Research Article | Open Access
Hongmei Chen, Wei Ouyang, Christopher Martoni, Satya Prakash, "Genipin Cross-Linked Polymeric Alginate-Chitosan Microcapsules for Oral Delivery: In-Vitro Analysis", International Journal of Polymer Science, vol. 2009, Article ID 617184, 16 pages, 2009. https://doi.org/10.1155/2009/617184
Genipin Cross-Linked Polymeric Alginate-Chitosan Microcapsules for Oral Delivery: In-Vitro Analysis
We have previously reported the preparation of the genipin cross-linked alginate-chitosan (GCAC) microcapsules composed of an alginate core with a genipin cross-linked chitosan membrane. This paper is the further investigation on their structural and physical characteristics. Results showed that the GCAC microcapsules had a smooth and dense surface and a networked interior. Cross-linking by genipin substantially reduced swelling and physical disintegration of microcapsules induced by nongelling ions and calcium sequestrants. Strong resistance to mechanical shear forces and enzymatic degradation was observed. Furthermore, the GCAC membranes were permeable to bovine serum albumin and maintained a molecular weight cutoff at 70 KD, analogous to the widely studied alginate-chitosan, and alginate-poly-L-lysine-alginate microcapsules. The release features and the tolerance of the GCAC microcapsules in the stimulated gastrointestinal environment were also investigated. This GCAC microcapsule formulation offers significant potential as a delivery vehicle for many biomedical applications.
Bioencapsulation describes a procedure where biologically active materials are enclosed within a semipermeable membrane . This technology has proven a valuable strategy to facilitate a wide range of pharmaceutical and biomedical processes in both fundamental research and industrial applications including drug delivery, artificial organs, and cell therapy [2–9]. The key required characteristics of microcapsules for such applications include biocompatibility, adequate resistance to environmental constraints, appropriate membrane stability, and permeability [10–17]. In particular, preservation of structural integrity of microcapsules is crucial in many applications such as immunoisolation in cell transplantation . Previous research has suggested that mechanically strong and durable capsules were less likely to rupture, thus prolonging in vivo functions of the encapsulated cells [11, 19–22].
Alginate, a polysaccharide isolated from brown algae, has been widely used in bioencapsulation due to its excellent biocompatibility and mild processing conditions. Addition of the outer poly-L-lysine (PLL)-alginate coating reduced the porosity of the alginate gel, rendering the alginate-PLL-alginate (APA) microcapsules promising as an immunoisolating device [18, 23–25]. One of the main limitations accounting for graft failures using this system was the capsular fragility and short-term durability [20, 26–29]. Insufficient membrane stability of the cell-containing microcapsules could lead to proteolytic degradation of the polyamino acid coating, destabilization of the alginate core matrix, and activation of the complement system, resulting in ultimate failure in immunoprotection . Chitosan, a naturally derived polycation, was investigated as an alternative to PLL for microcapsule coating. Microencapsulation by the alginate-chitosan (AC) membrane, formed via electrostatic interactions between the two opposite charged polysaccharides, has been extensively studied for the delivery of drugs [30–36], proteins [37, 38], enzymes , growth factors , DNA [41, 42], live microbes [43–46], and cells [47, 48]. However, the stability of the AC membrane remains limited [44, 49–52]. Hence, significant improvement in microcapsule chemistry is required for the delivery device to withstand long-term biological impediments.
Covalent cross-linking of microcapsules constitutes an effective way to generate polymeric networks giving rise to high strength and resistance to chemical, proteolytic, and mechanical stresses [53, 54]. Although enhancement in microcapsule stability using synthetic cross-linking reagents, such as bifunctional aldehydes [39, 55–57], carbodiimide (EDC) , and photosentitive molecules [58–60], has been reported, concerns about their cytotoxicity persist [61–65].
Genipin is an iridoid glucoside extracted from Gardenia fruits . It has traditionally been used as a Chinese herbal medicine [67–71] and an edible colorant in the food industry . In recent years, genipin has drawn considerable research interests as an alternative cross-linker due to its natural origin and low cytotoxicity, allowing for mild but effective chemical cross-linking [38, 63, 73–76, 76–91]. We have earlier reported the use of genipin to introduce covalent links into the microcapsule membrane for live cell encapsulation [90, 92]. As a follow-up study, we present herein the characterization of the microcapsule structure and key physical characteristics including mechanical properties, resistance, permeability, and durability.
