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The Effect of Estrogen Deprivation on the Cellular Stress
Response Following Muscle Damage
By
Stephanie Salerno
A thesis submitted in conformity with the requirements for the degree of Master of Science
Graduate Department of Exercise Sciences University of Toronto
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The Effect of Estrogen Deprivation on the Cellular Stress Response Following Muscle Damage
Stephanie Salerno
Master of Science
Graduate Department of Exercise Sciences
University of Toronto
2017 Abstract TA muscles from ovary-intact (OVI; n=12) and ovariectomized (OVX; n=12)
female Sprague-Dawley rats were subjected to either 20 or 40 LCs. No differences in
any muscle contractile properties were observed in TA muscles between OVI and
OVX animals. Skeletal muscle fibre changes following ovariectomy included
increased (P<0.001) fibre area in the contra-lateral (control) muscle from OVX
animal and increased (P<0.001) endomysial infiltration score following 20 and 40
LCs from OVX animals. Heat shock protein 25 (Hsp) TA muscle content was
increased (P<0.05; P<0.01, respectively) in TA muscle from OVX animals following
20 and 40 lengthening contractions (LC) and in OVI animals following 40 LCs
(P<0.01). A decreased constitutive expression of Hsp72 (P<0.05) in OVX animals
was observed. Following 40 LCs, TA muscle Hsp72 content was increased in OVI
animals (P<0.05). Thus, estrogen may play a role in regulating skeletal muscle
cellular stress response and damage following controlled LCs.
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Acknowledgements: I would like to extend my utmost gratitude to Dr. Marius Locke for providing me
with the opportunity to take on this research project. His guidance and patience
have helped navigate me through the trials and challenges of my research. Without
his guidance and support I could not have been successful. Thank you greatly for
your encouragement and direction. I would also thank the members of my
committee Dr. Daniel Moore and Dr. Cathy Amara for their support and guidance
throughout my research.
Many thanks to my friends, family, and lab mates who supported me through this
project and all the highs and lows.
My greatest heartfelt thanks to my good friend Dr. Lilia Topouzova, if not for her I
would not have taken on this challenge. I would like to thank her for believing in me
and pushing me to be my very best.
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Table of Contents Abstract ………………………………………………………………………………………………...…….…… ii Acknowledgements ……………………………………………………………………………….……….... iii Table of Contents ………………………………………………………………………………….….……… iv List of Tables ……………………………………………………………………………………………...….. viii List of Figures ……………………………………………………………………………………..…………… iv Abbreviations ………………………………………………………………………………...……………….... x Chapter I: Review of Literature 1.1 Introduction …………………………………………………………………………………..…………… 1 1.2 The Stress of Exercise ………………………………………………………………………..………... 2 1.3 The Structure of Skeletal Muscle ………………………………………………………………….. 2 1.4 Contraction Types ………………………………………………………………..…………………….. 3 1.5 Muscle Damage …………………………………………………………………………..……………….. 3
1.5.1 Consequences of Muscle Damage ………………………………………..…………….. 4 1.6 Possible Mechanisms of Muscle Damage ………………………………..…...……..…………. 7 1.7 Estrogen …………………………………………………………………………………...………………… 7 1.8 Proposed Mechanisms of Estrogen Protection ………………………………...……………. 8
1.8.1 The Antioxidant Properties of Estrogen ……………………………………..……... 9 1.8.2 The Membrane Stabilizing Properties of Estrogen ………………………….... 10
1.9 The Effect of Estrogen Loss or Deprivation on Skeletal Muscle ……………………………………………………………………………………………......………….. 11 1.10 The Loss or Deprivation of Estrogen on Human Skeletal Muscle ………….……. 11 1.11 Heat Shock Proteins ……………………………...………………………………………………… 13 1.12 Heat Shock Protein 25 …………………………………………………………………………...... 14 1.13 Heat Shock Protein 72 ………………………………………………………………………….….. 15 1.14 The Role of Heat Shock Proteins in Skeletal Muscle ………………………...………... 16 1.15 The Effect of Estrogen on Heat Shock Proteins ………................................................. 17 Chapter II: Study Rationale and Objectives 2.1 Study Rationale ……………………………………………………………………………………...…. 19 2.2 Objective ……………………………………………………………………………………………...…… 21 2.3 Hypothesis ……………………………………………………………………………………………...… 21 2.4 Study Question ………………………………………………………………………………………….. 21 Chapter III: Methods and Materials 3.1 Animals ……………………………………………………..……………………………………………… 22 3.2 Stimulation Protocol ………………………………….……………………………………………… 22 3.3 Tissue Collection and Uterus Dissection …..….………………………………………..…… 24 3.4 Biochemical Analysis ………..……………………………………….………………………………. 25
3.4.1 Tissue Homogenization ………………………………….………………………….....… 25 3.4.2 Protein Content Calculation …………………………….…..………………………….. 26 3.4.3 Lowry—Protein Concentrations ……………………….…………………………….. 26 3.4.4 One-Dimensional Sodium Dodecyl Sulphate Polyacrylamide Gel Electrophoresis …………………………………………………..……………………………. 27
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3.4.5 Western Blotting—Protein Analysis ……………………..………..…………......... 28 3.4.6 ELISA—Blood Serum Analysis ………………………..………………….…………… 29
3.5 Morphological Analysis …………………………………………………………………..………..... 30 3.5.1 Muscle Cross-Sectioning ………………………………………………………..……….. 30 3.5.2 Hematoxylin and Eosin Staining ……………………………….……………..……… 30 3.5.3 ImageJ Quantification ……………………………………………..………………..…….. 31 3.5.4 Histological Quantification ………………………………………………………....…... 32
3.6 Statistical Analysis …………………………………………………………………………………..… 33 Chapter IV: Results 4.1 Anatomical and Physiological Alterations ……………………………..…..………………... 34
4.1.1 Anatomical Changes Following Ovariectomy ………………………………….... 34 4.1.2 The Effect Lengthening Contractions on TA Muscle Mass ….……..……….. 35 4.1.3 Muscle Protein Concentration …………………………………………..…………..…. 39
4.2 Muscle Contractile Alterations …………………………..………………………….……............ 39 4.2.1 Muscle Contractile Properties ………………………..……………………..…………. 39 4.2.2 Torque Throughout 20 and 40 Lengthening Contractions ……….……….. 41 4.2.3 The Active Component of Tibialis Anterior Muscle Torque ………..…...… 44 4.2.4 The Passive Component of Tibialis Anterior Muscle Torque …...…..……. 48 4.2.5 Maximal Tetanic Tension Prior to and Following 20 and 40 Lengthening Contractions ………………………….………………………....… 52 4.2.6 Maximal Twitch Tension Prior to and Following 20 and 40 Lengthening Contractions ………………………………………………….....… 56
4.3 Muscle Fibre Morphological and Histological Changes Following Ovariectomy and/or Lengthening Contractions …………...………….……...……………….. 60
4.3.1 Histological Measures of Muscle Damage ………………..……………………..... 60 4.3.2 Muscle Fibre Morphology in the Contra-lateral (Control) TA Muscles from OVI and OVX Animals ……..……………………..…..……..………………... 60 4.3.3 Visual Analysis of Muscle Damage from TA Muscles from OVI and OVX Animals Subjected to Lengthening Contractions …….….………….…… 61 4.3.4 TA Muscle Fibre Area from OVI and OVX Animals Following Lengthening Contractions ……………….…………………………. 61 4.3.5 TA Muscle Fibre Circularity from OVI and OVX Animals Following Lengthening Contractions ………………….………………………. 62 4.3.6 TA Muscle Fibre Roundness from OVI and OVX Animals Following Lengthening Contractions …………..……………….…………….. 62 4.3.7 TA Muscle Fibre Necrosis from OVI and OVX Animals Following Lengthening Contractions ………..………………………………... 63 4.3.8 Endomysial Infiltration of TA Muscle Fibre from OVI and OVX Animals Following Lengthening Contractions ……………….………...…. 64 4.3.9 Endomysial Distension of TA Muscle Fibre from OVI and OVX Animals Following Lengthening Contractions ………………….………… 65 4.3.10 Perimysial Infiltration and Distension of TA Muscle Fibres from OVI and OVX Animals Following Lengthening Contractions …... 65
4.4 The Cellular Stress Response Following Ovariectomy and/or Lengthening Contraction …………………………………………………………………….. 71
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4.4.1 The Constitutive Expression of Heat Shock Protein 25 in Tibialis Anterior Muscle ………………………………………………………………….……… 71 4.4.2 The Constitutive Expression of Heat Shock Protein 72 in Tibialis Anterior Muscle ……………………………………………………………………….… 73 4.4.3 TA Muscle Heat Shock Protein 25 Content Following Lengthening Contractions ………………………………………………….…………………… 75 4.4.4 Heat Shock Protein 72 Content in the Lengthening Contracted TA Muscle …………………………………..……..………………….……………… 77 4.4.5 HSF1 Content ……………………………………………………………………….………... 79
4.5 Summary ……………………………………………………………………………………………….…. 81 4.5.1 Anatomical, Physiological and Muscle Contractile Changes Following Ovariectomy and/or Lengthening Contractions ……………..………… 81 4.5.2 The Changes in TA Muscle Fibre Morphology Following Ovariectomy and/or Lengthening Contractions …………………………….………… 81 4.5.3 The Muscle Cellular Stress Response Following Ovariectomy and/or Lengthening Contractions ……………………………………………………….….. 82
Chapter V: Discussion 5.1 Overview …………………………………………………………………..……………………………… 83 5.2 Lengthening Contractions vs. Downhill Treadmill Running ………………..……….. 84 5.3 Skeletal Muscle Contractility …………………………………………………………………..…. 86
5.3.1 Tibialis Anterior Muscle Torque ………………………………………………...…… 86 5.3.2 Maximal Tetanic Tension and Twitch Tension Recovery Following Lengthening Contractions ……………………………………….…………..….. 87 5.3.3 The Active Component of Tibialis Anterior Muscle Torque ………………………………………………………………...……………………... 90 5.3.4 The Passive Component of Tibialis Anterior Muscle Torque …………............................................................................................................ 90
5.4 Histological Characteristics ………………………………………………………………...……... 92 5.4.1 Muscle Fibre Area and Circularity in Ovary-Intact and Ovariectomized Animals ………………………………………………………...………... 92 5.4.2 Endomysial Infiltration …………………………………………………………………... 92 5.4.3 Endomysial Distension Between Ovary-Intact and Ovariectomized Animals ……………………………………………………………...…... 94
5.5 The Cellular Stress Response Following Ovariectomy and/or Lengthening Contractions ……………………………………………………………….…. 95
5.5.1 Differences in Heat Shock Protein 25 and 72 Content Following Lengthening Contractions ………………………………………….. 97 5.5.2 The Constitutive Expression of Heat Shock Protein 72 in the Tibialis Anterior ……………………………………………………………..…………….. 98 5.5.3 Heat Shock Factor 1 Content in Ovariectomized Animals ………….……… 99 5.5.4 Heat Shock Protein 72 Expression in Ovariectomized Animals ………… 99
5.6 Connections to Post-Menopausal Females …………….……………………..…………... 101 5.7 Conclusions ………………………………………………………………………………….…………. 102 5.8 Limitations ……………………………………………………………………….…………………….. 102
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Chapter VI: References ……………………………………………………..………………………… 105 Chapter VII: Appendix 7.1 Tissue Preparation and Sectioning Skeletal Muscle …………………………..………. 122 7.2 Tissue and Blood Collection ……………………………………………………………..……… 124 7.3 Muscle Homogenization ……………………………………………………………………..…… 126 7.4 Determination of Protein Concentration—Lowry Assay ………………………..….. 128 7.5 SDS-PAGE, Western Blotting and Development ……………………………………...…. 129 7.6 Enzyme-Linked Immunosorbent Assay (ELISA) ………………………………..……… 131 7.7 Muscle Cross-Sectioning …………………………………………………………………..……… 132 7.8 Hematoxylin and Eosin Staining ………………………………………………………..……... 134 7.9 Morphological Scoring System …………………………………………………………..…….. 135
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List of Tables Table 1: The Effects of Ovariectomy on Body, Muscle and Uteri Masses, and 17-β Estradiol Concentration …………………………………………….……………………… 37 Table 2: Tibialis Anterior Muscle Mass in the Lengthening Contracted and Contra-lateral (Control) Limbs …………………………….……………..….... 38 Table 3: Skeletal Muscle Fibre Alterations Following 20 and 40 Lengthening Contractions ……………………………….………………. 69 Table 4: Skeletal Muscle Fibre Damage Following 20 and 40 Lengthening Contractions …………………………………..…………… 70
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List of Figures Figure 1: The Active and Passive Component of TA Muscle Torque in Lengthening Contractions ……………………………………………………. 40 Figure 2: Muscle Torque is Similar Between OVI and OVX Animals Throughout 20 Lengthening Contractions …………………………………………………..…… 42 Figure 3: Muscle Torque is Similar Between OVI and OVX Animals Throughout 40 Lengthening Contractions …………………………………………..…………… 43 Figure 4: Ovariectomy Does Not Alter the Active Component of Muscle Torque Throughout 20 Lengthening Contractions ………………………………….………….. 46 Figure 5: Ovariectomy Does Not Alter the Active Component of Muscle Torque Throughout 40 Lengthening Contractions ……………………………………………... 47 Figure 6: Ovariectomized Animals Maintained the Passive Component of Torque Throughout 20 Lengthening Contractions ………………………...……………… 50 Figure 7: Ovariectomized Animals Maintained the Passive Component of Torque Throughout 40 Lengthening Contractions …………………………………….….. 51 Figure 8: Maximal Tetanic Tension is Similar Between TA Muscles from OVI and OVX Animals Following 20 Lengthening Contractions ……………………………...... 54 Figure 9: Maximal Tetanic Tension is Decreased Following 40 Lengthening Contractions ……………………………………………………….…….………………… 55 Figure 10: Maximal Twitch Tension is Decreased Following 20 Lengthening Contractions ………………………………………………………………….……….….. 58 Figure 11: Maximal Twitch Tension is Decreased Following 40 Lengthening Contractions …………………………………………………………………….….……… 59 Figure 12: Skeletal Muscle Changes in Ovary-Intact and Ovariectomized Animals Following 20 or 40 Lengthening Contractions …………………………….………. 66 Figure 13: Skeletal Muscle Damage Following Lengthening Contractions in Ovary-Intact Animals …………………..…………………………………………………..…….……. 67 Figure 14: Skeletal Muscle Damage Following Lengthening Contractions in Ovariectomized Animals ……………………………………………………………..……..……….. 68 Figure 15: Constitutive Hsp25 Content is Unchanged Following Ovariectomy …………………………………………………………………………….…….. 72 Figure 16: Constitutive TA Muscle Hsp72 Expression is Significantly Decreased Following Ovariectomy ……………………………………………………………………..………….… 74 Figure 17: TA Muscle Hsp25 Content Increases Following Lengthening Contractions ……………….………………………………………………………...……. 76 Figure 18: TA Muscle Hsp72 Content Following 20 and 40 Lengthening Contractions in Ovary-Intact and Ovariectomized Animals …………………………...….. 78 Figure 19: Heat Shock Factor1 Content in TA Muscles from OVX Animals …………………………………………………………………………………………………... 80
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Abbreviations Ca2+—Calcium CC—Control-Control CK—Creatine Kinase CSR—Cellular Stress Response DAMPs—Damage Associated Molecular Patterns EDL—Extensor Digitorum Longus ED1+--Subpopulation of macrophages (pro-inflammatory) ED2+--Subpopulation of macrophages (anti-inflammatory) ELISA—Enzyme-linked Immunosorbent Assay FOXO3A—Foxhead Box O3 G—Gauge g—gram H&E—Hematoxylin and Eosin HSP—Heat Shock Protein kDA—Kilodalton LC—Lengthening Contractions mg—Milligram ml—Milliliter MTT—Maximal Tetanic Tension MTw—Maximal Twitch Tension NFκB—Nuclear Factor-κ-Beta OVI—Ovary-intact OVX—Ovariectomized ROS—Reactive Oxygen Species SC—Shortening Contraction TA—Tibialis Anterior TNF-α—Tumor Necrosis Factor-α w/v—Weight per volume
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Chapter I: Review of Literature 1.1 Introduction
Hans Selye first characterized the body’s response to life’s challenges in the
mid 20th century. During periods of stress, the body exhibits a series of complex and
powerful responses that allows one to cope with the stressful condition/state
(Nickerson, 2006). Originally termed the ‘alarm response,’ stress was first
characterized as a general phenomenon (Selye, 1956; Tache and Selye, 1985).
Although stressors can affect the human body in a global manner, these effects can
also be observed within various systems or tissues including skeletal muscle. Daily
stressors, such as exercise, can impose physical demands activating the ‘alarm
response’ and other reactions responses in both muscle and the body. The goal of
the response is restore homeostasis.
With increased age both males and females are negatively affected by the
decline in skeletal muscle mass and strength. Termed sarcopenia, more than 30% of
individuals over 60 years of age are negatively impacted (Velders and Diel, 2013).
The age-related loss of skeletal muscle is thought to be a multi-factorial process
composed of numerous events, including inactivity, oxidative stress, nutritional
intake, inflammatory status and hormonal changes (Abbasi et al., 1998;
Baumgartner et al., 1999; Roubenoff and Hughes, 2000). The consequence of a
decreased muscle mass is the resultant increased health risks and decreased quality
of life.
In females, the presence of estrogen has been shown to provide some
resistance to cellular damage from certain pathological conditions such as
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cardiovascular disease, Parkinson’s disease and aging-related dementia
(Mendelsohn and Karas, 1999; Garcia-Segura et al., 2001; Brinton, 2004). In the
developed world, most females will spend one-third of their lifetime in a state of
estrogen deprivation (Barrett-Connor, 1993). Given that the risk for sarcopenia
increases with age, it suggests estrogen may play a role in protecting skeletal
muscle, thus emphasizing its importance.
1.2 The Stress of Exercise
Exercise can be a physical stress that ultimately results in cellular and
systemic adaptations. This may happen through two ways: the first is through
hypothalamic-pituitary axis, which is responsible for controlling and regulating
many vital bodily processes (Caston et al., 1995). The second involves hormones,
including estrogen, that bind to membrane receptors, move to the nucleus and alter
gene expression (Pinilla et al., 1992; Jarow et al., 1993; Chennaoui et al., 2002;
Vicdan, 2006). Both ways work together to cope with the stress of exercise (Viau,
2002) and restore homeostasis following exercise.
1.3 The Structure of Skeletal Muscle
Skeletal muscle is comprised of myofibres consisting primarily of actin and
myosin. The sarcomere is the functional unit of skeletal muscle and produces force
by actin and myosin cross bridge interaction. Skeletal muscle is comprised of
multiple bundles of cells known as muscle fascicles, surrounded by a layer of
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connective tissue. Each muscle fascicle is comprised of muscle fibres, which in turn
are constituted by myofibrils.
1.4 Contraction Types
Skeletal muscle contractions can be separated into isometric or dynamic
contractions. An isometric contraction results in no change in muscle length while a
dynamic contraction changes muscle length such that it shortens (concentric) or
lengthens (eccentric). With shortening contractions the collective forces generated
by the muscle fibres are greater than the opposing load and the sarcomeres shorten.
In contrast, a LC occurs when the muscle forces generated are insufficient to move
the load and the muscle is forcibly lengthened. For example, during a squat when
the load is lifted (up) the quadriceps performs a shortening contraction (SC).
Conversely, when the load is lowered (against the force of gravity) the quadriceps
undergo a LC. In comparison to SCs, LCs is associated with greater subsequent
muscle fibre damage and hence greater torque loss (Fridén et al. 1983; Evans et al.
1985; Fridén and Lieber, 1992).
1.5 Muscle Damage
As mentioned previously, skeletal muscle has evolved to shorten. However,
when the load is greater than the force, sarcomeres lengthen. As a result of LCs the
sarcolemma, sarcoplasmic reticulum and z-lines can become damaged, resulting in
protein leakage (Stupka et al., 2000). Following these primary events in muscle
damage, LC biased exercise results in the elevation of oxygen free radicals, further
4
propagating a secondary damage. The most noticeable consequences of muscle fibre
damage following LC exercise include delayed onset muscle soreness and an
immediate immune response (Stupka et al., 2000). These alterations may last up to
ten days following exercise (Tiidus, 2000).
1.5.1 Consequences of Muscle Damage Swelling
Muscle swelling or fluid accumulation often occurs following damaging
exercise and results in an increased muscle mass (McCully and Faulkner, 1985). An
increased muscle mass of approximately 10% has been observed immediately after
(t=0) forced LCs (Komulainen et al., 1998). Fibre swelling generally peaks 4-5 days
following muscle injury and gradually spreads throughout the muscle (Yu et al.,
2013). Fluid accumulation may remain in the intracellular space for as long as 5
days following damaging exercise (Yu et al., 2013).
Torque Loss
Following a sufficient stimulus of either SC or LCs, any subsequent
contractions may show a decreased torque. However, following SCs, the causes of
reduced muscle torque are generally due to metabolic fatigue. Indeed, SCs have been
shown to result in torque losses up to 30%, although torque generally returns
within hours following exercise (Newham et al., 1983; Jones et al., 1989). In
contrast, LCs may cause torque losses up to 60% (Newham et al., 1987, Nosaka et al.,
1991; Saxton et al., 1995) and depending on the severity, may persist for weeks
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(Newham et al., 1987). This long-term torque loss is thought to be due to the
damage to structural or cytoskeletal components that are associated with LCs
(Semmler, 2014). For example, central nuclei (Faulkner et al., 1989), z-line
streaming (Brooks et al., 1995) and ghost fibres (Komulainen et al., 1998; Holwerda
and Locke, 2014) are commonly observed following LCs. Thus, while both SCs and
LCs result in a decreased torque, a more persistent and greater magnitude of torque
loss is associated with LCs.
Leukocyte Infiltration
Following exercise induced muscle damage, leukocytes (neutrophils and
macrophages) migrate to the site of injury (Peake et al., 2005). The time-course of
this inflammatory response is dependent on the mode, duration, intensity and
muscle groups utilized during exercise (Smith et al., 1989; MacIntyre et al., 1995).
Within hours following LC, neutrophils invade the injured muscle fibres (MacIntyre
et al., 1996; MacIntyre et al., 2000; Malm et al., 2000; Stupka et al., 2000; Beaton et
al., 2002; Raastad et al., 2003) and may remain for up to 5 days (Yu et al., 2013).
High concentrations of neutrophils are required for proteolysis in order to remove
cellular debris, which are common signs of fibre damage and degeneration (Tidball,
2005). Following the initial fibre damage, neutrophils release proteolytic enzymes,
such as calpains, and oxygen free radicals, which can result in a further tissue
(secondary) degradation (Cannon et al., 1990; Pizza et al., 1995; Clarkson and Hubal,
2001). This allows for a greater efflux of muscle proteins such as creatine kinase
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(CK) (Cannon et al., 1990; Pizza et al., 1995), or even heat shock proteins (Hsp)
(Zheng et al., 2004).
Following muscle damage and the invasion of neutrophils, macrophages
typically enter the fibre 12 to 48 hours later (Tidball et al., 1995; Tiidus et al., 2001).
Two subpopulations of macrophages, termed ED1+ and ED2+ have been identified
(Honda et al., 1990; St. Pierre and Tidball, 1994). Approximately 12 hours following
damaging exercise, ED1+ macrophages invade (Clarkson and Sayer, 1999) whereas
ED2+ macrophages enter the fibre between 24 to 48 hours after exercise. ED1+
macrophages act as phagocytes and remove cellular debris in necrotic tissue (St.
Pierre and Tidball, 1994; Tidball, 2005) whereas ED2+ cells are necessary for
myoblast proliferation in muscle recovery (St. Pierre and Tidball, 1994; Massimino
et al., 1997; Tidball, 2005) and are thought to regulate the repair process (Clarkson
and Sayer, 1999). Thus, the increase in leukocyte infiltration following muscle
damage may be used as a measure or marker of muscle damage.
Neutrophil and macrophage infiltration and cytokine expression are
sensitive to ovarian hormone expression (Zuckerman et al., 1996; Angstwrum et al.,
1997; Komulainen et al., 1999; Tiidus et al., 2001, 2005). In support of this, female
rodents subjected to LCs displayed decreased macrophage invasion when compared
to males (St. Pierre-Schneider et al., 1999). Similarly, McClung et al. (2007) showed
the soleus muscle of OVX rats displayed elevated neutrophil and macrophage
concentrations following recovery from disuse injury. This work suggests that
estrogen deprived females may exhibit a greater inflammatory response following
exercise, which may lead to a delayed or decreased ability to recover.
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1.6 Possible Mechanisms of Muscle Damage Two mechanisms have been proposed to explain the decrement in torque
following exercise-induced muscle damage. The first is the “popping sarcomere”
hypothesis proposed by Morgan (1990). Also known as sarcomere disorganization,
this damage occurs when the muscle is stretched beyond optimal length pulling the
weakest sarcomeres (longest sarcomere) apart. These sarcomeres become
progressively weaker until the rising passive tension compensates for the
decreasing active tension (Morgan and Poske, 2004). This results in the sarcomeres
being stretched past the point of myofilament overlap and “popping” out (Morgan,
1990) thereby damaging the sarcomeres and decreasing muscle torque.
The second proposed mechanism for muscle damage following exercise is
the disruption of calcium (Ca2+) homeostasis. Lengthening contractions cause
membrane damage to the sarcolemma (Takekura et al., 2001) resulting in elevated
resting Ca2+ levels from an inward movement (Morgan and Allen, 1999). The
disrupted muscle sarcolemma is likely due to increased Ca2+ influx, which may also
disrupt the excitation-contraction coupling process (Jones, 1996; Ingalls et al., 1998)
and decreased muscle torque (Overgaard et al., 2002; 2004). Thus, current evidence
suggest LC damage decreases torque and may be the result of over-stretched
sarcomeres and/or disrupted Ca2+ homeostasis.
1.7 Estrogen
In eumenorrheic females, estrogen exists in three forms: the major form of
17-β estradiol and lesser quantities of estrone and estriol (Kirilovas et al., 2007). For
8
ease of communication in this thesis these forms will collectively be referred to as
estrogen. Primarily produced in the ovaries, estrogen is also synthesized in low
amounts in other tissue such as bone and skeletal muscle (Nelson and Bulun, 2001;
Chowdhury and Pickering, 2006; Aizawa et al., 2008). Estrogen is a pleiotropic
hormone and affects muscle function both directly as well as through the central
nervous system (McEwen and Alves, 1999). Estrogen replacement has beneficial
effects on bone, neurons, the cardiovascular system (Persky et al., 2000; Jia et al.,
2008) and skeletal muscle, thus attesting to its importance in musculoskeletal
health.
