dispersibility of phospholipids and its optimization for
TRANSCRIPT
Accepted Manuscript
Dispersibility of phospholipids and its optimization for efficient production ofliposomes using supercritical fluid technology
Faheem Maqbool, Peter M. Moyle, Kristofer J. Thurecht, James R. Falconer
PII: S0378-5173(19)30245-5DOI: https://doi.org/10.1016/j.ijpharm.2019.03.053Reference: IJP 18237
To appear in: International Journal of Pharmaceutics
Received Date: 2 February 2019Revised Date: 23 March 2019Accepted Date: 25 March 2019
Please cite this article as: F. Maqbool, P.M. Moyle, K.J. Thurecht, J.R. Falconer, Dispersibility of phospholipidsand its optimization for efficient production of liposomes using supercritical fluid technology, International Journalof Pharmaceutics (2019), doi: https://doi.org/10.1016/j.ijpharm.2019.03.053
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1
Dispersibility of phospholipids and its optimization for efficient production
of liposomes using supercritical fluid technology
Faheem Maqbool1, Peter M. Moyle
1, *, Kristofer J. Thurecht
2, James R. Falconer
1, *
1School of Pharmacy, The University of Queensland, Woolloongabba, QLD 4102, Australia
2The Centre for Advanced Imaging (CAI), The University of Queensland, Brisbane, QLD
4072, Australia
*Co-correspondence:
[email protected] (J.R.F) Tel: +61(4) 312 73844
and
[email protected] (P.M.M.) Tel: +61(7) 334 61869
2
Graphical Abstract:
3
Abstract
Liposomes are promising delivery vehicles and offer the added drawcard of being able to be 5
made functional to target tissues such as cardiac muscle and cancerous cells. Current methods
to manufacture liposomes need to be improved and supercritical fluid (SCF) technologies
may offer a solution. Herein, the dispersibility of six different phospholipids (PLs):
determined using supercritical carbon dioxide (scCO2), and 1,2-distearoyl-sn-glycero-3-
phosphocholine (DSPC) showed highest post-processing dispersibility, while 1,2-dioleoyl-sn-10
glycero-3-phosphocholine (DOPC), 1,2-dioleoyl-sn-glycero-3-phosphoethanolamine,
(DOPE) and 1,2-dioleoyl-3-trimethylammonium-propane (DOTAP) showed no dispersibility
at all in scCO2 at the assessed experimental conditions. The zetasizer results showed that the
SCF conditions at 37 °C, 250 bar and 200 RPM for 60 min provided nanoparticles with
narrowest polydispersity index (PDI) and spherical shaped as shown by cryo-transmission 15
electron microscopy (Cryo-TEM) supported these results. The mean diameter of liposomes
using the SCF method for DSPC-PEGylated and DOPC-PEGylated liposomes was 98.3±3.3
nm and 124.5±4.1 nm, while using thin film method it was 153.6 ± 4.5 nm and 131.3±3.4
nm, respectively. The stability of liposomes stored at different temperatures (25 °C, 4 °C and
-20 °C) using SCF technology was better over a period of 3 months. The current study would 20
provide green alternative method, less laborious, save time and energy.
Keywords: Green technology, Zwitter-ionic, Electron microscopy, Particle engineering, Drug
delivery, Size distribution
4
1. Introduction 25
Liposomes are nano/micro-sized spherical shaped vesicles, composed of an inner aqueous
layer enclosed by a phospholipids (PLs) bilayer. PLs are the structural building blocks of
liposomes that ; (i) are biocompatible (Daraee et al., 2016) (ii) have hydrophilic head groups
and hydrophobic tail (Torchilin, 2005) and have a similar structural composition to cell
membranes in the human body. Liposomes can be unilamellar or multilamellar, based on the 30
number of lipid bilayers; therefore, their size can vary from nano- to micro-meter range
(Gortzi et al., 2007; Joshi and Müller, 2009). Liposomes are useful drug delivery system, as
they can deliver either hydrophobic or hydrophilic drugs, even possible for both at the same
time.
Liposomes have had commercial success in delivering anticancer drugs at cancerous 35
tissues (Brannon-Peppas and Blanchette, 2012). As of writing, the FDA has approved 15
liposomal formulations on the market, seven are used for cancer therapy (Bulbake et al.,
2017). Research on liposomes in recent years has been rapidly growing, and liposomes have
progressed from basic delivery systems to immune evaded and targeted systems (Akbarzadeh
et al., 2013). Liposomes take advantage of tumor leaky microenvironment; thus liposomal 40
nanoparticles (100-400 nm) cross the endothelium gaps with the increased permeation effect
and enhanced retention at tumor site due to poor lymphatic drainage. In addition, stealth
liposomes possessing polyethylene glycol (PEG) can increase the circulation time of
liposomes by reducing immune-mediated clearance of liposomes by the reticoendothelial
system. The effects of polymers associated with different PLs (e.g. charge, liposome particle 45
size and stability) have shown promising results in targeting different types of cancerous cells
(He et al., 2010). Liposome-based drug delivery systems are also desirable due to being non-
toxic and biodegradable within the human body (Gregoriadis and Ryman, 1971; Liu and
Boyd, 2013; Sharma and Sharma, 1997).