Sodium alginate (low viscosity), bovine serum albumin (BSA, Mw 66 KD), lysozyme (58,100 units/mg protein), poly (L-lysine) hydrobromide (molecular weight, Mv 27.4 KD), and fluorescein isothiocyanate (FITC) labeled dextran (Mw 4, 20, 40, 70, and 2000 KD) were obtained from Sigma-Aldrich, USA. Chitosan (low viscosity, by viscometry, degree of deacetylation at 73.5% by titration) and genipin were purchased from Wako BioProducts, USA. All other reagents and solvents were of reagent grade and used as received without further purification.
2.2. Preparation of GCAC Microcapsules
The GCAC microcapsules were prepared according to the protocol as earlier described . Briefly, calcium alginate beads were formed by extruding an alginate aqueous solution (15 mg/mL) into a gelling bath containing 11 mg/mL Coating with chitosan was performed by immersing the Ca-alginate beads in a chitosan solution (10 mg/mL in 11 mg/mL ) for 30 minutes, resulting in the alginate-chitosan (AC) beads. Subsequently, the AC microcapsules were cross-linked by incubation in an aqueous solution of genipin (1.0 mg/mL) for 24 hours at 20 and 4 (the latter of which used for the test in the simulated gastrointestinal fluid only). The resulting microcapsules were washed with deionized prior to testing.
2.3. Preparation of Microcapsules Containing Blue Dye or High Molecular Weight Fluorescent Labeled Dextran
Microcapsules loaded with blue dye or FITC-dextran were prepared for the tests of long-term durability and enzymatic degradation, respectively. The preparation processes including alginate gelation, chitosan coating, and genipin cross-linking were performed using the aforementioned protocols except that a mixture of alginate solution with either a known amount of blue dye (Bleu ultramarine, Pb29, Kama Pigments), or with high molecular weight (HMW) FITC-dextran (FD2000, Mw 2000 KD) at a final dextran concentration of 2 mg/mL was used as the starting material.
2.4. Electron Microscopic Observations
Large Ca-alginate beads (approximately 1 mm in diameter) were prepared by extruding alginate solution into a receiving bath using a 1 mL syringe and a 27 gauge needle. Then the AC and GCAC beads were made according to the above-mentioned procedures. Beads were dehydrated by gradient ethanol and critical point drying (CPD, LADD Research Industries), and coated with Au-Pd using an Au-Pd sputtering coating unit (Hummer Polaron Au Sputter Coater). A minimum of three beads randomly selected from each formulation batch were initially scanned to ensure batch homogeneity, and the microscopic structure examined by scanning electron microscopy (SEM) (FEG_SEM, Hitachi model S-4700). To characterize the inner membrane structure, the microcapsules were dehydrated, embedded in Epon and cross-sectioned by using an ultramicrotome (Reichert Ultra Cut AV) prior to microscopic observations under transmission electron microscopy (TEM) (Tecnai 12 120 kV TEM).
2.5. Swelling and Membrane Resistance
To assess the swelling behavior and membrane resistance, aliquots of microcapsules were submerged in 2 mL of physiological solution (PS, 0.9% NaCl) or phosphate buffered saline (PBS, pH 7.4). The solution was refreshed every 2 hours in the first 8 hours and then once a day for up to 1 week. The morphology and physical integrity of the microcapsules were examined under an inverted light microscope (LOMO PC) at a magnification of 90 The microcapsule dimension was measured with an eyepiece micro-meter equipped on the microscope, and averaged from at least 8 beads per batch. The swelling ratio is expressed as percentage of diameter changed according to the following equation: % where and D were microcapsule diameters before and after the incubation, respectively.
To examine the membrane resistance to citrate chelation, microcapsules were exposed to a sodium citrate solution (50 mg/mL) at room temperature for 24 hours. The changes in morphology were studied by using an optical microscopy.
To test the long-term membrane durability, blue dye-entrapped microcapsules were incubated up to 6 months at room temperature in PS containing sodium azide (5 mM) to prevent microbial growth. The media were changed periodically. The morphology of the microcapsules was observed under the microscope, and images taken as records.