1.8 Proposed Mechanism of Estrogen Protection
Female sex hormones (estrogen and progesterone) have been shown to
enhance muscle mass, strength and attenuate muscle damage following LCs (Velders
and Diel, 2013). When subjected to exercise of a damaging nature such as LC,
ovariectomized animal displayed increased sarcolemma damage, increased blood
CK (Bar et al., 1985; Amelink and Bar, 1986) and an increased inflammatory
response (St. Pierre-Schneider et al., 1999). Thus, estrogen appears to play a role in
attenuating muscle damage.
Three mechanisms have been proposed to explain the protective effects of
estrogen on muscle. First, similar to vitamin E, estrogen may act as an antioxidant,
thereby inhibiting or decreasing membrane peroxidation (Nedergaard et al., 2013).
Second, estrogen may stabilize membrane integrity (McNulty et al., 2000) thereby
decreasing membrane disruption. Third, estrogen is known to regulate Hsp
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expression, thereby providing resistance against muscle damage (Bombardier et al.,
2009). Thus, estrogen may act through multiple mechanisms to provide protection
to skeletal muscle from the stress of exercise.
1.8.1 The Antioxidant Properties of Estrogen
Antioxidant membrane-stabilizing molecules are known to reduce
membrane fluidity (Wiseman et al., 1993; Behl et al., 1997). Estrogen is similar in
function to vitamin E in its chain-breaking action (Sugioka et al., 1987) and thus may
act as an antioxidant (Bar and Amelink, 1997; Tiidus, 1995; Whiting et al., 2000).
Studies have shown estrogen provides physiological protection to rat skeletal
muscle against free radical-mediated lipid peroxidation (Persky et al., 2000; Stupka
and Tiidus, 2001). This may be accomplished through the donation of a hydrogen
from its hydroxyl group to peroxyradicals (Carter et al., 2001). Thus, estrogen has
the ability to scavenge free radicals, thereby minimizing oxidative damage (Sugioka
et al., 1987; Subbiah et al., 1993; Strehlow et al., 2003). The conferred increase in
antioxidant ability via estrogen may promote muscle fibre survival following
damaging exercise.
Due to the structure of estrogens, it is plausible that estrogen may act to limit
free radical accumulation. It is not surprising that the removal of estrogen results in
a decreased ability to negate ROS production. In support if this, OVX rodents show a
decreased myocardial superoxide dismutase activity and expression (Barp et al.,
2002). Thus, estrogen deprivation may result in an increase in muscle fibre damage
10
due to the inability to negate the negative effects of increased ROS produced during
or following exercise.
1.8.2 The Membrane Stabilizing Properties of Estrogen
Membrane disruption is thought to be a key early event following skeletal
muscle damage (Kendall and Eston, 2002). Estrogen may prevent membrane
disruption through its receptor-mediated system (Tiidus, 1999; Tiidus, 2001) or by
directly interacting with the phospholipid membrane, thereby optimizing
membrane fluidity (Tiidus, 1999; Tiidus, 2003). Further support for the importance
of estrogen can be gleaned from the fact that following exercise, OVX female rats
supplemented with estrogen showed a reduction in blood CK (Bar et al., 1988;
Amelink et al., 1990; Persky et al., 2000; Tiidus et al., 2001; Feng et al., 2004). Thus,
estrogen appears to play a role in minimizing membrane disruption/damage
following exercise.
Estrogen also appears to protect muscle fibres by minimizing leukocyte
infiltration since neutrophil infiltration was attenuated by 1-2 hours following
exercise (Tiidus et al., 2001; Tiidus, 2003). Tiidus et al. (2001) observed that
skeletal muscle from estrogen-supplemented rodents showed an attenuated calpain
activity and neutrophil infiltration following downhill treadmill running. Overall,
estrogen appears to influence membrane stabilization, thus decreasing both CK
leakage and leukocyte infiltration following exercise.
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1.9 The Effect of Estrogen Loss or Deprivation on Skeletal Muscle
In female mice, estrogen has been shown to influence the development of
skeletal muscle size (Sciote et al., 2001). Multiple studies have also observed
estrogen affects muscle fatigue and twitch characteristics, including peak tetanic
tension and half-relaxation time (Hatae, 2001; McCormick et al., 2004; Schneider et
al., 2004; Enns and Tiidus, 2010). Thus, estrogen appears to play a role influencing
contractile measures of skeletal muscle.
Skeletal muscles from female rats showed a decreased loss of desmin
(Komulainen et al., 1999), a structural protein that contributes to z-discs alignment
and aids in tension transmission (Morgan and Allen, 1999). Ovariectomized rats
displayed a greater loss of desmin when compared to estrogen-supplemented rats
following treadmill running (Bar et al., 1988; Enns and Tiidus, 2010). Thus, the loss
of estrogen may predispose skeletal muscle to related z-disc damage. Taken
together, these data suggest estrogen may be necessary for the maintenance of
muscle fibre structure or structural proteins, thereby maintaining torque.
1.10 The Loss or Deprivation of Estrogen on Human Skeletal Muscle
Menopause is an age-related condition of female hypogonadism,
characterized by ovarian failure and exemplified by a rapid yet dramatic decline in
female sex hormone production including estrogen (Rannevik et al., 1986). During
menopause, females experience an accelerated loss of muscle mass (Aloia et al.,
1991). Rolland et al. (2007) showed each year following menopause, females lose
approximately 0.6% of muscle mass. This suggests estrogen promotes the
12
maintenance of muscle mass and that estrogen deprivation may hasten the onset of
sarcopenia. The declining estrogen concentrations following menopause may create
a pro-inflammatory state by increasing cytokines such as tumor necrosis factor-
alpha (TNF-α) (Roubenoff, 2003; Messier et al., 2011) and interleuklin-6 (Roubenoff,
2003). Not surprisingly, a link has been proposed between low estrogen
concentrations and decreased protein synthesis (Messier et al., 2011).
The large change in occurrence of “moderate sarcopenia” in females aged 40
to 49 years suggests the prevalence of sarcopenia increases at a time when
significant hormonal changes occur (Messier et al., 2011). In support of this, Jubrias
et al. (1997) reported post-menopausal females had twice the amount of non-
contractile muscle tissue, including intramuscular fat, when compared to younger
menstruating females. As age progresses beyond menopause, a decreased whole
body, trunk and lower extremity lean body mass, concurrent with an increase in
total body and visceral fat has been observed (Svendsen et al., 1995; Poehlman et al.,
1995; Pantopoulos et al., 1996; Douchi et al., 1998; Gambacciani et al., 1999; Douchi
et al., 2002; Lynch et al., 2002; Van Pelt et al., 2002). An increased adiposity (Phillips
et al., 1993; Poehlman et al., 1995; Aloia et al., 1991; Aloia et al., 1995; Douchi et al.,
1998; Poehlman and Tchernof, 1998) and a decreased bone mineral density also
occur (Carr, 2003). The decline in muscle performance following menopause may be
due to altered muscle contractile properties that result from the changes in
hormone concentrations (Pette and Stratin, 2001). In view of this, estrogen appears
to be necessary to maintain both muscle quantity and quality.
13
1.11 Heat Shock Proteins
Heat shock proteins are rapidly inducible, highly conserved proteins
(Kingston et al., 1987; Welch 1992) known to protect cells from stressors, such as
increased temperature (Landry et al., 1982; Tiidus, 1995; Bar and Amelink, 1997),
oxidative stress (Tiidus, 1995; Bar and Amelink, 1997; Bombardier et al., 2013),
decreased pH (Cohen et al., 1991) and reduced fuel (Febbraio et al., 2002). In the
unstressed cell, Hsps generally remain at low levels, but rapidly accumulate in
response to protein damaging stressors (Chiang et al., 1982; Hochstrasser, 1992;
Ellis and Heart, 1996). Hsps have been shown to minimize the aggregation of
unfolded proteins thereby preventing or limiting the detrimental consequences of
protein aggregation (Haslbeck and Viering, 2015). Given that many diseases of aging
result in protein aggregation, Hsps may play a vital role in maintaining or
preventing age-related diseases such as sarcopenia.
Hsps are known to facilitate protein chaperoning, folding, transport, as well
as the removal of damaged proteins (Lindquist and Craig, 1988; Welch, 1992). In
skeletal muscle, Hsps act as both chaperones and as an indicator of stress (Liu and
Steinacker, 2001). By interacting with damaged proteins, Hsps maintain
protetostasis (Liu and Steinacker, 2001). Thus, Hsps serve as both markers of
stress/damage, as well as preventing protein related problems. Both acute (Locke et
al., 1990; Salo et al., 1991; Skidmore et al., 1995; Hernando and Manso, 1997;
McArdle et al., 2001; Milne and Noble, 2002) and chronic (Gonzalez et al., 2000;
Mattson et al., 2000; Naito et al., 2000; Samelan, 2000) exercise has been shown to
14
increase Hsp content in skeletal muscle. Thus, any exercise mediated increase in
Hsps may play a key role in minimizing sarcopenia.
In addition to the Hsp protein chaperone related function, Hsps may also
provide protection to skeletal muscle through anti-inflammatory and apoptotic
mechanisms (Knowlton, 1995; Mosser and Morimoto, 2000; Christians et al., 2002).
Any inability to elevate Hsp content may result in increased muscle damage and
ultimately exacerbate muscle loss in the long-term. Thus, it is possible that estrogen
deficiency alters the skeletal muscle stress response, thereby rendering skeletal
muscle more susceptible to damage. This may increase muscle loss and have
detrimental effects for certain populations of females.
The regulation of Hsps is controlled through heat shock protein factors
(HSFs). In response to protein damaging stressors, the intracellular accumulation of
damaged proteins removes Hsps from heat shock factor 1 (HSF1), thus allowing
HSF1 trimerization (Chiang et al., 1982; Hochstrasser, 1992; Ellis and Heart, 1996).
This allows HSF1 to bind to the heat shock element-DNA (HSE) and initiate Hsp
transcription (Mosser et al., 1993). The subsequent increase in Hsps eventually
results in sequestration of HSF1, thereby ending the Hsp response (Kim et al., 1995;
Marber et al., 1995).
1.12 Heat Shock Protein 25
Heat shock proteins are grouped according to molecular weight. Small Hsps
(Hsp25, also known as Hsp27 in humans) are comprised of a family of nine proteins
sharing a highly conserved α-crystallin domain (Koh, 2002). Small Hsps are
15
molecular chaperones functioning independently of ATP and involved in a number
of cellular functions, including; modulating the cytoskeletal network, preventing
protein aggregation, regulating caspase activity and maintaining redox status
(Brinkmeier and Ohlendieck, 2014). Hsp25 is named due to its molecular mass of
25-kDa. In unstressed skeletal muscle fibres, Hsp25 is at low concentrations in the
cytosol. However, following stress, Hsp25 interacts with cytoskeleton and
myofilaments (Vissing et al. 2009). With the stress of LCs, Hsp25 binds to z-disk-
related structures (Koh, 2002) and possibly functions as a cytoskeletal protective
protein (Vasconsuelo et al., 2010). This may prevent cytoskeletal disruption during
high-force exercise (Koh, 2002). Using a C2C12 cell line, Vasconsuelo et al. (2010)
showed estrogen administration resulted in a time-dependent (5-60 minute)
increase in Hsp25 content. During contraction-induced muscle damage, Hsp25 has
been shown to interact with the myofilaments (Lutsch et al., 1997) and cytoskeleton
(Koh, 2002, 2004; Vissing et al., 2009) as well as with proteins involved with the
cytoskeletal structures (desmin). Thus, following exercise Hsp25 appears to attempt
to minimize cytoskeletal disruption.
1.13 Heat Shock Protein 72 Hsp70 refers to the markers of the 70-kDa family of proteins and consists of
four major Hsp70 isoforms have been characterized (Noble et al., 2008). Hsp78 is
the largest Hsp70 isoform and exists primarily in the endoplasmic and sarcoplasmic
reticulum, while Hsp75 is a mitochondrial import protein (Lui and Steinacker, 2001;
Noble et al., 2008). A 70kDa heat shock cognate (Hsc70 or Hsp73) is constitutively
16
expressed in a wide variety of cells; however, the main stress inducible form of
Hsp70 isoforms is Hsp72 (HspA1A) (Gabai et al., 1998; Yenari et al., 1998; Lui and
Steinacker, 2001; Bidmon et al., 2004; Noble et al., 2008). Locke et al. (1991) have
shown muscles containing type I muscle fibres constitutively express Hsp72,
possibly explaining why type I muscle fibres may be less susceptible to damage LC
biased exercise. Following LCs, Hsp72 accumulates in skeletal muscle (Thompson et
al., 2001; Khassaf et al., 2001; Thompson et al., 2003; Koh, 2004; Morton, 2006;
Paulsen et al., 2007; Morton et al., 2009; Paulsen et al., 2009; Holwerda and Locke,
2014). McArdle et al. (2004) observed that overexpression of Hsp70 in extensor
digitorum longus (EDL) from mice appeared to provide protection against LCs.
Hsp72 may be important in regulating specific atrophy signaling pathways
(Senf et al., 2008; Senf et al., 2010). Hsp72 has been shown to inhibit the
transcriptional activity of FOXO3a and nuclear factor-kappa beta (NF-κB), thereby
minimizing skeletal muscle atrophy (Senf et al., 2008; Senf et al., 2010). Thus,
following exercise, Hsp72 accumulation may play a key role in regulating atrophy
pathways thereby influencing muscle mass.
1.14 The Role of Heat Shock Proteins in Skeletal Muscle Hsps maintain protein synthesis and/or decrease the rate of muscle protein
breakdown, thereby perhaps slowing disuse muscle atrophy (Miyabara et al., 2012).
Hsps may also be involved in blunting the NF-κB pro-inflammatory pathway (Chen
et al., 2004b, 2004a; Chen and Currie, 2006), by inhibiting the degradation of IκB
complex and thus the subsequent activation of NF-κB (Noble, 2002). In view of this,
17
an increase in Hsps or the ability to increase Hsps may help protect or reduce
skeletal muscle damage by possibly negating the effect of pro-inflammatory
pathways.
Increased levels of Hsp27 and Hsp70 have been reported in human skeletal
muscle following high-force “eccentric exercise” (Reichsman et al., 1991; Thompson
and Scordilis, 1994; Febbraio and Kokoulas, 2000; Feasson et al., 2002; Thompson
et al., 2002; Thompson et al., 2003; Willoughby et al., 2003) and Hsps appear to be
involved in the remodeling and adaptation process (Feasson et al., 2002; Thompson
et al., 2003). In rodent models, during periods of overload stress, (resistance
exercise) Hsps are up-regulated (Oishi et al., 2005; Ogeta et al., 2005; O’Niell et al.,
2006; Paulsen et al., 2007). In addition, following muscle fibre damage, Hsps have
been shown to migrate to contractile protein structures, possibly in an attempt to
provide stabilization (Koh, 2004; Paulsen et al., 2007). An inverse relationship
between CK release and Hsp70 expression following exercise has also been reported
(Liu et al., 1999). Thus, Hsps appear to be initially involved following damaging
exercise (LC) and/or muscle contractions.
1.15 The Effects of Estrogen on Heat Shock Protein Content
Males and females present different profiles of muscle damage following
unaccustomed exercise (Paroo et al., 2002). Estrogen has been shown to decrease
post-exercise skeletal muscle damage and may be a factor involved in the
differences observed in post-exercise Hsp72 levels between males and females
(Paroo et al., 1999). Paroo et al. (2002) observed an estrogen mediated sex-specific
18
Hsp70 response following downhill treadmill running. Males and ovariectomized
female rodents demonstrated a greater Hsp70 response when compared to ovary-
intact females (Paroo et al., 1999; Gillum, 2010). Thus, estrogen may account for the
differences observed in Hsp content following exercise. In skeletal muscle,
Bombardier et al. (2009; 2013) showed estrogen regulates both basal and exercise-
stimulated Hsp70 content. Thus, estrogen appears to be a factor in mediating both
the constitutive expression and stress-induced expression of Hsps.
Myocytes from old ovariectomized rats showed an increased NF-κB activation,
cytokine expression and decreased ability to handle ROS (Stice et al., 2011). The loss
of Hsp content due to aging is thought to be the result of the loss of HSF1s ability to
bind to DNA inducing transcription (Heydari et al., 2000; Lee et al., 2009). Given the
available evidence, the loss of estrogen may play a role in the stress response of
muscle fibres and may augment protein damage from stressors such as LCs.
Studies have demonstrated estrogen-dependent activation of Hsp70 occurs
via the sequential stimulation of NF-κB and HSF1 (Hamilton et al., 2004; Stice and
Knowlton, 2008). The ability of estrogen to up-regulate Hsp72 content in skeletal
muscle may also provide increased protection by limiting the inflammatory
response following exercise (treadmill running) (Bombardier et al., 2009). Overall
these studies suggest estrogen may play a role protecting skeletal muscle from
exercise-induced damage by enhancing or maintaining the Hsp response. Ultimately,
less muscle damage overtime may result in a slowing of sarcopenia and an increased
quality of life.
19
Chapter II: Study Rationale and Objectives
2.1 Study Rationale
A connection between estrogen and the maintenance of muscle health has
been established. When skeletal muscle deprived of estrogen is subjected to
stressors, greater damage and inflammatory response, concurrent with an increased
Hsp content has been observed. Bombardier et al. (2013) found estrogen regulates
both the unstressed and exercise-stimulated Hsp response, suggesting both may be
altered following ovariectomy. This suggests estrogen deprivation may account for a
decreased capacity to protect skeletal muscle following LC exercise.
Downhill treadmill running as a form of exercise has been used to elucidate
the effects of estrogen on skeletal muscle damage (Paroo et al., 1999; Tiidus and
Bombardier, 1999; Tiidus et al., 2001; Bombardier et al., 2009, 2013). However, a
limitation of running models is the inability to control the specific response that
results from muscle contractions. Thus, the exact stressor responsible for the
increase in Hsp content remains unknown. An increase in body temperature
(Landry et al., 1982; Tiidus, 1995; Bar and Amelink, 1997), oxidative stress (Tiidus,
1995; Bar and Amelink, 1997; Bombardier et al., 2013), decreased pH (Cohen et al.,
1991) and decreased fuels (Febbraio et al., 2002) are all capable of inducing a stress
response. Given the vast number of factors capable of increasing protein damage, a
more controlled method, such as electrically stimulated LCs, may allow for a more
precise cause and effect relationship between estrogen deficiency and muscle
damage to be established.
20
A lowered Hsp content in the unstressed muscle from ovariectomized
animals may result in an inability to increase Hsp expression following LCs,
therefore increasing the extent of muscle damage. Using maximal electrically
stimulated LCs to induce muscle damage, this study intended to clarify the
relationship between estrogen deprivation and Hsp content and muscle damage.
By examining and assessing Hsp content and muscle damage following
damaging exercise (LCs) in estrogen deprived and intact states, the role of the CSR
can be assessed following LCs in skeletal muscle. To do this, one hind limb from OVX
and OVI animals was subjected to maximal electrical stimulation. Physiological (TA
muscle torque, maximal tetanic tension and twitch), biochemical (Hsp25, Hsp72 and
HSF1) and morphological (fibre area, circularity, roundess, fibre necrosis,
endomysial infiltration and distension following skeletal muscle cross-sectioning
and staining using hematoxylin and eosin) parameters following of the muscle were
analyzed.
Two different contraction repetitions (20 and 40) were selected to glean the
extent of differences in structural damage. Holwerda and Locke (2014) found large
amounts of structural damage eight hours following 100 LCs. However, to ensure a
range of muscle damage between OVI and OVX observed was the result of estrogen
loss and not a time dependent effect of LC overload, more moderate contraction
repetitions were selected. Pollock-Tahiri and Locke (2016) have observed increased
Hsp25 and 72 content and decreased torque throughout 20 contractions, with little
structural damage. Thus, to determine the role of ovariectomy in structural muscle
damage, 40 LCs was also selected.
21
2.2 Objective To characterize the CSR and muscle damage in TA skeletal muscle from
ovariectomized and ovary-intact animals following maximally stimulated
lengthening contractions.
3.3 Hypotheses
1) Muscles from OVX animals subjected to 20 or 40 LCs will show an increased
CSR response and muscle damage.
2) Following LCs, TA muscles from OVX animals will show an increased
physiological (contractile), biochemical (Hsps), and morphological markers
of skeletal muscle damage.
3.4 Study Question Does ovariectomy (estrogen deficiency) alter the cellular stress response following
electrically stimulated lengthening contractions?
22
Chapter III: Methods and Materials 3.1 Animals
At approximately two months of age, female Sprague-Dawley rats (n=12)
(Charles River Laboratories, Quebec, Canada) underwent surgical removal of the
ovaries (performed by Charles River Laboratories). Ovariectomized and ovary-
intact animals (N=29; consisting of 12 OVX, 12 OVI, 5 control-control [CC] animals
not subjected to any lengthening muscle contractions) were housed in the Ramsey
Wright laboratory (University of Toronto), two per cage with a 12-hour light-dark
cycle. Animals were fed and provided water ad libitum. All procedures were
approved by the Animal Care Committee at the University of Toronto, in accordance
with the Guidelines for Canadian Council on Animal Care. Three weeks after the
initial ovariectomy animals were subjected to experimentation.
3.2 Stimulation Protocol All procedures were performed under anesthesia (isoflurane/oxygen gas
mixture; 1L/min). Once anesthetized, animals were oriented in a supine position on
a small-animal warming platform (806D, Aurora Scientific Inc., Aurora, Canada)
maintained at 37°C. The left knee was secured between two vertical stabilizing posts
by the insertion of a 25G x 1.5-inch needle through the hind limb in a lateral
orientation, directly distal to the condyles. Two 25G x 0.5-inch needle probe
electrodes (Chalgren Enterprises, CA, USA) were inserted subcutaneously in a
longitudinal position, directly along the TA muscle. Adhesive tape was applied to
secure the left leg to the pedal of a computer-controlled servomotor (301C, Aurora
23
Scientific Inc., Aurora, Canada). The pedal was adjusted three-dimensionally until
the secured ankle was in line with the knee and the knee angle at 120°.
Electrical stimulation was produced from a bi-phase stimulator (701C Aurora
Scientific Inc., Aurora, Canada), controlled by a computer hardware interface (604A,
Aurora Scientific Inc., Aurora, Canada) synchronized to the servomotor (Cambridge
Technology, model #6650LR) movements. Once the correct orientation was
established, optimal stimulation voltage was determined by stimulating the TA
muscle to cause dorsiflexion of the secured foot against a rigid pedal for 0.5-second
periods in intervals of 1V. Generally voltages between 8-12V stimulations were
provided. Isometric torque (g/cm) output was measured and the optimal
stimulation voltage for animals was selected based on the lowest voltage needed to
achieve peak torque.
Lengthening contraction stimulation was performed using a bi-phase
stimulator connected to a computer controlled hardware interface (604A, Aurora
Scientific Inc., Aurora, Canada) that could be adjusted using Dynamic Muscle Control
software (DMC; 610A, Aurora Scientific Inc., Aurora, Canada). Pre-treatment tetanic
tetanus values were used from the peak isometric torque data collected from single
optimized stimulation. Pre-twitch tension values were also determined prior to the
start of LCs.
Electrical stimulation was initiated for 0.2s during the treatment protocol
prior to any servomotor movement allowing for adequate muscle force
development and to collect isometric torque data for each individual contraction.
The servomotor pedal was initiated causing plantar flexion (LC) while remaining
24
contracted over a range of 38° for the next 0.3 seconds, causing an angular velocity
of 127°/s. Upon completion of each contraction, stimulation was stopped and the
pedal passively maneuvered the foot back to the respective start position within 3
seconds. LCs protocols consisted of 20 or 40 stimulated contractions, sectioned into
1 set of 20 LCs, with 3 seconds of rest between each repetition, or 2 sets of 20 LCs,
with 3 seconds of rest between each contraction and 5 minutes rest was allowed
between each set. After completion of the LCs, peak tetanic tension and twitch
tension were re-measured immediately after and at 10-minutes following LCS using
a single 0.5-seconds stimulation against a rigid pedal. Rats were monitored for one
hour following electrical stimulation while they recovered before being returned to
their cage.
3.3 Tissue Collection and Uterus Dissection Animals were euthanized 24 hours following LCs while under anesthesia via
cardiac exsanguination. Blood was collected by inserting an 18G needle into the left
ventricle and blood slowly removed, and placed in evacuated collection tubes
(Vacutainer, BD, NJ, USA) free of anti-coagulant agent heparin. Blood was mixed at
4° for two hours and centrifuged at 3,000 rpm for 20 minutes at 4°. Serum was
stored in 1.5ml eppendorf tubes in a -70°C freezer until later analysis (Appendix
7.1).
TA muscles were excised from all CC animals, OVI and OVX lengthening
contracted and contra-lateral (control), weighed and portioned into three pieces.
Muscle samples were either placed in 1.5ml eppendorf tubes and snap-frozen in
liquid nitrogen, or coated in optimal cutting temperature medium (OCT) mounted
25
onto a corkboard and rapidly frozen in isopentane immersed in liquid nitrogen.
Embedded muscles were stored at -70°C for later cryosectioning and morphological
analysis.
To determine if ovariectomy altered uteri mass, the uteri were removed after
making an incision along the midline of the body to access the uteri. Once removed,
excess fat was trimmed away, and if present, ovaries were removed (OVI and CC).
For consistency with each dissection the uterus was cut at the bottom before the
junction of the bicornate uterine horns. Excess fat and connective tissue was
removed prior to weighing (Appendix 7.2).
3.4 Biochemical Analysis 3.4.1 Tissue Homogenization Frozen sections of TA muscle (30-140mg) were homogenized in 10 volumes
of RIPA buffer (Sigma Aldrich, Cat #: R0278; 50 mM Tris-HCl, pH 8.0, with 150 mM
sodium chloride, 1.0% Igepal CA-630 [NP-40], 0.5% sodium deoxycholate and 0.1%
sodium dodecyl sulphate) with 1:100 volumes of protease inhibitor cocktail (Sigma
Aldrich, Cat #: P8340; 104mM of AEBSF, 0.085mM of Aprotinin, 4mM of Besatin,
1.4mM of E-64, 2mM of Leupeptin and 1.5mM of Pepstain A) per volume of RIPA
buffer. A Bead Bug Microtube Homogenizer (Model D1030, Product Code:
1143051039) was used to homogenize muscle samples by vibrating tissue three
times for 45 seconds each. Samples were placed on ice between homogenizations to
avoid an increase in temperature. Homogenized muscle was centrifuged
(Eppendorf, Model #: 5415 C) for 30 seconds at 14,000 rpm to remove connective
26
tissue and supernatants were aliquoted and stored in a -70° freezer for later
analysis (Appendix 7.3).
3.4.2 Muscle Protein Determinations
TA muscle protein concentrations were determined by the method of Lowry
et al. (1951) using bovine serum albumin (BSA) as a standard. In short, triplicate
tubes with 5μl of sample added to 0.5ml of ddH2O in a 13 x 100mm glass test tubes
were used. Five milliliters of Lowry reagent (5 ml/250 ml of 2% w/v CuSO45H₂O, 5
ml/250 ml 4% w/v sodium tartrate in 240 ml of 3% w/v Na2CO3) was added,
vortexed and allowed to react for a minimum of 10 minutes. Phenol reagent (0.5 ml;
Sigma Aldrich, Cat #: F9252) diluted 1:2 times with ddH₂O was added while
vortexing and allowed to react for 30 minutes. Absorbance was measured at 660
nm in a spectrophotometer (Turner, model # 340). A standard curve consisting of
20, 40, 60, 80 and 100 µg of BSA was constructed and were determined using a
linear regression equation (y=mx+b) and compared to the net absorbance of
samples (Appendix 7.4).
