chapter 1 introduction -...
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CHAPTER 1
INTRODUCTION
1.1 Introduction to photosynthetic systems
Life on earth depends on the Sun. Higher plants,
eukaryotic algae and cyanobacteria (blue green algae) chemically
sequester light energy through photosynthesis, a light driven
process in which co2 is fixed to yield carbohydrates.
The chemical free energy stored in these substrates and
the oxygen evolved by photosynthetic organisms is what drives
practically all life processes.
1.1.1 Chloroplasts
The site of oxygenic photosynthesis in eukaryotes (algae
and higher plants) is the chloroplast. A cell of higher plants
contains typically 20 to 40 chloroplasts. Electron micr0graph of
a thin section of chloroplast shows a double layered envelope
membrane. The inner membrane surrounds stroma containing soluble
enzymes, genetic material and thylakoid membranes. The thylakoid
is probably a single highly folded vesicle although in most
organisms it appears as stacks of disk like sacs called grana,
which are interconnected by unstacked stroma lamellae.
Photosynthesis occurs in two distinct phases.
1. The 1 ight reactions, which use light energy to generate
NADPH, H+ and ATP.
2. The dark reactions, actually light independent reactions,
which use NADPH and ATP to drive the synthesis of carbohydrate
from co 2 and H2o.
1
The light reactions take place in thylakoids that contain
the li9ht absorbing pigments (antenna molecules) and the sites
where the primary photochemical reaction occurs (reaction
centres). Reaction centres generate the set of re:dox compounds
that are necessary for the overall process of photosynthesis. In
oxygen evolving organisms, two 1 ight driven photochemical
reactions, occurring at photosystem II (PSII) and photosystem I
(PSI), operate in series and drive electrons from the electron
donor H2o to the final electron acceptor NADP+. Eventually, the
Calvin cycle uses NADPH and ATP as substrates and reduces co~. L
1.1. 2 Absorption of light and the fate of absorl~d photon
Each of the photosynthetic pigments residing in the
thylakoids has a characteristic absorption spectrum when studied
in isolation outside the chloroplast i.e. in vitro. Each pigment
also has a characteristic fluorescence spectrum. 'rhe various
chlorophylls are highly conjugated molecules and strongly absorb
visible light. In fact, the peak molar extinction coefficients of
the various chlorophylls of over 10- 15 M- 1• cm- 1 , an:~ among the
highest known for organic molecules yet. The relatively small
chemical differences among the various chlorophylls greatly
affect their absorption spectra. These spectral differences are
functionally significant and ensure absorption from almost entire
visible solar spectrum. Inside the chloroplast, howE~ver, Chl b
fluorescence is not detected, even when the actinic light us,ed
is of a wavelength known to be absorbed predominantly by Chl b.
Similarly, fluorescence is never observed from the carotenoid
pigment and to only a small extent by the phycobilins in
cyanobacteria. Only Chl a fluoresces naturally inside the
chloroplast. This surprising phenomenon was explained by Duysens
(Duysens, 1952) He showed that Chl b, carotenoids and the
phycobilins act as "antennas" to harvest light energy. Their
2
energy is transferred very efficiently to Chl a. Only Chl a is
actively involved in the subsequent reactions of photosynthesis.
Absorption of light sends a molecule to the excited state. An
electronically excited molecule can dissipate its excitation
energy in one of the following ways,
1.1.2.1 Internal conversion
It is a common mode of decay in which electronic energy is
converted to the kinetic energy of molecular motion, i.e., to
heat. This proce~s is completed in ~lo-11s. Chl molecules usually
relax only to their lowest excited states. Therefore, the
photosynthetically applicable excitation energy of chlorophyll
molecule that has absorbed a photon in its short wavelength band,
which corresponds to its second excited state, is no different
than if it had absorbed a photon in its less energetic long
wavelength band.
1.1.2.2 Fluorescence
In this process an electronically excited molecule decays
to its ground state by emitting a photon. Such a process requ~res
~10-8 s, so it occurs much more slowly than internal conversion.
A photon emitted as fluorescence generally has a longer
wavelength (lower energy) than that initially absorbed.
Fluorescence accounts for the dissipation of only 3% to 6% of the
light energy absorbed by plants.
1.1.2.3 Excitation transfer (resonance energy transfer)
In this process an excited molecule directly transfers its
excitation energy to nearby molecules by resonance or Forster
transfer to neighbouring molecules.
3
1.1.2.4 Photochemical conversion
If trapped at the reaction centres, absorbed energy drives
the primary photochemical reactions. The reactions can be shown
to take place in an order as shown in fig. 1.1 (Z scheme). Every
photochemica 1 reaction involves transfer of one electron, thus
creating one positive and one negative charge. The charge
separation leaves a hole in the form of p+ 680 . This ·positive
charge is neutralized by electron donation from secondary donor
Z. z+, which has now been identified as a tyrosine residue of
the D1 protein of the PSII reaction centres (Debus et al, 1988)
in turn gets electron by oxidation of water. The process of
charge separation is very rapid (K -10 11 -10 12 s- 1 1. For
efficient photochemistry, the separated charges must be
stabilized, i.e. the probability of back reaction must be
minimized. This is achieved by spatial separation of the charges.
This process not only stabilizes the charge separation, but also
brings the reaction centre of PSII to a open state for the second
photochemical event. To make the rate of electrons transport
optimal, the quanta should arrive at the reaction cent:re at a
rate as fast as the removal of charges from the previous
photochemical event. The intensity of light which plants are
normally exposed is not sufficient. Therefore, the plants have
evolved a mechanism by which the effective cross section of
reaction centre for light absorption is considerably increased.
This is achieved by light harvest by several hundred antenna
chlorophylls as stated earlier. All the molecules absorb quanta
of different energy and transfer to reaction centre with such a
high efficiency that more than 90% of absorbed light is utilized
by photosynthesis.
4
Fig. 1.1
·------------ ----------------------------------------------------------------
-I :
-C€
-cs
-c ~ co
~ ·' -02 §
I G " :?. 0 c: '-'
·( ' 2 :> IJJ-0 < . g
<'6 0 Q
Fig. 1.1
photosynthetic
lifetimes of
"' c " 8 '? c
" ::; 0
~ c: ~
" -
An updated version of the 'Z'- scheme of
electron transport in higher plants showing the
various electron transfer reactions (After
Govindjee and Eaton-Rye, 1986).
1.2
1.2.1
1.2.1.1
organization of photosynthetic systems
Structure and function of the photosynthetic
apparatus in higher plants Cthylakoid membranes)
Structure and
lipids
distribution of the thylakoid acyl
Thylakoid membranes are made up of approximately 60%
protein, 30% lipid and 10% chlorophyll (by weight). The
predominant lipids of thylakoids are the uncharged galactolipids,
monogalactosyldiacylglycerol (MGDG) and
digalactosyldiacylglycerol {DGDG). Together they constitute about
75% of the total thylakoid lipid {50% and 25% respectively) (Webb
and Green, 1991) . The remaining 25% is comprised mostly of the
anionic lipids sulfoquinovosyldiacyl glycerol (SQDG) and
phosphatidylglycerol {PG) (Allen and Gord, 1971). Thylakoid
membranes do not contain sterols. Whether or not thylakoid
cont~fn phosphatidyl choline (PC) is debatable. There is strong
evidence (Dorne et al, 1990) that the endogenous levels of PC as
shown by Siegenthaler et al ( 1989) were contaminants from the
chloroplast envelope membranes. The remainder includes a wide
variety of lipophilic pigments, including the chlorophyll a and
Chl b, xanthophylls, B-carotene and the quinones. With the
possible exception of the specific quinones, these pigments are
non-covalently bound to the polypeptides of the pigment-protein
complexes (Murphy, 1986a; Murphy, 198Gb). A remarkable feature
of thylakoid lipids is the presence of high proportion of
polyunsaturated acyl groups, in particular that of the 18:3·
linolenic acid. However, a higher unsaturation index does not
confer a high membrane fluidity, probably because the motion of
acyl chains of lipids in the thylakoid membrane is considerably
5
ceduced by the presence of intrinsic membrane proteins. There is
no evidence for any specific lipid association with peptides
apart from the interaction of ch lorophy 11 with Chl-prote in
complexes. All chlorophyll molecules are bound to protein rather
than being 'free' in the lipid bilayer of the thylakoid membrane
(Markwell et al, 1979). The thylakoid membranes contain five
supramolecular assemblies embedded in the lipid bilayers.
1.2.1.2
1.2.1.2.1
Structure
complexes
and function of electron transJX>rt
Photosystem II (PSIIJ complex
PSII can be defined as the part of oxygenic photosynthesis
which catalyzes the photoinduced transfer of electrons from
water to plastoquinone (PQ).
The organization of all the components involved in this
reaction is shown in a pictorial model (fig. 1.2) given by
Hansson and Wydrzynski (1990). The genes of the proteins, their
molecular weight (MW) , the location of their transcri?tion and
probable function are shown in table 1.1. Biochemical
characterization of PSII suggests that around 22 polypeptides are
associated with PSII (Masojidek et al, 1987). In the hypothetical
picture cf PSII given by Hansson and Wydrzynski ( 1990), PSII is
subdivided into four functional parts.
1.2.1.2.1.1 Reaction core: The reaction core contains the primary
reactants, PSII reaction centre Chl a (P680 ), oxyqEm evolving
and plastoquinone (PQ) reducing components. Dl and 02 polypeptide
of PSII exhibit a significant degree of sequence homology with
the L and M subunits of the reaction centres of photosynthetic
6
Fig. 1.2 A schematic representation of the functior
organization of photosystem II (PSII) according to Hansson a
Wydrzynski (1990). The definition of symbols are as follows:
the primary electron donor chlorophyll (Chl) (P680); HA, t
primary electron acceptor pheophytin (Pheo); H8 , a second Phe
QA and Q8 , the first and second quinone electron acceptor
respectively; Fe, a non-heme iron atom; Y 2 , the tyrosine, fir
electron donor to P; Y0 , a second tyrosine; M, the manganes
containing component involved in oxygen evolution; cyt b55 Cytochrome b 559 heterodimer; D1 and D2, Reaction core subunit
QSP, Quinone-shielding protein; AIP, Accessory intrins
proteins; EP 33, EP 23 and EP 16, Extrinsic proteins of the
Regulatory Cap; AEP, Accessory extrinsic proteins; CP ~7 and CP
43, Chl proteins of the Proximal Antenna; ACP II, Accessory Chl
proteins of the Distal Antenna and LHC II, the Chl ajb light
harvesting complex.