2.6. Osmotic Pressure Test and Mechanical Stability of Microcapsules
The mechanical stability of the microcapsules was examined by the osmotic pressure and mechanical shear tests. Osmotic stress was applied to microcapsules using a modification of a previously described procedure . Specifically, the GCAC microcapsules were equilibrated for 30 minutes in hypertonic solution (10, 5, 2 or 1 of 0.85 wt% aqueous NaCl) prior to transferal to a hypotonic medium (deionized ), which led to a high osmotic pressure inside the microcapsules. During the following 1 hour, broken microcapsules were counted under an inverted microscope. In the mechanical stress experiments, microcapsules (2 mL) suspended in 10 mL deionized were subjected to agitation (600 rpm) for 3 hours. The percentage of destroyed microcapsules in at least three randomly picked observation fields was estimated under an optical microscope, and images taken as records. The experiments were performed in triplicate.
2.7. Membrane Permeability
In vitro permeability studies were performed to determine the ingress ratio of macromolecular markers and the microcapsule membrane molecular weight cutoffs (MWCO) using FITC-dextran (Mw 4, 20, 40, 70, and 2000 KD) as fluorescent molecular weight standards and BSA as a model protein permeant.
2.7.1. Penetration of FITC-Dextran into Microcapsules
Microcapsules (approx 150 beads) were equilibrated overnight in PS at room temperature, followed by addition of an FITC-dextran solution (150 L, 0.5 mg/mL dissolved in PS, with an exception of FD-4 at 1.0 mg/mL in PS due to the lower extent of FITC labeling). Incubation under light protection continued for 24 hours to reach equilibrium. Then, microcapsules along with the marker media were placed in a chambered coverglass system (Lab-TeK). The diffusion of FITC-dextran into the microcapsules was investigated by confocal laser scanning microscopy (Zeiss LSM 510, Jena, Germany) equipped with a Zeiss Axiovert 100 M microscope. An argon-ion laser was used at an excitation of 488 nm and the fluorescence was detected with the filter block BP500-550IR. For quantitative evaluation, rectangles with an area of at an equatorial, optical section of microcapsules inside the microcapsules and in the surrounding media were defined. Mean pixel grey values representing the relative fluorescence intensities were acquired using LSM 510 software command “Topography”. Standard deviations of pixels within the detected areas were consistently below 9 to ensure homogeneity of the fluorescence signals in the tested regions. Diffusion of dextran into ten individual capsules per batch was assessed and expressed as percent of fluorescence intensity in the microcapsule confines relative to that in the incubation solution (background reading). Microcapsule membranes with dextran diffusion less than 5% were considered cutoff to the tested marker.
2.7.2. Penetration of BSA into Microcapsules
Immediately after BSA solution (1.5 mg/mL in 1.5 mL PS) was added to the vials containing the tested microcapsules () and placed in an Environ shaker with gentle rotation at a speed of 125 rpm, the concentrations of BSA remaining in the supernatant was monitored for up to 8 hours using the Bradford method. The absorbance at 595 nm was recorded using a Quant Universal Microplate Spectrophotometer (Bio-Tek Instruments, Inc.) and the protein concentration was determined using a BSA standard curve. The BSA diffusion profile was plotted as relative BSA remaining in the medium as a function of incubation time.
2.8. BSA Encapsulation and In Vitro Sustained Release
2.8.1. BSA Encapsulation
To prepare the BSA encapsulated microcapsule, BSA was first dissolved in PS and mixed with alginate solution to give a final concentration of 15 mg/mL for both BSA and alginate. The mixture was extruded and droplets were gelled in a receiving bath (11 mg/mL) for 15 minutes. The subsequent coating with chitosan and cross-linking by genipin were performed according to the aforementioned protocol. Prior to assessment of protein release the microcapsules were equilibrated overnight in a physiological solution containing 15 mg/mL BSA to compensate for possible BSA loss during preparation.
2.8.2. In Vitro Release of Encapsulated BSA
The BSA loaded microcapsules (0.20 g) were suspended in 2.0 mL 0.01 M phosphate buffered saline (PBS, pH 7.4) with gentle rotation in an ENVIRON shaker at 37 At various time points, supernatant (1.0 mL) was withdrawn to determine the release of BSA by the Bradford assay as described above, and the medium was replaced with fresh PBS. Results of accumulated protein released from triplicate experiments were plotted as a function of incubation time.