3.4.3 Protein Content Calculation
To calculate muscle protein content, the weight of the tissue sample (mg)
was added to the volume of homogenizing buffer and a total volume (ml) obtained.
The volume was multiplied by the determined protein concentration (Lowry from
3.52) to provide a total protein amount (g). The wet weight mass of the
homogenized muscle protein (mg) was divided by the muscle protein concentration
27
value obtained, yielding a protein-to-mass ratio (mg of protein/g wet weight
muscle). Total protein content of the TA muscle was expressed as a ratio of the LC to
the CL.
3.4.4 One-Dimensional Sodium Dodecyl Sulphate Polyacrylamide Gel Electrophoresis
Known amounts (100μg -200μg) of muscle homogenates were separated by
one-dimensional sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-
PAGE) as previously described (Laemmli, 1970), with the exception of the resolving
gel, prepared as a 5-15% linear gradient. Glass plates were cleaned with 70%
ethanol and assembled as described by the manufacture (Bio-Rad, Mississauga,
Canada). The separating gel consisted of two parts; a 5% and 15% acrylamide
mixture. The 15% acrylamide was added to the back chamber and stirring applied.
The stopcock was closed and the air between the two chambers removed. The 5%
acrylamide mixture was added to the gradient maker chamber away from the spout.
Once the 15% acrylamide covered bottom portion of the cast, the stopcock was
opened and the acrylamide solutions mixed and drained into the gel. A 4:1 mixture
of H₂O and butanol was gently overlaid to remove any bubbles and gels were left to
polymerize for 1 hour or overnight. A stacking gel consisting ddH2O, stacking buffer
(0.8% SDS, 12.1% Tris pH6.8) and 3% acrylamide was overlaid over the resolving
gel and a 10 well 1.5mm teflon comb placed in the gel solution and allowed to
polymerize for two hours. Muscle homogenates (100μg-200μg) were loaded into
wells and electrophoresed at 60 volts until the dye front entered the separating gel.
Once into the separating gel voltage was increased to 110 volts until the dye reached
28
the bottom of the gel. A Bio-Rad Power Pac 1000 was used (Bio-Rad, Mississauga,
Canada) (Appendix 7.5).
3.4.5 Western Blotting—Protein Analysis
SDS-PAGE separated proteins were transferred from gels to nitrocellulose
membranes (0.22μm pore size), (Bio-Rad Laboratories, Mississauga, Canada) using
the method of Towbin et al. (1979) and modified to the Bio-Rad mini-protein II gel
transfer system described by Frier et al. (2008). Following transfer (~2 hours),
nitrocellulose membranes were blocked with 5% weight/volume non-fat skim milk
powder (NFSM) or 3% BSA dissolved in Tris-buffered saline (TBS) for one hour at
room temperature. TBS plus Tween-20 (TTBS) was used to wash the membranes
twice for five minutes each before being incubated overnight at 4°C with specific
antibodies for Hsp25 (ADI-SPP-715, ENZO, USA), Hsp72 (ADI-SPA-812, ENZO, USA),
HSF1 (H-311, SC-9144, Santa Cruz), diluted in TTBS with 2% NFSM or 3% BSA in
1:1000 concentration. Membranes were washed twice in TTBS for 5 minutes and
incubated for one hour at room temperature with appropriate secondary Goat Anti-
rabbit IgG HRP-linked antibody (BioRad Cat# 170-6515) and diluted in TTBS plus
2% NFSM or 3% BSA in 1:1000 concentration. Membranes were washed twice in
TTBS for five minutes and once in TBS for 30 minutes before being developed using
C-Digit (Mandel Scientific, Model #: CDG-001073 3600). Nitrocellulose membranes
were saturated with appropriate readymade substrates of eight mL of Luminata
Forte Western HRP Substrate (Millipore Corporation, Billerica, MA, Cat #:
WBLUF0100). Each blot was incubated separately for two minutes and developed
29
using Li-Cor C-Digit IS version 3.1 (Mandel Scientific, Model #: CDG-001073 3600).
Membranes were placed face down on the measuring surface of the C-Digit and
scanned at six minutes at normal sensitivity (Hsp25 and 72) or twelve minutes at
high sensitivity (HSF1). The optimal density of bands was quantified using the
Image Studio software (Image Studio Digits, version 5.2.5) and expressed as a fold-
increase of lengthening contracted TA muscle divided by contra-lateral (control) TA
muscle and values were expressed relative to CC animals, which was set to a value of
one (Appendix 7.5).
3.4.6 ELISA—Blood Serum Analysis Systemic circulation of serum 17-β estradiol concentration was measured
using an enzyme-linked immunosorbent assay (ELISA) (Abcam, ab108667). Serum
estradiol samples were determined by comparing a ratio of kit 17-β estradiol
control to animal serum samples. Blood serum samples were compared to a
reference standard. ELISA kit was brought to room temperature while tissue
samples thawed. Once thawed, 25μl of standards, kit control and tissue samples
were added to appropriate wells. Following this, 200μl of 17β-estradiol HRP
conjugate was added to each well and the 96 well plate was covered with aluminum
foil and left to incubate for two hours at 37°. Following incubation, the well contents
were removed and washed with the three times with 300μl of wash solution and
any excess solution was blotted from the wells. 100μl of TBM substrate was added
to each well and allowed to incubate for precisely 30 minutes at room temperature.
Stop solution (100μl) was added to each well and the 96 well plate was read at a
wavelength of 450nm within 30 minutes of final incubation (Appendix 7.6).
30
3.5 Morphological Analysis 3.5.1 Muscle Cross-Sectioning
Portions of skeletal muscle preserved in OCT medium, were cut using a
cryostat at -20°C (Cryo-Cut, American Optical Company, model #: 830) at a
thickness of 10 microns. The sections were air dried and stored at -20°C freezer
until stained for visualization using hematoxylin and eosin (H&E) (Appendix 7.7).
3.6.2 Hematoxylin and Eosin Staining
Cross-sections were stained using H&E. Staining was performed by placing
the slides in tap water for one minute, followed by hematoxylin (Sigma Aldrich; Cat
#: HHS32) for 3 minutes, the slides were rinsed in fresh tap water and placed into
distilled water for one minute, respectively. Cross-sections were moved through a
series of ethanol solution (30% and 50%) for one minute, before being placed in
eosin (Sigma Aldrich; Cat #: HT110180) stain for seven minutes. Slides were then
rinsed in a series of ethanol solutions of 70%, 90% and 95% for one minute each.
Cross-sections were placed in the first 100% ethanol for two minutes and a second
100% ethanol solution for two minutes, before being moved to xylene substitute
(Sigma Aldrich; Cat #: A5597) five minutes. Cross-sections were sealed with a VWR
micro glass cover (Cat #: 48366 067) and sealed using cytoseal 280 glue (Thermo
Scientific; Cat #: 8311-4). A small drop of the cytoseal glue was placed in the center
of the micro glass cover and placed directly over the centre of the stained slide.
Direct pressure was applied over the glass cover to force out air bubbles. Once the
sealed slides fully dried, slides were viewed using a Zeiss Axioskop and
31
photographed at 5x, 10x and 40x magnification using a Canon EOS 70D (Appendix
7.8).
3.5.3 ImageJ Quantification
ImageJ 64-bit software (National Institutes of Health; version 1.48v) was
used to quantify characteristics of skeletal muscle damage following H&E staining.
One hundred muscle fibres of each sample were counted to get an accurate
representation of muscle damage in each sample group. Characteristics of muscle
damage included fibre area, circularity and roundness. In addition, following the
model by Rizo-Roca et al. (2015) necrotic fibres were examined, as well as
endomysial and perimysial infiltration and distension. To do this, photos of
micrometers for 5x, 10x and 40x magnification were used to set the scale to count
measure fibre area, circularity and roundness. Photos of the micrograph were
loaded into ImageJ and line tool was selected to draw a straight line across a known
distance micron distance. The distance in pixels measured was set to the known
distance in microns and globally set to apply to images of the same magnification.
To examine the extent of muscle fibre damage, TA muscle fibre values from
the lengthening contracted TA muscles were compared to the CL values to
determine if LCs resulted in increased skeletal muscle damage, or in TA muscles
between OVI and OVX animals to examine if ovariectomy had an effect on muscle
fibre changes. In addition, values from the CL TA muscle were also compared
between OVI and OVX animals. Two hundred muscle fibres were counted in each
32
sample group to get an indication of focal or global damage and differences between
OVI and OVX animals (Appendix 7.9).
3.5.4 Histological Quantification Fibre roundness, circularity and area were quantified using the ImageJ tools
using ImageJ software 64-bit for Mac OS X. To count fibre roundness, circularity and
area, the polygon tool was used to carefully trace around the fibre. Once a fibre was
measured the paintbrush tool was selected and an “X” was drawn through the fibre
to ensure the fibre was not counted a second time.
Fibre area was quantified by the selected area, measured in square pixels and
calibrated in square units (e.g. mm2, μm2). Circularity is a measure that ranges from
0 (infinite polygon) to 1 (perfect circle). In contrast, roundness better captures
asymmetrical shapes, thus overall shape is accounted for.
In addition, following methods published by Rizo-Roca et al. (2015) fibre
damage was examined through multiple measures including; necrotic fibres
characterized by the infiltration of inflammatory cells (myophagocytosis),
fragmented sarcoplasm, dark staining (hypercontracted) and pale staining (necrotic
fibres). Furthermore, the extracellular inflammatory domain was examined,
consisting of endomysium and perimysial infiltration. Permysial infiltration
consisted of small, mononuclear cells found in the perimysium, while endomyisal
infiltration was similar but found within the endomysium. Lastly, the interstitial
compartment was analyzed and divided into endomysial and perimysial distention,
where space (distension) was present between the individual muscle fibres or
33
fascicles, respectively. Fibres were counted and marked using the paintbrush tool to
avoid recounting fibres. Two hundred fibres from each muscle sample were counted
to get an accurate representation of muscle damage (Appendix 7.9).
3.6 Statistical Analysis For all measures means and standard error of the mean were calculated to
compare differences from CC, OVI and OVX animals. When data was merged
between CC and OVI (CC/OVI) animals (body mass, contra-lateral control TA mass,
uterus mass and 17-β estradiol concentration) a Students T-test was performed. For
analysis of fibre morphology and biochemical analysis a one-way ANOVA test with a
Tukey’s post hoc analysis was used. A two-way repeated measures ANOVA was used
to analyze all measures of TA muscle torque, maximal tetanic tension and maximal
tetanic twitch. Statistical significance at an accepted P value of 0.05 was set and
GraphPad Prism version 6 software was used to perform data analysis.
34
Chapter IV: Results
4.1 Anatomical and Physiological Alterations 4.1.1 Anatomical Changes Following Ovariectomy To determine if ovariectomy (estrogen-removal) resulted in anatomical
changes, the mass of the body, TA muscles and uteri were measured. Given that
animals from CC groups are biologically identical to OVI animals, except for the
stimulation provided to the TA muscles, in cases where no differences between
these groups (OVI and CC animals), were observed, data were combined. Thus,
when the body mass of OVI/CC animals (285.0 ±6.1g) was compared to OVX animals
(335.9 ±6.0g), a 17.9% increase in the latter was observed (P<0.001; Table 1),
suggesting one effect of ovariectomy is an increased body mass.
Given that ovariectomy resulted in an increased body mass, it was
determined if muscle mass also increased. To do this, mass from the CL TA muscle
from OVI/CC animals (0.56 ±0.01g) were compared to the mass of the CL TA
muscles from OVX animals (0.66 ±0.02g). A significant increase (P<0.001; Table 1)
in TA muscle mass was observed in the CL TA muscles from OVX animals. To
determine if the observed elevation in TA mass was related to the increase in body
mass or to muscle hypertrophy, muscle mass to body mass ratios were determined.
Since no differences were observed in the TA muscle mass to body mass ratios
between OVI/CC and OVX animals (1.99 ±0.04 vs. 1.96 ±0.03) (Table 1), the
increased TA mass in ovariectomized animals was the result of increased body
mass. That is, TA mass was proportional to body mass.
35
The uterus is known to be an estrogen responsive organ (Astwood, 1939;
Jazbutyte et al., 2006). Thus, three weeks of estrogen deprivation via ovariectomy
would be expected to alter uteri mass. To assess this, uteri were removed from OVX
animals and their mass compared to OVI/CC uteri (0.57 ±0.03g vs. 0.17 ±0.01g). A
marked decrease of 70% was observed in the uteri mass from OVX animals
(P<0.001; Table 1), suggesting the loss of ovaries/estrogen dramatically affected the
mass of this organ.
To confirm that ovariectomy decreased blood estrogen levels, serum 17-β
estradiol levels were measured by enzyme-linked immunosorbent assay. OVX
animals displayed a significantly lower serum estradiol concentration (-48.6%)
when compared to all OVI/CC animals (19.6 ±2.1pg/ml vs. 38.1 ±4.4pg/ml; P<0.01;
Table 1). Taken together, the atrophy of the uteri in combination with decreased
serum 17-β estradiol concentrations suggest both tibilais anterior muscle and
estrogen sensitive tissues were markedly altered by ovariectomy.
4.1.2 The Effect of Lengthening Contractions on TA Muscle Mass
To determine if LCs altered the mass of TA muscles from OVX animals, TA
mass was measured twenty-four hours following LCs. An increase in TA mass was
observed following 20 LCs; such that, the mass of the lengthening contracted TA
increased in OVX animals by 13.9%, compared to TA masses from OVI animals
(0.72±0.02 vs. 0.62 ±0.03g; P<0.05). Similarly, following 40 LCs, the TA muscles
from OVX animals showed a 12.7% increase in mass when compared to lengthening
contracted TA muscle from OVI animals (0.63 ±0.01 vs. 0.55 ±0.01g; P<0.05; Table
36
2). When TA mass was expressed relative to body mass significance was negated
suggesting the observed increase in TA mass is due to the increased body mass
following ovariectomy.
Given that muscle swelling may occur following muscle contractions
(McCully and Faulkner, 1985), the absolute (g) TA muscle mass from CL and LC
limbs were compared. No statistical significances were found in the TA masses
between OVI and OVX groups following either 20 or 40 LCs (Table 2). Thus, the LCs
provided (20 or 40) did not result in an increased in TA mass.
37
Table 1: The Effects of Ovariectomy on Body, Muscle and Uteri Masses and 17-β Estradiol Concentration
Ovary-intact (OVI/CC)
n=17
Ovariectomized (OVX) n=12
Percent Difference
Body mass (g) 285.0 ±6.1 335.9g ±6.0*** + 17.9% Contra-lateral Control Tibialis Anterior Mass (g)
0.55 ±0.01 0.66 ±0.02*** + 20.0%
TA Muscle Mass/Body Mass
1.99 ±0.04 1.96 ±0.03 -1.51%
Uterus mass (g)
0.57 ±0.03 0.17 ±0.01*** - 70.2%
17-β Estradiol Concentration (pg/ml)
38.1 ±4.4 19.6 ±2.1** - 48.6%
Animal masses were measured following ovariectomy and/or LCs, OVX animals displayed significantly greater body. Twenty-four hours following LCs, TA muscles and uteri were removed and measured. Uteri mass was significantly decreased in OVX animals. In addition, blood serum 17-β estradiol concentration was measured via an ELISA and decreased serum 17-β estradiol concentration in OVX animals was observed. Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend **= P<0.01, ***= P<0.001.
38
Table 2: Tibilais Anterior Muscle Mass in the Lengthening Contracted and Contra-lateral (Control) Limbs
OVI OVX
Control
Contra-lateral (control)
20 LC
Contra-lateral (control)
40 LC
Contra-lateral (control)
20 LC Contra-lateral (control)
40 LC
Tibialis Anterior Muscle (g)
0.60 ±0.02
0.58 ±0.03
0.62 ±0.03
0.51 ±0.02
0.55 ±0.01
0.69 ±0.03
0.72 ±0.02**
0.63 ±0.01
0.63 ±0.01*
Treatment TA/Contra-lateral Control TA
1.00
1.07 1.07 1.04 1.00
Characterization of the LC and CL TA mass and the ratio of LC limb divided by the CL, 24 hours following LC. Groups consisted of an n=5 for control TA muscles and an n=6 for both 20 and 40 LCs in each animal group. Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend *= P<0.05, **= P<0.01.
39
4.1.3 Muscle Protein Concentration
Protein concentration expressed as the amount of protein per mg muscle wet
weight was used to determine if the observed increase in OVX TA mass following
LCs was the result of increased protein concentration, an increased overall size or
merely due to water retention. For TA muscles subjected to LCs, a ratio of
lengthening contracted muscle mass value over CL mass was determined. For
animals not subjected (CC) to any LCs, a ratio of the right to the left TA muscle was
used. Ratios from the lengthening contracted limbs were compared to ratios of CL
TA muscle from CC animals. As expected, left and right TA muscle from CC animals
showed no differences in TA muscle protein content (ratio = 0.98 ±0.06). Following
20 LCs (1.0 ±0.08) or 40 LCs (1.0 ±0.08) the TA muscle protein content from OVI
animals was lower than CC animals although not statistically significant. Similarly,
no differences in TA muscle protein content from TA muscles from OVX animals was
detected when compared to CC animals. Thus, despite changes in the quantity of
muscle mass, muscle protein concentration was not significantly altered in the TA
muscle following ovariectomy.
4.2 Muscle Contractile Alterations 4.2.1 Muscle Contractile Properties To determine the effect of ovariectomy on skeletal muscle contractile
properties, TA muscle torque was measured throughout the 20 or 40 LCs as
described in methods and materials. Prior to undergoing LCs, maximal muscle
tetanic tension (MTT) and maximal twitch tension (MTw) were determined.
Following the cessation of LCs, tetanic tension and twitch tension were also
40
measured immediately after and at ten minutes following the last (20th or 40th) LC.
During an LC muscle torque can be separated into an active and a passive
component. The active component of torque is equal to MTT and was reached at
0.2ms, prior to lever movement (Figure 2). The passive component is the torque
resulting from the stretching of the TA muscle and occurred while the lever was
actively moving. The passive component of torque is an indirect measure of stretch
(or connective tissue tolerance) (Figure 1). To normalize for alteration in muscle
mass, such as that observed in OVX animals, data are expressed in relation to muscle
mass, known as specific torque. That is, torque (g/cm) divided by TA mass (mg) to
provide a value in g-cm/mg muscle wet weight.
Figure 1: The Active and Passive Components of TA Muscle Torque During a Lengthening Contraction A lengthening contraction can be divided into the active (A) and passive (B) components of a cotraction. The active component of torque is the summation of tetanic tension, and occurs prior to the lever moving. The passive component if torque develops after the lever movesm and is an indirect measure of connective tissue tolerance or stretch.
41
4.2.2 Specific Total Torque Throughout 20 and 40 Lengthening Contractions When compared to the first LC, TA muscle torque was progressively
decreased by the ninth contraction for both groups (OVI: 0.71 ±0.04 vs. OVX: 0.70
±0.04g-cm/mg; P<0.001; Figure 2). When specific torque was measured no
difference in TA muscle torque was observed between OVI and OVX animals at any
contraction throughout the 20 LCs.
In TA muscles subjected to 40 LCs, TA torque was gradually decreased
(P<0.001) in OVI animals such that, after the thirteenth contraction in the first set
(0.63 ±0.04g-cm/mg; compared to contraction one) torque decrease was significant.
In the second set, when compared to the first contraction, a significant decrease
(P<0.001) in TA muscle from OVI animals was detected after the fourth contraction.
When TA muscles from OVX animals were examined, a decreased (P<0.001) in TA
muscle torque (0.65 ±0.04g-cm/mg) was noted after the tenth contraction in the
first set. When compared to the first contraction in the second set, a significant
decrease (P<0.001; Figure 3) in TA muscles from OVX animals was detected by the
fifth contraction. Overall, given that the TA muscle torque of OVI and OVX animals
decreased at similar points, it suggests ovariectomy does not change the ability of
skeletal muscle to generate torque.
42
Figure 2: Specific Muscle Torque is Similar Between OVI and OVX Animals Throughout 20 Lengthening Contractions No differences in TA muscle torque between OVI and OVX animals were observed throughout 20 LCs. TA muscle torque decreased in the ninth contraction in both OVI and OVX animals (P<0.001). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend ***= P<0.001.
43
Figure 3: Specific Muscle Torque is Similar Between OVI and OVX Animals Throughout 40 Lengthening Contractions No differences in TA muscle torque were observed throughout 40 LCs between OVI and OVX animals. TA muscles from OVI animals decreased torque in the thirteenth and fourth contraction in set one and two, respectively (P<0.001). While TA muscles from OVX animals decreased torque in the tenth and fifth contraction in set one and two, respectively (P<0.001). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend ***= P<0.001.
44
4.2.3 The Active Component of Tibialis Anterior Muscle Torque The active component of muscle torque is a measure of tetanic tension prior
to the foot pedal actively lengthening the TA muscle and peaks between 0-0.2ms
following stimulation. To determine if the active component of TA muscle torque
was altered between OVI and OVX animals, the active component was measured and
compared for each LC. In TA muscles from OVI animals subjected to 20 LCs, the
active component of TA muscle torque was significantly decreased by the fifth
contraction, while TA muscles from OVX animals showed a significant decrease by
the seventh contraction (0.61 ±0.03 vs. 0.64 ±0.03g-cm/mg; P<0.001). No
differences were observed between the active components of TA muscle torque of
OVI and OVX animals for any of the repetition time points examined during the 20
LCs (Figure 4). Thus, ovariectomy does not appear to alter the active component of
muscle torque during lengthening contractions.
To investigate muscle torque beyond 20 LCs, TA muscles were subjected to
40 LCs. In this case, the active component of TA muscle torque from OVI animals
was significantly decreased (from the first contraction of the first set) at the eighth
contraction (0.54 ±0.04g-cm/mg; P<0.001). In the second set, TA muscles from OVI
animals showed a decreased (P<0.001) torque at the fifth contraction when
compared to the first contraction. Similarly, TA muscle torque from OVX animals
significantly decreased at the seventh contraction of the first set (0.58 ±0.04g-
cm/mg; P<0.001) and at the sixth contraction of the second set (compared to the
first contraction of the second set; P<0.001). No differences in the active component
of TA muscle torque were observed between TA muscles from OVI and OVX animals
45
at any repetitions during the 40 LCs. A similar pattern of active component TA
torque loss was observed between OVI and OVX animals during 40 LCs (Figure 5).
Taken together, these data suggest that although LCs tended to decrease in the
active component of TA muscle torque, ovariectomy does not result in any
additional losses in the active component of muscle torque.
46
Figure 4: Ovariectomy Does Not Alter the Active Component of Muscle Torque Throughout 20 Lengthening Contractions No differences were observed in the active component of TA muscle torque between OVI and OVX animals throughout 20 LCs. TA muscle from OVI animals decreased the active component of TA muscle torque at the fifth contraction from the first contraction (P<0.001). In contrast, TA muscle from OVX animals decreased the active component of TA muscle torque at the seventh contraction from the first contraction (P<0.001). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend ***= P<0.001.
47
Figure 5: Ovariectomy Does Not Alter the Active Component of Muscle Torque Throughout 40 Lengthening Contractions No differences were observed in the active component of TA muscle torque between OVI and OVX animals throughout 40 LCs. In TA muscle from OVI animals the active component of torque decreased at the eighth contraction compared to the first contraction (set one) (P<0.001) and fifth contraction compared to the first contraction in set two (P<0.001). In TA muscle from the active component of TA muscle torque decreased by the seventh contraction compared to the first contraction (set one) (P<0.001) and sixth contraction compared to the first contraction in set two (P<0.001). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend ***= P<0.001.
48
4.2.4 The Passive Component of Tibialis Anterior Muscle Torque The passive component of torque refers to the torque generated after MTT
has plateaued. This reflects the stretch of the muscle generated by the tension (pull)
from the foot pedal moving and occurs between 0.3ms to 1.0 seconds. The passive
component of torque may be considered as an indirect measure of muscle and
connective tissue resistance to stretch. For the ease of presentation, decreases in the
passive component of TA muscle torque are presented in relation to the peak TA
obtained during contractions (Figure 6 and 7). Following 20 LCs, this occurred at
repetition five for TA muscles from OVI animals and at repetition eight for TA
muscles from OVX animals. A steady decrease (P<0.001) in the passive component
of TA muscle torque occurred at the eleventh contraction in TA muscles from OVI
animals (0.10 ±0.01g-cm/mg). In contrast, the passive component of TA muscle
torque from OVX animals was gradually but significantly decreased (P<0.01) by the
sixteenth (0.07 ±0.01g-cm/mg). Again no differences were observed in the passive
component of TA muscle torque between OVI and OVX animals. However, it should
be noted that TA muscles from OVI animals reached their peak passive torque prior
to the TA muscles from OVX animals (fifth vs. eighth contraction; Figure 6). Taken
together, these data suggest that following ovariectomy, the passive component of
torque and perhaps connective tissue may stiffen and be able to resist greater TA
stretch.
During 40 LCs, no significant differences were observed in TA muscles
between OVI and OVX animals at any contraction time point. Decreases in the
passive component of TA muscle torque following 40 LCs are presented in relation
49
to the peak contraction torque (eight vs. seven, OVI vs. OVX). TA muscles from OVI
animals were decreased by the sixteenth contraction while TA muscles from OVX
animals were decreased by the eighteenth contraction during the first set (0.09
±0.01 vs. 0.07 ±0.005g-cm/mg; P<0.001, P<0.05, respectively).
When compared to the first contraction in the second set, TA muscle torque
from OVI animals showed a decreased passive component by the seventh
contraction while TA muscles from OVX animals showed a decrease by the ninth
contraction (P<0.001; Figure 7). When TA muscles from OVI and OVX animals were
compared, a trend of maintaining the passive component of TA muscle torque was
observed in OVX animals. In addition, TA muscles from OVI animals reached peak
passive torque prior to TA muscles from OVX animals. Lastly, although no difference
in the passive component of TA muscle torque was observed between OVI and OVX
animals throughout 40 LCs, the TA muscles from OVI animals lost the passive
component of torque prior to that of TA muscles from OVX animals. Thus,
ovariectomy may influence the onset of the passive component of TA muscle torque
loss throughout LCs.