Fig. 1.2
LUMEN
Approximate Location Apparent Mo-
Gene (Eukaryotes) Product lecular Mass
psbA chloroplast D1 (PS II-A) 32,000 psbB chloroplast CP47 (PS II-B) 47,000 psbC chloroplast CP43 (PS II-C) 43,000 psbD chloroplast D2 (PS II-D) 32,000 psb£ chloroplast cyt b-559 (PS 11-E) 9,000 psbF chloroplast cyt b-559 (PS II-F) 4,000 psbH chloroplast "10,000 M, phosphoprotein" (PS II-H) 10,000 psbl chloroplast reaction center component (PS II-I) 4,800 psbf chloroplast n.d. ("PS 11-J") n.d. psbK chloroplast PS Il-K 2,400 psbL chloroplast PS Il-L 5,000 IISb!v: chloroplast PS 11-M 4,700 IISbN chloroplast PS II-N 4,700 IISbO nuclear MSP; PS 11-0 33,000 psbP nuclear 24,000-M, protein (OEE2; PS 11-P) 24,000 /ISbQ nuclear 18,000-M, protein (0EE3; PS 11-Q) 18,000 /ISbR nuclear 10,000-M.-protein (PS 11-R) 10,000 cab nuclear (family) LHC lis 21,000-29,000
Table 1.1 PSII genes and their products as listed by Erickson
and Rochaix (1992).
bacteria (Rochaix et al, 1984; Youvan et al, 1984). This has led
to speculation that 01 and 02 constitute the reaction centre in
PSII of higher organisms. Isolation of a minimal unit of PSII
which can do photochemistry and contains 01, 02 and 10 KOa (Nanba
and Satoh, 1987; Okamura et al, 1987) subunit of Cyt b559 has
supported this speculation. cyt b559 is also associated with the
reaction centre. The molecular structure of Cyt b559 was recently
established to be an inter molecular heme cross-linker dimer of
14 KOa (Cramer et al, 1986), which could be either a homodimer or
heterodimer (Tae et al, 1988). The stoichiometry of Cyt b599 and
P680 a stripped 01-02-Cyt b559 reaction centre particle is 1. 3
(Nanba and Satoh, 1987)~ suggesting that the stoichiometry could
be one Cyt b559 heme per PS II centre (Barber et al, 1987;
Gounaris et al, ·1987). There is a lot of ambiguity regarding the
functional role of Cyt b559 , which led researchers to propose
following hypothesis for its function,
1. An electron transfer intermediate on the oxidizing side of
PSII (Knaff and Arnon, 1969).
2. In a bypass or cyclic electron
(Ben-Hayyim, 1974); Arnon and Tang,
(1990) proposed that the primary role
transfer route around PSII
1988) . Canaani and Havaux
of Cyt b 559 in vivo is to
direct excess photons from linear to a cyclic electron flow at
high light intensities for protection of the 01 and 02 proteins
against photodamage. In addition to this, cyt b559 is suggested
to have a role in the deactivation of the powerful oxidant z+ in
the dark, also (Canaani and Havaux, 1990).
3. Linking the two photosystems (Ortega et al, 1989) in non-
cyclic electron transfer.
1.2.1.2.1.2 Regulatory cap: Regulatory cap of PSII contains a set
of three proteins having molecular weight of 33, 23 and 16 KDa.
All the three proteins are extrinsically bound to the luminal
surface of the thylakoid membrane. In addition to these proteins
regulatory cap may contain another extrinsic protein of 5 KDa
7
(Ljungberg et al, 1986}. The regulatory cap proteins have been
assigned a role in regulating the ionic requirement (i.e. Cl and
ca++) of o2 evolution and in controlling the exchange of
reactants with the manganese (Mn) cluster. One of the important
component associated with regulatory cap is Mn clusters. The Mn
stoichiometry has been determined by various external extraction
procedures (Yocum et al, 1981}. It is generally agreed that
stoichiometrically, four Mn ions are associated with each PSII.
'Despite extensive studies, the exact location and functional
operation of the Mn is still under considerable debate (Hansson
and Wydrzynski, 1990). Valance state changes of the Mn ions are
shown to be associated with the S state transitions. Mn ions are
believ1~d to be located within a restricted compartment toward~.
the luminal side of the membrane.
1. 2. 1. 2. 1. 3 Proximal antenna: The proximal antenna of PSII
comprises two pigment-protein complexes CP47 and CP43 (Green,.
1988). The polypeptides of these complexes have molecular weight
of 4.5-51 and 40-45 kDa, respectively. Each of these proteins
binds 20-25 Chl a and about 5 molecules of 8-carotene, but no Chl _
b or Pheo. The proximal antenna is apparently tightly coupled to
the reaction core. The CP4 7 and CP4 3 proteins are always
present in oxygen evolving preparations of PSII from higher
plants. Studies show that electron transfer from exogenous donors
to QA can take place in the absence of CP47 and CP43 (Yamaguchi
et al, 1980) but that the ability to reduce QA is lost when both
CP43 and CP47 are removed (Akabori, et al 1988}. Inactivation of
the genes for CP47 or CP43 by site directed mutagenesis prevents
or reduces, respectively, the assembly of reaction core (Vermaas
et al, 1988). Therefore, the earlier belief that these complexes
may directly bind the reaction centre and primary acceptor of
PSII (Nakatani et al, 1984; Inoue, 1983; de Vitry et al, 1984} or
have a role in the regulation of early photochemical events can
not be totally excluded.
8
1.2.1.2.1.4 Distal antenna: The distal antenna of PSII in higher
plants is light harvesting chlorophyll protein complex (LHCII).
The smallest, resolvable natural unit of LHCII is a dimer
consisting of two polypeptides with approximate molecular weights
of 25 and 27 kDa. LHCII has a Chl ajb ratio of 1.2 ± 0.2 and
contains xanthophyll as the major carotenoid. About 30% of LHCII
can be phosphorylated by a membrane bound kinase. The extent of
phosphorylation is regulated by the levels of reduced PQ.
Following phosphorylation, LHCII migrates laterally from
appressed to nonappressed regions of thylakoids, where it is
proposed to enhance the light harvesting capacity of PSI (Larsson
et al, 1987a and b; Bassi et al, 1988). LHCII is also shown to
have a role in cation dependent stacking of thylakoid membranes
to form grana (Mullet and Arntzen, 1980; Steinback et al, 1982).
PSII distal antenna also contains Chl protein complexes which are
not a part of LHCII. Among these components are CP 29 (Green,
1988), CP 26 and CP 24 (Dunahay and Staehlin, 1986; Bassi et al,
1987). The Chl ajb ratio of these complexes vary from 2 to 3.
None of these proteins are phosphorylated. According to Hansson
and Wydrzynski ( 1990) , these compl"exes may be closer to the
proximal antenna and the reaction core and may serve as 'linker'
or 'anchor' for the LHCII proteins. One suggestion has been that
these Chl proteins may participate in the dissipation of excess
excitation energy arriving at the reaction core to counter
photoinhibition (Bassi et al, 1987).
1.2.1.2.2 Heterogeneity in PSII
The notion of functionally, and possibly structurally,
distinct populations of PSII centres within the thylakoid
membranes is well established for long. The existence of two
types of primary acceptor, Q, (Q1 and Q2) was suggested on the
basis of differences in the fluorescence yield after single
9
turnover light flashes (Joliet and Joliet, 1977; 1979; 1981;
1983).
On redox considerations, QA has been shown to exist: in two
forms; low potential (QL, - 250mv) and high potential (QH, 0 mv)
(Cramer and Butler, 1969; Horton and Croze, 1979). Since the QL
and QH are believed to be associated with different reaction
centre proteins, two forms of PSII one with QL and another with
QH are expected in vivo (Vermaas and Govindjee, 1981; DinE~r and
Delosme, 1983; van Gorkom, 1985; Govindjee, 1990).
Measurements of the ability of spinach chloroplasts to reduce PQ
indicate that there are about 1. 7 m mol of active PSII centres
per mol of Chl (Graan and Ort, 1984). Measurement of the ability
of chloroplasts to oxidize water in the presence of DMQ yielded
similar results (Whitmarsh and Ort, 1984). However, estimates of
the reduction of the primary quinone electron acceptor QA (Melis
and Anderson, 1983; McCauley and Melis, 1986) suggestE~d the
number of PSII centres about 3 m mol per mol Chl. The <estimate
of active centres per mol Chl was increased to a similar number
( 3 m mol), when certain halogenated benzoquinones (e.g. DCBQ)
were used as electron acceptors (Graan and ort, 1986).
Quantitative estimates of the oxidation of the electron donor Z
also supports these results (Babcock et al, 1983). This
difference in the quantities of PSII per mol Chl as revealed by
different techniques was explained on the basis of a population
of PSII centres deficient in sustained water oxidation capacity.
The evidence regarding the heterogeneity in PSII has also
come from the interpretation of Chl a fluorescence induction in
the thylakoids. Melis and Homann (1975) analyzed the induction of
Chl a fluorescence in DCMU poisoned chloroplasts (DCMU inhibits
electron transfer from the primary acceptor QA to QB) 1n terms of
two distinct p)1ases, an initial sigmoidal phase (o<J and a slower
exponential phase (8). These two phases are assumed to be because
of two different type of PSII centres in thylakoid membranes
occurring in vivo which are designated as PSIIac and PSII 8
10
centres. The analysis method of Melis (Melis and Homann, 1975;
1976) involved calculation of the growth of complementary area,
defined by the induction curve and the line of the maximum
fluorescence level (FM), with time and the semilogarithmic plot
of such an analysis. However, since it is difficult to determine
asymptotic level of FM , it is always difficult to determine the
precise value of complementary area. Assuming that the last part
of the fluorescence induction curve is exponential, Hsu et al
( 1989) determined FM using mathematical analysis and curve
fitting. They analyzed the Chl a fluorescence induction in DCMU
poisoned chloroplasts into three phases, a major rapid sigmoidal
~phase followed by two minor slower exponential phases B and t.