5
Several methods have been developed to produce liposomes. These include the 50
original Bangham method, also known as the thin film method (Bangham et al., 1965),
reverse phase evaporation, ether injection (Deamer and Bangham, 1976; Schieren et al.,
1978), freeze thaw (Pick, 1981), detergent depletion (Torchilin and Weissig, 2003),
membrane contactor (Charcosset and Fessi, 2005), microfluidics (Jahn et al., 2007), post-
formation/homogenisation, and emulsion methods (Batzri and Korn, 1973; Deamer and 55
Bangham, 1976). Each method has its own drawbacks, such as the use of large amounts of
organic solvents, multiple steps (thus time consuming), environmental waste issues, and
stability complications. Supercritical fluid (SCF) technology has the potential to provide an
alternative to address these problems. SCF as a solvent method can be utilised with less/no
use of organic solvent, thus a green/er technology, and operating can use cheap, readily 60
available and non-flammable gas like carbon dioxide (Alnaief and Smirnova, 2011; Prosapio
et al., 2015), producing a solvent-free end product.
Supercritical carbon dioxide (scCO2) is one of the most commonly used SCFs due to
its low critical temperature (Tc) i.e. approx. 32 °C (305 Kelvin) in pure form, which is less
likely to cause degradation to a thermolabile compound and only requires a small amount of 65
heat (energy), thus adding to the green method banner, its critical pressure (Pc) in pure form
is approx. 73 bar (1059 psi) (Esfandiari, 2015; Poliakoff et al., 2014; Zheng et al., 2016). It is
interesting to note, that scCO2 methods produce a zero-net change in atmosphere amounts of
CO2, as the CO2 used in processing is gathered from industrial sites. In addition, SCF
technologies can be scaled up, so simpler lab-bench equipment is sufficient for optimising 70
methods that can be extrapolated to much larger sized equipment (Cansell et al., 2003;
Cardea et al., 2010; Hakuta et al., 2003; Huang et al., 2005; Kim et al., 2007; Shariati and
Peters, 2003; Wu et al., 2015). These desirable attributes create a need to explore new
methodologies using scCO2 in the field of liposomal drug delivery and nanotechnology.
6
Although, use of acCO2 has been previously reported in many studies for natural product 75
extraction from plants and in the area of polymer chemistry (Ewing and Kazarian, 2018;
Lorenzen et al., 2017; Nuchuchua et al., 2017; Stadie et al., 2015; Trucillo et al., 2017), the
gap needs to be filled in the field of liposomal drug delivery and nanotechnology. The
minimal work has been done on the dispersibility of different charged groups of PLs in
scCO2 and production of liposomes using these PLs and SCF technology. Although some 80
studies using other techniques have been published before but all of these studies have used
anti-solvents techniques and other PLs. Thus, there is need to provide novel data for
manufacturing liposomes using six PLs and SCF technology. In this study, SCF has been
used as main solvent and co-solvent has been used to improved dispersibility of few PLs.
The aim of this study was to determine the dispersibility of six different charged PLs 85
in scCO2 to optimize the production of liposomes using a SCF method. The PLs were
selected based on those used in the market and classed as either having a +ve or -ve charged
head group or zwitterionic, viz having opposite dual charges. There were six PLs selected; a.
DSPC, b. DOPC, c. 1,2-dihexadecanoyl-sn-glycero-3-phospho-(1'-rac-glycerol) (DPPG), d.
1,2-dioleoyl-sn-glycero-3-phospho-(1'-rac-glycerol) (DOPG), e. DOTAP, f. DOPE. (See 90
Table 1). In addition, the PEGylation of these PLs was evaluated for scCO2 dispersibility and
to produce stealth liposomes. These were DSPC-PEG and DOPC-PEG liposomes, which
were produced with the similar molar ratio using SCF technology, as available in the market.
The scCO2 conditions were screened for effects on PL dispersibility and included;
varying temperature, pressure, time, and their effects were evaluated on the particle size, PDI 95
and liposome morphology. Moreover, liposomes produced using SCF technology were
compared to the traditional thin film method. Moreover, for stability studies, the liposomes
stored at different temperatures (25 °C, 4 °C and -20 °C) were analysed in terms of change in
the PDI and particle size for the period of 3 months.
7
2. Materials and methods 100
2.1. Materials
DSPC, 1,2-dihexadecanoyl-sn-glycero-3-phospho-(1'-rac-glycerol) (DPPG), 1,2-dioleoyl-sn-
glycero-3-phospho-(1'-rac-glycerol) (DOPG), DOPE, DOPC, DOTAP and 1,2-distearoyl-sn-
glycero-3-phospho- ethanolamine-N-[methoxy(polyethylene glycol)-2000] (ammonium salt)
(DSPE-PEG-2000) were purchased from Avanti Polar Lipids, Alabama, USA. Ethanol and 105
carbon dioxide liquid cylinder were obtained from Merck Millipore (Kilsynth, VIC,
Australia) and BOC Australia, respectively. All solvents used in the study were of analytical
or high-pressure liquid chromatography (HPLC) grade.