50
Figure 6: Ovariectomized Animals Maintained the Passive Component of Torque Throughout 20 Lengthening Contractions No differences were observed in the passive component of TA muscle torque between OVI and OVX animals. The passive component of TA muscle torque from OVI animals decreased in the eleventh contraction from the peak of contraction five (P<0.001). In contrast, the passive component of TA muscle torque decreased in the TA muscle of OVX animals in the sixteenth contraction using the eighth contraction as the peak (P<0.01). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend **= P<0.01, ***= P<0.001
51
Figure 7: Ovariectomized Animals Maintained the Passive Component of Torque Throughout 40 Lengthening Contractions No differences were observed in the passive component of TA muscle torque between OVI and OVX animals. In TA muscle from OVI animals the passive component of torque decreased in the sixteenth contraction, while TA muscle torque from OVX animals decreased by the eighteenth in the first set (P<0.001, P<0.05, respectively). Both OVI and OVX animals were compared to their respective peak torque in the passive component. In the second set, the passive component of TA muscle torque decreased in the seventh contraction in TA muscles from OVI animals (P<0.001) when compared to the first contraction in the second set. Similarly, in the second set the passive component of TA muscle torque from OVX animals decreased by the ninth contraction, when compared to the first contraction. Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend *= P<0.05, **= P<0.01, ***= P<0.001.
52
4.2.5 Maximal Tetanic Tension Prior to and Following 20 and 40 Lengthening Contractions
To determine if ovariectomy altered the maximal tetanic tension of TA
muscle, measurements of MTT were reported prior to (pre), directly after (t=0) and
at 10-minutes after the last LC. Prior to 20 LCs, maximal tetanic tension was 0.64
±0.05g-cm/mg and 0.66 ± 0.04g-cm/mg in TA muscles from OVI and OVX animals,
respectively. Thus, prior to any LCs there was no significant difference in pre-tetanic
tension in TA muscles between OVI and OVX animals. Directly following the 20th LC
(t=0; 0.45 ±0.02g-cm/mg), TA muscle MTT from OVI animals was decreased
(P<0.001) by ~31% when compared to pre-tetanic tension. Similarly, TA muscle
MTT of OVX animals directly after (t=0; 0.43 ±0.02g-cm/mg) the 20th LC was also
significantly (P<0.001) decreased (~ 26%) when compared to pre-tetanic tension.
After ten minutes of recovery following the 20th LC, TA MTT (0.49 ±0.03g-
cm/mg) remained significantly (P<0.01) decreased in TA muscles from OVX animals
by ~35% compared to pre-MTT. In contrast, MTT TA tension of OVI animals (0.55
±0.02g-cm/mg) recovered such that is was not significantly reduced at ten minutes
following the last LC when compared to pre-MTT. This suggets ovariectomy may
alter the ability of skeletal muscle to recover following moderate LCs. No differences
were observed in MTT in TA muscles between OVI and OVX animals at any of the
three time points in 20 LCs (Figure 8).
In animals subjected to 40 LCs, TA muscle MTT was 0.68 ±0.03g-cm/mg and
0.70 ± 0.04g-cm/mg for OVI and OVX animals, prior to any LCs and showed no
significant difference in TA muscle pre-MTT between OVI and OVX animals. Directly
after (t=0) the 40th LC, MTT of TA muscles from OVI and OVX animals was
53
significantly (P<0.001) decreased (~60 and 61%; 0.27 ±0.02 vs. 0.27 ±0.05g-
cm/mg) when compared to pre-tetanic tension. At 10 minutes after the 40th LC, TA
muscle tetanic tension remained significantly (P<0.001) decreased when compared
to pre-tetanic tension for both OVI and OVX (~37% vs. 34%) TA muscles (0.43
±0.02 vs. 0.46 ±0.05g-cm/mg). When compared to tetanic tension directly after
(t=0) the 40th LC, the TA tetanic tension had significantly (P<0.001) recovered in
TAs from both OVI and OVX animals to 63% and 65% of pre-tetanic tension values
(Figure 9). However, no differences were observed in TA muscle tetanic tension
between OVI and OVX animals at any of the three time points examined.
54
0.0
0.2
0.4
0.6
0.8
Time
Teta
nic
Ten
sio
n (
g-c
m/m
g m
uscle
wet
weig
ht)
OVI
OVX
*****
Pre 0 +10 Pre 0 +10
***
NS
NS
NS
Figure 8: Maximal Tetanic Tension is Similar Between TA Muscles from OVI and OVX Animals Following 20 Lengthening Contractions No differences were observed in TA muscle MTT between OVI and OVX animals. Immediately following the 20th LC, TA MTT was significantly reduced in TA muscle from both OVI and OVX animals (P<0.001). Ten minutes following 20th LC, MTT was significantly decreased in only OVX animals (P<0.01). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend **= P<0.01, ***= P<0.001.
55
0.0
0.2
0.4
0.6
0.8
Time
Teta
nic
Ten
sio
n (
g-c
m/m
g m
uscle
wet
weig
ht)
OVI
OVX
***
***
******
***
***
Pre 0 +10 Pre 0 +10
NS Figure 9: Maximal Tetanic Tension is Similar Between TA Muscles from OVI and OVX Animals Following 40 Lengthening Contractions No differences were observed in TA muscle MTT between OVI and OVX animals. Immediately after and ten minutes following the 40th LC TA muscle MTT from both OVI and OVX animals compared to pre-MTT (P<0.001). In addition, post 10-minute recovery MTT was increased in TA muscle from both OVI and OVX animals when compared to TA muscle MTT directly the 40th LC (P<0.001). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend***=P<0.001.
56
4.2.6 Maximal Twitch Tension Prior to and Following 20 and 40 Lengthening Contractions Maximal twitch tension (MTw) is defined as the force generated from a single
muscle contraction in response to a single stimulus and was used to measure muscle
recovery following LCs. Similar to MTT, MTw was measured prior to (pre), directly
after (t=0) and at 10 minutes after the last LC. Prior to any LCs, TA MTw was 0.09
±0.01g-cm/mg for OVI animals and 0.12 ±0.02g-cm/mg for OVX animals and was
not significantly different. Directly after (t=0) the 20th LC, TA muscle twitch tension
was not significantly decreased in OVI animals or OVX animals (OVI: 0.10 ±0.01;
OVX: 0.10 ±0.01g-cm/mg) when compared to pre-MTw. At 10 minutes after the last
LC, both OVI and OVX TA muscle MTw was significantly decreased (P<0.01;
P<0.001), respectively when compared to pre-MTw. Ten minutes after the 20th LC
MTw was significantly decreased (P<0.001) in both TA muscle from OVI and OVX
animals when compared to MTw directly after the 20th LC (Figure 10). When the TA
muscles from OVI and OVX animals were compared, no differences were observed
between treatments at any of the three contraction time points examined.
To determine if an additional set of LCs influenced muscle function, animals
were subjected to a second set of 20 LCs. Similar to 20 LCs, TA muscle twitch tension
was measured at identical time points and no differences in maximal TA muscle pre-
twitch tension were observed between OVI and OVX animals. When compared to
pre-twitch tension (0.11 ±0.01g-cm/mg) TA muscles from OVI animals were
significantly (P<0.001, all conditions) decreased after the 40th LC such that a ~64%
loss at 0- (0.04 ±0.01g-cm/mg) and ~82% reduction at 10 minutes (0.02 ±0.003g-
cm/mg) was observed. When pre-TA muscle twitch tension (0.11 ±0.01g-cm/mg)
57
from OVX animals was compared to 0- (0.04 ±0.01g-cm/mg) and 10 minutes (0.04
±0.01g-cm/mg) a significant (P<0.001) decrease of approximately 64% for both
time points was observed. Notably, when compared to pre-twitch tension, TA
muscles from OVX animals recovered 36% of TA pre-twitch tension, while TA
muscles from OVI animals only recovered 18% at 10-minutes after the 40th LC.
However, similar to 20 LCs, no significant differences in TA twitch tension between
OVI and OVX animals were observed at any of the three time points examined
(Figure 11).
58
0.00
0.05
0.10
0.15
Time
Tw
itc
h T
en
sio
n (g
-cm
/mg
mu
sc
le
we
t w
eig
ht)
OVI
OVX
**
***
***
***
Pre 0 +10 Pre 0 +10
NS Figure 10: Maximal Twitch Tension is Decreased Following 20 Lengthening Contractions No differences were observed in TA muscle MTw between OVI and OVX animals. No difference was observed in TA muscle pre-MTW when compared to TA muscle MTw directly following the 20th LC in both OVI and OVX animals. At ten minutes following the 40th LC TA muscle MTw was significantly decreased in 10- compared to pre-MTw from both OVI and OVX animals (P<0.01, P<0.001, respectively). Furthermore, post 10-minute MTw was significantly reduced in the TA muscles of both OVI and OVX animals when compared to MTw directly after the 20th LC (P<0.001). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend **= P<0.01, ***= P<0.001.
59
0.00
0.05
0.10
0.15
Time
Tw
itc
h T
en
sio
n (g
-cm
/mg
mu
sc
le
we
t w
eig
ht)
OVI
OVX
***
***
***
***
Pre 0 +10 Pre 0 +10
NS
NS NS
Figure 11: Maximal Twitch Tension is Decreased Following 40 Lengthening Contractions No differences were observed in TA muscle MTw between OVI and OVX animals. In the TA muscle from both OVI and OVX animals, MTw was significantly decreased at 0 and 10-minute following the 40th LC when compared to TA muscle pre-MTw (P<0.001). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend ***= P<0.001.
60
4.3 Muscle Fibre Morphological and Histological Changes Following Ovariectomy and/or Lengthening Contractions 4.3.1 Histological Measures of Muscle Damage To determine if ovariectomy and/or exposure to LCs resulted in differences
in muscle damage, TA muscle cross-sections from both the CL and lengthening
contracted muscles were stained with H&E and examined by light microscopy. Fibre
area, circularity and roundness were measured (Table 3). Photomicrographs were
quantified using ImageJ as described in methods and material. In addition, a scale of
muscle fibre damaged developed by Rizo-Roca et al. (2015) was used to examine the
extent of muscle fibre necrosis, endomysial and perimysial infiltration of immune
cells and distension. The scale used a score of 0 as the absence of damage, 1 as
moderate damage and 2 as severe damage [Rizo-Roca et al. (2015)] (Table 4).
4.3.2 Muscle Fibre Morphology in the Contra-lateral (Control) TA Muscles from OVI and OVX Animals
Fibre area of CL TA muscles from OVX animals were 17.5% greater (P<0.001)
when compared to TA muscle fibre area from OVI animals (4169 ±60.0 vs. 3441 ±
53.0μm2). The CL TA muscles from OVX animals also displayed a 7.3-fold increase
(P<0.01) in endomysial distension (altered space between the individual muscle
fibres), when compared to the CL from OVI animals. Necrotic fibres of CL TA
muscles from OVX animals were increased 7.5-fold compared to CL TA muscles from
OVI animals (OVI: 0.06 ±0.06 vs. OVX: 0.45 ±0.15).
61
4.3.3 Visual Analysis of Muscle Damage from TA Muscles from OVI and OVX Animals Subjected to Lengthening Contractions
Visible signs of muscle damage include fibre necrosis, rounded fibres and
endomysial infiltration of immune cell. Figures 12-14 show photomicrographs of TA
muscle fibres from 20 or 40 LCs from OVI and OVX animals stained by H&E and
visualized using light microscopy. Necrotic fibres were considered those with
infiltrating inflammatory cells, fragmented sarcoplasm and dark or lightly stained
fibres [Rizo-Roca et al. (2015)]. In addition, endomysial infiltration of immune cells
was characterized by the presence of mononuclear cells within the muscle fibres.
Figure 12, panels A and F show fibre necrosis following both 20 and 40 LCs. The
presence of rounded fibres appears to be increased following LCs (Figure 13; Panel
C, Figure 14; Panel A). An increased endomysial infiltration was also observed
following 20 and 40 LCs (Figure 14; Panel A and D). Thus, LCs resulted in the
appearance of an increased extent of muscle fibre damage markers in the TA
muscles from both OVI and OVX animals.
4.3.4 TA Muscle Fibre Area from OVI and OVX Animals Following Lengthening Contractions
When LC TA muscle fibre area from OVI animals were compared to OVI
animals, TA fibres area from OVX animals was increased (P<0.001) by 21%
following 20 LCs (OVX: 4010 ±83.2 vs. OVI: 3159 ±61.9μm2). When subjected to 40
LCs, TA muscles from OVI animals only showed a 9.7% increase (3810 ± 75.9μm2;
P<0.01) in fibre area when compared to TA muscles from the CL. These findings
suggest estrogen deprivation alters fibre area when subjected to LCs.
62
4.3.5 TA Muscle Fibre Circularity from OVI and OVX Animals Following Lengthening Contractions
To further confirm if ovariectomy altered fibre morphology, fibre circularity
was measured. When compared to the CL TA muscles, no differences in fibre
circularity was observed in lengthening contracted TA muscle from OVI animals
following 20 LCs. In contrast, when compared to the CL TA muscles, lengthening
contracted TA muscles from OVX animals showed a small but significant (3.6%)
increase (P<0.001) in fibre circularity following 20 LCs. Following 40 LCs, TA muscle
fibres from OVI animals also exhibited a small but significant (2.4%; P<0.001)
increase in the muscle fibre circularity measure when compared to their respective
contra-lateral (control) TA muscles. Similarly, when compared to the CL TA muscle,
lengthening contracted TA muscles from OVX animals also showed a 3.6% increase
(P<0.001) in fibre circularity when subjected to 40 LCs. No differences in fibre
circularity were observed in CL or LC TA muscles between OVI and OVX animals.
4.3.6 TA Muscle Fibre Roundness from OVI and OVX Animals Following Lengthening Contractions
Since muscle damage from LCs is known to cause fibre swelling (McCully and
Faulkner, 1985), muscle fibre roundness was also examined. Following 40 LCs, TA
muscle fibres from OVI animals displayed an increased measure of roundness
(4.0%; P<0.001) when compared to their respective CLs. Similar to OVI animals,
OVX animals also displayed an increased (5.0%; P<0.001) roundness measure
following 40 LCs when compared to their respective CLs.
63
Figure 13, panel A and figure 14, panel C show photomicrographs of rounded
in TA muscle fibres subjected to LCs from OVI and OVX animals, respectively. A
representative rounded TA muscle fibre from an OVI animal subjected to 20 LCs is
presented in figure 13, panel A while a fibre from an OVX animal following 40 LCs is
shown in figure 14, panel C. Perhaps not surprisingly, LCs resulted in increased fibre
roundness. Fibre roundness was greater in the lengthening contracted TA muscles
from both OVI and OVX animals subjected to 40 LCs when compared to fibres from
unstressed contra-lateral (control). When the CL TA muscles were compared to the
lengthening contracted TA muscles, no differences in TA muscle fibre roundness
between muscle fibres from OVI and OVX animals was observed.
4.3.7 TA Muscle Fibre Necrosis from OVI and OVX Animals Following Lengthening Contractions
The scale by developed by Rizo-Roca et al. (2015) considers necrotic fibres as
those with infiltrating inflammatory cells, fragmented sarcoplasm and dark or
lightly stained fibres. When compared to the CL TA muscles, TA muscles from OVI
animals subjected to 20 LCs showed a 18-fold increase (P<0.01) in necrotic fibre
score. Similarly a 17-fold increase (P<0.05) was observed in necrotic fibre score
following 40 LCs. In contrast, lengthening contracted TA muscles from OVX animals
subjected to 20 LC, showed only a 3.1-fold increase (P<0.01) in necrotic fibre score
when compared to their respective CL TA muscles, similarly a 3.3-fold increase
(P<0.01) in necrotic fibre score was observed following 40 LCs (Figure 14; Panel B).
The difference in fold increase between OVI and OVX was due to the decreased basal
necrotic fibres in OVI animals compared to OVX animals (Table 4). When TA
64
muscles from OVI and OVX animals subjected to 20 or 40 LCs were compared, no
differences in the extent/number of necrotic fibres were observed. Thus, an
increased presence of necrotic muscle fibres in TA muscle from OVI and OVX
animals was only observed following 20 or 40 LCs.
4.3.8 Endomysial Infiltration of TA Muscle Fibres from OVI and OVX Animals Following Lengthening Contractions The endoymisum encases individual muscle fibres and is the smallest
component of connective tissue of the muscle. To determine if this was altered
following ovariectormy and/or LCs, endomysial infiltration of immune cells was
measured as described in methods and materials. Muscle fibre (endomysial)
infiltration in OVI animals was un-altered following 20 LCs. However, following 40
LCs, infiltration was observed such that TA muscles showed a 3.6-fold increase
(P<0.01) in endomysial infiltration [score of mononuclear cells (endomysial
infiltration)] when compared to their respective CL TA muscles (Figure 14; Panel C).
A photomicrograph of TA muscle fibres from an OVI animal subjected to 40 LCs
displaying an increased endomysial infiltration is presented in Figure 12, panel G. In
contrast, TA muscles from OVX animals showed a dramatic 8.7-fold increase
(P<0.001) in the score of mononuclear cells (endomysial infiltration) following both
20 and 40 LCs when compared to their respective CL TA muscles (0.15 ±0.08).
Photomicrographs showing an increased immune cell infiltration in the TA muscle
fibres from OVX animal after 20 and 40 LCs are presented in Figure 12, panel F and
Figure 14, panels A and D, respectively. When TA muscle fibres were subjected to 20
65
or 40 LCs, no differences in endomysial infiltration of immune cells in TA muscle
fibres between OVI and OVX animals were detected.
4.3.9 Endomysial Distension of TA Muscle Fibres from OVI and OVX Animals Following Lengthening Contractions Endomysium distension is characterized by an altered or distended space
between individual muscle fibres. When CL TA muscles subjected to 20 LCs from
OVI animals were compared muscles, showed a 9.0- and 10.0-fold increase (P<0.01)
in the endomysial distension score following 20 and 40 LCs, respectively. In
contrast, TA muscle fibres from OVX animals subjected to LCs showed no increase in
endomysial distension following either 20 or 40 LCs.
4.3.10 Perimysial Infiltration and Distension of TA Muscle Fibres from OVI and OVX Animals Following Lengthening Contractions
The perimysium consists of the sheath of connective tissue surrounding a
bundle of muscle fibres. When perimysial infiltration (altered mononuclear cells in
the perimysium) and distension (altered space between the muscle fascicles) was
examined, no observable differences were detected between TA muscle fibres from
OVI and OVX animals, or between LC and CL TA muscle fibres following 20 or 40
LCs.
66
Figure 12: Skeletal Muscle Changes in Ovary-Intact and Ovariectomized Animals Following 20 or 40 Lengthening Contractions A visual representation showing skeletal muscle focal damage at 24 hours following 20 or 40 LCs. Panel A: OVI CL; Panel B: OVX CL; Panel C: OVI CL; Panel D: OVX CL. Panel E: 20 LC OVI, Panel F: 20 LC OVX, Panel G: 40 LC OVI and Panel H: 40 LC OVX fibres were stained using H&E as described in methods and materials and scale bars represent 100μm.
67
Figure 13: Skeletal Muscle Damage Following Lengthening Contractions in Ovary-intact Animals Focal damage at 24 hours following either 20 or 40 LCs in OVI animals. Panels A and B: muscle fibres following 20 LCs and Panel C and D: muscle fibres following 40 LCs. Panel A: displays a rounded fibre (denoted by the *). Panel B: is a fibre that has been surrounded and infiltrated by immune cells (denoted by the pointing arrow). Panel C: represents fibre infiltration by immune cells (signified by an X). Lastly, Panel D: is characterized by central nuclei (denoted by the pointing arrows). Fibres were stained using H&E as described in methods and materials. Scale bars represent 100µm.
68
Figure 14: Skeletal Muscle Damage in Ovarectomized Animals Following Lengthening Contractions Focal damage at 24 hours following either 20 or 40 LCs in OVX animals. Panels A and B: muscle fibres following 20 LCs and Panel C and D: muscle fibres following 40 LCs. Panel A: represents fibre infiltration from immune cells (denoted by the *). Panel B: displays fibre splitting and the transition to a ghost fibre, along with immune cell infiltration (signified by the #). Panel C: is a rounded fibre (denoted by the X). Lastly, Panel D: is characterized by immune cell infiltration of a rounded fibre (denoted by the diagonal arrow). Fibres were stained using H&E as described in methods and materials. Scale bars represent 100µm.
69
Table 3: Skeletal Muscle Fibre Alterations Following 20 or 40 Lengthening Contractions A B C D E F Fibre Histology
OVI CL (n=10)
OVX CL (n=10)
OVI 20 LC (n=5)
OVX 20 LC (n=5)
OVI 40 LC (n=5)
OVX 40 LC (n=5)
Area (μm2) 3441 ±53.0 4169 ±60.0A 3159 ±61.9 4010 ±83.2B/C 3810 ±75.9D 4000 103.1 Circularity 0.82 ±0.002 0.81 ±0.002 0.83 ±0.003 0.84 ±0.003B
0.84 ±0.003A
0.84 ±0.003B
Roundness 0.67 ±0.003 0.68 ±0.004 0.67 ±0.006 0.69 ±0.007 0.70 ±0.006A 0.72 ±0.006B Quantified measures of fibre area, circularity and roundness in unstressed CL TA and LC TA muscles from OVI and OVX animals. ASignificant in relation to OVI CL (P<0.001), BSignificant in relation to OVX CL (P<0.001), CSignificant in relation to 20 LC OVI (P<0.001), DSignificant in relation to 40 OVI (P<0.001). TA muscle fibre area was increased in the CL TA muscle from OVX animals, when compared to CL TA muscles from OVI animals (A). In addition, following 20 LCs, TA muscles from OVX animals showed increased fibre area when compared to the TA muscles from CL (B). OVI animals increased TA muscles fibre area after 40 LCs (D). Furthermore, following 20 LCs TA muscles from OVX animals increased fibre area when compared to OVI animals (C). TA muscles fibre circularity increased in OVI animals following 40 LCs (A) and in TA muscles from OVX animals (B). After 20 LCs, fibre circularity was increased in TA muscles from OVX animals (B). Lastly, roundness increased in TA muscles from both OVI and OVX animals following 40 LCs when compared to CL TA muscles (A and B). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM.
70
Table 4: Skeletal Muscle Fibre Damage Following 20 or 40 Lengthening Contractions A B C D E F Histological Markers of Damage
OVI CL (n=10)
OVX CL (n=10)
OVI 20 LC (n=5)
OVX 20 LC (n=5)
OVI 40 LC (n=5)
OVX 40 LC (n=5)
Necrotic Fibres
0.06 ±0.06 0.45 ±0.15A 1.1 ±0.28A 1.4 ±0.22B
1.0 ±0.26C
1.5 ±0.27B
Endomysial Infiltration
0.39 ±0.14 0.15 ±0.08 0.60 ±0.27
1.3±0.3B
1.4 ±0.27A
1.3±0.26B
Endomysium Distension
0.11 ±0.08 0.8 ±0.09A 1.0 ±0.26A
1.1 ±0.28
1.1 ±0.23A
1.1 ±0.18
Presented are the quantified scores of necrotic fibres, endomysium infiltration and distension in the TA muscles of the CL and LC TA muscles. ASignificant in relation to OVI CL (P<0.01), BSignificant in relation to OVX CL (P<0.01), CSignificant in relation to OVI CL (P<0.05). Necrotic fibres increased in CL TA muscle fibres from OVX animals (A). Necrotic fibres were increased in the TA muscles from both OVI and OVX animals following both 20 (A and B) and 40 LCs (C and D). After 20 LCs, endomysial infiltration increased in TA muscles from OVX animals when compared to the CL TA muscles (B). In addition, endomyisal infiltration increased in the TA muscles from both OVI and OVX animals following 40 LCs when compared to the CL TA muscles (A and B). Lastly, endomysial distension increased in the CL TA muscles from OVX animals when compared to CL TA muscles from OVI animals (A). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM.
71
4.4 The Cellular Stress Response Following Ovariectomy and/or Lengthening Contractions 4.4.1 The Constitutive Expression of Heat Shock Protein 25 in Tibialis Anterior Muscle
Hsps may be used as markers of stress following exercise, or they may reflect
the extent of cell protection prior to a stress. In this study, a three-week period of
ovariecotmy was provided rending the possibility such that muscle (fibre) changes
in gene expression may have occurred. To determine if the constitutive expression
of Hsp25 and/or 72 were altered in TA muscles from OVI and OVX animals, Hsps
were assessed by Western blotting in unstressed muscles (not subjected to LCs).
Following band quantification, a ratio of right over left limb was determined for CC
animals, while TA muscle exposed to LCs had the Hsp values expressed as LC over
CL. When expressed to CC animals (1.0 ±0.16), no difference was found between the
TA muscle Hsp25 content for OVI and OVX animals CL TA (Figure 15). This suggests
estrogen deprivation does not alter the constitutive expression of Hsp25.
72
Figure 15: Constitutive Hsp25 Content is Unchanged Following Ovariectomy Characterization of constitutive expression of TA muscle Hsp25 from both OVI and OVX animals. No differences were observed in the CL TA muscle between OVX and OVI animals. Panel A: shows Western Blot bands for Hsp25. Lane 1: represents band intensity from the TA muscle from CC animals, Lane 2: depicts band intensity from the TA muscle from OVI animals and Lane 3: shows the band intensity from TA muscle from OVX animals. Panel B: displays the percent increase Hsp content (control-control right limb/contra-lateral control limb). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM.
73
4.4.2 The Constitutive Expression of Heat Shock Protein 72 in Tibialis Anterior Muscle To determine if ovariectomy altered the constitutive level of Hsp72 TA
muscle content, Hsp72 content was measured in the unstressed CL TA muscles from
CC, OVI and OVI animals. When expressed to CC animals, no change in TA muscle
Hsp72 content from OVI animals was observed. However, Hsp72 content in TA
muscles from OVX animals showed a marked reduction such that Hsp72 content
was significantly (P<0.05) decreased by 57%, (0.57 ±0.08 vs. 0.99 ±0.14; Figure 16).
Thus, estrogen deprivation (ovariectomy) appears to significantly decrease the
constitutive expression of HSp72 content in skeletal muscles.
74
Figure 16: Constitutive TA Muscle Hsp72 Expression is Significantly Decreased Following Ovariectomy Characterization of constitutive expression of TA muscle Hsp72 from both OVI and OVX animals. TA muscle from OVX animals displayed significantly less Hsp72 expression compared to TA muscle from OVI animals (P<0.05). Panel A: shows Western Blot bands for Hsp72 expression. Lane 1: shows band intensity of TA muscle from CC animals, Lane 2: represents band intensity of TA muscle from OVI animals, Lane 3: displays the band intensity of TA muscle from OVX animals. Panel B: displays the percent increase Hsp content (control-control right limb/contra-lateral control limb). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend *= P<0.05.
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4.4.3 TA Muscle Heat Shock Protein 25 Content Following Lengthening Contractions To examine the CSR in TA muscles from OVI and OVX animals, Hsp25 content
was examined 24 hours after LCs and the removal of the TA muscle. Given that the
constitutive expression of Hsp25 was similar between CC, CL OVI and CL OVX
animals, Hsp25 content was expressed as a ratio of the lengthening contracted value
relative to its respective CL value. In animals not subjected to LCs a ratio of right
over left TA muscle was computed. When compared to CC animals, no difference
was observed in TA muscle Hsp25 content from OVI animals following 20 LCs.