The kinetic analysis both in the case of Melis and Homann (1975;
1976) and Hsu et al (1989) showed that rate constant of the oC
phase is light intensity dependent and is affected by presence of Mg++.
Chylla et al (1987) reported that certain PSII centers are
slow in the reduction of Q8 and take around 1.7 s before they are
ready for a second photochemical act. The authors designated them
as slow turning over PSII centres (inactive PSII) centres in ,,
comparison· to normal PSII units (active). They further showed
that around 44 % of PSII centres exist in inactive state (Chylla
et al, 1987; Chylla and Whitmarsh, 1989). Cao and Govindj ee
(1989) suggested that Fo to F1 rise seen in the Chl a
fluorescence induction occurs due to inactive centres. Hsu et al
(1989) studied the kinetics of this rise (F0 to F1 rise). They
found this rise to be monoexponential. Kinetic parameters show
that rate constant and response of this phase towards Mg++
depletion is very similar to oC phase in DCMU poisoned
chloroplasts (F0 to F1 rise was studied in absence of DCMU).
Depending on these observations, these authors suggested that F0 ·
to F1 rise is due to PSII ~ centres, a pool of which are inactive
in PQ reduction. In their analysis they found out that
complementary area of growth phase due to F0 to F1 rise is 10% to
11
the total area occupied by oe. phase. This suggests that only 10%
out of total pool of PSII centres are inactive which is contrary
to Chylla and Whitmarsh (1987) who suggested this number to be
40%. Hsu and Lee (1991) tried to explain the reason for this
discrepancy. They suggested that a large portion of the inactive
PSII centres are not detectable in fluorescence rise from F0 to
FI. They also mention that probably these left over centres,
which escape detection in their experiments represent inactive
PSII centres with low fluorescence yield. They further suggested
that the population of the inactive PSII centres is likely to be
heterogeneous. So, methods qther than fluorescence induction are
required to clarify this suggestion. In a recent study, Chylla
and Whitmarsh (1990) using light saturation curves of flash
induced absorbance change at 518 nm have shown that inactive PSII
centres require twice as many photons as the active: reaction
centres to achieve the same yield. They suggested that the
inactive PSII centres have a smaller effective absorption cross
section, due to a smaller antenna size, or due to a lower quantum
yield for photochemistry.
These studies thus suggest that PSII population in
thylakoids is heterogenous. The heterogeneity has been shown to
exist in terms of antenna size (oe, B heterogeneity; Melis and
Homann, 1975; Anderson and Melis, 1983; Melis, 1985; Guenther et
al, 1988). In addition to~' B heterogeneity, PSII centres also
display heterogeneity on the reducing side of QA with respect to
electron flow to the plastoquinone pool. several investigators
have shown that a number of PSII centres, though photochemically
competent are unable to transfer electrons from QA to QB
(Thielen and van Gorkom, 1981; Lavergne, 1982; Melis, 1985; Graan
and Ort, 1986; Greene et al, 1988; Guenther et al, 1988).
In Lavergne's nomenclature ( 1982) these centres are termed as
PSII Q8-non reducing centres.
12
-
1.2.1.2.3 Plastoquinone ~
Plastoquinone acts as a mobile electron carrier between
QB (PSII) and Cyt b 6/f
Barber, 1984; Whitmarsh,
molecule and consists of
and an isoprenoid side
complex (Anderson,
1986). It is a
a quinone ring with
chain attached to
1980; Millner and
relatively small
two methyl groups
it. The size of
plastoquinone pool has been estimated to be between i (in the
cyanobacterium Anabaena var.:i,.abilis and 40 (in chloroplasts and
Anacystis nidulans) molecules per P700 (Hauska and Hurt, 1982).
Thus, this component provides a large pool of electron acceptors
near PSII. Each quinone molecule transfers two electrons during
a reduction-oxidation reaction, which must be accompanied by the
uptake of two H+ ions (Jagendorf, 1977). The flux of electrons
through the plastoquinone pool seems to be the rate-limiting step
in photosynthetic electron transport. Oxidation of PQH2 by the
Cyt b 6/f complex is linked to translocation of protons from the
stromal phase into the lumen, generating a proton gradient across
the thylakoid membranes (Velthuys, 1978; Whitmarsh, 1986).
Plastoquinone also plays a role in the regulation of
excitation energy distribution between PS II and PSI under
changing environmental conditions. Reduced state of
plastoquinone is reported to activate a kinase (Bennett et al,
1980; Howarth et al,. 1982; Allen, 1992) , which phosphorylates
LHCII. Phosphorylated pool of LHCII molecules decouple themselves
energetically (functionally) and migrate to non-appressed
membrane region where they are known to associate with the PSI
(Fork and Satoh, 1986; Bennett, 1991; Allen, 1992).
1.2.1.2.4
The cytochrome b 6-f complex mediates electron flow between
the plastoquinone generated by PSII activity and the diffusible
plastocyanin carrier. In this way, it links the electron
13
transport chains of PSII and PSI. The complex is made up of four
polypeptides of M.W. higher than 15 KDa; a 19-23 KDa (P'et c gene
product), which binds one high potential (2Fe-2S)' Rieske' group
(Widger and Cramer, 1991), a Cyt f (pet A gene product, =32 KDa),
Cyt b 6 (pet B gene product,=25 KDa), subunit IV (pet D gene
product, -18 KDa). In addition to this, two to three small
polypeptides of molecular weight less than 6 KDa have also been
reported as a part of purified Cyt b 6 /f complex (W'idger and
Cramer, 1991). This complex transports protons as: well as
electrons from the outside to the inside of the thylakoid
membrane. It has been suggested that much of the electrochemical
proton gradient needed for the synthesis of ATP is qenerated
because of electron transport activity of Cyt b 6-f complex. This
complex is shown to be uniformly distributed in the grana and
stromal membranes (Cox and Andersson, 1981; Anderson, 1982;
Peters et al, 1983) . However, a model has also been proposed
according to which this complex is placed in the region around
the grana. (Barber, 1983; Ghirardi and Melis, 1984; Webber et al,
1988).
1.2.1.2.5 Photosystem L (PSIJ complex
PSI acts as a plastocyanin ferredoxin photoxidoreductase,
which transfers the electron from plastocyanin (located on the
luminal side of the membrane) through a series of five or six
electron carriers to ferredoxin (towards the stromal side of the
membrane). Figure 1.3 represents the diagrammatic picture of PSI
as suggested by Golbeck (1992). The genes of proteins associated,
their molecular weight (MW) , the location of their transcription
and probable function are shown in table 1. 2. PSI is a
multiprotein complex and can be divided into two structu1~al units
based on functional considerations.
14
Fig. 1.3
Fig. 1·3
STI{0;\1A
I
LUMEN
!'sa:\ 1\3.2-ki>a
The architecture
proposed by Golbeck ( 1992). The
l'saB S2.5-kDa
l'saF I'I;L\IOC)'allin Dock in~-:
for the
symbols
PSI
are
1.2 and also in section 1.2.1.2.5.
PsaL
reactio.n centre as
described in table
Protein Site Residues· Mass Cofactors Function 'Pr0J.H:>rt ie:' (kDa)•
Hydrophobic PSI core proteins
PsaA c 750 83 Antenn:1e chloro--100Chla
phyll and photo· 12- 15 {1-Carotene
chemical charge s;ep-2 Ph,·Iloquinone
a ration (Vit K 1)
1 ]-lfe-4S]
PsaB c 734 82 Antennae and pho-
toprotN'tion
Char[!<' >'tahi!tzat ion
Ch.arg,· ;tahiliz:nion
PsaF N 154 17.3 None Pla;otocyantn· dock-
ing protein
p,aG" N 98 10.8 !'one
Psal c 36 Tran:-:.nH·mhrant' )
h<>!tx
P<aJ c 44 5 Tran~mt.•mhr;1nt· ,.
helix
P<aK N !;I 1:'.4 !\on~ lntrin:::.ic mt·n:br;tllt'
protein
PsaL N 169 18 None lntrin~ir mt·n:hrant.·
prot(~in
Psa~l· c 30 32 :1.5 ~one lntrin~ic nwmhrane
protein
P,-aN· C? -50-{;() Vi None Intrinsic nH'mhr;1nt'
protein
PsaO•' N -90 9.0 None lntrin~ic nwmhrttne
prote1n
H~·drophilic PSI peripheral prot .. ins
P,;aC c 81 8.9 2]4Fe-4S] Terminal el<·ctron
acct-ptors
PsaD N 162 1/.9 None Ferreooxin-duck in~ protC'in·p,,.c l11nd-
ing
PsaE N 91 9.7 !'lone Cyclic ele\tron
flow .'ft·rn·doxin-
dockinr:?
PsaH" N 95 10.2 None LHC I Jink(•r pro-
tein?
Hydrophobic Chi a/b binding proteins (eukaryotes only)
Cab-6Ai6B ~ 201-2 ~2 Chi a. Chi b. Xan- Ant~nna: LHCI-~:lO:
thophylls T,p.-1 C-'.1:!' Cab-7 ~ 209-10 24.9 Chi a. Chi b. Xan- Antt·nna: LHCI-6i<O:
thophylls T,·p~ II CAB'
Cab-8 s 2-l0-241 26.1 Chi a. Chi b. Xan- Antenna: LHCI-6:'0:
thophylls • Type Ill CAB' Cab-11/12 ~ 200 0•? Chi a. Chi b, Xan- Antt-nna: LHCI ~:lO:
thophylls Typ<· l\" C.-\ B'
Table 1. 2 PSI genes and their products (Golbeck, 1992).
1. 2. 1. 2. 5. 1 PSI core complex Two high molecular weight Chl
binding subunit proteins of about 83 KDa and 82 KDa (psa A and
psa B gene products) comprise the PSI core complex. The electron
transfer components associated with the PSI core complex include,
a) A primary electron donor P700 , possibly a dimer of Chl a
molecules (Philipson et al, 1972; Bengis and Nelson, 1977; Mullet
et al, 1980).
b) A0 , a Chl a monomer which acts as primary electron acceptor
(Shuvalov et al, 1986).
c) A1 , a quinone (probably phylloquinone) (Biggins and Mathis,
1988)
d) Three non-sulfur centres, Fx, F8 , and FA, which are probably
associated with two low molecular weight proteins ( 15 and 18-19
KDa, Bonnergea et al, 1985), or 12 KDa polypeptide (Lagoutte et
al, 1984) of the PSI complex.