2.2. General method of processing phospholipids using SCF technology.
110
In this section, the general method to process PLs using scCO2, for determination of
dispersibility and manufacture liposome has been described in detail. The modifications of
different parameters including optimization for screening the best processing conditions is
explained in the later sections. The stainless steel (SS) vessel (360 grade with 60 mL
capacity) was used as reaction/processing vessel for the experiment. At first, the SS vessel 115
was sealed, and liquid CO2 was injected by a syringe pump and converted into scCO2. The
CO2 becomes scCO2 above Tc and Pc and for each experiment, a specific temperature and
pressure was used, as explained in the following sections in detail. It took 2-3 min to fill the
CO2 into SS vessel when steady state was achieved. The overhead stirrer fitted above the SS
vessel used to rotate the peddle (hanging in the high-pressure SS vessel) for mixing and 120
provide agitation and the temperature of the system was controlled by the heating jacket and
monitored using an inlet probe passing through the SS vessel (see Figure 1, schematic
diagram for experimental set-up). At the end of experiment, the vessel was slowly
8
depressurized to atmospheric conditions and sudden drop of pressure led to the formation of
CO2 gas from scCO2, which was then released back into the air. 125
2.3. Determination of dispersibility of phospholipids using subcritical and supercritical
carbon dioxide
To determine dispersibility of all PLs, based on the different head groups charge; DSPC,
DPPG, DOPG, DOPE, DOPC and DOTAP were processed using liquid (subcritical) and
scCO2 in separate experiments. For all experiments 20 ± 0.1 mg of the PLs were used in 130
individual set of experiment. The processing conditions were set at 37 °C and 60 bar (for
liquid/subcritical CO2) and 37 °C with 250 bar (for scCO2) with 200 RPM, in a 60 mL high-
pressure SS vessel for 60 min. The steps of this experiment were performed in similar order,
as explained above in the general method section. At the end of experiment, to
assess/determine the dispersibility of PLs in scCO2 bird-eye images of the inner section/lining 135
of SS vessel were collected before processing (0 min) and after depressurization.
9
Figure 1: Schematic diagram of the experimental setup to determine the dispersibility of
phospholipids (PLs) for production of liposomes using scCO2 in a high-pressure stainless
steel (SS) vessel. 140
2.4. Manufacturing conventional liposomes using SCF technology
The SCF technology was first used in the current study to manufacture conventional/non-
stealth liposomes of the all PLs (See Table 1). To manufacture 5 mM (94: 6 molar ratios
(PLs: DSPE-PEG-2000) of conventional liposomes of six PLs, the experiments were 145
performed at 37 °C, 250 bar, 200 RPM in 60 mL of scCO2. After completion of experiment,
the thin film of proliposomes was formed, which was processed for hydration to manufacture
liposomes using 5 mL of normal saline for 30 min above transition temperature (TT) (60 ˚C
for DSPC and 50 ˚C for all other PLs). To perform hydration of the thin film of
10
proliposomes, 5 mL of the normal saline was added into the high pressure stainless steel 150
vessel and placed on the hot plate to perform hydration and stirring (100 RPM using
magnetic stirrer/hot plate, at temperature above TT of respective PLs) to manufacture
liposomes.
2.4.1. Asses the effect of transition temperatures
To see the effect of temperatures above TT of the PLs, additional experiments were 155
performed for DSPC (at 56 °C) and DPPG (at 42 °C) (see Table 1 for TT of PLs). The
particle size analysis of the liposomes was performed and compared with the liposomes
manufactured using temperature below TT of PLs.
2.4.2. Effect of co-solvent
To assess the effect of co-solvents with scCO2 on the dispersibility of PLs, such as: DOPC, 160
DOPE and DOTAP; 0.5 mL (~ 0.74 % of the total mass ratio of PLDs and DSPE-PEG-2000)
of ethanol was used with 60 mL of scCO2. To do this, first PLs were dissolved in ethanol and
then the solution was added into the high-pressure SS vessel. The similar SCF general
method was used, as explained in above section at 37 °C, 250 bar, 200 RPM. After
depressurized of the of SS vessel proliposomes were hydrated using 5 mL of normal saline 165
above TT of the PLs for 30 min.
2.4.3. Effect of sonication
To see the effect of sonication on particle, size, population distribution and morphology of
the manufactured liposomes, sonication was performed using Grant XUB18 Ultrasonic Water
Bath for 15 min. To analyse these effects the particle size analysis was performed of the 170
manufactured liposomes before and after sonication and compared accordingly.
11
Table 1. Transition temperatures and surface charges of the selected phospholipids (PLs)
used in the study.