However, when subjected to 40 LCs TA muscle Hsp25 content from OVI animals
increased (P<0.01) by 260% (Figure 17). In comparison, TA muscle Hsp25 content
from OVX animals was increased (P<0.05) by 190% following 20 LCs and increased
(P<0.01) by 240% following 40 LCs (Figure 17). These data show that although
skeletal muscles from OVI and OVX animals are both capable of mounting a cellular
stress response, the stress may be experienced differently.
76
Figure 17: TA Muscle Hsp25 Content Increases Following Lengthening Contractions TA muscle Hsp25 content was increased in the TA muscle from OVX animals 24 hours following 20 and 40 LCs (P<0.05, P<0.01, respectively) and in TA muscle from OVI animals following 40 LCs (P<0.01) compared to the TA muscle from CC animals. Panel A: shows Western bands for TA muscle Hsp25 content. Lane 1: shows band intensity of TA muscle from CC animals. Lane 2: displays band intensity of TA muscle from OVI animals following 20 LCs. Lane 3: depicts band intensity of TA muscle from OVX animals following 20 LCs and Lane 4: represents band intensity of TA muscle from OVI animals following 40 LCs. Lane 5: shows band intensity of TA muscle from OVX animals following 40 LCs. Panel B: the percent increase of TA muscle Hsp25 content (LC divided by CL). Data was displayed in one graph for clarity. Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Legend *= P<0.05, **= P<0.01.
77
4.4.4 Heat Shock Protein 72 Content in the Lengthening Contracted TA Muscle
Given that Hsp72 content was decreased in the TA muscles from the CL OVX
animals, it was not possible to express a ratio of lengthening contracted TA value to
its respective CL value. To control for the decreased constitutive expression of
Hsp72 in OVX animals, Hsp72 content has been expressed relative to the value
obtained from CC animals. The Hsp72 content of TA muscles subjected to
lengthening contractions from OVI animals showed no increase following 20 LCs
when compared to CC animals (Figure 18). However, following 40 LCs, the TA
muscle Hsp72 content of OVI animals showed a 5-fold increase (P<0.05) when
compared to TA muscles from CC animals. In contrast, Hsp72 TA muscle content
from OVX animals remained unchanged following both 20 and 40 LCs when
compared to CC animals. These data suggest skeletal muscle from ovariectomized
animals demonstrates a compromised CSR in that its capacity to protect skeletal
muscle may be decreased due to decreased Hsp72 content following LCs.
78
Figure 18: TA Muscle Hsp72 Content Following 20 and 40 Lengthening Contractions in Ovary-Intact and Ovariectomized Animals TA muscle from both OVI and OVX animals did not increase Hsp72 content following 20 LCs. However, after 40 LCs, the TA muscle from OVI animals increased (P<0.05) compared to TA muscle from CC animals. Hsp72 content was not increased in TA muscle from OVX animals following LCs. Panel A: shows Western bands for TA muscle Hsp72 content. Lane 1: shows band intensity of TA muscle from CC animals. Lane 2: displays band intensity of TA muscle from OVI animals following 20 LCs. Lane 3: depicts band intensity of TA muscle from OVX animals following 20 LCs and Lane 4: represents band intensity of TA muscle from OVI animals following 40 LCs. Lane 5: shows band intensity of TA muscle from OVX animals following 40 LCs. Panel B: the percent increase of TA muscle Hsp72 content (LC divided by CL). Statistical significance was set at a P<0.05 and data are expressed as mean ±SEM. Data was displayed in one graph for clarity. Legend *= P<0.05.
79
4.4.5 HSF1 Content Stress induced increases in Hsps are regulated through the trimerization and
binding of heat shock factor-1 (HSF1) to the heat shock element (HSE) (Sarge et al.,
1993). The observed increase in TA muscle Hsp content following 20 or 40 LCs in
OVI and OVX animals suggests involvement of an HSF in the regulation of Hsp
expression following LCs. When HSF1 content was examined by Western blotting, a
ratio of CL TA muscles from OVI and OVX animals were compared to the value from
CC animals. A decrease in HSF1 content in the TA muscles of OVX animals was noted
when compared to TA muscles from OVI animals. Although a 31.0% reduction in
HSF1 content of TA muscle was observed in OVX animals, significance was not found
(Figure 19).
80
Figure 19: Heat Shock Factor1 Content in TA Muscles from OVX Animals No significant differences were observed in HSF1 content in TA muscle from OVI and OVX animals. Panel A: shows Western Blot bands for TA muscle HSF1 content and Panel B: displays the ratio of TA muscle HSF1 content between OVI and OVX animals. Lane 1: shows band intensity of TA muscle from OVI animals, Lane 2: shows band intensity of TA muscle from OVX animals. Data are expressed as mean ±SEM.
81
4.5 Summary 4.5.1 Anatomical, Physiological and Muscle Contractile Changes Following Ovariectomy and/or Lengthening Contractions Both body and TA mass were increased in OVX animals when compared to
OVI animals; however, uteri mass was markedly decreased in OVX animals. LCs
resulted in decreased torque throughout 20 and 40 LCs, as well as decreased tetanic
tension and twitch tension in all TA muscles examined. Ovariectomy did not
influence TA muscle MTT and MTw and no observable differences in TA muscles
torque were found throughout 20 or 40 LCs between OVI and OVX animals. The
passive component of LCs showed a decrease in TA muscle torque from OVI animals
prior to that observed from OVX animals, suggesting that an earlier onset of torque
loss in the passive component of torque may be mediated by estrogen. Lastly, the
active component of torque during LCs was also not affected by estrogen
deprivation.
4.5.2 The Changes in TA Muscle Fibre Morphology Following Ovariectomy and/or Lengthening Contractions
Ovariectomy resulted in an increased fibre area in the CL TA muscles from
OVX animals, when compared to CL TA muscles from OVI animals. CL TA muscles
from OVX animals also displayed an increased presence of endomysial distension
when compared CL TA muscles from OVI animals. Lastly, ovariectomy and LCs,
resulted in TA muscles from OVX animals showing an increased endomysial
infiltration after both 20 and 40 LCs. These findings suggest estrogen deprivation
may facilitate an increased level or extent of muscle damage.
82
4.5.3 The Muscle Cellular Stress Response Following Ovariectomy and/or Lengthening Contractions When compared to TA muscle from OVI animals, the constitutive expression
of TA muscle Hsp72 but not Hsp25 was decreased in OVX animals. In addition, TA
muscle Hsp72 content in the lengthening contracted TA muscles from OVX animals
was blunted in comparison to TA muscles from OVI animals. However, both TA
muscles from OVI (20 LCs) and OVX (20 and 40 LCs) animals were capable of
increasing Hsp25 content following LCs. These data suggest estrogen loss or
deprivation may selectively down regulate the expression of specific Hsps, thereby
decreasing the ability of muscles from OVX animals to mount a cellular stress
response following a single bout of LCs.
83
Chapter V: Discussion 5.1 Overview
The connection between menopause (estrogen health) and decreased energy
expenditure (Poehlman et al., 1995) may be related to a loss of metabolically active
muscle tissue. Menopause combined with decreased physical activity acts to elevate
central adiposity, oxidative stress and inflammatory markers associated with
sarcopenia (Sites et al., 2002; Bauer and Sieber, 2008; Maltias et al., 2009). Exercise
may help to attenuate many of the negative consequences associated with the
transition of menopause on body composition, physical fitness and overall health
(Roussel et al., 2009).
This study sought to determine the role of estrogen deprivation
(ovariectomy) on the CSR and muscle damage following maximally controlled
stimulated lengthening contractions of rodent TA muscles. It was hypothesized that
TA muscles from OVX animals would show a greater loss of muscle torque following
LCs relative to OVI animals. In addition, morphological markers of muscle damage
were expected to increase in TA muscles from OVX animals when compared to OVI
animals. Lastly, Hsp content (Hsp25 and 72) was expected to be elevated in TA
muscles from OVX animals following LCs.
When physiological measures of muscle function were compared this study
showed no contractile differences in skeletal muscle were observed between TA
muscles from OVI and OVX animals. Thus, estrogen deprivation, at least in the short-
term does not appear to compromise muscle function. However, TA muscles from
OVX had increased immune cell infiltration following muscle damage, suggesting the
84
muscles from OVX animals may be more susceptible to damage. TA muscle Hsp25
content was increased in OVI (20 LCs) and OVX (20 and 40 LCs) animals; however,
TA muscle Hsp72 content was only increased following 40 LCs in OVI animals. This
suggests estrogen deprivation (ovariectomy) may alter the muscle CSR. A decreased
Hsp72 expression was found in the constitutive TA muscles from OVX animals.
Taken together, these findings suggest certain changes in skeletal muscle may
commence shortly after estrogen deprivation occurs. Although, short-term estrogen
deprivation does not appear to effect skeletal muscle torque, the histological and
biochemical responses to LCs appear to be altered following ovariectomy. In the TA
muscles of ovariecotmized animals, an increased immune cell infiltration and an
inability to increase Hsp72 content following 20 and 40 LCs was observed. This
suggests as few as 20 LCs may be a sufficient stress to invoke muscle damage. In
OVX animals the CSR is altered such that skeletal muscle is unable to cope with the
demands of exercise, possibly resulting in additional muscle damage.
5.2 The Anatomical and Physiological Changes Following Ovariectomy
The TA muscles from ovary-intact and ovariectomized animals were
examined three weeks after surgical removal of the ovaries to ensure early changes
in anatomical characteristics had stabilized prior to being subjected to LCs. At the
time, ovariectomy resulted in an 18% increase in body mass and a 20% increase in
TA muscle mass. In addition, uteri mass was decreased by 70% and serum 17-β
estradiol concentration was also significantly decreased in OVX animals. These
85
changes suggest removal of ovaries substantially decreased estrogen and likely
resulted in the alterations to these anatomical parameters.
In agreement with this, Fisher et al. (1998), Christgau et al., (2004) and
Fontenelle et al. (2013), showed increases of 22%, 17.6% and 13.4% in body mass
of OVX animals, respectively. Ovariectomized animals have shown decreased cage
activity (Fisher et al., 1998) and increased food intake (Wade, 1972), resulting in a
positive energy balance (Fisher et al., 1998), thereby becoming more sedentary in
nature. This may also contribute to the increased body mass. In addition, Fisher et
al. (1998) also observed an increase soleus masses by 18% in OVX rats. These
studies support the observation of an increased TA mass in OVX animals observed
herein. Thus the current findings are in agreement with previous studies suggesting
estrogen deprivation results in an increased body mass.
With regards to the uterus, Christgau et al. (2004) and McCormick et al.
(2004) found uteri mass was significantly decreased by 69.2% and 65% in OVX
animals. These values are similar to decreases observed in the present study. These
data support the current findings of increased body and muscle mass and decreased
uteri mass following ovariectomy. Thus, the present study is consistent with other
studies showing estrogen deprivation via ovariectomy results in specific anatomical
changes.
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5.3 Skeletal Muscle Contractility
5.3.1 Tibialis Anterior Muscle Torque
To determine if ovariectomy altered skeletal muscle torque, TA muscles from
both OVI and OVX animals were subjected to 20 and 40 LCs. In general, no
differences in contractile measures were observed in TA muscle torque between
OVI and OVX animals during or following either 20 or 40 LCs. Following 20 LCs, TA
muscle MTT from OVI animals recovered a greater percentage of pre-MTT
compared to OVX animals, suggesting estrogen deprivation may impair skeletal
muscle recovery following LCs.
In humans, studies have observed an estrogenic affect in the maintenance of
skeletal muscle mass and torque (Greeves et al., 1997; 1999; Dionne et al., 2000;
Meeuwsen et al., 2000). In contrast, 60 days after ovariectomy OVX mice generated
less contractile tension, possibly due to an altered interaction between actin and
myosin (Moran et al., 2006). Moran et al. (2007) observed up to a 20% loss in
muscle torque in OVX mice following 30 days of estrogen deprivation. The lack of
any difference between OVI and OVX animals in the current study supports Wohlers
et al., (2009) where no difference in MTT was observed. The lack of observable
differences in TA muscle torque between OVI and OVX animals, in our hands,
suggests the role of estrogen on skeletal muscle torque is minimal.
The results of estrogen on skeletal muscle loss are mixed. In humans, studies
have observed an estrogenic effect on the maintenance of skeletal muscle mass and
torque (Greeves et al., 1999; Dionne et al., 2000; Meeuwsen et al., 2000). However,
animal models tend to shown no differences in skeletal muscle mass between OVI
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and OVX (Moran et al., 2006). The exact reasons for these differences remain
unclear but may be related, in part, to a variety of factors, such as the length of
estrogen deprivation, and fibre type. In the current study, the lack of differences
may be due to the short period of estrogen deprivation (three weeks), the
exercise/stimulation protocol used, the fibre type of the muscle examined (slow vs.
fast twitch). Fridén et al. (1983) observed type II fibres have narrower z-lines,
reflecting fewer attachments for thick and thin filaments (Yamaguchi et al., 1985).
Type II fibres contain fewer sarcoplasmic proteins, myomension and nebulin, which
play roles in sarcomere assembly (Agarkova et al., 2004; Pardo et al., 2005). The TA
muscle is a predominately type II or fast twitch muscle containing very few (<5%)
type I fibres (Locke et al., 1991). Thus, a relatively greater stress is applied to the
cytoskeleton of type II fibres, which may contribute to their greater susceptibility in
fibre damage (Choi, 2014). Estrogen deprivation has been shown to reduce the
relative amount of type IIX muscle fibres (Piccone et al., 2004). The age of animals at
the time of ovariectomy, or species differences may also explain the differences in
skeletal muscle torque.
5.3.2 Maximal Tetanic Tension and Twitch Tension Recovery Following Lengthening Contractions To gain an understanding of potential differences in skeletal muscle recovery
in an estrogen deprived state, TA muscle MTT and MTw were measured prior to,
directly after (t=0) and 10-minutes following LCs in OVI and OVX animals. Ten
minutes following the last (20th) LC, MTT tetanic tension of the TA muscles showed
a significant decrease in OVX animals when compared to pre-MTT. However,
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muscles from OVI animals at ten minutes after the 20th LC had significantly
recovered from pre-tetanic tension. This suggests estrogen may either minimize the
loss of MTT following LCs and/or facilitate recovery following LCs. A similar
response has been observed in aged rat muscle, where maximal tetanic force was
decreased and a ~60% decrease in recovery from intermittent isometric
contractions (Degens and Always, 2003). Thus, OVX animals may be similar to an
“aged” condition, in this respect.
Estrogen deprivation may alter MTT and MTw through multiple mechanisms
including due to interference with Ca2+ binding sites (Martinez-Azorin et al., 1992).
Diethylstilbestrol, an endocrine disruptor, directly inhibited rabbit muscle
sarcoplasmic reticulum Ca2+ ATPase by interfering with Ca2+ binding sites
(Martinez-Azorin et al., 1992). Estrogen deprivation may affect Ca2+ reuptake into
skeletal muscle, indicated by an increase in soleus half-relaxation time (McCormick
et al., 2004). Ovariectomy may also result in decreased fast myosin heavy chain
expression observed in the soleus muscle (Kadi et al., 2002), indicating the estrogen
deprivation may reduce contraction speed (McCormick et al., 2004).
Using an in vitro model, McCormick et al. (2004) showed that time to peak
tension was decreased in OVX animals, although maximal isometric torque
remained unchanged in the soleus from OVX animals. In addition, using a similar
model, after three weeks of ovariectomy, Hubal et al. (2005) observed no significant
difference in peak isometric torque in TA and EDL muscles from OVX mice and sham
mice; however, peak isometric torque tended to be ~5-10% lower in OVX mice.
Furthermore, using an in situ model Fisher et al., (1998) found no significant
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differences in peak tetanic tension in the EDL and soleus of OVX rats with a two-
week period of ovariectomy. Similar to the current study, in vivo or in situ models of
exercise do not appear to alter MTT following ovariectomy. However, in vitro
measures of contractility resulted in decreased skeletal muscle MTT. Using a three-
week period of estrogen deprivation, Warren et al. (1996) showed an 18% decrease
in in vitro pre-peak isometric torque in EDL muscles from OVX mice, although no
significant difference was observed in post-peak isometric tension in EDL muscles
from OVI and OVX mice. Taken together, these differences in MTT observed may be
the result of different models of muscle damage used (in vivo, in vitro and in situ), as
well as the length of estrogen deprivation prior to contractile measures.
In the present study, TA muscle MTw was examined with no differences
observed between OVI and OVX animals. Bunratsami et al. (2015) showed twitch
tension was significantly decreased in EDL muscles from OVX rats. Using an in vitro
model, isometric MTw in the EDL was significantly decreased in OVX mice compared
to sham mice (Lai et al., 2016). Similar to MTT, mixed results were observed in MTw
between OVX and sham animals from the current study when compared to past
results. The differences in the present study to others may again be the model (in
vivo versus in vitro) to determine MTw. Furthermore, neither Bunratsami et al.
(2015) or Lai et al. (2016) employed an exercise protocol to induce muscle fatigue
or damage. In contrast, the present study examined the role of ovariectomy on
skeletal muscle torque using both 20 and 40 LCs.
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5.3.3 The Active Component of Tibilais Anterior Muscle Torque
The active component of muscle torque is a measure of tetanic tension prior
to the foot pedal actively lengthening the TA muscle and peaks between 0-0.2ms of a
LC. No differences were observed in the active components of TA muscle torque
between OVI and OVX animals. To date, no literature is available on the active
component of skeletal muscle torque measured during in vivo contraction. In the
closest study available, Moran et al. (2007) used 4 weeks of estrogen deprivation
and showed a 10% decrease (in vitro) in the active stiffness in the soleus, which is
predominantly a slow oxidative muscle. Whether differences between this finding
and the present study are due to in vivo versus in vitro muscle contraction, or some
other factor(s) remains to be determined.
5.3.4 The Passive Component of Tibialis Anterior Muscle Torque
The passive component of torque refers to the torque generated after MTT
has plateaued. This reflects the stretch of the muscle generated by the tension (pull)
from the foot pedal moving and occurs between 0.3ms to 1.0 seconds. The passive
component of torque may be considered as an indirect measure of muscle and
connective tissue resistance to stretch. The passive component of TA muscle torque
decreased in OVI animals prior to TA muscles from OVX animals throughout both 20
and 40 LCs, suggesting tissues from OVX animals may be stiffer or be beginning to
show an increased stiffness compared to connective tissues from OVI animals.
Moran et al. (2007) examined the (in vitro) soleus (passive) stiffness in OVX mice
and showed it increased by 7.7% after four weeks of ovariectomy. Skeletal muscle
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connective tissue is essential for the transmission of force and stability throughout
skeletal muscle structures (Kjaer, 2004). An increased collagen formation has been
reported in articular cartilage from ovariectomized rats (Fontenelle et al., 2013).
Estrogen deprivation has been shown to increase collagen production, thereby
increasing ossification and decreasing mechanical resistance (Fontenelle et al.,
2013). Taken together, the observations and the present work suggest estrogen
deprivation may result in an increased connective tissue stiffness and a slow but
progressive loss in the passive component of muscle torque.
In the present study, no differences in the passive component of TA muscle
torque were observed between OVI and OVX animals. However, a trend towards an
elevated passive component of TA muscle torque was observed in OVI animals
(compared to OVX animals) suggesting a decreased elasticity in connective tissues
may have commenced. The passive component of TA muscle torque from OVI
animals decreased before TA muscles from OVX animals. The production of passive
tension and storage and release of elastic recoil energy in skeletal muscle may be
necessary for energy transmission in LCs (Lindstedt et al., 2001). Tendons are
capable of returning 85-95% of the stored energy (Shadwick, 1990; Matson et al.,
2012). A stiffer spring may enhance the amount of elastic recoil energy available in
the stretch shortening cycle (Komi, 2000). Thus the increase in articular cartilage in
OVX animals may allow for greater energy transmission allowing for prolonged
torque production and may enhance the “spring like” (Lindstedt et al., 2001)
property of the muscle. Seyfarth et al., (2000) showed an increased muscle stiffness
(tighter muscle spring) allowed for improvements in lengthening exercises, such as
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jumping. Taken together, estrogen deprivation may result in increased tissue
stiffness allowing for greater transmission of energy.
5.4 Histological Characteristics
5.4.1 Muscle Fibre Area and Circularity in Ovary-Intact and Ovariectomized Animals
Estrogen deprivation increases body mass, which would account for the
increased fibre area observed since it would require a greater muscle mass to cope
with the increased body mass. Following ovariectomy, TA muscle fibre area of the
CL limb was increased in OVX animals when compared to the CL limb of OVI
animals. Given that both body mass and skeletal muscle mass were increased
following ovariectomy, the increased body mass observed herein may account for
the observed increase in CL TA muscles fibre area from OVX animals. Fibre
circularity (a measure of a perfect circle) was also increased in the TA muscles from
OVX animals following both 20 and 40 LCs. In contrast, TA muscles from OVI
animals only showed an increase in fibre circularity after 40 LCs. Although the
absolute stress of LCs was the same for both OVI and OVX animals, the different
response observed between the two suggests 20 LCs was an insufficient stress to
invoke fibre area and circularity increases in OVI animals.
5.4.2 Endomysial Infiltration
Using the visual scale developed by Rizo-Roca et al. (2015) H&E stained
muscle fibres were examined for damage by light microscopy. An increase in the
infiltration of immune cells was observed in the endomysium of TA muscle fibres
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from OVX animals following both 20 and 40 LCs. In contrast, endomysial infiltration
was only increased following 40 LCs in TA muscles from OVI animals. Similar to
fibre circularity, this suggests muscles from OVX animals may be more susceptible
to the stress imposed by LCs. Twenty LCs may be experienced as a relatively greater
stress in OVX animals. It appears that the changes due to estrogen deprivation may
alter either the permeability of connective tissue or the activity of immune cells.
Given that LCs require the absorption of energy, a muscle incapable of this action
may be more easily damaged (Roberts, 2016).
Neutrophil and macrophage infiltration are known to be sensitive to ovarian
hormone (progesterone and estrogen) concentrations (Zuckerman et al., 1996;
Angstwrum et al., 1997; Komulainen et al., 1999; Tiidus et al., 2001, 2005). McClung
et al. (2007) observed increased neutrophil and macrophage invasion in the soleus
muscle from OVX animals during the initial week of recovery from disuse injury.
Multiple studies using downhill treadmill running have shown estrogen attenuates
neutrophil infiltration (St. Pierre-Schneider et al., 1999; Enns and Tiidus, 2010;
Nedergaard et al., 2013). The present work suggests estrogen deprived skeletal
muscle may not recover from the injury induced by LC-biased exercise. Similarly,
Tiidus et al. (2001) showed an estrogenic effect on post-exercise neutrophil
invasion, suggesting estrogen mediated leukocyte infiltration following exercise and
may result in a reduction of intramuscular leukocyte infiltration (Iqbal et al., 2008).
Thus, following LCs, TA muscles from OVX animals are likely to experience greater
muscle damage when compared to TA muscles from OVI animals.
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Whether estrogen attenuates the primary or secondary phase of muscle
damage through the localized inflammatory response remains to be determined
(Savage and Clarkson, 2002). Stupka and Tiidus (2001) examined neutrophil
infiltration following ischemia-reperfusion injury in the hind limb of female rats and
showed OVX rats exhibited an increased myeloperoxidase activity when compared
to OVI animals. In addition, Iqbal et al. (2008) observed an increased neutrophil and
macrophage invasion in the soleus and vastus lateralis muscles from OVX rats
following downhill treadmill running. These data suggest estrogen attenuates
leukocyte infiltration following injury or exercise. Whether estrogen acts in
conjunction with Hsps or other cellular mechanisms, thereby providing resistance
against muscular damage, to limit leukocyte infiltration remains to be determined.
5.4.3 Endomysial Distension (Between Ovary-Intact and Ovariectomized Animals)
Endomysial distension refers to a distended space in the connective tissue
between the individual muscle fibres. Not surprisingly, TA muscles from OVI
animals showed significant increases in endomysial distension following both 20
and 40 LCs. This finding may be due to an increase in connective tissues in TA
muscles from OVX animals. In the aged animal, Nielsen et al. (1998) has shown
increased stiffness in the TA tendons of aged rats and better energy-absorption
(Nielsen et al., 1998). Similar to aged animals, OVX animals show increased articular
cartilage (Fontenelle et al., 2013). Thus, the increased connective tissue may allow
for greater energy absorption and possible torque transmission. The increased
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tensile stiffness in OVX animals may explain the decreased distension or stretch in
connective tissue from OVX animals.
5.5 The Cellular Stress Response Following Ovariectomy and/or Lengthening Contractions Increased levels of Hsp27 and 70 have been reported in human skeletal
muscle following high-force ‘eccentric’ exercise (Reichsman et al., 1991; Thompson
and Scordilis, 1994; Febbraio and Kokoulas, 2000; Feasson et al., 2002; Thompson
et al., 2002; Thompson et al., 2003; Willoughby et al., 2003). Whether increased Hsp
levels are indicative of the response to skeletal muscle damage or an attempt to
prepare against (protect) future stressful events is unclear. However, estrogen may
be involved in the regulation of Hsp expression following damaging exercise.
The significant decrease (57%) of constitutive expression of Hsp72 in TA
muscles from OVX animals observed in the present study is supported by other
findings. Bombardier et al. (2013) observed similar decreases in the constitutive
expression of Hsp70 in the soleus muscles from OVX animals. Sexual dimorphism of
the Hsp72 response to a variety of stressors is well-documented and following
stress the up-regulation of Hsp72 appears to be partially mediated by estrogen
interacting with the sympathetic nervous system (Nickerson, 2006). Since the
constitutive Hsp72 expression level may be necessary for skeletal muscle to mount
an immediate cellular stress response, any observed decrease in constitutive
expression of Hsp72 in OVX animals may result in a reduced ability to protect
against skeletal muscle damage. In support of this, McArdle et al. (2004) observed
mice expressing Hsp70 showed increased protection from secondary damage three
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days following LCs. McArdle et al. (2004) suggest Hsp70 might be a necessary
component of cellular repair machinery, indicating that the presence of Hsp70 may
help repair skeletal muscle more readily following LCs. This may also augment an
increased immune cell or inflammatory response following LCs. The observed
presence of an increased endomysial infiltration of immune cells in TA muscles from
OVX animals following 20 and 40 LCs supports this idea. Hsps may also function as
damage associated molecular patterns (DAMPs) that may be released from damaged
cells under necrotic conditions (Broere et al., 2011). If the constitutive expression of
Hsp72 is decreased it may result in a decreased DAMPs signal when a fibre is
damaged, thus decreasing any subsequent repair responses. Taken together, the
decrease in Hsp72 may result in a decreased capacity of OVX animals to protect
skeletal muscles against damage.
