Mechanical and transport properties of chitosan-zwitterionic phospholipid vesicles
Graphical abstract
Introduction
Liposomes are vesicles formed by the self-assembly of phospholipid bilayers in an aqueous phase. Even as liposomes are increasingly used for controlled and targeted drug delivery, their detection and rapid clearance by the reticuloendothelial system is a major challenge [[1], [2], [3]]. To overcome this hurdle, several efforts have been reported where surface properties of liposomes were modified with both, natural and synthetic polymers [4].
Chitosan, a cationic linear polysaccharide composed of N-acetyl-d-glucosamine and β-(1,4)-linked d-glucosamine units has been widely used in drug delivery because of its biodegradability, biocompatibility, non-toxicity and mucoadhesive properties [[5], [6], [7]]. For instance, when compared to non-coated liposomes, oral administration of liposomes coated with chitosan (MW:150kDa) showed a 30 % increase in adhesion to the intestinal lining of male wistar rats [8]. Additionally, it was shown that chitosan-coated liposomes, which are negatively-charged at physiological pH, become positively-charged at acidic pH [9,10]. This pH sensitive property of chitosan was used to selectively improve cellular uptake efficiency of doxorubicin-loaded liposomes in tumors which have an acidic environment [11].
Interactions between chitosan and the liposomal phospholipid bilayer have been shown to change the thickness and charge of the bilayer as well as the size and polydispersity of the liposomes [12]. Electron paramagnetic resonance spectroscopic studies have shown that, while at a lower chitosan concentration the polymer chains are well-extended and their adsorption to the lipid bilayer leads to a reduction in membrane fluidity, at a higher concentration, the chitosan chains self-aggregate resulting in an increase in membrane fluidity [13,14]. Moreover, Quemeneur et.al demonstrated that the stability of pure and chitosan-decorated 1,2-dioleoy-sn-glycero-phosphocholine (DOPC) liposomes was adversely affected on reduction of pH or by increasing salt concentration of the suspending medium [10]. At an acidic pH of 4.5 and in the presence of chitosan, Henriksen and coworkers observed significantly higher aggregation of negatively-charged liposomes comprising of phosphatidylcholine (PC) and phosphatidylglycerol (PG) (PC:PG ratio 90:10), when compared to neutral liposomes made of pure PC [15]. The acidic pH below 4.5 is critical to chitosan solubility and its incorporation into liposomes. Mertins and Dimova concluded that at acidic pH, the chitosan chains become positively-charged and cause bridging of liposomes made of negatively-charged phospholipids thereby resulting in liposome aggregation [16]. In contrast, in the case of liposomes comprising of chitosan and neutral phospholipids, the net charge on the bilayer becomes positive resulting in repulsion between vesicles and thereby preventing their aggregation [16]. Another study by Mertins and Dimova conducted at pH 4.5 showed that strong electrostatic interaction between chitosan and negatively-charged phospholipids resulted in pore formation and leakage in the liposomes [17]. Other studies showed that an increase in degree of unsaturation and/or reduction in the length of the hydrocarbon chain of the phospholipid itself results in increased water permeability of the vesicle membrane [18] as well as faster leakage of water soluble drugs [19].
Differences in chitosan organization on the bilayer was observed to depend on the preparation method of chitosan-lipid vesicles [12,20]. Previous studies reported two different approaches for the incorporation of chitosan into the lipid bilayer: (i) incubation method and (ii) inverse phase precursor method [17,21,22]. In the first approach, pre-formed vesicles were incubated in a chitosan solution leading to chitosan adsorption only to the outer leaflet of vesicle bilayer. In the second method, chitosan is incorporated into the lipid bilayer during its self-assembly prior to vesicle formation, resulting in chitosan presence on both the inner and outer leaflets of the vesicles [22]. Using small angle x-ray scattering, Mertins et.al have shown that for dried chitosan-phospholipid films prepared by inverse phase precursor method (also known as reverse phase emulsion method), presence of chitosan reduces the thickness of the phospholipid bilayer in the organogel [22]. This suggests that the bilayer is sandwiched between polymer chains, and vesicles formed from the organogel contain chitosan in inner and outer leaflet of the membrane [22].