175
2.5. Manufacturing PEGylated liposomes using SCF technology
To manufacture PEGylated liposomes of DSPC and DOPC using SCF technology, same
method was used, as described in the above section. The conditions were 37°C, 250 bar, 200
RPM in 60 m L of scCO2. The initial data of dispersibility and conventional liposomes using
scCO2, provided further direction to manufacture PEGylated liposomes. The composition of 180
PLs and DSPE-PEG used to manufacture liposomes was like the market available stealth
liposomes (DOXIL®
). DSPC with DSPE-PEG-2000 (94: 6 molar ratio) and DOPC with
DSPE-PEG-2000 (94: 6 molar ratio) were dispersed into 60 mL of scCO2 (SS vessel) and
processed at various conditions detailed in the following sections (Naik et al., 2010). For
DOPC PL, 0.5 mL of ethanol was used as co-solvent with 60 mL of scCO2. The unsaturated 185
PL e.g. DOPC show maximum drug loading capacity for hydrophobic drugs compared to the
saturated PL. The basic reason of this high loading is associated with wide lipid bilayer,
compared to the saturated PL (Hong et al., 2015). To do this, first DOPC was dissolved in
ethanol and the solution added into high-pressure SS vessel. The effect of different
modifications was studied and is explained in the following sections. 190
2.5.1. Effect of varying temperature and pressure
To see the effect of varying temperature, pressure on the hydrodynamic particle size and PDI
of PEGylated liposomes, number of experiments were performed with different combinations
of temperature and pressure. The conditions used were 100, 150, 250 and 300 bar processed
at constant temperature i.e. 37 °C in separate experiments. Moreover, DSPC-PEGylated 195
Type of PLs DSPC DOPE DOPC DOTAP DPPG DOPG
Charge on PLs
Zwitter-
ionic
Zwitter-
ionic
Zwitter-
ionic
Cationic Anionic Anionic
Transition
Temperature (°C)
55 -16 -17 5 41 -18
12
liposomes were also prepared at 56 °C (above TT) and 250 bar. The particle sizing data and
PDI of the liposomes was taken after each experiment and compared accordingly.
2.5.2. Effect of time and sonication
To see the effect time (experiment time) on particle, size, distribution and morphology,
separate experiments were performed at 30 and 60 min with similar pressure and temperature 200
combinations, as explained above. In addition, effect of sonication was evaluated using Grant
XUB18 Ultrasonic Water Bath for 15 min. The sonication was performed after hydration and
manufacturing of PEGylated liposomes. In addition, particle size and PDI of the PEGylated
liposomes was determined before and after sonication and compared accordingly.
2.6. Manufacturing PEGylated liposomes using thin film (Bangham) method 205
To prepare (5 mM of liposomes with 94: 6 molar ratio (PLs: DSPE-PEG-2000)) DSPC-
PEGylated and DOPC-PEGylated liposomes using the thin film method, DSPC with DSPE-
PEG-2000 and DOPC with DSPE-PEG-2000 were first dissolved in 10 mL of ethanol. The
organic solvent/ethanol was removed by rotary evaporation at 60 C and 50 C (above TT of
respective PLs) in 30-40 min, respectively. When thin film was formed, it was allowed to dry 210
in vacuum desiccator overnight. The following day, thin film was hydrated using 5 mL of
normal saline at 60 C and 50 C to prepare DSPC-PEGylated and DOPC-PEGylated
liposomes respectively. Sonication was then performed, using Grant XUB18 Ultrasonic
Water Bath for 15 min, to see the effect on hydrodynamic particle size, PDI and morphology
of liposomes before and after sonication. 215
2.7. Particle analysis
2.7.1. Mean size and distribution by dynamic light scattering (DLS)
The hydrodynamic particles size and PDI of liposomes were measured by dynamic light
scattering (DLS) Zeta-Sizer Nano ZS (Malvern, UK). Disposable cuvettes with 1 mL of the 5
13
mM suspended liposomes were taken to measure particle size and PDI. All runs were 220
performed in triplicate and each run comprised of 100 measurements at 25 °C.
2.7.2. Morphological analysis by cryo-TEM
Liposome samples were imaged by cryo-TEM. The samples of prepared liposomes were
applied to 300 mesh EM carbon coated film grids (EMS, Hatfield PA,USA) using a FEI
Vitrobot Mark IV plunge freezer set (100% humidity) at 22 C. The samples were vitrified 225
using thin ice and plunged by liquid ethane at -180 C. Frozen grids were cryo-transferred
into a FEI Tecnai F30 transmission electron microscope (FEI, Einhoven, Netherlands) using a
Gatan cryo holder. The microscope was operated at 300 kV and the samples were imaged at -
179 C under low dose conditions using a Gatan K2 summit camera (Gatan, Pleasonton CA,
USA). This was operated in counting mode at a dose rate of 9 e/px/s, a 10 s total exposure 10 230
s and a dose fractionation of 0.2 s. For acquisition of the image, Serial EM was used. The 50
frames were later motion corrected using the ‘Align’ function of Serial EM (Hyatt, 1984;
Mastronarde, 2005; Vuitton, 2009).
2.8. Stability study
Liposomes were tested for physical stability at different storage conditions. For this, that 235
manufactured liposomes using both SCF and conventional methods i.e. DSPC-PEGylated and
DOPC-PEGylated (5 mM with 94: 6 molar ratios in normal saline) were stored at -20 °C, 4
°C and 25 °C. To compare the results PDI and the hydrodynamic mean particle size (Z-
average) were recorded immediately after manufacturing and over a period of 3 months.
2.9. Statistical analysis 240
GraphPad Prism version 7.04 (GraphPad software Inc., San Diego, USA) was used and the
data is presented as mean ± standard deviation (S.D). Two-way analysis of variance
(ANOVA) was carried out, followed by Sidek post hoc multiple comparison test to determine
the statistical difference among different groups.