Recently, Krauss et al, ( 1993). determined the three
dimensional structure of PSI trimers isolated from Synechococcus
sp. at 6A resolution which has provided further information
regarding the arrangement of 4Fe-4S clusters, oC-helices of
reaction centre protein and Chl a in reaction centre.
1. 2. 1. 2. 5. 2 Chl a/b light harvesting complex (LHCI) : This
constitutes a peripheral antenna of PSI reaction centre. LHCI
contains three polypeptides with apparent molecular weights of
17-26 kDa (Haworth et al, 1983) and one of about 10 kDa. The Chl
ajb ratio of LHCI is 3.5 to 4.0. The major function of LHCI is to
hold pigment molecules in the right orientation for efficient
light harvesting and subsequent transfer of excitation energy to
the reaction centre. However, Ikegami and Katoh (1991) have shown
that Chl a of antenna has a structural role in stabilizing the
functional conformation of P700 chlorophyll -protein complexes.
The LHCI contains a long wavelength absorbing Chl a species
(Chl 705 ) which is responsible for the 735 fluorescence band of
PSI at 77K (Mullet et al, 1980).
15
1.2.1.2.6 Heterogeneity in.PSI
Rurainski (1981), using isolated broken chloroplasts with
ferredoxin and NADP as substrates, showed that the total pool of
P700 ban be divided into at least two smaller pools. These pools
differ in their relaxation times and magnitudes and are proposed
to have different functions in photosynthetic electron transport.
This showed a heterogeneity in the reaction centre of PSI. In
contrast to PSII, the antenna size of PSI has previously been
thought to b~ fairly homogeneous. However, recent studies have
shown that there exists a heterogeneity in PSI as well with
respect to antenna size. (Andereasson et al, 1988) . · Under green
light illumination, the antenna size of PSI of the oC vesicles
(PSioe) was 40% larger than that of PSI of the B (PSI8 ) vesicles
(Svensson et al, 1991) . The oe and .B vesicle were suggested to
originate from grana and stroma lamellae, respectively
(Andereasson et al, 1991). A heterogeneity was also reported in
their localization; PSioC being located in the periphery of grana
and PS t 8 in the stroma lamellae (Svensson et al, 1991).
1.2.1.2.7 Plastocyanin
Plastocyanin, a copper containing peripheral membrane
protein is localized on the luminal ~urface of thylakoids (Katoh,
1977; Haehnel et al, 1981). The monomeric form of this protein
has a molecular weight of about 10.5 KDa (Katoh, 1977; Boger,.
1978). It is a flattened barrel like structure with dimensions of
4. Ox3. 2x2. 8 nm (Coleman et al, 197 8) . The X-ray structure of
plastocyanin shows that the Cu atom is coordinated with distorted
tetrahedral geometry by one Cys, one Met and two His residues.
Plastocyanin mediates the electron transport between Cyt b6-f
complex and PSI.
16
1.2.1.2.8 ATPase-ATP synthase
This complex comprises intrinsic protonopore CF0 , and an
extrinsic enzyme CF1 , \\·~ i ~h catalyzes ATP synthesis and
hydrolysis. CF 1 also serves as a plus to prevent uncontrolled
leakage of protons through CF0 . Chloroplast '-'l'P synthase is
located in the unstacked portions of the thylakoid memb.c;;;:,,c_:_ Cr'0 has four sub- units, I (18-19 KDa), II (16 KDa), III (8 KDa) and
IV (27 KDa). (Hudson and Mason, 1988). All subunits are coded by
the chloroplast genome exc~pt subunit II, which is coded by
nuclear genome ( Ne'J,:Son et al, 1980; Westhoff et al, 1985) .
Subunit III forms hexamer, which appears as rods in the eiectron
microscope. (Fromme et al, 1987). It also forms a proton channel
and contains the binding sites of DCCD. ( Sigrist-Nelson et al,
1978; Sebald and Hoppe, 1981). It is suggested that proton pore
made by subunit III is stabilized by the interaction of one of
the alpha-helix cf the subunit II polypeptides. The carboxy
tcr~~n~~ ~f subunit I, which protrudes into the stroma, provides
an anchor for CF1 attachment (Otto and Berzbom, 1989). Thus CF0 serves a dual purpose; very rapid and specific proton conductance
through the membrane and CF1 binding. CF1 is comprised of five
subunits, designated oe, B, i , b and € , present in the ratio of
3:3:1:1:1 ·(Stratmann and Bickel-Sand Kotter, 1984). The
~subunit has a molecular mass of 55-56 kDa. This subunit contains
adenylate binding site, which may occur at some part of the~/B
interface. B subunit has a molecular weight of 52-54 kDa. Both
~and B are encoded in chloroplasts. The isubunit has a molecular
mass of about 3 7 KDa and encoded by nuclear genome. The most
clearly defined function of t is in regulation of ATP synthesis
activity. This is achieved by oxidation and reduction of Cys
residues. The b subunit ranges from 21 to 25 kDa and is nuclear
genome encoded. The function of the <£ subunit has been only
partly elucidated. Studies show that this subunit is required to
block the leakage of protons. Thus, it lS required for
17
photophosphorylation. However, removal of this subunit has no or
little effect on ATPase activity of CF1 . The € subunit, a 14-
kDa polypeptide, is a chloroplast- _encoded protein. This subunit . ~-· ......
has been attributed a :.o;.e . in the regulation of activity of
ATPase. Remov:'· ' c-,: S subunit causes a marked increase in the
A.TPase · a.::ti. "~'t.Y. The CF 1 forms a more or less globular head,
which is bound to the CF0 by weak electrostatic fofces (Sigrist
Nelson et al, 1978) on the thylakoid membrane surface.
1. 3. Chl a fluorescence analysis
Chlorophyll in organic solvents emits fluorescence with a
quantum yield of around 30-40 % (Latimer et al,
since the yield of photochemistry is very high
1956). However,
in vivo (around
90%}, the yield of fluorescence is only around 3-4% (Weber,
1960}. The light reactions saturate at high light intensities.
When added, the inhibitors of photosynthetic electron transport
block the flow of electrons at specific sites. Under both of
these conditions, photochemical yield decreases and the decreased
yield is accompanied by a complementary increase in the
fluorescence yield. As stated earlier Duysens and Sweer {1963}
showed that yield of fluorescence is regulated by the redox state
of PSII acceptor, Q (quencher of fluorescence in its oxidized
state}. The fluorescence yield and concentration of Q are not
linearly related. This is reflected in a sigmoidal rise of Chl a
fluorescence in presence of DCMU which blocks the flow of
electrons from QA to Q8 . The sigmoidicity arises as a result of
migration of excitation energy between PSII units (Joliot and
Joliot, 1964).
The relationship of Chl a fluorescence emission and redox
state of Q in vivo has been extensively studied and both the
kinetics and steady state measurements of Chl a fluorescence
18
have been used to get information regarding photochemical events
and other reactions.
The rate of fluorescence emission , F, is given by
(1.1}
Absorbed light
KF, Rate constant of fluorescence
K1 , Sum of rate constants of all competing reactions
that result in the return of the Chl molecule to ground state.
The most important of these deactivation rates are,
photochemical reaction (Kp), thermal deactivation (K0 ) and
excitation energy transfer to non-fluorescent pigments (PSI)
(KT) ' The fluorescence yield may, therefore, be expressed as,
Yield of photochemical conversion of energy is maximum
when KP>> Kp+K0+KT. For example when primary stable electron
acceptor of PSII (QA) is fully reduced (i.e. all PSII reaction
c~ntres are in the state, z+ P680 Pheo QA-), excitation of P680 can not result in stable charge separation (Kp=O). This state of
PSII reaction centres is known as closed state against an open
state where all the QA molecules are in oxidized state. Under
the closed state of PSII reaction centres, the yield of
deexcitation via fluorescence becomes maximum, (FM). The yield
under these conditions is around 3 to 5 fold of the minimal
fluorescence yield obtained when all the PSII reaction centres.
are open ( F 0 ) . The increase from F 0 (open state of reaction
centres) to FM (closed state of reaction centre) represents
variable fluorescence (Fv) and reflects the reduced state of QA,
i.e. (QA-) at any particular time.
19
1. 3.1 Chl g_ fluorescence emission characteristics
1.3.1.1 Room temperature measurements
Characteristics of Chl a fluorescence emission spectra
vary with the state and nature of photosynthetic apparatus.
Isolated thylakoids, intact chloroplasts and intact leaves at
room temperature show a characteristic predominant band with a
peak at about 685 nm and a shoulder at 735 nm (fig. 1.4A). As
stated earlier, this emission emanates mostly from PSII while the
contribution from PSI is quite small.
1.3.1.2 Low temperature measurements
At 77 K, the thylakoid membrane from higher plants and
green algae show three emission bands with peaks at about 685 nm
(F685), 695 nm (F695), and a predominant 715 to 740 nm band
((fig., 1.4b) (Govindjee, 1963; Bose, 1982)). Second-derivative
spectroscopy and curve fitting methods reveal four additional
bands at about 680 nm (F680), 705 nm (F705), 715-725 nm (F720)
and 735-745 nm (F735). F680 has been attributed to LHCII
(Vernotte et al, 1976; Rijersberg et al, 1979) whereas F685 is
assigned to core antenna of PSII (Gasanov et al, 1979). F695
arises as
recombine
luminescence when
(Briantais et al,
the separated charges
1986). Igekami and Ke
in PSII
(1984)
proposed that F705 originates from charge recombination in PSI
reaction centre (P700+ A1-). Core antenna and peripheral antenna
(LHCI) of PSI produce F720 and F735, respectively (Butler and
Kitajima, 1975a and b; Bose, 1982; Briantais et al, 1986; Siffel
and Sestak, 1988).
20
Fig. 1. 4 Typical fluorescence emission spectra of higher
plants thylakoids under unstacked conditions, A. Room
temperature Ch 1 a fluorescence emission spectrum, B. Low
temperature (77 K) Chl a fluorescence emission spectrum.