This study also observed an increased TA Hsp25 content for both OVI and
OVX animals following 40 LCs whereas only Hsp25 increased in the TA muscle from
OVX rats following 20 LCs. The lack of increase in TA muscle Hsp25 content in OVI
animals following 20 LCs suggests the stress was insufficient to warrant an Hsp
response. Conversely, the increased Hsp25 expression in OVX animals suggests
estrogen deprivation does not affect Hsp25 expression.
A ‘critical amount’ or threshold of Hsp72 has been suggested to be necessary
to provide protection (Locke and Tanguay, 1996). Thus, the decreased constitutive
expression of Hsp72 TA muscle may thereby prevent or not allow an adequate CSR
response. Thus, the decreased constitutive Hsp72 expression may lead to the loss in
the capacity to cope with the stressors of daily life. It should be noted that an
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increased number of necrotic fibres was observed in CL TA muscles from OVX
animals. Therefore, the decreased constitutive expression of TA muscle Hsp72
content in OVX animals may result in the inability to handle the stressors of
everyday life, resulting in an increased presence of necrotic fibers observed in the
CL TA muscles from OVX animals.
5.5.1 Differences in Heat Shock Protein 25 and 72 Content Following Lengthening Contractions Heat shock proteins act as protein chaperones ensuring the correct folding
refolding of damaged proteins from stressful events. Hsp72 content is known to
stabilize both the structure and function of the sarcoplasmic reticulum Ca2+ pump in
muscle subjected to heat stress (Tupling et al., 2004; Fu and Tupling, 2009). Hsp25
predominately binds to cytoskeletal/myofibrillar proteins, such as desmin, α-
actinin, actin and myosin, possibly protecting them from the stress of converting
energy through a structure (Hernado and Manso, 1997; Atomi et al., 2000; Koh and
Escobedo, 2004; Paulsen et al., 2009). In mouse models, Hsp25 has been found to
accumulate at the z-disk and within intermediate structures, (possibly desmin [Koh
and Escobedo, 2004]) following damaging eccentric exercise (Larkins et al., 2012).
In addition, some of the Hsp25 present in the ‘unstressed’ muscle fibres is localized
within the sarcolemma (Larkins et al., 2012), suggesting different functions for
Hsp25 and Hsp72. Given that Hsp25 content was over expressed in OVX animals
following 20 LCs, it underlines its potential importance in protecting skeletal muscle
from mechanical insult. These data suggest Hsp25 and Hsp72 may have different
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protective mechanisms, possibly resulting in the differences observed in expression
between Hsp25 and 72.
5.5.2 The Constitutive Heat Shock Protein 72 Expression in the Tibialis Anterior
Skeletal muscle fibre types may play a role in the observed differences for
Hsp72 content. The TA muscle is comprised primarily of type II fibres. Locke et al.
(1991) observed decreased constitutive expression of Hsp72 in the TA muscle in the
regions expressing primarily type IIB fibres. In support of this, Bombardier et al.
(2009) observed that independently of hormone treatment type II fibres showed
decreased Hsp70 expression compared to type I skeletal muscle fibres. This could
suggest that type II fibres may be subject to increased damage as any further loss of
Hsp72 content may result a decreased capacity to protect skeletal muscle following
exercise.
In aged cells and tissues a decreased Hsp content results in a decreased
protection. Vasilaki et al. (2002) observed a diminished Hsp response in the muscles
of elderly rodents. Using a transgenic Hsp70 overexpression mouse model and LCs
to induce muscle damage, McArdle et al. (2004) showed muscles from Hsp70
transgenic mice had less fibre damage when compared to wild type mice. The
decreased constitutive TA muscle Hsp72 expression observed following
ovariectomy may render the muscles from OVX animals more susceptible to usage
or stress.
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5.5.3 Heat Shock Factor 1 Content in Ovariectomized Animals
HSF1 content mediates the stress induced up-regulation of Hsps (Yasuhara et
al., 2011). Yasuhara et al. (2011) showed soleus regrowth following a four-week
recovery was partially inhibited in HSF1-null mice HSF1. Interestingly, this was not
the case for Hsp25. The presence of HSF1 content may be necessary for the up-
regulation of Hsp72 content. There may be a ‘critical level’ in the ‘baseline
expression’ of Hsps, thereby influencing the regulation of skeletal muscle mass
(Yasuhara et al., 2011). The observed difference in Hsp25 and 72 content following
20 and 40 LCs in OVI and OVX animals may be an indication of their different
regulatory mechanisms (Yasuhara et al., 2011). This suggests Hsp25 expression may
be increased by factors other than HSF1, given the lack of Hsp25 increase observed
following 20 or 40 LCs in OVI animals. The p38 mitogen-activated protein kinase
pathway is activated by stress and also plays an important role in the immune
response, as well as in the regulation of cell survival in differentiation (Cuadrado
and Nebreda, 2010). p38 is involved in the balance of protein synthesis and
degradation (Evertsson et al., 2014). p38 has been identified as a likely mediator of
catabolic signaling in skeletal muscle (Tracey, 2002) and Hsp25 is phosphorylated
through the p38 pathway (Stokoe et al., 1992). Thus, Hsp25 may function through
the p38 pathway to maintain protein integrity following muscle damage.
5.5.4 Heat Shock Protein 72 Content in Ovariectomized Animals
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In the current study, TA muscle Hsp72 content in the lengthening contracted
limb was not increased following both 20 and 40 LCs and thus OVX animals
appeared to similar to an “aged” like condition. Hsps have been shown to protect
cells and tissues, including skeletal muscle; however, tissues from aged animals
show a decreased Hsp content and therefore a diminished protection (Blake et al.,
1991; Heydari et al., 1993; Nitta et al., 1994; Locke and Tanguay, 1996). For
example, following exercise, when hearts from adult and aged animals were
examined, the hearts from aged animals showed a decreased HSF1 activation, Hsp72
content and myocardial protection (Locke and Tanguay, 1996). Whether the same
lack of protection occurs in OVX animals remains to be determined.
The stress-inducible transcription of Hsp72 and other Hsps are mediated by
HSF1 (Amin et al., 1988). In the current study, although HSF1 expression was not
significantly reduced in TA muscles from OVX animals, a decreased trend was
observed. The finding of non-significance in HSF1 content may be due to the lack of
power (n=4). Thus, it follows that if HSF1 is decreased then the ability to increase
Hsp72 content may also be attenuated. If ovariectomy (estrogen deprivation) alters
HSF1 content similar to aged cells and tissues, then ovariectomy may render the
cells and tissues more susceptible to stressors due to their decreased ability to
protect cells and tissue from damage.
Yasuhara et al. (2011) showed that in HSF-null mice, Hsp72 content was
significantly decreased when compared to wild-type mice. A similar trend of
decreased HSF1 was observed in the present study in TA muscles from OVX animals.
In view of this, skeletal muscle from OVX animals may be unable to translate the
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stress signals into the biochemical responses necessary to invoke the protective
stress response. Thus, it may be the case that a decreased CSR observed with OVX
animals may result in a decreased ability to protect skeletal muscle from LCs,
thereby increase muscle damage.
5.6 Connections to Post-Menopausal Females
These findings support the well-established fact that estrogen deprivation
results in increased body mass. In addition, females in the early phase of menopause
may not show changes in skeletal muscle performance (Sewright et al., 2008). Post-
menopausal females will experience the loss of elastic properties resulting in an
increased connective tissue stiffness. Furthermore, following a single bout of
moderate LCs (20 LCs) menopausal females may be more likely to exhibit a localized
inflammatory response, as observed by increased endomysial infiltration of immune
cells in TA muscle following both 20 and 40 LCs in OVX animals. This suggests, that
even moderate forms of exercise may result in an increased inflammatory response.
Lastly, the decreased Hsp72 content following LCs suggests that similar to aging,
menopausal females may have a decreased stress response following a single bout
of LCs. Thus, since menopausal females may have decreased cellular and tissue
protection following a single bout of mild or moderate LCs, females initially
beginning exercise should avoid excessive exercise and begin gradually until the
muscles have adapted. Given the daily stressors of life, such as stair descending
involve LCs, skeletal muscle of menopausal females may have a decreased capacity
to mount a CSR, thus decreasing muscles protection following daily activities or
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exercise. Whether this contributes to the onset, or an earlier onset of sarcopenia
remains to be determined.
5.7 Conclusions
This study observed no difference in TA muscles contractile properties
between OVI and OVX animals following both 20 and 40 LCs. An increased immune
cells presence was detected in TA muscles from OVX animals. A decreased
constitutive TA muscle Hsp72 expression in OVX animals, as well as, no elevation in
Hsp72 content in TA muscle from OVX animals following LCs was observed.
However, Hsp25 content was increased in OVX animals following 20 and 40 LCs.
This work suggests during the early phases of menopause changes to the CSR may
occur prior to contractile changes. Post-menopausal females may not be able to
mount an adequate cellular defense to a low number of LCs.
5.8 Limitations
The effects of estrogen deprivation on skeletal muscle after LCs were
examined. In the current study the period of estrogen deprivation lasted three
weeks prior to the LC procedure. Three weeks of estrogen deprivation may not have
been sufficient time to observe long-term alterations in TA muscle torque between
OVI and OVX animals. Thus, future studies should examine the effects on a longer
term of estrogen deprivation on skeletal muscle. On average, the lifespan of a rat is
approximately two years; in the current study OVX animals were estrogen-deprived
following surgical removal of the ovaries and prior to LCs for only 3 weeks. In the
life of a rodent, this time is approximately equivalent to 2.4 years of a human
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lifespan. Thus, it is possible that short-term estrogen deprivation may not
immediately cause the differences in muscle contractility, as some alterations may
take longer to develop. In view of this, long-term estrogen deprivation may be
necessary to observe significant estrogen related changed to take place/occur in
skeletal muscle torque and markers of muscle damage.
An enzyme linked immunosorbent assay was used to measure 17-β estradiol
serum concentrations. Serum 17-β estradiol concentration from OVX animals was
only reduced by ~48%. While it remains possible that estrogen was decreased. A
likely explanation for the less than half decrease in serum 17-β estradiol is the
antibodies used bound to other molecules, including the two other forms of
estrogen (i.e. estrone and estriol) or other mineralcorticoids such as testosterone
may have also bound to the epitope resulting in non-specific binding. Also,
menstruating rodents go through four phases of the estrous cycle (proestrus, estrus,
metestru and diestrus). These phases are associated with varying levels of 17-β
estradiol, with highest levels during proetsrus. Thus, non-specific binding or varying
stages of estrous may account for the levels of serum 17-β estradiol concentrations
measured in OVX animals when compared to the blood serum of OVI animals.
Although the effects of estrogen were examined in skeletal muscle
contractility and muscle damage, this study did not account for the effect of
progesterone on skeletal muscle. Progesterone concentrations were not measured
and thus, the effect of circulating progesterone on skeletal muscle cannot be
accounted for in the current study. Whether the removal of estrogen was
compensated by an increase in progesterone remains unlikely.
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Since morphology was only examined 24 hours after LCs it is not possible to
determine the role of estrogen plays in endomysial infiltration in the days following
LCs and thus the role of estrogen in skeletal muscle recovery cannot be examined. In
addition, when skeletal muscles were examined the investigator was not blinded,
potentially resulting in some bias in measurements. Lastly, this study examined
medial sections of skeletal muscle by Western blotting. Thus, it is not possible to
determine if the Hsp response observed was localized to that area of the skeletal
muscle or throughout the entire muscle.
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Chapter VI: References Abbasi A, Duthie Jr. EH, Sheldahl L, Wilson C, Sasse E, Rudman I and Mattson DE
(1998). Association of dehydroepiandrosterone sulfate, body composition, and physical fitness in independent community-dwelling older men and women. Journal of American Geriatrics Society, 46, 263-273.
Aizawa K, Iemitsu M, Otsuki T, Maeda S, Miyauchi T and Mesaki N (2008). Sex differences in steroidogenesis in skeletal muscle following a single bout of exercise in rats. Journal of Applied Physiology, 104, 67–74.
Agarkova I, Schoenauer R, Ehler E, Carlsson L, Carlsson E, Thornell LE and Perriard JC (2004). The molecular composition of the sarcomeric m-band correlates with muscle fiber type. European Journal of Cell Biology, 83, 193–204. Aloia JF, McGowan DM, Vaswani AN, Ross P and Cohn SH (1991). Relationship of
menopause to skeletal and muscle mass. American Journal of Clinical Nutrition, 53, 1378-1383.
Aloia JF, Vaswani A, Russo L, Sheehan M and Flaster E (1995). The influence of menopause and hormonal replacement therapy on body cell mass and body fat mass. American Journal of Obstetrics Gynecology, 172, 896– 900.
Amelink GJ and Bar PR (1986). Exercise-induced muscle protein leakage in the rat: effects of hormonal manipulation. Journal of Neurological Science, 76, 61–68.
Amelink GJ, Koot RW, Erich WB, Van Gijn J and Bar PR (1990). Sex-linked variation in creatine kinase release, and its dependence on oestradiol, can be demonstrated in an in-vitro rat skeletal muscle preparation. Acta Physiologica Scandinavia, 138, 115–124.
Amin J, Anathan J and Voellmy R (1988). Key features of heat shock regulatory elements. Molecular Cellular Biology, 8, 3761-3769.
Angstwurm MW, Gartner R and Ziegler-Heitbrock HW (1997). Cyclic plasma IL-6 levels during normal menstrual cycle. Cytokine, 9, 370–374.
Astwood EB (1939). Changes in the weight and water content of the uterus of the normal adult rat. American Journal of Physiology, 126, 162-170.
Atomi Y, Toro K, Masuda T and Hatta H (2000). Fiber-type-specific alphaB-crystallin distribution and its shifts with T(3) and PTU treatments in rat hindlimb muscles. Journal of Applied Physiology, 88, 1355–1364.
Bar PR and Amelink GJ (1997). Protection against muscle damage exerted by oestrogen: hormonal or antioxidant action? Biochemical Society Transcripts, 25, 50-54.
Bar PR, Amelink GJ, Oldenburg B and Balnkenstein MA (1988). Prevention of Exercise induced muscle membrane damage by oestradiol. Life Sciences, 42, 2677–2681.
Bar PR, Dressen M, Rikken B et al. (1985). Muscle protein leakage after strenuous exercise: sex and chronological differences. Neuroscience Letters, 22, S288.
Bauer JM and Sieber CC (2008). Sarcopenia and frailty: a clinician’s controversial
106
point of view. Experimental Gerontology, 43, 674 – 680. Brinkmeier H and Ohlendieck K. (2014). Chaperoning heat shock proteins:
Proteomic analysis and relevance for normal and dystrophin-deficient muscle. Proteomics. Clinical Applications, 1–67.
Barp J, Araujo AS, Fernandes TR, Rigatto KV, Llesuy S, Bello-Klein A and Singal P (2002). Myocardial antioxidant and oxidative stress changes due to sex hormones. Brazilian Journal of Medical and Biological Research, 35, 1075-1081.
Barrett-Connor E (1993). Estrogen and estrogen-progestogen replacement: therapy and cardiovascular diseases. American Journal of Medicine, 95, 40S-43S.
Baumgartner RN, Waters DL, Gallagher D, Morley JE and Garry PJ (1999). Predictors of skeletal muscle mass in elderly men and women. Mechanism of Ageing and
Development, 107, 123-136. Beaton LJ, Tarnopolsky MA and Phillips SM (2002). Contraction-induced muscle damage in humans following calcium channel blocker administration. Journal
of Physiology, 544, 849–859. Behl C, Skutella T, Lezoualch F, Post A, Widmann M, Newton CJ and Holsboer F
(1997). Neuroprotection against oxidative stress by estrogens: structure-activity relationship. Molecular Pharmacology, 51, 535–541.
Bidmon B, Endemann M, Arbeiter K, Ruffingshofer D, Regele H, Herkner K, Eickelberg O and Aufricht C (2004). Overexpression of HSP-72 confers cytoprotection in experimental peritoneal dialysis. Kidney International, 66, 2300-2307.
Blake MJ, Udelsman R, Feulner GJ, Norton DD and Holbrook NJ (1991). Stress induced heat shock protein 70 expression in adrenal cortex: an adrenocorticotropic hormone-sensitive, age-dependent response. PNAS, 88, 9873-9877.
Bombardier E, Vigna C, Bloemberg D, Quadrilatero J, Tiidus PM and Tupling AR (2013). The role of estrogen receptor-α in estrogen-mediated regulaition of basal and exercise-induced Hsp70 and Hsp27 expression in rat soleus. Canadian Journal of Physiological Pharmacology, 91, 823-829.
Bombardier E, Vagna C, Iqbal SP, Tiidus PM and Tupling AR (2009), Effects of ovarian sex hormones and downhill running on fiber type-specific Hsp70 expression in the rat soleus. Journal of Applied Physiology, 106, 2009-2015.
Brinton RD (2004). Impact of estrogen therapy on Alzheimer’s disease: fork in the road? CNS Drugs, 18, 405-422.
roere F, van der Zee R and van Eden (2011). Heat shock proteins are no DAMPs, rather ‘dampers’. Nature Review Immunology, Correspondence.
Brooks SV, Zerba E and Faulkner JA (1995). Injury to muscle fibre after single stretches of passive and maximally stimulated muscles in mice. Journal of Physiology, 2, 459-469.
Bunratsami S, Wandee U, Kumarnsit E, Vongvatcharanon S and Vongvatcharanon U (2015). Estrogen replacement improves skeletal muscle performance by increasing parvalbumin levels in ovariectomized rats. Acta Histochemica, 117, 163-175.
107
Cannon JG, Orencole SF, Fielding RA, Meydani M, Meydani SN, Fiatarone MA, Blumberg JB and Evans WJ (1990). Acute phase response in exercise: interaction of age and vitamin E on neutrophils and muscle enzyme release. American Journal of Physiology, 259, R1214-R1219.
Carr MC (2003). The emergence of the metabolic syndrome with menopause. Journal of Clinical Endocrinology and Metabolism, 88, 2404-2411.
Carter A, Dobridge J and Hackney AC (2001). Influence of estrogen on markers of muscle tissue damage following eccentric exercise. Human Physiology, 27, 626-630.
Caston Al, Farrell PA and Deaver DR (1995). Exercise training-induced changes in anterior pituitary gonadotrope of the female rats. Journal of Applied Physiology, 79, 194-201.
Chen Y, Arrigo AP and Currie RW (2004a). Heat shock treatment suppresses angiotensin II induced activation of NF-kappaB pathway and heart inflammation: a role for IKK depletion by heat shock? American Journal of Physiology and Heart Circulation Physiology, 287, H1104-H1114.
Chen Y and Currie RW (2006). Small interfering RNA knocks down heat shock factor-1 (HSF-1) and exacerbates pro-inflammatory activation of NF-kappaB and AP-1 in vascular smooth muscle cells. Cardiovascular Research, 69, 66-75.
Chen Y, Ross BM and Currie RW (2004b), Heat shock treatment protects against angiotensin II-induced hypertension and inflammation in aorta. Cell Stress Chaperones, 9, 99-107.
Chennaoui M, Gomez Merino D, Lesage J, Drogou C and Guezennec CY (2002). Effects of moderate and intensive training on the hypothalamic-pituitary-adrenal axis in rats. Acta Physiologica Scandinavia, 175, 279-286.
Chiang HL, Trelecky SR, Plant CP and Dice JF. (1982). A role for a 70-kiladalton heat shock protein in lysosomal degradation of intracellular proteins. Science, 246, 382-385.
Choi SJ (2014). Differential susceptibility of myosin heavy chain isoform following eccentric-induced muscle damage. Journal of Exercise Rehabilitation, 10, 344-348.
Chowdhury S and Pickering LM (2006). Ellis PA Adjuvant aromatase inhibitors and bone health. Journal of British Menopause Society, 12, 97–103.
Christgau STL, CLOOS PAC, Mouritzen U, Christiansen CMD, Delaissé JM and Hoegh Anderson P (2004). Suppression of elevated cartilage turnover in postmenopausal women and ovariectomized animals by estrogen and selective estrogen receptor modulator (SERM). Menopause, 11, 508–518.
Christians ESP, Yan L-JP and Benjamin IJMD (2002) Heat shock factor 1 and heat shock proteins: Critical partners in protection against acute cell injury. [Review]. Critical Care Medicine, 30, S43–S50.
Clarkson PM and Hubal MJ (2001). Are women less susceptible to exercise-induced muscle damage? Clinical Nutrition and Metabolic Care, 4, 527-531. Clarkson PM and Sayers SP (1999). Etiology of exercise-induced muscle damage.
Canadian Journal of Applied Physiology, 24, 234–248. Cohen DS, Palmer E, Welch WJ and Sheppard D. (1991). The response of guinea pig
108
airway epithelia cells and alveolar macrophages to environmental stress. American Journal of Respiratory Cellular Molecular Biology, 5, 13-143.
Cuadrado A and Nebreda AR (2010). Mechanisms and functions of p38 MAPK signaling. Journal of Biochemistry, 429, 403-417.
Degens H and Always S (2003). Skeletal muscle function and hypertrophy are diminished in old age. Muscle and Nerve, 27, 339-347.
Dionne IJ, Kinaman KA and Poehlman ET (2000). Sarcopenia and muscle function during menopause and hormone-replacement therapy. Journal of Nutritional Health and Aging, 4, 156–161.
Douchi T, Yamamoto S, Nakamura S, Ijuin T, Oki T, Maruta K and Nagata Y (1998). The effects of menopause on regional and total body lean mass. Maturitas, 29, 247-252.
Douchi T, Yamamoto S, Yoshimitsu N, Andoh T, Matsuo T and Nagata Y (2002). Relative contribution of aging and menopause to changes in lean and fat mass in segmental regions. Maturitas, 42, 301-306.
Ellis RJ and Heart FU (1996). Protein folding in the cell: competing models of chaperoning function. FASEB Journal, 10, 20–26.
Enns DL and Tiidus PM (2010). The influence of estrogen on skeletal muscle. Sports Medicine, 40, 41-58.
Evans WJ, Meredith CN, Cannon JG, Dinarello CA, Frontera WR, Hughes VA, Jones BH and Knuttgen HG. (1985). Metabolic changes following eccentric exercise in trained and untrained men. Journal of Applied Physiology, 61, 1864-1868.
Evertsson K, Fjällström AK, Norrby M and Tågerud S (2014). P38 mitogen-activated protein kinase and mitgen-activated protein kinase-activated protein kinase 2 (MK2) signaling in atrophic and hypertrophic denervated mouse skeletal muscle. Journal of Molecular Signaling, 9, 2-13.
Feasson L, Stockholm D, Freyssenet D, Richard I, Duguez S, Beckmann JS and Denis C (2002). Molecular adaptations of neuromuscular disease-associated proteins in response to eccentric exercise in human skeletal muscle. Journal of Physiology, 543, 297–306.
Febbraio MA and Koukoulas I (2000). HSP72 gene expression progressively increases in human skeletal muscle during prolonged, exhaustive exercise. Journal of Applied Physiology, 89, 1055–1060.
Febbraio MA, Steensberg A, Walsh R, Koukoulas I, van Hall G, Stalin B and Pedersen BK (2002). Reduced glycogen availability is associated with an elevation in HSP72 in contracting human skeletal muscle. The Journal of Physiology, 538, 911-917.
Feng X, Li GZ and Wang S (2004). Effects of estrogen on gastrocnemius muscle strain injury and regeneration in female rats. Acta Pharmacologica Singapore, 25, 1489–1494.
Fisher JS, Hasser EM and Brown M (1998). Effects of ovariectomy and hind-limb unloading on skeletal muscle. Journal of Applied Physiology, 85, 1316–1321.
Fontenelle RG, Mariotto VB, Vazzoleré AM, Ferrão JSP, Junior JRK and De Souza RR (2013). Menopause, exercise, and knee. What happens? Microscopy Research and Technique, 76, 381-387.
Fitts RH (1994). Cellular mechanisms of muscle fatigue. Physiological Reviews, 74, 49
109
94. Fridén J and Lieber RL (1992). The structural and mechanical basis of exercise
induced muscle injury. Medicine and Science in Sport and Exercise, 24, 521-530.
Fridén J, Sjostrom M and Ekblom B (1983). Myofibrillar damage following intense eccentric exercise in man. International Journal of Sports Medicine, 4, 170–176.
Friden J, Sjostrom M and Ekblom B (1983). Myofibrillar damage following intense eccentric exercise in man. International Journal of Sports Medicine, 4, 170–176.
Fu MH and Tupling AR (2009). Protective effects of Hsp70 on the structure and function of SERCA2a expressed in HEK-293 cells during heat stress. American Journal of Physiology Heart Circulation Physiology, 296, H1175–H1183.
Gabai VL, Meriin AB, Yaglom JA, Volloch VZ and Sherman MY (1998). Role of Hsp70 in regulation of stress-kinase JNK: implications in apoptosis and aging. FEBS Letters, 438, 1-4.
Gambacciani M, Ciaponi M, Cappagli B, Benussi C, De Simone L and Genazzani AR (1999). Climacteric modifications in body weight and fat tissue distribution. Climacteric, 2, 37-44.
Garcia-Segura LM, Azcoitia I and Don Carlos LL (2001). Neuroprotection by estradiol. Progress in Neurology, 63, 29-60.
Gill SS and Tuteja N (2010). Reactive oxygen species and antioxidant machinery in abiotic stress tolerance in crop plants. Plant Physiology and Biochemistry, 48, 909-930.
Gillum TL (2010). Sex differences in heat shock protein 72 expression and inflammatory response to acute exercise in the heat. Thesis Dissertation.
Gonzalez B, Hernando R and Manso R (2000). Stress proteins of 70 kDa in chronically exercised skeletal muscle. Pflugers Archives, 440, 42–49.
Greeves JP, Cable NT, Luckas ML, Reilly T and Biljan MM (1997). Effects of acute changes in oestrogen on muscle function of the first dorsal interosseus muscle in humans. Journal of Physiology, 500, 265–270.
Greeves JP, Cable NT, Reilly T and Kingsland C (1999). Changes in muscle strength in women following the menopause: a longitudinal assessment of the efficacy of hormone replacement therapy. Clinical Science (London), 97, 79–84.
Haizlip KM, Harrison and Leinwand LA (2015). Sex-based differences in skeletal muscle kinetics and fibre-type composition. Physiology, 30, 30-39.
Hamilton KL, Gupta S and Knowlton AA (2004). Estrogen and regulation of heat shock protein expression in female cardiomyocytes: cross-talk with NF kappa B signaling. Journal of Molecular Cell Cardiology, 36, 577-584.
Haslbeck M and Viering E (2015). A first line of stress defense: small heat shock proteins and their function in protein homeostasis. Journal of Molecular Biology, 427, 1537-1548.
Hatae J (2001). Effects of 17beta-estradiol on tension responses and fatigue in the skeletal twitch muscle fibers of frog. Japanese Journal of Physiology, 51, 753
759. Hernando R and Manso R (1997). Muscle fibre stress in response to exercise:
110
synthesis, accumulation and isoform transactions of 70 kDa heat shock proteins. European Journal of Biochemistry, 243, 460–467.
Heydari AR, Wu B, Takahashi R, Strong R and Richardson A (1993). Expression of heat shock protein 70 is altered by age and diet at the level of transcription. Molecular Cell Biology, 13, 2909-2918.