14
3. Results and discussion 245
3.1. Dispersibility of PLs in subcritical and supercritical CO2
The results showed that DSPC has the highest dispersibility in scCO2, while DPPG and
DOPG showed “moderate” and “the least” dispersibility respectively (see Figure 2). The
dispersibility of chemical material have a significant role in physiochemical interaction and
processes. Different simulations, and calculative formulas have been developed previously, 250
to predict the solubility or dispersibility of different materials/compounds in scCO2 (Bian et
al., 2015; Del Valle and Aguilera, 1988). Although prediction of solubility is helpful to some
extent, its accuracy and application is not that much reliable though. Therefore, in the current
study to determine the dispersibility of six types of PLs, a method was developed and for this
birdseye view images of the SS vessel were collected before and after processing with scCO2 255
at the assessed supercritical conditions. PLs, like DOPE, DOPC and DOTAP were not
dispersed in scCO2 (were named as scCO2 non-dispersible PLs) thus a co-solvent i.e. ethanol
used to manufacture liposomes (see following sections). In addition, it was also found that
none of the PLs showed dispersibility at subcritical conditions in liquid CO, thus for the later
experiments just supercritical conditions were used to manufacture liposomes using scCO2. 260
The visual images taken at 0 min and after depressurization (at 60 min) of scCO2 SS
vessel showed no change, while PLs such as DSPC, DOPG and DPPG showed different
levels of dispersibility in scCO2 (Figure 2). It is fact that scCO2 has high solubility power
because it has viscosity like that of liquid and diffusivity power like that of gases. The extent
of dispersibility of dispersible PL’s (DSPC, DPPG and DOPG) was determined based on the 265
visual changes and area of the SS vessel covered by layer of dispersed PLs. It is obvious from
the Figure 2 that DSPC showed the highest dispersibility compared to DPPG (showed poor
dispersibility) and DOPG (showed very poor dispersibility). The estimated semi-quantitative
results of the visual dispersibility of the PLs in scCO2 are explained in the Table 2. DOPC
15
was further selected to manufacture PEGylated liposomes, based on the better particle size 270
range and PDI compared to conventional DOPE, and DOTAP liposomes and results are
detailed in the following sections.
It can be derived from the results that the higher the TT of PLs, the more they show
dispersibility in scCO2. The more dispersibility shown by DSPC could be referred to strong
bonds between long hydrocarbon chains and CO2 interactions. Such interactions are due to 275
strong van der Waals forces and quadruple induced dipole with hydrocarbon chains of PLs.
As a result, long fatty acyl chain helps CO2 to be surrounded by more hydrocarbon chains
with improved distribution of PL molecules (Shin-ichiro et al., 2005; Zhao et al., 2015). In
addition, cationic PL did not show any dispersibility, while zwitter-ionic and PLs with higher
TT value i.e. DSPC showed a visible dispersibility. 280
16
Figure 2. Birdseye view of SS vessel containing PLs, pre- and post-exposure to scCO2.
Pre-exposures are (1a) DSPC, (2a) DPPG and (3a) DOPG and post-exposures to scCO2 are
(1b) DSPC, (2b) DPPG and (3b) DOPG. 285
17
Table 2. Visual estimation of dispersibility using a semi-quantitative/visual dispersibility of
phospholipids (PLs) in scCO2.
No. PLs Visual dispersibility in scCO2
1 DSPC completely dispersible
2 DPPG ≥ 50 % dispersible
3 DOPG ≤ 50% dispersible
4 DOPC not dispersible
5 DOPE not dispersible
6 DOTAP not dispersible
290
3.2. Manufacturing conventional (non-stealth) liposomes using SCF technology
In the first set of experiments, at the highest density (893 kg/dm3
based on pure CO2) at 37 °C
and 250 bar, the conventional/non-PEGylated liposomes were manufactured using six types
of PLs and the results of particle size are shown in Figure 3 A and B. The effect of different
conditions on particle size of manufactured liposomes using scCO2 explained in the following 295
sections.
3.3. Asses the effect of transition temperatures
The effect of varying temperature showed that below TT (See Table 1 for TT values and
Figure 3 A for results) with 250 bar pressure liposomes had showed nano-range, for both
DSPC and DPPG PLs and particle size was significantly lower (i.e. **, where **: P ≤ 0.0) 300
compared to the liposomes manufactured above TT of the used PLs (see Table 1 for TT
values). The lesser of density on increasing the temperature is one of the reason, which result
in reduction of the solubility power of scCO2 and hence end in increase of the particle size of
the liposomes. In addition, the SCF generally does not follow the ideal gas law, meaning that
the trend of increase/decrease in viscosity and density behaves differently from normal fluids 305
and varies at every point upon changing the temperature and pressure (Span and Wagner,
1996).
18
3.4. Effect of co-solvent
The ethanol, as a co-solvent with scCO2, used to assess its effect on (PLs e.g. DOPE, DOPC,
DOTAP) solubility (of scCO2) and particle size of liposomes. The results of the particle size 310
analysis are presented in Figure 3 B. Based on the initial experiments of dispersibility, (as
described in the above sections) three PLs i.e. DOPE, DOPC and DOTAP did not show
dispersibility in scCO2, while DOPG showed “least” dispersibility. DOPE (inhibit endosomal
reuptake), and DOPC best suited for high drug loading and delivery of hydrophobic drugs,
while DOTAP (cationic), improve targeting of negatively charged cancer cells with enhanced 315
gene and DNA delivery effect (Zhang et al., 2004). At the end of depressurization
suspended/dissolved particles precipitated out after depressurisation (and proliposomes were
formed) which were hydrated to manufacture liposomes. Atomization and nucleation effect
during scCO2 processing with the aid of ethanol provided a uniform sized particle distribution
with nanoparticle size range (See Figure 3 B). The hydrodynamic particle size of DOPC, 320
DOPE and DOTAP liposomes was 557±17 nm, 642.5±44.5 nm and 233±25.5 nm
respectively. DOPC was further selected (from non-dispersible PLs) to prepare
stealth/PEGylated liposomes and to see the effect on particle size and morphology.