2.8.3. BSA Stability Assay
To confirm the integrity and stability of the encapsulated BSA, freshly made BSA-containing microcapsules were immersed in a sodium citrate aqueous solution (10 wt%), followed by pressing the bead suspension through needles with gradually increasing gauge (from 18 to 27G) to break the capsules and liberate the entrapped BSA. Subsequently, the suspension was centrifuged at 5000 g for 5 minutes and the supernatant was pressed through a 0.22 m syringe filter. The clear filtrate was analyzed by a high-performance liquid chromatographic system (HPLC, Varian Inc. Canada) equipped with a column of Biosep-SEC3000 (Phenomenex). The mobile phase, 50 mM phosphate buffer solution (pH 6.8), was prefiltered through 0.22 m vacuum-driven filter unit (Millipore, Japan) and run at a flow rate of 0.5 mL/min at room temperature. The injection loop was set at 20 L and UV detection at 280 nm. A standard BSA solution was used as reference.
2.9. In Vitro Degradation by Lysozyme
A known amount () of the microcapsules containing high molecular weight fluorescent-labeled dextran (2000 KD) were placed in amber vials containing lysozyme solutions (2.0 mL) at different concentrations (15 g/mL, 150 g/mL, and 15 mg/mL) in PBS and incubated at 37 in a platform shaker with gentle rotation of 100 rpm for either 7 or 30 days. The leakage of fluorescent marker from the microcapsules was assessed as indicative of membrane defects induced by lysozyme degradation and erosion. Supernatant (0.2 mL) was withdrawn at different intervals and assessed spectrofluorometrically using a Microplate Fluorescence Reader (FLx800, Bio-Tek Instruments, Inc.) with the absorption and emission wavelengths at 485 and 528 nm, respectively. The volume of the media was kept constant by adding fresh lysozyme solution after sampling. Data are presented as from triplicate experiments.
2.10. Membrane Resistance to Simulated Gastrointestinal Fluids
To examine the potential of microcapsules for oral applications, the simulated gastric fluid (SGF, pH 1.2) and the simulated intestinal fluid (SIF, pH 7.5) were prepared according to United States Pharmacopoeia XXII protocol, and used to test the microcapsule resistance. The morphological changes of the tested microcapsules were observed by optical microscopy (LOMO PC), and microphotographs were recorded using a digital camera (Canon Power shot G2).
3. Results and Discussion
3.1. Surface and Internal Structure of Microcapsules
The surface and internal structure of the microcapsules were examined by electron microscopy and images are shown in Figures 1–4. We found that these microcapsules were essentially spherical in geometry, possessing a homogenous, smooth, and compact structure on the surface (Figure 1). The GCAC microcapsule had a denser and smoother surface than the AC membrane (Figures 1(c) and 1(d)), though sporadic small nubs were seen in both cases. Preliminary energy-dispersive x-ray (EDX) analysis did not show differences in chemical compositions on these small nubs when compared to the other regions of the membrane. At higher magnifications, the presence of clusters and small spheres on the cross-linked surface was observed (Figure 1(f)). Porous structure was found inside the microcapsules without discernible differences in porosity and density of the network between the AC and GCAC capsules (Figures 2 and 3). The internal morphology of the microcapsule membranes at the boundary regions was assessed by TEM. In comparison to the alginate (Figures 4(a) and 4(b)) and AC capsules (Figures 4(c) and 4(d)) where a more granular pattern of structure was observed, a smoother and denser structure was seen for the GCAC membranes (Figures 4(e) and 4(f)). These structural differences were most likely caused by different membrane chemistries.
3.2. Effect of Genipin Cross-Linking on Microcapsule Swelling and Resistance
Alginate is highly hydrophilic because of the presence of –OH and –COOH groups in its chain. At neutral pH, water penetrates into the chains of alginate to form hydrogen bridges through the –OH and groups, and fills up the space along the chains and/or the centre of wide pores or voids . As a consequence, the alginate beads tend to swell substantially. Additional swelling and destabilization are promoted by the presence of non-gelling ions and chelators, such as sodium, magnesium, phosphate, lactate, and citrate. For example, a substantial quantity of sodium and phosphate ions in physiological conditions induce osmotic swelling. Chelation of the bound cross-linking calcium ions results in the loss of the egg-box structure and dissolution of the alginate matrix [22, 95]. Previous studies suggested that creating a strong membrane and minimizing the matrix swelling may stabilize the alginate-based microcapsules [22, 27, 96, 97]. In our study, morphological changes in microcapsules exposed to non-gelling media and citrate chelation were investigated. Results showed that the GCAC microcapsules remained intact and swelled and in PS and PBS, respectively. Both AC and APA microcapsules experienced substantial swelling in PBS, increasing in size by approximately 46% and 80%, respectively (data not shown). After 24 hours of citrate treatment, the AC microcapsules showed significant swelling with worn out and thinner membrane though resistant against complete dissolution (compare Figure 5(a) with Figure 5(b)). In contrast, the GCAC microcapsules underwent limited swelling and remained morphologically stable (compare Figure 5(c) with Figure 5(d)). In addition, the cross-linked microcapsules retained their structural integrity for at least 6 months in PS, compared to the AC capsules showing membrane defection (roughly 8%) over the same period of investigation (Figure 6). These observations demonstrate the enhancement of microcapsule resistance and durability by the covalent links on the membrane.