Heydari AR, You S, Takahashi R, Gutsmann-Conrad A, Sarge KD and Richardson A (2000). Age related alterations in the activation of heat shock transcription factor 1 in rat hepatocytes. Experimental Cell Research, 256, 83–93.
Holwerda A and Locke M (2014). Hsp25 and Hsp72 content in rat skeletal muscle following controlled shortening and lengthening contractions. Journal of Applied Physiology, Nutrition and Metabolism, 39, 1-8.
Hochstrasser M (1992). Ubiquitin and intracellular protein degradation. Current Opinion in Cellular Biology, 4, 1024–1031.
Honda H, Kimura H and Rostami A (1990). Demonstration and phenotypic characterization of resident macrophages in rat skeletal muscle. Immunology, 70, 272-277.
Hubal, ML, Ingalls CP, Allen MR, Wenkw JC, Hogan HA and Bloomfield SA (2005). Effects of eccentric exercise training on cortical bone and muscle strength in estrogen-deficient mice. Journal of Applied Physiology, 98, 1674-1681.
Iqbal S, Thomas A, Bunyan K and Tiidus PM (2008). Progesterone and estrogen influence postexercise leukocyte infiltration in overiectomized female rats. Applied Physiology: Nutrition and Metabolism, 33, 1207–1212.
Ingalls CP, Warren GL and Armstrong RB (1998). Dissociation of force production from MHC and actin contents in muscles injured by eccentric contractions. Journal of Muscle Research and Cell Motility, 19, 215-224.
Jarow JP, Kirkland J, Koritnik DR and Cefalu WT (1993). Effect of obesity and fertility status on sex steroid levels in men. Urology, 42, 171-174.
Jazbutyte V, Hu K, Kruchten P, Bey E, Maier SK, Fritzemeier KH, Prelle K, Hegele Hartung C, Hartmann RW, Neyses L, Ertl G and Pelzer T (2006). Aging reduces the efficacy of estrogen substitution to attenuate cardiac hypertrophy in female spontaneously hypertensive rats. Hypertension, 48, 579–586.
Jia J, Guan D, Zhu W, Alkayed NJ, Wang MM, Hua Z and Xu Y (2008). Estrogen inhibits Fas-mediated apoptosis in experimental stroke. Experimental Neurology, 215, 48–52.
Jones DA (1996). High-and low-frequency fatigue revisited. Acta Physiological Scandinavia, 156, 265-270.
Jones DA, Newham DJ and Torgan C (1989). Mechanical influences on long-lasting human muscle fatigue and delayed-onset pain. Journal of Physiology, 412, 415-427.
Jubrias SA, Odderson IR, Esselman PC and Conley KE (1997). Decline in isokinetic force with age: muscle cross-sectional area and specific force. Pflugers Archives, 434, 246-253.
Khassaf M, Child RB, McArdle A, Brodie DA, Esanu C and Jackson MJ (2001). Time course of response of human skeletal muscle to oxidative stress induced by nondamaging exercise. Journal of Applied Physiology, 90, 1031-1035.
111
Kendall B and Eston R (2002). Exercise-induced muscle damage and the potential protective role of estrogen. Sports Medicine, 32, 103–123.
Kingston RE, Schuetz TJ and Larin Z (1987). Heat-inducible human factor that binds to a human hsp70 promoter. Molecular Cellular Biology, 7, 1530–1534.
Kim D, Ouyang H and Li GC (1995). Heat shock protein hsp70 accelerates the recovery of heat-shocked mammalian cells through its modulation of heat shock transcription factor HSF1. Proceedings of the National Academy of Science USA 92, 2126–2130.
Kirilovas D, Schedvins K, Naessén T, Von Schoultz B and Carlström K (2007). Conversion of circulating estrone sulfate to 17beta-estradiol by ovarian tumor tissue: a possible mechanism behind elevated circulating concentrations of 17beta-estradiol in postmenopausal women with ovarian tumors. Gynecological Endocrinology, 23, 25–8.
Kjaer M (2004). Role of extracellular matrix in adaptation of tendon and skeletal muscle to mechanical loading. Physiology Review, 84, 649–698.
Knowlton AA (1995). The role of heat shock proteins in the heart. Journal of Molecular Cell Cardiology, 27, 121–131.
Koh T J (2002). Do small heat shock proteins protect skeletal muscle from injury? Exercise and Sport Sciences Reviews, 30, 117–121.
Koh TJ (2004). Cytoskeleton disruption and small heat shock protein translocation immediately after lengthening contractions. American Journal of Physiology: Cell Physiology, 286, 713C-722.
Koh TJ and Escobedo J (2004). Cytoskeletal disruption and small heat shock protein translocation immediately after lengthening contractions. American Journal of Physiology and Cell Physiology, 286, C713–C722.
Komi PV (2000). Stretch-shortening cycle: a powerful model to study normal and fatigued muscle. Journal of Biomechanics, 33, 1197−1206.
Komulainen J, Koskinen SO, Kalliokoski R, Takala TE and Vihro V (1999). Gender differences in skeletal muscle fibre damage after eccentrically biased downhill running in rats. Acta Physiologica Scandinavia, 165, 57–63.
Komulainen J, Takala TES, Kuipers H and Hesselink MKC (1998). The disruption of myofibre structures in rat skeletal muscle after forced lengthening contractions. Journal of European Physiology, 436, 735-741.
Labbadia J and Morimoto RI (2015). The biology of proteostasis in aging and disease. Annual Review of Biochemistry, 84, 435-464.
Laemmli UK (1970). Cleavage of structural proteins during the assembly of the head of bacteriophage T4. Nature, 227, 680-685.
Lai S, Collins BC, Colson BA, Karaigas G and Lowe DA (2016). Estradiol modulates myosin regulatory light chain phosphorylation and contractility in skeletal muscle. American Journal of Physiology, Endocrinology, and Metabolism, 310, E724-E733.
Landry J, Bernier D, Chrétien P, Nicole LM, Tanguay RM and Marceau N (1982). Synthesis and degradation of heat shock proteins during development and decay of thermotolerance. Cancer Research, 42, 2457-2461.
Larkins NT, Murphy RM and Lamb GD (2012). Absolute amounts and diffusibility of
112
Hsp72, Hsp25, and αB-crystallin in fast- and slow-twitch skeletal muscle fibres of rat. American Journal of Physiology and Cell Physiology, 302, C228-C239.
Lee YK, Liu DJ, Lu J, Chen KY, Liu AYC (2009). Aberrant regulation and modification of heat shock factor 1 in senescent human diploid fibroblasts. Journal of Cellular Biochemistry, 106, 267–278.
Lindquist S and Craig EA (1988). The heat shock protein. Annual Review of Genetics, 22, 631-677. Lindstedt SL, LaStayo PC and Reich TE (2001). When Active Muscles Lengthen:
Properties and Consequences of Eccentric Contractions. News in Physiological Science, 16, 256-261.
Liu Y, Lormes W, Baur C, Baur S, Steinacker JM and Lehmann M (1999). Human HSP 70 response to training is not dependent on exercise volume. International Journal of Sports Medicine, 20 (Suppl 1): S53
Liu Y and Steinacker, JM (2001). Changes in skeletal muscle heat shock proteins: pathological significance. Frontiers in Bioscience, 6, 12–25.
Locke M, Noble EG and Atkinson BG (1990). Exercising mammals synthesize stress proteins. American Journal of Physiology and Cell Physiology, 258, C723–C729.
Locke M, Noble EG and Atkison BG. (1991). Inducible isoform of HSP70 is Constitutively expressed in a muscle fiber type specific pattern. American Journal of Physiology, Cellular Physiology, 261, C774-C779.
Locke M and Tanguay RM (1996). Diminished heat shock response in the aged myocardium. Cell Stress and Chaperones, 1, 251-260.
Lowry OH, Rosenbrough NJ, Farr AL and Randall RJ (1951). Protein measurement with the folin phenol reagent. Journal of Biological Chemistry, 193, 265-275.
Lutsch G, Vetter R, Offhauss U, Wieske M, Gröne H-J, Klemenz R, Schimke I, Stahl J and Benndorf (1997). Abundance and location of small heat shock proteins HSP25 and αβ-crystallin in rat and human heart. Circulation, 96, 3466-3476.
Lynch NA, Ryan AS, Berman DM, Sorkin JD and Nicklas BJ (2002). Comparison of VO2max and disease risk factors between perimenopausal and postmenopausal women. Menopause, 9, 456-462.
MacIntyre DL, Reid WD, Lyster DM, Szasz IJ and McKenzie DC (1996). Presence of WBC, decreased strength, and delayed soreness in muscle after eccentric exercise. Journal of Applied Physiology, 80, 1006-1013.
MacIntyre DL, Reid WD, Lyster DM and McKenzie DC (2000). Different effects of strenuous eccentric exercise on the accumulation of neutrophils in muscle in women and men. European Journal of Applied Physiology, 81, 47-53.
MacIntyre DL, Reid WD and McKenzie DC (1995). Delayed muscle soreness: the inflammatory response to muscle injury and its clinical implications. Journal of Sports Medicine, 20, 24-40.
Malm C, Nyberg P, Engstrom M, Sjodin B, Lenkei R, Ekblom B and Lundberg I (2000). Immunological changes in human skeletal muscle and blood after eccentric exercise and multiple biopsies. Journal of Physiology, 529, Pt 1, 243-262.
Maltais ML, Desroches J and Dionne IJ (2009). Changes in muscle mass and strength after menopause. Journal of Musculoskeletal Neuronal Interaction, 9, 186-197.
113
Marber MS, Mestril R, Chi SH, Sayen MR, Yellon DM and Dillmann WH (1995). Overexpression of the rat inducible 70-kDa heat stress protein in transgenic mouse increases the resistance of the heart to ischemic injury. Journal of Clinical Investigation, 18, 355-357.
Martinez-Azorin F, Teruel JA, Fernandez-Belda F and Gomez-Fernandez JC (1992). Effect of diethystilbestrol and related compounds on the Ca21-transportingATPase of the sarcoplasmic reticulum. Journal of Biology and Chemistry, 267, 11923–11929.
Massimino ML, Rapizzi E, Cantini M, Libera LD, Mazzoleni F, Arslan P and Carraro U (1997). ED2+ macrophages increase selectively myoblast proliferation in muscle cultures. Biochemical Biophysiology Research Communication, 235, 754–759.
Matson A, Konow N, Miller S, Konow PP and Roberts TJ (2012). Tendon material properties vary and are interdependent among turkey hindlimb muscles. Journal of Experimental Biology, 215, 3552-3558.
Mattson JP, Ross CR, Kilgore JL and Musch TI (2000). Induction of mitochondrial stress proteins following treadmill running. Medicine Science and Sports Exercise, 32, 365–369.
McArdle A, Dillmann WH, Mestril R, Faulkner JA and Jackson MJ (2004). Overexpression of Hsp70 in mouse skeletal muscle protects against muscle damage and age-related muscle dysfunction. FASEB Journal, 18, 355-370.
McArdle A, Pattwell D, Vasilaki A, Griffiths RD and Jackson MJ (2001). Contractile activity-induced oxidative stress: cellular origin and adaptive responses. American Journal of Physiology and Cell Physiology, 280, C621–C627.
McClung JM, Davis JM and Carson JA (2007). Ovarian hormone status and skeletal muscle inflammation during recovery from disuse atrophy. Experimental Physiology, 92, 219-232.
McCormick KM, Burns KL, Piccone CM, Gosselin Le and Brazeau GA (2004). Effects of ovariectomy and estrogen on skeletal muscle function in growing rats. Journal of Muscle Research and Cell Motility, 25, 21–27.
McCully KK and Faulkner JA (1985). Injury to skeletal muscle fibres of mice following lengthening contractions. Journal of Applied Physiology, 59, 119-126.
McEwen BS and Alves SE (1999). Estrogen actions in the central nervous system. Endocrine Reviews, 20, 279–307.
McNulty PH, Jagasia D, Whiting JM and Caulin-Glaser T (2000). Effect of 6-wk estrogen withdrawal or replacement on myocardial ischemic tolerance in rats. American Journal of Physiology and Heart Circulatory Physiology, 278, H1030–H1034.
Meeuwsen IB, Samson MM and Verhaa HJ (2000). Evaluation of the applicability of HRT as a preservative of muscle strength in women. Maturitas, 36, 49–61.
Mendelsohn ME and Karas RH (1999). The protective effects of estrogen on the cardiovascular system. The New England Journal of Medicine, 340, 1801-1811.
Messier V, Rabasa-Lhoret R, Barbat-Artigas S, Elisha B, Karelis AD, Aubertin- Leheudre M (2011). Menopause and sarcopenia. A potential role for sex
114
hormones. Maturitas, 68, 331-336. Milne KJ and Noble EG (2002). Exercise-induced elevation of HSP70 is intensity
dependent. Journal of Applied Physiology, 93, 561–568. Miyabara EH, Nascimento TL and Rodrigues DC (2012). Overexpression of inducible
70kDA heat shock protein in mouse improves structural and functional recovery of skeletal muscle from atrophy. Pflugers Archives, 463, 733-741.
Moran AL, Nelson SA, Landisch RM, Warren GL and Lowe DA (2007). Estradiol replacement reverses ovariectomy-induced muscle contractile and myosin dysfunction in mature female mice. Journal of Applied Physiology, 102, 1387–1393.
Moran AL, Warren GL and Lowe DA (2006). Removal of ovarian hormones from mature mice detrimentally affects muscle contractile function and myosin structural distribution. Journal of Applied Physiology, 100, 548–559.
Morgan DL (1990). New insights into the behavior of muscle during active lengthening. Biophysical Journal, 57, 209–221.
Morgan DL and Allen DG (1999). Early events in stretch-induced muscle damage. Journal of Applied Physiology, 87, 2007-2015.
Morgan DL and Poske U (2004). Popping sarcomere hypothesis explains stretch induced muscle damage. Clinical and Experimental Phramacology and Physiology, 31, 541-545.
Morton JP (2006). Time course and differential responses of the major heat shock protein families in human skeletal muscle following acute nondamaging treadmill exercise. Journal of Applied Physiology, 101, 176-182.
Morton JP, Holloway K, Woods P, Cable NT, Burniston J, Evans L, Kayani AC and McArdle A (2009). Exercise training-induced gender-specific heat shock protein adaptations in human skeletal muscle. Muscle & Nerve, 39, 230-233.
Mosser DD, Duchaine J and Massie B (1993). The DNA-binding activity of the human heat shock transcription factor is regulated in vivo by hsp70. Molecular Cellular Biology, 13, 5427–5438.
Mosser DD and Morimoto RI (2000) Molecular chaperones and the stress of oncogenesis. Oncogene, 23, 2907–2918
Naito H, Powers SK, Demirel HA and Aoki J (2000). Exercise training increases hea shock protein in skeletal muscles of old rats. Medicine Science and Sports Exercise, 33, 729–734.
Nedergaard A, Henriksen K, Karsdal MA and Christiansen C (2013). Menopause, estrogens and frailty. Gynecological Endocrinology, 29, 418-423.
Nielsen HM, Skalicky M and Viidik A (1998). Influence of physical exercise on aging rats. III. Life-long exercise modifies the aging changes of the mechanical properties of limb muscle tendons. Mechanisms of Ageing and Development, 100, 243–260
Nelson LR and Bulun SE (2001). Estrogen production and action. Journal of American Academy Dermatology, 45(3 Suppl), S116–S124.
Newham DJ, Jones DA and Clarkson PM (1987). Repeated high-force eccentric exercise: effects on muscle pain and damage. Journal of Applied Physiology, 63, 1381-1386.
Newham DJ, Mills KR, Quigley EM and Edwards RH (1983). Pain and fatigue after
115
concentric and eccentric muscle contractions. Clinical Science (London), 64, 55-62.
Nickerson M, Kennedy SL, Johnson JD and Fishner M (2006). Sexual dimorphism of the intracellular heat shock protein 72 response. Journal of Applied Physiology, 101, 566-575.
Nitta Y, Abe K, Aoki M, Ohno I and Isoyama S (1994). Diminished heat shock protein 70 mRNA induction in aged rat skeletal muscles after ischemia. American Journal of Physiology, 267 (Skeletal Muscle and Circulatory and Physiology 36), H1795-H1803.
Noble EG (2002). Heat shock proteins and their induction with exercise. In: Exercise and Stress Response: Role of Stress Proteins. (eds. M. Locke and E.G. Noble). CRC Press. Boca Raton, Florida. pp. 43–78.
Noble EG, Milne KJ and Melling CWJ (2008). Heat shock proteins and exercise: a primer. Applied Physiology, Nutrition, and Metabolism, 33, 1050-1065.
Nosaka K, Clarkson PM, McGuiggin and Byrne JM (1991). Time course of muscle adaptation after high force eccentric exercise. Journal of Applied Physiology, 63, 70-76.
Ogata T, Oishi Y, Roy RR and Ohmori H (2005). Effects of T3 treatment on HSP72 and calcineurin content of functionally overloaded rat plantaris muscle. Biochemical and Biophysical Research Communications, 331, 1317–1323.
Oishi Y, Ogata T, Ohira Y, Taniguchi K and Roy RR (2005). Calcineurin and heat shock protein 72 in functionally overloaded rat plantaris muscle. Biochemical and Biophysical Research Communications, 330, 706–713.
O'Neill DET, Aubrey FK, Zeldin DA, Michel RN, and Noble EG (2006). Slower skeletal muscle phenotypes are critical for constitutive expression of Hsp70 in overloaded rat plantaris muscle. Journal of Applied Physiology, 100, 981–987.
Overgaard K, Fredsted A, Hyldal A, Ingemann-Hansen T, Gissel H and Clausen T (2004). Effects of running distance and training on Ca2+ content and damage in human muscle. Medicine and Science in Sports and Exercise, 36, 821-829.
Overgaard K, Lindstrom T, Ingemann-Hansen T and Clausen T (2002). Membrane leakage and increased content of Na+ -K+ pumps and Ca2+ in human muscle after a 100-km run. Journal of Applied Physiology, 92, 1891-1898.
Pantopoulos K, Weiss G and Hentze (1996). Nirtic oxide and oxidative stress (H2O2) control mammalian iron metabolism by different pathways. Molecular and cellular Biology, 16, 3781-3788.
Paroo Z, Dipchand ES and Noble EG (2002). Estrogen attenuates postexercise Hsp70 expression in skeletal muscle. American Journal of Physiology and Cellular Physiology, 282, 245-251.
Paroo Z, Tiidus PM and Noble EG (1999). Estrogen attenuates Hsp72 expression in acutely exercised male rodents. European Journal of Applied Occupational Physiology, 80, 180-184.
Paulsen G, Lauritzen F, Bayer ML, Kalhovde JM, Ugelstad I, Owe SG, Hallen J, Bergersen LH and Raastad T. (2009). Subceullar movement and expression of HSP27, B-crystallin, and HSP70 after two bouts of eccentric exercise in humans. Journal of Applied Physiology, 107, 570-582.
Paulsen G, Vissing K, Kalhovde JM, Ugelstad I, Bayer ML, Kadi F, Schjerling P, Hallen
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J and Raastad T (2007). Maximal eccentric exercise induces a rapid accumulation of small heat shock proteins on myofibrils and a delayed HSP70 response in humans. American Journal of Physiology: Regulatory, Integrative and Comparative Physiology, 293, R844–R853.
Peake J, Nosaka K and Suzuki K (2005). Characterization of inflammatory responses to eccentric exercise in humans. Exercise Immunology Review, 11, 64-85.
Persky AM, Green PS, Stubley L, Howell CO, Zaulyanov L, Brazeau GA and Simpkins JW (2000). Protective effect of estrogens against oxidative damage to heart and skeletal muscle in vivo and in vitro. Proceedings for the Society of Experimental Biology and Medicine, 223, 59–66.
Phillips SK, Rook KM, Siddle NC, Bruce SA and Woldedge RC (1993). Muscle weakness in women occurs at an earlier age than in men, but strength is preserved with hormone replacement therapy. Journal of Clinical Science (London), 84, 95-98.
Piccone CM, Brazeau GA and McCormick KM (2004). Effect of oestrogen on myofibre size and myosin expression in growing rats. Experimental Physiology, 90, 87–93.
Pinilla L, Garnelo P, Gaytan F and Aguilar E (1992). Hypothalamic-pituitary function in neonatally oestrogen-treated male rats. Journal of Endocrinology, 134, 279-286.
Pizza FX, Mitchell JB, Davis, Starling RD, Holtz RW and Bigelow N (1995). Exercise induced muscle damage: effect on circulating leukocyte and lymphocyte subsets. Medicine and Science in Sports and Exercise, 27, 363-370.
Poehlman ET and Tchernof A (1998). Traversing the menopause: changes in energy expenditure and body composition. Coronary Artery Disease, 9, 799-803.
Poehlman ET, Toth MJ, Fishman PS, Vaitkevicius P, Gottlieb SS, Fisher ML and Fonong T (1995). Sarcopenia in aging humans: the impact of menopause and disease. Journal of Gerontology A: Biological Sciences and Medical Science, 50, 73–77.
Pollock-Tahiri E and Locke M (2016). Heat shock proteins as markers of contraction-induced muscle damage. FASEB Journal, 30, 769.5.
Prado LG, Makarenko I, Andresen C, Kruger M, Opitz CA and Linke WA (2005). Isoform diversity of giant proteins in relation to passive and active contractile properties of rabbit skeletal muscles. Journal of General Physiology, 126, 461–480.
Raastad T, Risoy BA, Benestad HB, Fjeld JG and Hallen J (2003). Temporal relation between leukocyte accumulation in muscles and halted recovery 10-20 h after strength exercise. Journal of Applied Physiology, 95, 2503-2509.
Rannevik G, Jeppsson S, Johnell O, Bjerre B, Laurell-Borulf Y and SvanbergL (2008). A longitudinal study of the perimenopausal transition: altered profiles of steroid and pituitary hormones, SHBG and bone mineral density. Maturitas, 61, 67–77.
Reichsman F, Scordilis SP, Clarkson PM and Evans WJ (1991). Muscle protein changes following eccentric exercise in humans. European Journal of Applied Physiology and Occupational Physiology, 62, 245–250.
117
Rizo-Roca D, Rios-Kristjánsson JG, Núñez-Espinosa C, Ascensão AA, Magalhães J, Torrella JR, Pagès T and Viscor G (2015). A semiquantitative scoring tool to evaluate eccentric exercise-induced muscle damage in trained rats. European Journal of Histochemistry, 59, 310-316.
Roberts TJ (2016). Contribution of elastic tissues to the machanisms and energetics of muscle function during movement. Journal of Experimental Biology, 219, 266-275.
Rolland YM, Perry 3rd HM, Patrick P, Banks WA and Morley JE (2007). Loss of appendicular muscle mass and loss of muscle strength in young postmenopausal women. Journal of Gerontology Series A: Biological Science and Medical Sciences, 62, 330–335.
Roubenoff R (2003). Catabolism of aging: is it an inflammatory process? Current Opinion in Clinical Nutrition and Metabolism and Care, 6, 295–299.
Roubenoff R and Hughes VA (2000). Sarcopenia: current concepts. Journals of Gerontology: A Biological Sciences and Medical Sciences, 55, M716-M724.
Roussel M, Garnier S, Lemoine S, Gaubert I, Charbonnier L, Auneau G and Mauriège P (2009). Influence of a walking program on the metabolic risk profile of obese postmenopausal women. Menopause, 16, 566-575.
Salo DC, Donovan CM and Davies KJA (1991). HSP70 and other possible heat shock or oxidative stress proteins are induced in skeletal muscle, heart and liver during exercise. Free Radical Biology and Medicine, 11, 239–246.
Samelan TR (2000). Heat shock protein expression is increased in cardiac and skeletal muscles of Fischer 344 rats after endurance training. Experimental Physiology, 85, 97–102.
Savage K and Clarkson P (2002). Oral contraceptive use and exercise-induced muscle damage and recovery. Contraception, 66, 67–71
Saxton JM, Clarkson PM, James R, Miles M, Westerfer M, Clark S and Donnelly AE (1995). Neuromuscular dysfunction following eccentric exercise. Medicine and Science in Sports and Exercise, 27, 1185-1193.
Schneider BS, Fine JP, Nadolski T and Tiidus PM (2004). The effects of estradiol and progesterone on plantarflexor muscle fatigue in ovariectomized mice. Biological Research for Nursing, 5, 265–275.
Sciote JJ, Horton MJ, Zyman Y, and Pascoe G (2001). Differential effects of diminished oestrogen and androgen levels on development of skeletal muscle fibres in hypogonadal mice. Acta Physiologica Scandinavia, 172, 179–187.
Selye H. 1956. The stress of life. New York: McGraw-Hill Book Co. Semmler JG (2014). Motor unit activity after eccentric exercise and muscle damage
in humans. Acta Physiologica, 210, 754-767. Senf SM, Dodd SL and Judge AR (2010). FOXO signaling is required for disuse muscle
atrophy and is directly regulated by Hsp70. American Journal of Physiology and Cellular Physiology, 298, C38–C45.
Senf SM, Dodd SL, McClung JM and Judge AR (2008). Hsp70 over-expression inhibits NF-kappaB and Foxo3a transcriptional activities and prevents skeletal muscle atrophy. FASEB Journal, 22, 3836– 3845.
Sewright KA, Hubal MJ, Kearns A, Holbrook MT and Clarkson OM (2008). Sex differences in response to maximal eccentric exercise. Medicine and Science
118
in Sports and Exercise, 40, 242-251. Seyfarth A, Blickman R and vanLeeuwen JL (2000). Optimum take-off technique and
muscle design for long jump. Journal of Experimental Biology, 302, 741−750. Shadwick RE (1990). Elastic energy storage in tendons: mechanical differences
related to function and age. Journal of Applied Physiology, 68, 1033-1040. Sites CK, Toth MJ, Cushman M, L’Hommedieu GD, Tchernof A, Tracy RP and
Poehlman ET (2002). Menopause-related differences in inflammation markers and their relationship to body fat distribution and insulin-stimulated glucose disposal. Fertility and Sterility, 77, 128-135.
Skidmore R, Gutierrez JA, Guerrio V and Kregal KC (1995). HSP70 induction during exercise and heat stress in rats: role of internal temperature. American Journal of Physiology, Regulatory, Integrative and Comparative Physiology, 268, R92–R97.
Smith LL, McCammon M, Smith S, Chamness Ms, Israel RG and O’Brien KF (1989). White blood cell response to uphill walking and downhill jogging at similar metabolic loads. European Journal of Applied Physiology and Occupational Physiology, 58, 833-837.
Stice JP, Chen L, Kim SC, Jung JS, Tran AL, Liu TT and Kowlton AA (2011). 17β estradiol, aging, inflammation, and the stress response in the female heart. Endocrinology, 152, 1589-1598.
Stice JP and Knowlton AA (2008) Estrogen, NF-B, and the heat shock response. Molecular Medicine, 14, 517–527.