3.5. Effect of sonication
The results of the effect of sonication on particle size of liposomes are shown in 325
Figure 3. It was observed for DOPE, DOPC, DOPG and DOTAP conventional liposomes, the
particle size was significantly reduced (i.e. ***, where ***: P ≤ 0.001) after 15 min
sonication, which proved that sonication at the assessed conditions helped to reduce the
particle size of liposomes. The nano-sized liposomes are formed due to the formation of tiny
droplets called proliposomes. This could be due to interaction among the PL mixture, scCO2 330
and ethanol.
19
Figure 3. Particle size analysis of conventional liposomes using scCO2 at 250 bar, 200 RPM and
60 min (n=3 ±S.D) before and after sonication. (A) DSPC and DPPG liposomes using scCO2
below TT (37°C) and above TT (56 °C for DSPC and 42 °C for DPPG). (B) DOPG, DOPE, 335
DOPC and DOTAP liposomes using scCO2 at 37°C. Where **: P ≤ 0.01 and *** P ≤ 0.001
(Two way ANOVA with Sidek post hoc test).
3.6. Manufacturing PEGylated (stealth) liposomes using SCF technology
The particle size, morphological analysis and the stability studies of the PEGylated 340
liposomes manufactured using SCF technology are described in the following sections. The
process yield was also calculated using SCF method and it was found to be 83.65 %. This
could be associated due to depressurization at high pressure when SCF is released at last step
then it may take some particles outside of the vessel. This yield could be improved on large
scale SCF processing. Effects of different varying conditions on DSPC (a scCO2 dispersible 345
PL) and DOPC (non-dispersible PL in scCO2) PEGylated liposomes is explained in the
following sections.
3.6.1. Effect of varying temperature and pressure
The results of liposomes manufactured using different conditions such as: pressure
and temperature explained in Figures 4-5. It has been shown that at 37 °C and 250 bar the 350
liposomes had nano-range with better PDI of nanoparticles/liposomes. This could be due to
20
high density of CO2 i.e. 893 kg/dm3
at these conditions, which is very close to density of its
liquid and show high solubility. The higher density increases the solvation power of scCO2
and thus increases mass transfer rate, which reduces the particle size of liposomes. It has been
shown that the particle size of liposomes at 250 bar was significantly lower (see Figures 4-5, 355
for significant P values) than the other pressures (150, 200 and 300 bar) and the temperature
below TT reduced particle size range effectively, compared to the liposomes manufactured at
temperature above TT. The reduction in density of scCO2 on increasing pressure has been
described previously (Span and Wagner, 1996). So increasing the temperature did not
increase the density (i.e. solubility would reduce on increasing temperature at fixed pressure 360
of 250 bar) and hence particle size was bigger than the particle size of liposomes
manufactured at lower temperature.
3.6.2. Effect of time and sonication
The effect of time and sonication has been shown in Figures 4-5. It is obvious from
Figures that more experimental time i.e. 60 min provided better results in terms of particle 365
size and PDI compared to 30 min. In addition, the effect of sonication on particle size of
liposomes played a vital role and significantly reduced the particle size and PDI of liposomes.
The particle size of liposomes is inversely proportional to processing time and has been
reported elsewhere in the literature (Span and Wagner, 1996), which states that lengthy
processing time reduces the particle size more effectively. At constant temperature, the 370
increase in the pressure did not help in the reduction of particle size of DSPC-PEG and
DOPC-PEG liposomes.
21
375 Figure 4. Particle size optimization of DSPC-PEGylated liposomes using scCO2 at varying
conditions of temperature, time and pressure and effect of sonication (n=3 ± S.D). (A) DSPC-
PEG liposomes at 150, 200 and 250 bar after 30 min, below TT at 37 °C (for all pressures)
and above TT at 56°C (for 250 bar). (B). DSPC-PEG liposomes at 150, 200, 250 and 300 bar
after 60 min below TT at 37 °C (for all pressures) and above TT at 56°C (for 250 bar). Where 380
*: P ≤ 0.05 and ** P ≤ 0.01 (Two way ANOVA with Sidek post hoc test).
22
Figure 5. Particle size optimization of DOPC-PEGylated liposomes using scCO2 at varying
conditions of temperature, time and pressure and effect of sonication (n=3 ± S.D). (A) DOPC-
PEG liposomes at 150, 200 and 250 bar after 30 min and 37 °C. (B). DOPC-PEG liposomes at 385
150, 200, 250 and 300 bar after 60 min and 37 °C. Where * P ≤ 0.05, ** P ≤ 0.01 and *** P ≤
0.001 (Two way ANOVA with Sidek post hoc test).
3.7. Manufacturing liposomes using thin film method and comparison with SCF
technology 390
The results of the PEGylated liposomes manufacture using thin film method are explained
and compared with SCF technology in the following sections.