Fig. 1.5 Kinetics of Chl a fluorescence emission at room
temperature, A) Fast fluorescence induction transients in
isolated thylakoids. Broken line represents the transients
obtained in the DCMU poisoned thylakoids. B) Slow fluorescence
transients (in intact leaves); F0 , 'Minimal' level of
fluorescence; FM, 'Maximal' level of fluorescence; I, Inflection
point (intermediate level); D; Dip level; Sl and S2 represent,
Steady states levels 1 and 2 and Ml and M2 denote, Relative
maxima 1 and 2 M2; T, Terminal level.
lfl c ClJ ....... c
QJ
u c QJ
u V'l (lJ L
0 ::J
I.J...
>--iii c ~
c
i1J u c i1J u V'l i1J .._ 0 ::J -
LL
Fig. 1.4
600
Fig.1.5
® ~ON
I
-682 ® ®
( PS II) 695
(PS II I
685 ...
( PS I ) 735
700 800 700 800 '
Wave length ( nm)
® t OFF J ON
Fm p --- -- - - - --- -~
~ / p / M· I
M2 i I 1S1 I I I Fcj 52
L ~ 200 ms
OFF j
T
1. 3. 2 Kinetics of Chl ~ fluorescence emission
1.3.2.1 Fast fluorescence induction kinetics
Kautsky and Hirsch (1931), showed that when dark adapted
photosynthetic cells were illuminated with light, th~ yield of
Chl a fluorescence follows a particular time course, These
transient changes in the fluorescence yield are known as Kautsky
phenomenon. At physiological temperatures Chl fluorescence is
emitted· mostly from Chl associated with PSII with weak
contributions from PSI (Duysens and Sweers, 1963; Mathis and
Paillotin, 1981). Figure 1. SA represents a typical fast
fluorescence Chl a induction curve. The various symbols represent
the levels of fluorescence attained after a given time period of
illumination. The .F0 represents the basal level of fluorescence
emissions, originating from light harvesting antenna (LHCII)
when all PSII re~ction centres are in the open state (Telfer et
al, 1983). There are a variety of technical problems in measuring
F0 , precisely. For the determination of F0 , rapid transients
should be captured using a device such as a digital Oscilloscope,
transient recorder or a microcomputer attached with an analogue
to-digital signal converter. An electronic shutter with fast
opening time of the order of 2 ms is usually used. The data
points captured by the detector at the end of opening of shutter
is an operational measure of F0 . The intensity of excitation
light within this time period is assumed to be too weak to induce
photochemistry. A data sampling rate of 10 KHz (i.e. 1 data point
per 100 us) may permit measurement of a point which may be taken
as a reliable measure of F0 . This point is the meeting point of
extrapolated lines of the initial variable fluorescence rise and
of F0 rise. However, it is difficult to consider it to be the
true F0 . This problem may be overcome, at least, in principle, by
the use of modulated fluorometers where fluorescence yield can be
measured by exciting with a modulated light of low intensity
21
which is assumed to be too weak to induce any· photochemical
event. In these instruments also, sensitivity of detection puts a
limit for choosing a light of sufficiently weak intensity for
such purpose. Thus most instruments measure a ''so called " F0 , a
value that closely approximates the true F0 . It is termed as Fi
(for F initial). Fi can be taken as F0 if its yield does not
depend .on the intensity of exciting light (Munday and Govindjee,
1969; Lavorel and Etienne, 1977) and is not quenched by added ...
electron acceptors like bCBQ (Cao and Govindjee, 1989). 'I'·~
represents fluorescence intensity at the first inflection point.
Melis (1985) suggested that 0 to I rise represent an increase in
the variable fluorescence yield due to PSIIB centres. According
to Cao and Govindjee (1989), the oro phase of the fluorescence
transients is contributed by the inactive PSII centres i.e.
centres which are slow in the reduction of Q8 . Fluorescence
decrease from I to D is indicative of the oxidation of QA or
electron transfer from QA to Q8 . D to P rise reflects reducti6n
of QA to QA-. Majority of photosynthetic systems can not attain a
maximum value of fluorescence (FM) even at a high intensity of
light so as P level is often lower than FM, which is attained by ~
the addition of DCMU to the sample (Arnold and Sherwood (1957).
1.3.2.2 Slow fluorescence induction kinetics
After reaching the level P, Chl a fluorescence level
decreases slowly through points S and M to a steady state
terminal level T ((fig. 1.5b) (Papageorgiou, 1975; Mohanty and
Govindjee, 1974; Briantais et al, 1986)). Since these transient
points are attained in a time scale of several seconds after
illumination, the fluorescence induction is termed to be slow. P
to T decline of Chl a fluorescence has been shown to result due ~
to two independent quenching mechanisms; photochemical and non
photochemical.
22
1.3.2.2.1 Photochemical quenching ~ of Chl ~ fluorescence
This quenching occurs due to oxidation of QA which in turn
results from a high rate of non-cyclic e~ectron transport.
Modulated fluorometers permit measurement of slow fluorescence
induction of Chl a with repetitive application of saturation
light pulses. These saturation pulses imposed during the course
of fluorescence (Kautsky transients) make it possible to resolve
the photochemical and non-photochemical components of
fluorescence ·quenching (Schreiber et al, 1986).
a typical slow induction curve of Chl a
application of saturation pulses. The dark
Figure ·1. 6 shows
with repetitive
adapted state is
characterized by absence of non-photochemical quenching and
maximal photochemical quenching as all PSII reaction centers are
open in dark. At this state, fluorescence yield is defined as F0 .
When a brief saturation pulse (duration -500 ms of intensity,
2000 fE.m- 2 .s-1 ) is given at this stage, all PSI! reaction
centres become closed and system attains a state of maximum
fluorescence which in fig. 1. 6 is shown by FM. The point FM
represents the maximal yield of variable fluorescence when all QA
molecule are in the reduced state. The yield of FM, therefore,
consists of maximum yield
fluorescence (F0 ) and variable
period, following the flash,
stage if the actini6 light
of two components constant
fluorescence (Fv>· During the dark
reduced QA are oxidized. At this
is switched on for fluorescence
induction, the system attains a level of variable fluorescence,
(Fv), the yield of which depends on the intensity of actinic
light used. At any given intensity, Fv is suppressed compared to
the ma~ima 1 variable fluorescence ( Fv) M, by the amount of
fluorescence quenching.
The quenching is caused by two independent mechanisms, the
23
coefficients of which consist of two parts, qQ and qE. To
differentiate between these two, saturation flashes are given
during the Chl · a fluorescence induction. Following each
saturating pulse, fluorescence is pushed to (Fv>s because qQ is
eliminated. (Fv}s is, therefore, expressed as,
(Fv} s 'is less than (Fv}M, because of among other
factors, the generation of a proton gradient and its associated
quenching (qE} so that,
Using this technique, Schreiber et al (1986}, derived
equations to determine the value of qQ and qE at any point of
induction curve for variable fluorescence (Fv).
qQ = [ <Fv> s- <Fv> l I <Fv> s
qE = [(FV)M-(Fv)g]/(Fv)M
Thus qQ and qE bear a direct relationship to _ Chl a
fluorescence so that qE follows the lowering of· fluorescence
yield by the development of the proton gradient and qQ reflects
the degree of redox state of QA.
1.3.2.2.2 Non-photochemical
fluorescence
quenching
qE arises because of an increase in the trans-thylakoid
proton gradient (Govindjee et al, 1967; Murata and sugahara,
1969}. It is formed in the light and relaxes in the dark within
2-10 minutes (Horton and Hague, 1988; Quick and Stitt, 1989). qE
24
Fig.
Fig. 1.6
F.--+ m --------------
0
J
\.
'""--....... _
-----~~------------
' saturating _ e_ul~e- __ _
t measuring
beam
1--20 s --1
t actinic
beam
qE ·(F)m
----qa· (~~
Fv
-------+
·(F)m
(F)s
1.6 Definition of quenching coefficients etc. by
Schreiber et al ( 1986). F0 : Fluorescence displayed by a dark
adapted leaf in very weak modulated light, (Fv)M: Maximum
variable fluorescence first seen when a pulse of saturating
actinic light is applied, (Fv): Variable fluorescence induced due
to continuous actinic light, (Fv) 5 : Peak fluorescence attained
when pulses of saturating light is applied in presence of
continuous actinic light, qE: Non-photochemical quenching
coefficient, qQ: Photochemical quenching coefficient.
has been assigned a role both in the protection of PSII apparatus
from excess light (Krause et al, 1982) and in the dynamic control
over the rate of electron transport through PSII (Weis and Berry,
1987; Genty et al, 1989).
Photochemical and non-photochemical quenching are the two
main mechanisms which cause the decline of Chl a fluorescence
yield from P to T. However, other than these two, depletion of
cation levels, phosphorylation of LHCII and generation of reduced
pheophytin has also been shown to cause Chl a fluorescence
quenching.
1.4 THERMOLUMINESCENCE
Thermoluminescence results due to the emission of light
induced by heating of preilluminated photosynthetic materials
Arnold and Sherwood, 1957). When illuminated, photosystem
reaction centres undergo charge separation. These charges are
quickly removed away, to other neighbouring species. This
process, known as charge stabilization, ensures that the charges
do not recombine . .If same sample is frozen quickly just after or
during the illumination, the system gets frozen in the charge
separated state. If the sample is then warmed slowly, opposite
charges come near to each other and recombine.
provides the necessary energy for this process
Temperature
(Arnold and
Sherwood, 1957). The recombination of charges produces an
excited state of Chl a which finally deexcites to produce
luminescence. Light emission from various photosynthetic
materials have been observed to have at least 13 bands in the
range of temperature from 77 K to 373 K (Sane and Rutherford,
1986). A lot of variation has been reported in the position and
number of thermoluminescence (TL) peaks in the glow curves (Sane
and Rutherford, 1986). The characteristics of different TL peaks
25
are summarized in table 1.3.
1. 4.1 Effects of electron transport inhibitors which act at
the acceptor side of PSII
pattern
transport on thermoluminescence
All the herbicides which interrupt electron transport
between QA and Q8 (like DCMU) modify the glow pattern (Arnold and
Azzi, 1968; shuvalov and Litvin, 1969). Since DCMU can be taken·
as an ·ideal representative of this class of herbicides, the
effect of DCMU on TL has extensively been studied. Treatment of
chloroplasts with other herbicides which have site of action
similar to DCMU, also cause
curve pattern (Droppa et al,
et al ( 1982) , found out
characteristic changes in the glow
1981; Horvath et al, 1986). Demeter
that in presence of DCMU, band B
disappears arid a new band (Q band) emerges at a temperature lower
than B. They also found that peak position and activation energy
of this band vary depending on the group of herbicide used.