Mertins and coworkers measured chitosan content in chitosan-DOPC vesicles and showed that chitosan incorporation in the bilayer by the inverse phase precursor method remains stable over time and that the thermodynamic stability bilayer is also enhanced due to effective shielding of phospholipid head group by chitosan [20,23]. Using fluctation analysis, Mertins and Dimova showed that at low concentrations chitosan, the bending rigidity of chitosan-DOPC giant unilamellar vesicles (GUVs) was found to decrease [17]. However, measurements could not be made for higher chitosan: DOPC molar ratios (≥2 × 10−4) as membrane undulations reduce to unobservable levels thereby rendering fluctation analysis inapplicable [17].
In the present work, chitosan-bearing 1-stearoyl-2-oleoyl-sn-glycero-3-phosphocholine (SOPC) GUVs prepared by inverse phase precursor method [23]. We employed micropipette aspiration assay which enabled us to measure the mechanical and transport properties of the GUVs at high chitosan : SOPC molar ratios (upto 3 × 10−3). We confirmed the presence of chitosan in the bilayer by laser scanning confocal microscopy (LSCM) and also quantified the amount of chitosan associated with vesicles. Further, we estimated the bending and area compressibility moduli, water permeability and lysis tension of these chitosan-SOPC GUVs. In addition, the impact of solution pH on surface charge as well as bending and area compressibility moduli of chitosan-SOPC vesicles was measured. Phospholipid diffusivity in chitosan-SOPC supported lipid bilayers (SLBs) was also estimated.
Section snippets
Materials
1-stearoyl-2-oleoyl-sn-glycero-3-phosphocholine (SOPC) and 1,2-dipalmitoyl-sn-glycero-3-phosphoethanolamine-N-(lissamine-rhodamineB sulfonyl) (DPPE-Rh) in chloroform (25 mg/ml) were procured from Avanti Polar Lipids Inc. (Alabaster, AL, USA) and used without further purification. Chitosan in powder form (Mol. Wt. 150 kDa) with 90 % degree of deacetylation was gifted by Meron (Kerala, India). Bovine serum albumin (BSA) (fraction V, low heavy metals) and fluorescein isothiocyanate (FITC) was
Quantification of chitosan and SOPC in GUVs
In this work, we measured the mechanical properties and water permeability of chitosan-SOPC GUVs. To this end, we prepared chitosan-SOPC GUVs by first drying a water-in-chloroform emulsion containing SOPC and chitosan, and subsequently rehydrating the chitosan-SOPC film under an electric field [21]. Chitosan is a pH sensitive polymer that remains de-protonated at pH 7 but at pH 4.5, its amino groups get protonated resulting in electrostatic repulsion within and between polymer chains [16,40].
Conclusion
In summary, we characterized the effect of incorporating chitosan in SOPC GUVs on various mechanical properties of the lipid bilayer. At a neutral pH of 7, bending modulus of chitosan - SOPC vesicles increased with chitosan concentration when compared to pure SOPC lipid vesicles while area expansion modulus remained unaffected. However, at an acidic pH of 4.5 the presence of chitosan in SOPC vesicles did not show this pronounced effect. Chitosan incorporation also led to a slight decrease in
Credit authorship contribution statement
Sameer Jadhav supervised the design and analysis of the study and contributed towards writing of the manuscript. Honey Priya James designed and performed the experiments, carried out the analysis and wrote the manuscript.
Declaration of Competing Interest
The authors declare that they have no known competing financial interests or personal relationships that could have appeared to influence the work reported in this paper.
Acknowledgments
Authors acknowledge financial support from Department of Science and Technology (DST), (Government of India). HPJ was supported by DST Inspire Fellowship (DST/INSPIRE/03/2014/001092). The authors thank IRCC, IIT Bombay for providing access to the laser scanning confocal microscopy facility.
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