3.7.1. Particle size characterization
The particle size and PDI of the DSPC-PEG and DOPC-PEG liposomes manufactured using
thin film and its comparison with SCF technology using scCO2 (with high density at 250 bar 395
and 37 °C) is described in Table 3. The mean particle size diameter of DSPC-PEG and
DOPC-PEG liposomes using thin film method was 274.4±16.5 nm and 131.3±3.4 nm
respectively. The data shows that the mean particle size of the liposomes i.e. DSPC-PEG and
DOPC-PEG liposomes using SCF technology at 250 bar and 37 °C was 98.3±3.3 nm and
124.5±4.1 nm respectively. The particle size and PDI of the SCF processed liposomes was 400
23
relatively smaller, compared to conventional thin film method. (Table 3). The better PDI
results show that SCF assisted DSPC-PEG liposomes were homogenous with narrow range
of particle sizes, while liposomes manufactured using thin film method were of different
sizes/heterogeneous and size distribution graph also support and show the multiple size
populations of nanoparticles. The further reduction of particle size and PDI could be achieved 405
in conventional methods by using: sonication, homogenization or extrusion techniques.
Whereas particle size and PDI of the liposomes obtained using SCF method avoids the use of
such techniques for reduction of particle size and PDI (Park et al., 2012; Wagner and
Vorauer-Uhl, 2011). Moreover, SCF as a green technology could be better alternative to
traditional used methods, which would save time, avoid use large amounts of energy and 410
organic solvents, and also save environment from waste products (as produced by
conventional Bangham method). The particle sizing data and morphology of liposomes was
further confirmed by electron microscopy, detailed in the following section.
24
Table 3. Comparison of DSPC-PEGylated and DOPC-PEGylated liposomes manufactured using SCF and Bangham method. 415
No. Method
Composition and conditions
(PL + polymer + solvent/co-solvent &
volume)
Total time for
preparation of
liposomes (h)
Mean Particle
Size ± S.D
(n=3)
Mean PDI ± S.D
(n=3)
1 Thin
Film
DSPC and DSPE-PEG-2000 (94:6) + 10 mL
ethanol 24 – 32 153.6 ± 4.5 0.4 ± 0.02
2 SCF
DSPC and DSPE-PEG-2000 (94:6) 250 bar,
37 °C, 200 RPM 2 98.3 ± 3.3 0.2 ± 0.01
3 Thin
Film
DOPC and DSPE-PEG-2000 (94:6) + 10 mL
ethanol 24 - 32 131.3 ± 3.4 0.3 ± 0.01
4 SCF
DOPC and DSPE-PEG-2000 (94:6) + 0.5 mL
ethanol, 250 bar, 37 °C, 200 RPM 2 124.5 ± 4.1 0.2 ± 0.01
25
3.7.2. Morphological analysis using cryo-TEM
The images taken by cryo-TEM are shown in Figures 6- 7. Results showed that DSPC and
DOPC stealth/PEGylated liposomes manufactured using thin film and SCF technology were
spherical and nano-vesicles with absence of any aggregation. The particle size and 420
homogeneity observed by Cryo-TEM was similar to the results obtained by Zeta-sizer, with a
slight difference. This difference in the particle size obtained using DLS and Cryo-TEM
might be due to hydration shells surrounding liposomes, and show a bit larger particle size
using DLS machine when compared to the results obtained from cryo-TEM. The effect on
differences in the particle size due to hydration shells is well explained in the literature (Mahl 425
et al., 2011; Müller et al., 2004). The results showed that liposomes have unilamellar
structure for both SCF and thin film method but that manufactured using SCF method are
more smaller and have lower PDI compared to that manufactured using the thin film method.
This nanosize range could better help to cross the cell membranes and targeting the cancerous
cells, which would help to achieve increased intracellular uptake. The size distribution graph 430
in Figure 6 C, 6 D of DSPC-PEGylated liposomes showed that liposomes manufactured using
SCF method were homogenous with single population (PDI: 0.2± 0.01), whereas liposomes
manufactured using thin film method are heterogeneous with multiple sized populations
(PDI: 0.4± 0.02). The improved particle size reduction of SCF assisted liposomes is
associated with process of atomization and nucleation too. This could be reason when thin 435
film is hydrated then liposomes manufactured using SCF process are more better, and
homogenously dispersed as explained in the detail in the above sections. SCF of CO2 is
reason of atomization and nucleation of the liposomal nanoparticles and after hydration; the
manufactured liposomes were of better PDI with more reduction in the particle size compared
to thin film liposomes. SCF technology could provide a better alternative approach to 440
26
manufacture liposomes with number of benefits such as, use of less amount of organic
solvents, cheap, rapid and less intensive technique.
Figure 6. Cryo-TEM images and size distribution data by DLS of DSPC-PEGylated liposomes. (A)
Cryo- TEM image of DSPC-PEG liposomes prepared using thin film method (B) Cryo- TEM image 445
of DSPC-PEG liposomes, prepared using SCF technology at 250 bar, 37 °C, 200 RPM processed
for 1 h. (C) Particle size distribution graph of thin film-DSPC-PEG liposomes by Zetasizer (DLS
machine). (D) Particle size distribution graph of SCF-DSPC-PEG liposomes by Zetasizer (DLS
machine).