Treatment with urea, pyridazinone, phenyl carbazide and DSPD
shifts the Q band at +6°c whereas triazines and hydroxyquinone
give a band at o0c. Phenolic herbicides (hydroxybenzonitrite and
dinitrophenol) shift the Q bani to -14°C (Droppa et al, 1981).
All the above mentioned groups of herbicides inhibit electron
transport at the same site i.e. between QA and Q8 (Pfister and
Arntzen, 1979; Demeter et al, 1979). Thus, the source of negative
charge needed for recombination to generate thermoluminescence is
QA in all the cases. On the other hand, it is generally
considered that activation energy and peak positions are defined
by the redox span between the donor ( +ve) and acceptor ( -ve)
molecules participating in the charge recombination (Crofts et
al, 1971; Vass et al, 1981). To explain this discrepancy, three
explanations have been put forward.
1. Other than inhibiting at donor side of PSII, herbicides also
26
Table 1.3 Thermoluminescence in Plants
Peak
Approximate emission temperature (°C) Origin
z
I (A)
II
-160
-70 (variable)
-20
-0.0 (D or Q)
III 10
IV(B) 25
V(C) 48
No. Author
?
+ -Z Q8 (?) and/
+ -or Z QA (?)
Signal II-slow
1. Sane et al, 1974 2. Arnold and Azzi, 1968 3. Vass et al, 1984 4. Inoue et al, 1977 5. Inoue and Shibata, 1978 6. Rutherford and Inoue, 1984 7. Demeter et al, 1982
Characterstics
Emission max. 740 nm (1); excitation max. blue light (2)
Oscillates with preflash number; maxima coincide with s 1 (3) Insensitive to Tris (4) and NH20H (3)
Oscillates with preflash number maxima coincide with s3 (5)
Insensitive to Tris (6)
Oscillates with flash number when diuron is added after excitation· maxima coincide with s 2 and s 3 (7,8) Sensitive to Tris and tetranitro methane treatment (9)
Formed in leaves or in the _presence of DCCD (9,10) Sensitive to Tris and NH 2oH (11)
Oscillates with flash number maxima coincide with s 2 and s 3 (5) Sensitive to Tris and NH 20H treatment ( 4, 12)
Oscillates with flash number when diuron is added after excitation; maxima coincide with s 0 and s 1 (13) Insensitive to Tris treatment (14)
No. Author
8. Demeter, 1982 9. Sane et al, 1983b 10. Sane et al 1 1977 11. Sane et al, 1983a 12. Rozsa and Demeter, 1982 13. Demeter et al, 1984 14. Inoue et al, 1977
shift the redox potential of S states.
2 . There may be one intermediary species existing in between
P680 and QB and herbicides of above mentioned three groups
inhibit electron flow at the site of these intermediary
acceptors.
3. The three group of herbicides bind to different position in
the QB binding protein and thus cause different extent of shifts
in the redox state of QA. This difference in shift in the redox
potential of primary acceptor presumably produces difference in
the peak position and redox potential.
1.5 stoichiometry of
photosynthesis
reaction centres in oxygenic
As recently as 1980, it was widely accepted that PSII and
PSI centres existed in 1:1 ratio in the thylakoid membranes.
Experimental data obtained from the measurements of the
electrochromic band-shift at 518 nm supported this assertion
(Schliephake et al, 1968).
In recent years, development of many techniques such as
sensitive absorbance difference spectrophotometry (Melis and
Brown, 1980), measurement of QB/herbicide binding sites in the
thylakoid membranes (Vermaas and Arntzen, 1983; Jursinic and
Stemler, 1983), the Cyt b559 content (Lam et al, 1983; Murata et
al, 1984) and amounts of Mn and Z (Babcock et al, 1983; Yocum et
al, 1981), have permitted direct quantitation of integrate
components in the reaction centre of PSI! (QA, P680 , Phe) and PSI
(P760 ). Repetitive flash illumination of photosynthetic material
in vivo and in vitro leads to oxidation of water. Oxygen yield
per flash, measured from the experimental data of such
experiments have also been used to quantitate the number of PSI!
units (Whitmarsh and Ort, 1984; Myers et al, 1980; Kawamura et
27
al, 1979; Chow et al, 1990) . Quantitative measurements with
thylakoids from spinach and from other sun-adapted plants showed
the presence of one PSII reaction centre per 350 Chl (a+b)
molecules and the presence of one PSI reaction centre per about
600 Chl (a+b) molecules (Melis, 1991). This shows a photosystem
stoichiometry of PSII: PSI, 1.7: l.O (Melis and Anderson, 1983;
Melis and Brown, 1980; Melis and Harvey, 1981). Moreover, the
measurement regarding the ratio of PSII/PSI varied in diverse
photosynthetic species.
The information as available regarding the organization of
thylakoid membranes thus suggest that photosynthetic organisms
have the ability to regulate the photosystem stoichiometry in the
thylakoid membrane and, thereby, to adjust and optimize the
process of light absorption and linear electron transport {Melis
and Brown, 1980; Whitmarsh and Ort, 1984; Jursinic and
Dennenberg, 1989; Melis, 1985; Ort and Whitmarsh, 1990).
1.6 Dynamics of thylakoid structure and function
1. 6.1 stater-state!! transition
Light energy absorbed by the antenna molecules is
distributed between the two photosystems. Since photosystems
absorb at different region of the spectrum of incident radiation,
any change in the quality of light causes an imbalance in the
distribution of excitation energy between PSII and PSI. Murata
{1969) and Bonaventura and Myers {1969) independently showed that
thylakoid membranes have an in vivo regulatory mechanism, which
corrects for any imbalance in the excitation of photosystem II
reaction centres. This process by which antenna molecules can
reorient themselves to direct excitation energy to either of the
28
photosystem reaction centres is known as state change. There is
now evidence (Bennett, 1979b; Horton and Black, 1980; Allen et
al, 1981; Barber, 1982) that such regulatory mechanism (state
change) which compensates for the imbalance in excitation energy
distribution involves phosphorylation/dephosphorylation dependent
reorganisation of thylakoid membranes. The phosphorylation and
dephosphorylation takes place in the thylakoid membranes by a
membrane bound kinase and phosphatase, respectively in a
reversible fashion (Bennett, 1979a). The preferred substrate for
these reactions is the surface exposed domain of LHCII. The
activity of kinase is regulated by the redox state of PQ pool
(Bennett, 1979a}. How many kinase(s) are involved in LHCII
phosphorylation is not certain. There are observations which
support ·a single thylakoid protein
et al, 1981; Coughlan and Hind,
multiple kinase (Lin et al, 1982;
1991). Under the conditions
kinase (Berinett, 1979b; Horton
1987; Bennett et al, 1988) or
Farchaus et al; 1985; Bennett,
when PSII mediated electron
transport is high· and PQ pool is reduced, phosphorylation of
LHCII polypeptides takes place. Under the conditions when PSI
activity is higher or there. is no PSII · electron transport,
depletion of reduced PQ pool takes place which leads to kinase
inactivation. As a consequence, dephosphorylation of LHCII
occurs. Phosphorylation of LHCII
residues on the outer surface
polypeptide occurs at threonine
near the N-terminus. This
increases the net negative charge on the surface of LHCII
complex. A negative surface charge destabilizes the aggregation
of these complex in appressed regions of thylakoid membranes
(Barber, 1980; Kyle and Arntzen, 1983) and has been assumed to
trigger the lateral migration of LHCII from grana lamellae to
stroma lamellae (Andersson et al, 1982; Kyle et al, 1983). Under
these conditions excitation energy is preferentially directed to
PSI and thylakoids are said to be in stater. Under Stateii
condition, LHCII is dephosphorylated and functions as antenna
of PSII reaction centre. Thus, the stater - stateii conversion is
29
regulated by redox level of PQ, which in turn depends, as well as
decides, the turnover rate of the two reaction "centres through
phosphorylation and dephosphorylation. It is proposed that this
is the regulating mechanism by which plants adapt to changing
wavelengths of light (Allen et al, 1981; Bennett et al, 1991;
Allen, 1992).
1.7 Review of Literature
1. 7.1 Pyridazinones as photosynthetic herbicides
Figure above Rl
common
. ;
.. '
structure for pyridazinone
derivatives. Depending on the various substitutions, R1, R2 and
R3, more than forty derivatives of pyridazinone have been.
synthesized and tested for their interaction with plant systems
(St. John et al, 1979). Though some of the derivatives like
pyrazon ( 5-amino-4-chloro-2-phenyl pyridazin-3-one) are used in
agriculture for weed control, most of the pyridazinone
derivatives are used as experimental photosynthetic herbicides
because they can affect structure or function of photosynthetic
apparatus in many ways. In general effects of pyridazinone
herbicides on photosynthesis can be classified as follows,
1. Inhibition of photosynthetic electron transport
2. Alteration in the fatty acid composition of thylakoid
membranes lipid.
3. Inhibition of pigment formation
4. Changes in the 'structure-function' relationship of
thylakoids.
30
1.7.1.1 Inhibition of photosynthetic electron transport
Many of the substituted pyridazinone compounds have been
shown to inhibit Hill reaction in isolated chloroplasts. (Hilton
et al 1969; Tischer and Strotmann, 1977; Mannan and Bose,
1985a). They are also known to inhibit light induced o2 evolution
from isolated leaf mesophyll cells (Hilton et al, 1969) and
intact algae cells (Herczeg et al, 1979; Karapetyan et al, 1981).
However, there is a large variation in the pyridazinone
derivatives in their efficiency to inhibit photosynthetic
electron transport in isolated chloroplast. The concentration of
SAN 6706 to obtain 50% inhibition of electron flow (I 50 ) in
isolated chloroplast was 5 pM while for SAN 9789 it was 90 pM.
The r 50 value reported for SAN 97_85 were 14 p.M (Hilton et al,
1969) and 20 fM (Mannan and Bose, 1985a). Thus,, pyridazinone
compounds are 100-150 fold weaker inhibitors of photosynthetic
electron transport as compared to DCMU and atrazine. This is
attributed to their 100-150 fold lower binding constant as
compared to DCMU (Tischer and Strotmann, 1977). The competition
experiments have shown that pyridazinones and DCMU inhibit
electron transport by interaction with the same component (QB
protein); the mode of action being similar as well (Tischer and
Strotmann, 1977).