Stokoe D, Engel K, Campbell DG, Cohen P and Gaestel M (1992). Identification of MAPKAP kinase 2 as a major enzyme responsible for the phosphorylation of the small mammalian heat shock proteins. FEBS Letters, 313, 307–313.
St. Pierre-Schneider BA, Correia LA, and Cannon JG (1999). Sex differences in leukocyte invasion of injured murine skeletal muscle. Research in Nursing
Health, 22, 243-251. St. Pierre BA and Tidball JG (1994). Differential response of macrophage
subpopulations to soleus muscle reloading after rat hindlimb supesnion. Journal of Applied Physiology, 77, 290-297.
Strehlow K, Rotter S, Wassmann S, Adam O, Grohé, Laufs K, Böhm, M and Nickenig G (2003). Modulation of antioxidant enzyme expression and function by estrogen. Circulation Research, 93, 170–177.
Stupka N, Lowther S, Chorneyko K, Bougeois JM, Hogben C and Tarnoposlky MA (2000). Gender differences in muscle inflammation after eccentric exercise. Journal of Applied Physiology, 89, 2325–2332.
Stupka N and Tiidus PM (2001). Effects of ovariectomy and estrogen on ischemia reperfusion injury in hindlimbs of female rats. Journal of Applied Physiology, 91, 1828–1835.
Subbiah MT, Kessel B, Agrawal M, Rajan R, Abplanalp W and Rymaszewski Z (1993). Antioxidant potential of specific estrogens on lipid peroxidation. Journal of Clinical Endocrinology Metabolism, 77, 1095–1097.
Sugioka K, Shimosegawa Y and Nakano M (1987). Estrogens as natural antioxidants of membrane phospholipid peroxidation. FEBS Letters, 210, 37–39.
Svendsen OL, Hassager C and Christiansen C (1995). Age- and menopause
119
associated variations in body composition and fat distribution in healthy women as measured by dual-energy x-ray absorptiometry. Metabolism, 44, 369-373.
Tache J and Selye H (1985). On stress and coping mechanisms. Issues in Mental Health Nursing, 7, 3–24.
Takekura H, Fujinami N, Nishzawa T, Ogasawara H and Kasuga N (2001). Eccentric exercise induced morphological in the membrane systems involved in excitation-contraction coupling in rat skeletal muscle. Journal of Physiology, 533, 571-583.
Thompson HS, Clarkson PM and Scordilis SP (2002). The repeated bout effect and heat shock proteins: intramuscular HSP27 and HSP70 expression following two bouts of eccentric exercise in humans. Acta Physiologica Scandinavia, 174, 47–56.
Thompson HS, Maynard EB, Morales ER and Scordilis SP (2003). Exercise-induced HSP27, HSP70 and MAPK responses in human skeletal muscle. Acta Physiologica Scandinavia, 178, 61–72.
Thompson HS and Scordilis SP (1994). Ubiquitin changes in human biceps muscle following exercise-induced damage. Biochemical and Biophysical Research Communications, 204, 1193–1198.
Thompson HS, Scordilis SP, Clarkson PM and Lohrer WA (2001). A single bout of eccentric exercise increases HSP27 and HSC/HSP70 in human skeletal muscle. Acta Physiological Scandinavian, 171, 187-193.
Tidball JG (1995). Inflammatory cell response to acute muscle injury. Medicine and Science in Sports and Exercise, 27, 1022–1032.
Tidball JG (2005). Inflammatory processes in muscle injury and repair. American Journal of Physiology. Regulatory, Integrative and Comparative Physiology, 288, R345–R353.
Tiidus PM (1995). Can estrogens diminish exercise induced muscle damage? Canadian Journal of Applied Physiology, 20, 26–38.
Tiidus PM (1999). Chapter 11: Nutritional implications of gender differences in metabolism: Estrogen and oxygen radicals: Oxidative damage, inflammation, and muscle function. In M. A. Tarnopolsky (Ed.), Gender differences in metabolism: Practical and nutritional implications (pp. 265-281). Boca Raton: CRC Press.
Tiidus PM (2000). Estrogen and gender effects on muscle damage, inflammation, and oxidative stress. Canadian Journal of Applied Physiology, 25, 274-287.
Tiidus PM (2001). Oestrogen and sex influence on muscle damage and inflammation: evidence from animal models. Current Opinion in Clinical Nutrition and Metabolic Care, 4, 509-513.
Tiidus PM (2003). Influence of estrogen and gender on muscle damage, inflammation and repair. Exercise Sport Science Review, 31, 40–44.
Tiidus PM and Bombardier E (1999). Oestrogen attenuates post-exercise myeloperoxidase activity in skeletal muscle of male rats. Acta Physiologica Scandinavia, 166, 85–90.
Tiidus PM, Deller M and Liu XL (2005). Oestrogen influence onvmyogenic satellite cells following downhill running in malevrats: a preliminary study. Acta
120
Physiologica Scandinavia, 184, 67–72. Tiidus PM, Holden D, Bombardier E, Zajchowski S, Enns D and Belcastro A (2001).
Estrogen effect on post-exercise skeletal muscle neutrophil infiltration and calpain activity. Canadian Journal of Physiological Pharmacology, 79, 400–406.
Tracey KJ (2002) Lethal weight loss: the focus shifts to signal transduction. Science STKE, PE21.
Tupling AR, Gramolini AO, Duhamel TA, Kondo H, Asahi M, Tsuchiya SC, Borrelli MJ, Lepock JR, Otsu K, Hori M, MacLennan DH and Green HJ (2004). HSP70 binds to the fast-twitch skeletal muscle sarco(endo)plasmic reticulum Ca2+-ATPase (SERCA1a) and prevents thermal inactivation. Journal of Biological Chemistry, 279, 52382–52389.
Van Pelt RE, Evans EM, Schechtman KB, Ehsani AA and Kohrt WM (2002). Contributions of total and regional fat mass to risk for cardiovascular disease in older women. American Journal of Physiology, Endocrinology, and Metabolism, 282, E1023- E1028.
Vasconsuelo A, Milanesi L and Boland R (2010). Participation of Hsp27 in the antiapoptotic action of 17β-estradiol in skeletal muscle cells. Cell Stress and Chaperones, 15, 183-192.
Vasilaki A, Jackson M and McArdle A (2002). Attenuated HSP70 response in skeletal muscle of aged rats following contractile activity. Muscle Nerve, 25, 902–905.
Velders M and Diel P (2013). How sex hormones promote skeletal muscle regeneration. Sports Medicine, 43, 1089-1100.
Viau V (2002). Functional cross-talk between the hypothalamic-pituitry-gonadal and-adrenal axes. Journal of Neuroednocrinology, 14, 506-513.
Vicdan K (2006). Erkek üreme sisteminin gilişimi ve fonksiyonlari üzerinde östrojenin rolü. Androloji Bülteni, 26, 213-216.
Vissing K, Bayer ML, Overgraad K, Schjerling P and Raastad T (2009). Heat shock protein transolcation and expression response is attenuated in response to repeated eccentric exercise. Acta Physiological Scandinavian, 196, 830-839.
Wade GN (1972). Gonadal hormones and behavioral regulation of body weight. Physiological Behaviour. 8, 523–553.
Warren GL, Lowe DA, Inman CL, Orr OM, Hogan HA, Bloomfield, SA and Armstrong (1996). Estradiol effect on anterior crural muscles-tibial bone relationship and susceptibility to injury. Journal of Applied Physiology, 80, 1660-1665.
Welch WJ (1992). Mammalian stress response: cell physiology, structure/function of stress proteins, and implications for medicine and disease. Physiology Review, 72, 1063-1081.
Willoughby DS, Rosene J and Myers J (2003). HSP-72 and ubiquitin expression and caspase-3 activity after a single bout of eccentric exercise. Journal of Exercise Physiologyonline, 6, 96–104.
Wiseman H, Quinn P and Halliwell B (1993). Tamoxifen and related compounds decrease membrane fluidity in liposomes. Mechanism for the antioxidant action of tamoxifen and relevance to its anticancer and cardioprotective actions? FEBS Letters, 330, 53–56.
Wohlers LM, Sweeney SM, Ward CW, Lovering RM and Spangenburg EE (2009).
121
Changes in contraction-induced phosphorylation of AMP-activated protein kinase and mitogen- activated protein kinases in skeletal muscle after ovariectomy. Journal of Cell Biochemistry, 107, 171-180.
Wolf MR (2009). Effects of estrogen on muscle damage in response to an acute resistance exercise protocol. These Paper.
Yamaguchi M, Izumimoto M, Robson RM and Stromer MH (1985). Fine structure of wide and narrow vertebrate muscle z-lines. A proposed model and computer simulation of z-line architecture. Journal of Molecular Biology, 184, 621–643.
Yasuhara K, Ohno Y, Kojima A, Uehara K, Beppu M, Sugiura T, Fujimoto M, Nakai A, Ohira Y, Yoshioka T and Goto K (2011). Absence of heat shock transcription factor 1 retards the regrowth of atrophied soleus muscle in mice. Journal of Applied Physiology, 111, 1142-1149.
Yenari MA, Fink SL, Sun GH, CHnag LK, Patel MK, Kunis DM, Onley D, Ho DY, Sapolsky RM and Steinberg GK (1988). Gene therapy with Hsp72 is neuroprotective ion rat models of stroke and epilepsy. Annals of Neurology, 44, 584-591.
Yu JD, Liu JX, Carisson L, Thornell LE and Stäl PS (2013). Re-evaluation of sarcolemma injury and muscle swelling in human skeletal muscles after eccentric exercise. PLoS One, 8, Doi: 10.1371/journal.pone.0062056.
Zheng L, He M, Long M, Blomgran R and Stendahl O (2004). Pathogen-induced apoptotic neutrophils express heat shock proteins and elicit activation of human macrophages. Journal of Immunology, 173, 6319-6326.
Zuckerman SH, Ahmari SE, Bryan-Poole N, Evans GF, Short L and Glasebrook AL (1996). Estriol: a potent regulator of TNF and IL-6 expression in a murine model of endotoxemia. Inflammation, 20, 581–597.
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Chapter VII: Appendix 7.1 Tissue Preparation and Sectioning Skeletal Muscle Materials:
Tempered glass plate Single edged blade (Personna American Safety razor Co., Cat #: 94-120-71) 2-18G needles Cut cork sections (~3cm x 3cm) Dewar for liquid nitrogen and Isopentane Suspension apparatus
o Sturdy stand with a vertical bar o Horizontal arm secured by a vertical bar o Thin rope to suspend the metallic bowl
Small metallic bowl (~250mL) Tongs Liquid Nitrogen (~1L) Isopentane (Methylbutane or 3-methylbutane) (~150mL) Optimal Cutting Temperature medium (OCT) (VWR, Cat #: CA95057-838)
Preparation:
1. Label cork pieces on the bottom and side with the subject, condition and muscle.
2. Pour liquid nitrogen into the dewar. 3. Set up the thin rope and metal bowl on the suspension apparatus above the
dewar of liquid nitrogen. 4. Pour isopentate (~150mL) into the metal bowl and lower into the liquid
nitrogen in order for isopentane to cool (the bottom of the metallic bowl will begin to turn white).
Procedure:
1. Raise the metal bowl out of the liquid nitrogen. 2. Section the muscle into 100-150mg pieces by using the both single edged
blades in a scissors manner, cutting perpendicular to the fibres (cross-section).
3. Dab a small dollop of OCT onto the cork and submerse it into the isopentane quickly to solidify the outside layers, while the inside remains gelatinous.
4. Repeat step 3 to build up another layer of OCT. 5. Using the two 18G needles, orient and submerge the muscle section with the
fibres facing directly upwards. 6. Cover the muscle section with OCT and submerge the completed cork and
muscle section into isopentane face down. 7. Remove the muscle section from the isopentane and place in dewar of liquid
nitrogen while preparing other muscle samples.
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8. Remove from liquid nitrogen, place the samples in a plastic container, add some liquid nitrogen to the container and store the samples at -80°C.
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7.2 Tissue and Blood Collection Materials:
1.5mL eppendorf tubes 18G needles Evacuated Collection Tubes (Vacutainer, BD, NJ, USA) heparin and heparin-
free Centrifuge (Beckman Coulter, Model #: Allegra 6R, Serial #: ALR01F81) Surgical scissors Rat toothed tweezers Blunt probe Clamp Plastic cutting board Isoflurane/oxygen gas mixture; 1L/min Oscillator (Lab-Line International Inc., Orbit P4, Model #: 322) Suction pipets
Preparation:
1. Label eppendorf tubes on the top and side with the subject, condition and muscle.
2. Label evacuated collection tubes with the subject and blood sample. 3. Turn on the centrifuge and set to 4°C.
Procedure:
1. Under anesthesia pick up the rodent’s abdomen with the rat toothed tweezers and cut through the abdomen and diaphragm using the scissors.
2. Extract the blood from the heart using an 18G needle and place half the blood sample in the evacuated collection tubes containing heparin and heparin-free tubes.
3. Place the blood samples on the oscillator for 15 minutes at room temperature and than store in the fridge at 4°C on an oscillator until ready for centrifuge.
4. Pull away fur and skin on the rodent’s treatment limb and use fine scissors to cut away at the epimysium.
5. Use a blunt probe to tear away the epimysium at the top near the patella in order to free the tibilais anterior.
6. Clamp the tendon at the bottom neat the foot and cut the tendon with fine scissors, using the clamp to gently pull the muscle away.
7. Use the fine scissors to cut the tibilais anterior at the top of the knee.
8. Place in a small weight boat the weight the muscle before sectioning for analysis.
9. Repeat steps 4-8 for the contra-lateral control limb. 10. Following collection of all rodent tissue, place the evacuated collection tubes
in the centrifuge, making sure they are balanced.
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11. Centrifuge the blood samples at 4°C for 15 minutes, at 3,000rpm. 12. Gently use the suction tubes to extract the plasma and serum and place them
into pre-labeled 1.5mL eppendorf tubes and store at -80°C for later analysis.
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7.3 Muscle Homogenization Materials:
Bead Bug Microtube Homogenizer (Model D1030, Product Code: 1143051039)
Acid Washed, Stainless Steel Prefilled Tubes (2.8mm diameter) (Benchmark, Item #: D1033-28)
RIPA buffer (Sigma Aldrich, Cat #: R0278) Protease inhibitor (Sigma Aldrich, Cat #: P8340) Ice bucket for samples Cut muscle samples (in ice) Centrifuge (Eppendorf, Model #: 5415 C) Eppendorf Pipets Labeled 1.5ml Eppendorf tubes
Preparation:
1. Place frozen muscle samples on ice in order to keep cool. Procedure:
1. Label prefilled tubes to designate appropriate muscle sample. 2. Add ten times the amount of RIAP buffer solution (based on muscle weight)
to the prefilled tube and 0.100μl of protease inhibitor per mg of muscle to prefilled tubes.
3. Place the frozen sample into prefilled tubes with RIPA buffer and protease inhibitor on and then place on ice to keep cool.
4. Repeat step 2 and 3 for all muscle samples. 5. Orient prefilled tubes into the Bead Bug homogenizer the same way, place
the control tube in the uppermost slot and the treatment in the lowest slot, leave the center slot empty.
a. Orientation image 6. Homogenize sample at a set speed of 400, set timer to 45 seconds. 7. After each homogenate, place the prefilled tubes back on ice to cool for
30seconds-1minute. 8. Place the prefilled tubes back into the Bead Bug homogenizer and repeat
steps 6 and 7 two more times. 9. Place prefilled tubes into centrifuge and spin for 30 seconds or longer at
3,000 rpm, to get rid of bubbles and determine if further homogenization is needed.
10. If further homogenization is needed place the prefilled tubes back on ice to allow for cooling for 30 seconds to 1 minute.
11. Repeat step 5-7 two to three more times. 12. Again, place the prefilled tubes into centrifuge and spin for 30 seconds or
longer at 3,000 rpm, to get rid of bubbles and determine if further homogenization is needed.
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13. Once the muscle sample is fully homogenized, extract it with an Eppendorf pipet along the side of the prefilled tubes, in order to avoid the beads and connective tissue at the bottom.
14. Place homogenate into labeled Eppendorf tube and place in -20°C freezer for short-term storage.
15. Once all samples are ground, place all in -80°C freezer for long-term storage.
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7.4 Determination of Protein Concentration—Lowry Assay Lowry-Protein Determination Loaded Sample
ddH2O STD Sample Reagent Phenol
Blank 0.5 ml - - -
20μg 0.48 20μl 5ml 0.5ml
40μg 0.46 40μl 5ml 0.5ml
60μg 0.44 60μl 5ml 0.5ml
80μg 0.42 80μl 5ml 0.5ml
100μg 0.40 100μl 5ml 0.5ml
Samples ddH2O STD Sample 1 0.500ml 5μl 2 0.500ml 5μl 3 0.500ml 5μl 4 0.500ml 5μl 36 0.500ml 5μl Preparation: 1ml (2% weight/volume) CuSO45H20 4ml (3% weight/volume) Na2CO3 in 0.1 N NaOH
In sets of three tubes (16) add 5ml of Lowry reagent = 240ml o Make up 250ml of Lowry reagent
Lowry Reagent
5ml Na-Tartrate 5ml CuSO45H20 240ml of Na2CO3 1. In a beaker, place 240ml of Na2CO3 and add Na-Tartrate first (5ml), than add
CuSO4 (5ml). 2. Add standards and samples together. 3. Add Lowry reagent to tubes than vortex and let rest for 10 minutes. 4. Mix the Phenol reagent with ddH2O, in a 1:2 ratio, i.e., for 45 tubes 70ml is
needed (0.5ml/tube). a. Make up 70ml, i.e., 20ml of phenol in 50ml of ddH2O.
5. Add 0.5ml of phenol reagent to each tube while vortexing tubes. Let each tube sit for 5 minutes before reading.
6. Read the tubes at a wavelength of 660nm (Turner, model # 340).
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7.5 SDS-PAGE, Western Blotting and Development
1. Assemble pouring apparatus for SDS-PAGE, pour gels o Add 1mL of APS to 1mL of ddH2O
2. Load sample with 1:1 ration of sample buffer o Load between 50-100μg per lane o Run the gel between 100-120 volts, until the dye runs off the gel o Ensure bubbles are present o It should take approximately 1.5 hours for the dye to run off the gel
3. While the gel is running gather materials to transfer to Western Blot (large casserole dish) and make transfer buffer.
4. Transfer buffer: 100ml of 10x Running Buffer, 700mL of ddH2O, 200mL of methanol.
o Mix in this order in order to avoid salt loss from the solution. o Equilibrate the gel and nitrocellulose paper for ten minutes and set up
transfer sandwich. o Mark the nitrocellulose: one diagonal for the first well, one square for
the last well. 5. Sandwich: Black part of the apparatusBrillo pad, three filter papers,
Nitrocellulose, white part of the apparatus3 filter papers, Brillo pad, close and lock the apparatus to create the sandwich.
o Repeat for both sandwiches 6. Ensure no bubbles are present, use a test tube to smooth the gel down,
carefully lift the ends of the gel remove bubble. 7. Insert the ice pack and fill with transfer buffer. Run at 60 volts for two hours.
o Ensure bubbles are present before turning on the stir bar o Replace the ice pack every hour
8. Remove blot and block in 5% blotto for one hour or overnight 9. 5% Blotto: 5g of non-fat milk powder, 100mL of TBS 10. Wash blot:
o First wash: 1x TTBS for five minutes o Second wash: 1x TTBS for five minutes
11. Incubate in 2% blotto with primary anti-body oscillating in the fridge for 3 hours or overnight
12. 2% Blotto: 2g of non-fat milk powder and 100mL of TBS 13. Primary anti-body dilution:
o 10mL of 2% blotto o Add 0.010μl of primary anti-body to make a 1:1000 dilution
14. Wash blot in TTBS for two washes at five minutes each and wash once in TBS for five minutes
15. Incubate in 2% blotto with secondary goat anti-rabbit IgG HRP-linked antibody (BioRad Cat# 170-6515) anti-body for 1 hour at room temperature on tectator (Lab-Line Instruments Inc., model #: 3520)
16. Secondary anti-body dilution: o 20mL of 2% blotto o Add 0.020μl of secondary anti-body (goat anti-rabbit HRP)
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17. Place in solution developer o Add 8ml of Luminata Forte Western HRP Substrate (Millipore
Corporation, Billerica, MA, Cat #: WBLUF0100) o Incubate each blot separately for 5 minutes.
18. Place blot face down on Li-Cor C-digit IS version 3.1 (Mandel Scientific, model #: CDG-001073 3600).
19. Scan image at “standard” sensitivity for six minutes, using Image Studio Digits (version 5.2.5)
20. Select best image and quantify lanes and safe quantified values in an Excel file.
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7.6 Enzyme-Linked Immunosorbent Assay (ELISA) Materials:
17 beta Estradiol ELISA Kit (Abcam, ab108667) Orbit Environ Shaker (Lab-Line Instruments, Inc., Model #: 3527) Deionised distilled water Serum samples Kimtech wipes Aluminum foil
Preparation:
Bring ELISA kit to room temperature. Place serum samples on ice to thaw. Turn on incubator and set to 37°C. Make wash solution by adding 50ml of Wash Solution to 450ml of ddH20.
Procedure:
1. Add 25μl of standards, control and sample to appropriate wells. 2. Add 200μl of 17β-Estradiol HRP Conjugate to each well. 3. Cover 96 well plate with aluminum foil and incubate at 37°C for two hours. 4. Remove the well contents and wash the each well three times with 300μl of
Wash Solution each time. a. Blot excess solution from wells following last wash.
5. Add 100μl of TBM Substrate to each well and incubate for exactly 30 minutes at room temperature.
6. Add 100μl of Stop Solution to each well and read the 96 well plate at a wavelength of 450nm within 30 minutes.
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7.7 Muscle Cross-Sectioning Materials:
Croystat, Myotome (Cryo-Cut, American Optimal Company, model #: 830) Honeycomb block/chuck Single edged blade (Personna American Safety razor Co., Cat #: 94-120-71) Microscope slides (stored at room temperature) (VWR, Cat#: CA48323-190) Paint brush (Chinese boar bristles, 1/4 inch, flat or bright, cut at a 45 degree
angle) OCT compound (VWR, Cat #: CA95057-838) 70% Ethanol 95% Ethanol Slide rack Kimtech wipes
Preparation: 1. Turn the cryostat and, place a single edged blade in the cryostat and the
apparatus to reach -20°C. 2. Take the cryostat blade out of the -20°C freezer and position the blade inside the
cryostat. Tighten the furthest knob to the left. 3. Remove the sample being sectioned from the cork using the cooled single edged
blade and bond the section to the chuck with a small amount of OCT compound. To fully bond leave the chuck inside the cryostat for 10-15 minutes.
4. Trim and remove excess OCT compound from the periphery of the sample into a triangle shape, with the most arrow part being the first cut (pointed up).
5. Insert the chuck into the holder and tighten. Procedure: 1. Adjust the angle of the blade to 4° with the black knob closets to you (may be
done). 2. Adjusting the knob behind the curved ruler at the back of the cryostat in order
to just the section thickness (10-12μm). 3. Adjust the blade cart height by locking and unlocking the lever closest to you. 4. Cut off a few sections in order to get nice consistent slices and ensure the blade
is cutting properly. 5. Crank the black hand wheel on the right of the machine to cut sections. Ensure
that the cutting is even and not curling, folding or tearing (caused by crevasses in the blade).
A. Ensure that the axel does not become unhinged after numerous sections. B. Reset the axel by using the knob at the front of the machine and readjusting
the blade. 6. Hold the slide on the frosted end and place the frosted end down towards the
blade. 7. Adhere the slide by using a room temperature slide and angling it at a 45° angle
above the blade. Slowly move the slide towards the section and allow it to
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adhere. A. Minimize drying time, as the tissue will undergo alterations and it warms
and dries. 8. Once the section has adhered to the slide, submerse in fixation solution (95%
ethanol) and than add it to the slide rack while cutting the rest of the sections. 9. If residue is left in the blade, wipe away large chunks of residue with the paint
brush and than spray 70% ethanol onto a Kimtech wipe a carefully wipe the blade and allow to air dry.
A. Always wipe away from the from the edge of the blade to ensure safety. 10. Label each slide on the frosted end and place in slide box at -20° for storage until
further processing. Notes:
It is best to cut approximately 12 sections with the settings in order to keep consistency.
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7.8 Hematoxylin and Eosin Staining Materials:
Slide rack Transfer containers and apparatus VWR micro glass cover (VWR, Cat: 48366-067) Cytoseal 280 glue (Thermo Scientific, Cat #: 8311-4)
Procedure: Container # Reagent Time 1 1x Phosphate Buffered Saline 1 minute 2 Erlich’s Hematoxylin 5 minutes 3 Tap Water (change every time) 1 minute 4 Distilled Water (change every time) 1 minute 5 30% Ethanol 1 minute 6 50% Ethanol 1 minute 7 Eosin 3 minutes 8 70% Ethanol (alternate the contents of this Rinse x 2 and the next dish after each use) 9 90% Ethanol Rinse 10 95% Ethanol Rinse 11 100% Ethanol 2 minutes 12 100% Ethanol 5 minutes 13 Xylene Substitute 5 minutes 14 Xylene Substitute 5 minutes Notes:
Refresh the Xylene Substitute after every 200 slides (substitute can be left of evaporate in the fume hood).
Eosin and Hematoxylin should stain thousands of slides, although filtering the stains prior to use if they have been sitting for longer than two days is best to remove lumps.
Eosin and Hematoxylin may be poured down the sink once no longer needed.
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7.9 Morphological Scoring System - Frequency of occurrence (items with a very low frequency of occurrence
were discarded) - Physiological relevance (items strongly related to eccentric exercise-induced
muscle damage) - 3 pictures of each sample taken~120 fibres per picture
0—absence of damage 1—moderate damage 2—severe damage Muscle Fibre
- Abnormal morphology (small, angulated or rounded fibres, swollen appearance of fibre splitting)
o 0= <4 o 1= 4-7 fibres o 2 > fibres or an entire fascicle
- Necrotic/(re)degenerating fibres [presence of infiltrating inflammatory cells (myophagocytosis), fragmented sarcoplasm, dark staining (hypercontracted fibres) and pale staining (necrotic fibres)
- Regenerating fibres were represented by early stage small basophilic myotubes and later by bluish-stained myofibres with central nuclei
o 0= absent o 1= 1-2 fibres o 2= >2 fibres
Inflammatory State
- Endomysial infiltrationsmall, mononuclear cells found in the endomysium o 0= <6 cells o 1= one cluster or ≥ 6 cells o 2= > 1 cluster of an entire fascicle infiltrated
- Perimysial infiltrationsmall, mononuclear cells found within the perimysium
o 0 = ≤ 10 cells o 1= >10 cells o 2= >2 clusters of widely diffused
Interstitial compartment
- Endomysium distensionspace b/w individual muscle fibres o 0= tight space o 1= moderately distended o 2= completely distended
- Perimysium distentionspace b/w fascicles o 0= tight space o 1= moderately distended o 2= completely distended