450
27
Figure 7. Cryo-TEM images and size distribution data by DLS of DOPC-PEGylated liposomes (A)
Cryo- TEM image of DOPC-PEG liposomes prepared using thin film method (B) Cryo- TEM
image of DOPC-PEG liposomes, prepared using SCF technology at 250 bar, 37 °C, 200 RPM
processed for 1 h. (C) Particle size distribution graph of Thin film-DOPC-PEG liposomes by 455
Zetasizer (DLS machine). (D) Particle size distribution graph of SCF-DOPC-PEG liposomes by
Zetasizer (DLS machine).
3.8. Stability study
The difference between stability results of the particle size and PDI of the liposome stored at 460
4 °C or – 20 °C was very less after 3 months. However, room temperature did not show
promising results in terms of stability of the liposomes. The results showed that liposomes are
best stable at 4 °C or – 20 °C (Table 4). While comparing the stability of DSPC-PEGylated
liposomes manufactured using SCF method with that of thin film method, it can be seen that
liposomes manufactured using SCF technology showed better stability. Summarizing this, the 465
changes observed in the particle size were minimal by SCF liposomes and were more stable
compared to thin film method. These stability results also match with that obtained by Otake
28
et al (Otake et al., 2006) and some other researcher (Aburai et al., 2011; Kadimi et al., 2007).
Static repulsion of the carbonic acids incorporated into the bilayer membrane, well explain
the long-term stability of liposomes prepared using scCO2 (Bothun et al., 2005). Liposomes 470
manufactured using thin film showed more increase in the particle size, and one of the
possible reasons could be oxidation of polyunsaturated acyl chains of lipids and hydrolysis of
ester bonds.
475
Table 4. Stability of DSPC-PEGylated and DOPC-PEGylated liposomes over the period of 3
months stored at different temperatures.
Mean= ±S. D, n=3
Liposomes Particle Size (nm) Storage
(°C)
Particle Size (nm)
Initial After 1 Month After 2
Months
After 3
Months
DSPC-
PEG- Film
153.6 ± 4.5 4 ± 2 157.8 ± 3.5 156.5 ± 5.4 158.2 ± 3.5
-20 ± 2 159.1 ± 4.34 163.8 ± 3.2 167 ± 5.25
25 ± 2 161.7 ± 3.4 165.1 ± 4.6 166.6 ± 4.6
DSPC-
PEG- SCF
98.3±3.3 4 ± 2 99.8 ± 2.5 98.3.5 ± 4.74 100.7 ± 3.8
-20 ± 2 100.8 ± 4.3 102.3 ± 2.6 102.4 ± 4.6
25 ± 2 102.8 ± 3.4 103.4 ± 5.1 104.3 ± 2.8
DOPC-
PEG- Film
131.3±3.4 4 ± 2 132.5 ± 5.5 137.5 ± 5.6 140.4 ± 4.6
-20 ± 2 136.2 ± 2.6 136.6 ± 3.31 138.8 ± 3.8
25 ± 2 138.4 ± 4.9 136.5 ± 4.9 145.4 ± 4.3
DOPC-
PEG- SCF
124.5±4.1 4 ± 2 122.4 ± 2.5 125.5 ± 3.6 126.4 ± 3.6
-20 ± 2 127.2 ± 3.5 126.6 ± 5.4 128.8 ± 2.9
25 ± 2 126.6 ± 3.8 127.2 ± 2.8 131.4 ± 3.9
29
4. Conclusion 480
In our study, the method was developed to determine the dispersibility of PLs and to
manufacture conventional liposomes from six types of PLs using SCF technology. The two
PLs (DPSC and DOPC) were selected to manufacture PEGylated/stealth liposomes using
scCO2 and results were compared with the liposomes manufactured using the thin film
method. It was observed that DSPE-PEG2000 caused reduction of particle size and PDI. The 485
method was optimized for best combination of processing time, temperature and pressure, to
manufacture liposomes and it was found that 37 °C, 250 bar for 1 h provided best results in
terms of particle size and morphology. DLS data and cryo-TEM images showed that SCF
mediated liposomes were better in particle size and morphology when compared with the thin
film method. The stability of particle size at various temperatures was tested which shows 490
that DSPC-PEG liposomes manufactured using SCF technology were more stable over the
period of 3 months. The data from this study provides original information about the
dispersibility and manufacturing of liposomes using SCF green technology and a better
alternative to traditional used methods; it is less intensive, rapid, nontoxic and easily scalable.
Our study provides a good starting point for future formulation studies and to manufacture 495
drug loaded liposomes using SCF technology.
5. Author information
All authors approved the final version of the manuscript.
Author Contributions
James Falconer and Peter Moyle conceived and designed the project. Faheem Maqbool 500
performed the experiments and wrote the manuscript. Kristofer Thurecht provided conceptual
input and revised manuscript.
30
Acknowledgement
Faheem Maqbool is a recipient of Australian Government Research Training Program 505
Scholarship from The University of Queensland, Brisbane, Australia. The authors thank
Professor Andrew K. Whittaker of the Australian Institute for Bioengineering and
Nanotechnology (AIBN), The University of Queensland, Brisbane, QLD 4072 Australia, for
his support and access to specialized equipment, including the SCF unit used in this research.
Conflict of interest 510
The authors declare no conflict of interest.
31
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