The substructures as mentioned below have been identified
as features common to all inhibitors which inhibit PSII dependent
electron transport (Buchel, 1972; Trebst and Harth, 1974)
Pyridazinone compounds fulfill these requirements,
1. the group >N-C-CX, Where X = 0 or N, but not S and
2. a hydrophobic residue in close vicinity to the above
mentioned group
A model which encompasses biochemical, biophysical and
structure-activity considerations for PSII herbicides considers
31
that all these compounds are non-reducible analogues of
plastoquinone or its semiquinone anion (Gardner, 1989). The model
suggests that sp2-carbon of the essential element of the
herbicide corresponds to the sp2 carbon of the quinone carbonyls,
and thus there are two possible sites to which this element may
bind. The essential features of Gardner's model are,
1. Plastoquinone molecule is asymmetric and, therefore, receptor
should also have asymmetry.
2. A hydrophobic domain in the vicinity of essential element of ~
the herbicide should be present, which corresponds to isoprenoid
tail of the plastoquinone. A hypothetical picture depicting how
one of the PSII inhibitors (atrazine) supposedly acts on PSII
shown in fig. 1.7.
is
1.7.1.2 Alteration in the fatty acid composition of thylakoid
membrane lipids
Substituted pyridazinone compounds e.g. SAN 9785 cause an
increase in the linoleic acid content of thylakoid membrane
lipids (St. John, 1976; Frosch et al, 1979; Ashworth et al, 1981
and Mannan and Bose, 1984), when the plants are grown in their
presence. In vitro studies using 14c acetate and leaf discs
have shown that this specific increase in the linoleic acid was
due to the inhibition of desaturation of linolenic acid to form
linoleic acid (Murphy et al, 1980; Willemot et al, 1982). Out
of forty-four substituted pyridazinones tested for their ability
to induce a specific decrease in 1 inolenic acid content, SAN
9785 was found to be the most efficient (St.John, 1979).
1.7.1.3 Inhibition of pigment formation
Depending on the nature of substitution in pyridazinone
32
\
.....
Fig. 1.7
Fig. 1.7 Schematic figure of the plastoquinone/herbicide binding
pocket of the 01 protein. Dashed lines represent hydrogen bonds;
dotted lines represent hydrophobic interactions, A.
Plastoquinone binds to the Dl protein, accepts two electrons and
two protons, and is released as plastohydroquinone. B. Atrazine
binds to the 01 protein and prevents the binding of
plastoquinone. Adopted from Fuerst and Norman (1991).
compounds, these herbicides cause bleaching of photosynthetic
pigments to varying degree in higher plants and algal cells
(Kleudgen, 1979; Kummel and Grimme, 1975) . Urbach et al ( 1976)
have proposed certain features in the structure of the herbicide
which are necessary for efficient bleaching activity. SAN 9785 is
expected not to have any bleaching activity on this basis. In
fact SAN 9785 did not cause any significant bleaching in many
plant species upto a concentration of 100 fM (Urbach, 1976; St.
John, 1976; Mannan and Bose, 1985b). Therefore, SAN 9785 is
considered to be a non-bleaching or weakly bleaching herbicide
(St. John, 1976). The bleaching activity of pyridazinone
compounds is highly dependent on light intensity. When seeds ~ere
germinated and seedlings were raised in presence of 100 pM SAN
9789, carotenoid biosynthesis was inhibited by 99% (Lehoczki et
al, 1982). Therefore, under these conditions the plants can grow
only if the light intensity is kept extremely low and thus avoids
Chl bleaching. The mechanism of bleaching of photosynthetic
pigments by pyridazinone compounds is still not certain
(Karapetyan, 1993). However, three hypothesis have been proposed
to explain the bleaching phenomenon.
1. Su.bsti tuted pyr idazinone compounds inhibit carotenoid
biosynthesis, directly. Sandmann et al ( 1980) showed that SAN
9789 inhibits phytoene synthetase. Ben- Aziz and Koren ( 1974)
noted that SAN 6706 interfered with the cyclization reactions in
the biosynthesis of carotenoids whereas Bartels and McCullough
(1972) and Bartels and Watson (1978) found that this compound
inhibits dehydrogenation reactions. Carotenoids are shown to have
a protective role against chlorophyll bleaching (Frosch et al,
1979) . Since coloured carotenoids are decreased in presence of
SAN 6706, chlorophyll molecules get photodegraded.
2. According to the second hypothesis, pyridazinone derivatives
do inhibit carotenoid biosynthesis. However, this hypothesis does
not consider that carotenoids have a protective role against the
bleaching of chlorophylls. Instead, the hypothesis considers that
33
carotenoid biosynthesis is highly coordinated with chlorophyll
biosynthesis. Though this type of control mechanism was seen in
Euglena gracilis by Vaisberg and Schiff ( 1976) it was not found
in higher plants in the studies of Frosch et al (1979) and Pardo
and Schiff (1980).
3. The third hypothesis considers a more generalized effect of
pyridazinones. According to this hypothesis, pyridazinone
derivatives cause a decrease in the content of 70 S ribosomes.
This in turn causes a decrease in the synthesis of enzymes which
are responsible for carotenoid and chlorophyll biosynthesis
(Lichtenthaler and Kleudgen, 1977). Direct evidence in support of
this hypothesis is, however, still lacking.
1.7.1.4 Changes in the structure-function
thylakoids
relationship of
The structural and functiona 1 changes rn the thylakoids
induced in response to substituted pyridazinone tre:atment vary
to a great extent and depend upon the derivative of pyridazinone
used. Herczeg et al (1980) reported an increase in the light
induced oxygen evolution in Chlorella cells grown in presence of
sublethal concentrations of SAN 6706, SAN 9785 and SAN 9789.
Plants treated or grown in presence of SAN 9785 exhibit several
a 1 terations in the structure and function of their thylakoids.
Plants grown in presence of SAN 9785 show an increased stacking
(Khan et al, 1979) whereas those grown in presence of SAN 6706
and SAN 9789 show a disorganization of thylakoid membrane
structure (Laskay et al, 1983; Karapetyan, 1993). Many
investigators have reported an increased emission of Chl a
fluorescence and a higher rate of PSII catalyzed electron
transport in thylakoids isolated from SAN 9785 grown plants in
comparison to thylakoids of control plants on Chl basis (Bose et
al, 1984; Leech et al, 1985; Mannan and Bose, 1985; Laskay and
34
Lehoczki, 1986). It was suggested that such increase in rate of
PSII electron transport rate in SAN 9785 grown wheat seedlings
occurred due to a preferential synthesis of PSII units in these
plants (Bose et al, 1984). These results suggested that PSI! to
PSI ratio increased in thylakoids of SAN 9785 grown plants (Bose
et al, 1984). Such an increase in the ratio of PSII/PSI explains
the increase in the relative area occupied by appressed membranes
in SAN 9785 grown plants as revealed by ultrastructural studies
done using electron microscopic studies (Khan et al, 1979; Leech
et al, 1985; Bose et al, 1992). However, this effect seems to be
specific to SAN 9785 as SAN 9789 (norflurazon} treatment have
been reported to result in a drastic decrease in PSI! to PSI
ratio in the thylakoids of barley plants (Lehoczki et al, 1982;
Karapetyan, 1993}.
In general, the alterations in the thylakoid membrane
structure and function in the plants grown in presence of
·sublethal concentrations of one of the pyridazinone derivatives,
SAN 9785 can be summarized-in the following way,
1.
2 •
3 •
4.
5.
Characteristic
Parameters
Chl ajb
CPII/CPI
PSI to total
Chlorophyll
QA/PQ
F0 and Fv/Fo
35
Response Reference
Decreased ( 1} , (2)
Increased ( 1) , (2)
Decreased ( 3)
Decreased ( 3)
Decreased ( 3)
~I
I '
Number
(1)
(2)
(3)
Reference
Leech et al, 1985
Mannan and Bose, 1985a and b
Bose et al, 1984
Based on the energy flux theory for biomembranes
(Strasser, 1978), Graf et al (1986) have proposed a model of the
modified organisation of the photosynthetic system in the leaves
of SAN 9785 treated plants. According to model the t:hylakoid
membranes of treated plants exhibit following changes compared to
thylakoids of control plants.
1. A decrease in the excitation energy transfer (:spillover)
from PSII to PSI
2. A decrease in co-operativity (grouping) between PSII units.
3. Inhibition of LHCII phosphorylation induced changes in
electron transport.
4. Decrease in the antenna s1ze of PSII
Above mentioned changes in functional organizat.ion of
thylakoids of SAN 9785 treated plants were speculated to occur
because of an altered lipid matrix in these plants. However,
these conclusions
temperature (77K)
biochemical evidence.
were based on room temperature and low
fluorescence studies only, and lacked
SAN 9785 grown plants also show an inhibition of cation
mediated modulation of structure-function relationship of
thylakoid membranes. Bose et al (1992) showed an inhib~tion of
cation regulation of room temperature Chl a fluorescence emission
and absorption properties of thylakoids in SAN 9785 grown plants.
Based on these observations Bose et al ( 1992) proposed that
cation induced changes in the excitation energy distribution were
inhibited in the thylakoids isolated from Pisum sativum plants
grown in the sublethal concentration of SAN 9785. Simu11:aneous
measurement of PSII and PSI fluorescence emission kinetics at 77K
36
~------------------------ -~~------------~
showed that the ability of cations to regulate excitation energy
spillover from PSII to PSI was also inhibited in the thylakoids
of SAN 9785 grown. The authors correlated these functional
changes with the ultrastructural changes in the thylakoid
membranes of SAN 9785 grown plants and concluded that the
observed inhibition of cation induced spillover changes occurs
due to loss in the ability of thylakoids to undergo unstacking in
low salt medium.
1.8 Adaptive
membranes
herbicides
changes in
of plants
the chloroplasts
grown/treated
thylakoid
with PSII
Plants grown or treated with sublethal concentrations of
herbicide have a partially inhibited PSII electron transport
capacity. This generates a significant imbalance of electron
transport between PSII and PSI. Such imbalance in electron
transport between PSII and PSI is suggested to induce an
adaptive change in the structure-function relationship of
thylakoids (Melis et al, 1985; Melis, 1991} as a result of which
thylakoid structure in the plants ·grown in presence of sublethal
concentration of PSII herbicides and strong light appears very
much similar to shade (low intensity} grown plants (Leong and
Anderson, 1984; Davies et al, 1986; De la Torre and Burkey,
1990). The physiological changes induced in herbicide grown
plants are, therefore, commonly said to produce a shade
phenotype.
Various studies have been conducted to observe the
herbicide induced physiological changes in the thylakoid
structure and function. Lichtenthaler (1979), studied the effect
of two biocides, bentazon and triadimefon on the growth response
of raddish seedlings (Raphanus sativus L.}. Plants grown in
37
presence of fungicide, triadimefon (10- 5M) induced strong light
growth response and the formation of sun-type chloroplasts. The
total chlorophyll content, ratio of Chl ajb and content of prenyl
quinones all increased in triadimefon treated plants. On the
contrary, PSII herbicide, bentazon induced a shade type
adaptation, when the plants were grown under a regime of strong
light intensity. The content of chlorophyll, carotenoids and
ratio of Chl ajb, all decreased in bentazon treated plants
relative to control plants. However, the ratio of Chl a f prenyl
quinones and xanthophyll/carotenoides increased in bentazon
treated plants. Such effects of bentazon were strongly dependent
on the light intensity under which the plants were grown as
chloroplast composition and organization in the plants grown at
low light intensity was affected very little (Lichtenthaler,
1979). Shade type adaptation in bentazon treated plants were
also characterized by increased formation of chloroplast lamellae
and grana stacks. Lichtenthaler et al ( 1982) latE!I' showed that
bentazon treated plants grown under strong light conditions show
low levels of CPI+CPia in comparison to that shown by control
plants. Fedtke (1979) obtained similar results when plants were
treated with metabenzthiazuron (MBT) instead of bentazon.
Chloroplasts of MBT-treated plants exhibited a higher degree of
stacking of thylakoids (Fedtke et al, 1977) as well as lower Chl
aj b ratios, lower amounts of b-carotene and prenylquinones
(Kleudgen, 1978). It was later shown that a shade type
adaptation similar to that induced by bentazon and MBT can also
be induced by DCMU (Lichtenthaler et al, 1980).
Similar kinds of results were
treated with atrazine. Matteo et
obtained when plants
al (1984b) showed
were
that
cul ti vat ion of Spirodela oligorrhiza on a sublethal dose of
atrazine induces a shade type of response. Chloroplast structure
of plants grown in presence of sublethal concentration of
herbicide was very much similar to that in triazine resistant
plants. Vaughn and Duke ( 1984) found out that chloroplasts of
38
atrazine susceptible (S) biotypes could be modified to
ultrastructural phenocopies of those in resistant (R) biotypes by
treatment with sublethal levels of the PSII inhibiting
herbicides, bentazon, diuron and prometon. In a recent study, De
la Torre and Burkey (1992) reported the physiological effects of
sublethal (0.07 mM) concentrations of atrazine on thylakoid
membrane activity and composition of barley. Thylakoids from
plants treated with sublethal concentrations of atrazine showed
an increased level of the LHCII and lower levels of CPI in
comparison to that shown by thylakoids of control plants. The
number of PSII and PSI,reaction centre and Cyt b 6 /f.complex per
unit Chl were not a·ffected by sublethal concentrations. of
atrazine. This suggests an overall effect of atrazine treatment
on redistribution of chlorophyll associated with PSI to PSII with
no effect on the number of thylakoid membrane protein complexes
associated with electron transport (De ld Torre and Burkey,
1992).
The shade tY.pe adaptations of thylakoids by sublethal
concentrations of herbicides is also shown to be induced . in
cyanobacteria. Koenig, (1987 a,b) showed that shade .type·
appearance can be induced· in Anacystis nidulans in high light
intensity in the presence of sublethal conc;:entrations of DCMU
type inhibitors. The cell types grown in presence of sublethal
concentrations of herbicides· were characterized by higher
concentrations of both Chl a and phycocyanin , (PC) per cell and,
in addition, by a higher ratio of PC to Chl ,as compared to the
corresponding control cells (Sun-type).
Various workers have tried to explain: the physiological
significance of adaptive changes induced in 'the thylakoids of
plants grown in presence of sublethal concentration of herbicide.
Mel is et al ( 1985) proposed that such changes are regulatory
mechanism of the plants to balance the electron transport between
PSII and PSI. Fedtke (1977; 1979) assumed that the adap~ive
changes are produced due to the lower level of soluble sugars.and
39
other photosynthetic products, as a result of the strongly
inhibited photosynthesis. From the observations that exogenous
cytokinins induce the formation of sun-type chloroplasts and the
, plants grown at high light intensities contain more cytokinins
t:han shade-plants (Kohler, 1977), Lichtenthaler et al, 1980
assumed that PSII-herbicides decreases the endogenous cytokinin
level. Lichtenthaler (1979) interpreted the increased formation
of chloroplast lamellae and grown stacks in bentazon treated
plants as a part of an inactivation mechanism for the herbicide
through providing more binding sites within a chloroplast. Mattoo
et al (1984b) proposed that adaptive reorganization of thylakoid
components in plants grown in presence of sublethal concentration
of PSII herbicide (atrazine) may be a compensatory mechanism for
maintenance of a functional interaction of the proteins and
lipids of the PSI! complex.
As discussed above, the physiological changes produced in
the thylakoids of plants grown in presence of sublethal
concentrations of herbicides are generally believed to arise as a
result of an in situ inhibited PSII activity which generates an
imbalance of electron transport between PSI! and PSI (Melis,
1985; Melis, 1991). However, Koenig (1990) showed that the shade
type adaptation grown under Anacystis nidulans under strong
light in the presence of sublethal concentrations of DCMU-type
inhibitors is not due to an imbalance of electron transport
because such changes can not be prevented or reverted by using a
electron donor like thiosulphate. Since thiosulphate is known
to feed electrons at the Cyt b6 /f complex (Utkilen, 1976;
Peschek, 1978; Koenig, 1990), it is expected to compensate for
any imbalance between PSII and PSI created by in situ inhibition
of PSII electron transport by herbicide.
40
1.9 About this investigation
Upon reviewing the SAN 9785 action on photosynthetic
system of higher plants suggests that SAN 9785 is an effective
inhibitor of electron transport in isolated thylakoids in vitro;
the site and mode of action of this inhibitor is, however, not
well elucidated. The in vivo action of SAN 9785 on photosynthesis
has also been investigated by various workers (Bose et al, 1984;
Mannan and Bose, 1985b; Leech et al, 1985; Karapetyan, 1993; Bose
et al,. 1992). Thus, SAN 9785 becomes an useful tool to study the
structural and functional changes produced in the thylakoid
membranes in . response to in situ partial inhibition o,f PSII
mediated electron transport. However, among the pyridazinone
derivatives this compound has maximum ability of increasing the
ratio of saturated to unsaturated fatty acids with no or ~ittle
changes in the pigment content in plants grown in presence of
pyridazinone compounds (St. John et al, 1979). Thus, any
alteration in the structure and function of thylakoid membranes
in SAN 9785 grown plants may be considered to arise as a result
of partial inhibition of PSII mediated electron transport or \due
to changes in the lipid environment of the thylakoid membranes.
It was shown by other workers (Murphy · et al, 1985) that
alterations in the fatty acid composition of thylakoid membranes
in response to SAN 97"85 varied depending upon the plant species
used and P. sativum shown to be resistant against such changes·.
In spite of this, P. sati vum remains highly susceptible to SAN
9785 dependent photosynthetic changes .. Thus, P. sativum as an
experimental system, offers a special advantage where the';
structural and functional changes induced in the thylakoid
membranes in response to SAN 9785 treatment can be considered to
arise only due to the ability of SAN 9785 to cause in situ.
partial inhibition of PSII electron transport and not due to the
SAN 9785 mediated fatty acid changes.
The subject matter reviewed in relation to adaptive
41
- '
capacity of plants to the stress given in the form of a sub
lethal concentration of PSII herbicide suggests that treated
plants undergo an adaptive change in the organizat~ion of their
thylakoids so that structural organization of thylakoids of
treated plant become very similar to the thylakoids of shade
grown plants. Though the information is available regarding the
nature of herbicide induced changes, not much information is
available regarding the structure-function ?relationship of
thylakoids in the plants grown or treated with herbicide and
associated alterations in the excitation energy distribution
between photosystems.
In view of this, we were encouraged to focus attention on
adaptive capability of thylakoids of P. sativum plants treated
with SAN 9785, especially on the potential for change in
composition and function (long term changes) and the capacity to
undergo short term changes. This essentially involved,
1. Studies regarding further characterization of site of action
of SAN 9785, the PSII inhibitor used in this study.
2. Measurement of the extent of in situ inhibition of PSII
electron transport rate
the extent of stress.
in SAN 9785 treated plants to evaluate
·3. Characterization of structure-function relationship of
thylakoids isolated from plants treated with SAN 9785.
4. To determine the dynamic ability of thylakoids of SAN 9785
treated plants to undergo state-transition and phosphorylation
mediated energy distribution.
Our experimental protocol involved transferring either 11
day old seedlings of P. sativum or 41 d old seedlings of
Chenopodium album to a 125 fM solution of SAN 9785 in 0.5 S
Hoagland solution, where plants were allowed to grow for further
72-84 h. This type of treatment is different from those. of
previous investigations (Leech et al, 1985; Bose et al, 1984;
Mann an
plants
and Bose, 1985a and b;
were grown in presence
42
Bose et al, 1992) , where the
of SA.N 9785 from the onset of
germination. In the latter treatments, it was extremely difficult
to identify the sites of action responsible for changes in the
photosynthetic apparatus. For instance, certain developmental
changes that occur in the chloroplasts during maturation may
overlap with the adaptive changes that occur due to partial
inhibition of PSII. Further, presence of SAN 9785 may affect the
normal process of development, itself. H~nce, in the present
investigation, normally grown seedlings were treated with SAN
9785 as mentioned above. Since the possibility of developmental
changes being incorporated in the photosynthetic apparatus is
excluded, adaptive structural and functional changes in the
thylakoids of SAN 9785 treated plants can be considered to arise
due to an in situ partially inhibited PSII mediated electron
transport.
43