3.3. Mechanical Stability of GCAC Microcapsule Membrane
Mechanical properties of microcapsule membranes are of key importance for their integrity preservation and in vivo performance. It was previously reported that microcapsules with strong membranes were more durable and less likely ruptured, which allows for prolonged functions of the encapsulated cells [20, 21, 27]. Despite being crucial, precise determination of the microcapsule mechanical strength is difficult because of the size (generally 100 m to 2 mm in diameters)  and fragile nature of the microcapsule. A number of assessment techniques have been explored [13, 16, 28, 93, 96, 99], but standard testing methods have yet to be established. In this study, the membrane strength was evaluated by subjecting the microcapsules to osmotic pressure and mechanical agitation. It was found that after exposure to an osmotic shock, none of the GCAC microcapsules burst, in contrast to the complete fracture of the APA capsules (data not shown). In the mechanical shear test, the vigorous agitation accelerated the breakage of the microcapsules. After 3 hours of continuous mechanical agitation, the APA microcapsules became totally fragmented; 70–80% of the AC beads were ruptured; whereas approximately 30% of the cross-linked microcapsules were destroyed (Figure 7). Noticeably, some of the GCAC microcapsules had changed into an elliptical shape under mechanical force, indicating the elasticity of the cross-linked capsules (Figure 7(c)). This improvement in mechanical stability was correlated with the reduced swelling of the GCAC capsules, showing that covalent cross-linking by genipin considerably stabilized the microcapsules.
3.4. Permeability of Microcapsules
In cell microencapsulation, live cells are isolated from the external environment by an artificial, semipermeable membrane, which should allow for ingress of oxygen and nutrients, and egress of waste products and therapeutic molecules. Proper encapsulated cell functions require strict control over permeability of the microcapsule membrane. In permeability research, the use of neutral polysaccharide molecular weight standards precludes the problems of absorption, aggregation, and other charge/hydrophobic interactions, while proteins are thought to be more appropriate in determining the permeability of microcapsules designed for biological systems [100, 101]. In our study, permeability measurements were carried out with individual microcapsules using confocal laser scanning microscopy (CLSM) to examine the ingress of fluorescent dextran markers, and by batch experiments detecting the decrease in concentration of the protein marker in incubating media containing plain microcapsules.
Dextran is a linear and neutral polysaccharide, whereas globular BSA bears negative charges at and hydrophobic character. Results from our dextran experiments using CLSM are shown in Figures 8–10. Figure 8 depicted the significant difference in light intensity within tested regions of the two red rectangles (mean pixels 125 versus 242), suggesting the nonhomogeneous dissemination of FITC-dextran (20 KD) inside and outside the microcapsule. The representative CLSM images shown in Figure 9 demonstrated that the dextran ingress was significantly reduced with increasing molecular weights of fluorescent markers. Irrespective of microcapsules, low Mw dextran (4 KD) infiltrated to the interior of the microcapsules at a great extent (diffusion ratio 70%), whereas permeation of larger dextrans, 40 KD and 70 KD, was greatly restricted, with the inflow ratio around 20% and below 5%, respectively (Figure 10). The cut-off for the GCAC membrane was on the order of 70 KD (for FITC-dextran), and same as for the APA and AC microcapsules, which corroborated with the published results [100, 102–106].
As the diameter of BSA may correspond to dextran with molecular weight of 20 KD, which is below the above-described exclusion limit, BSA should theoretically penetrate the studied microcapsule membranes. Our observation on BSA diffusion confirmed this postulation. Despite initial retardation, BSA was able to diffuse into the GCAC microcapsules, as seen by a gradual decline of BSA remaining in the media (Figure 11). After 4 hours, the BSA infiltration reached a similar level to that for the APA microcapsules, with 55% of BSA remaining in the media. In the GCAC and AC systems, the membrane thickness was mainly governed by the binding of chitosan . This may account for their similar permeability for dextran diffusion (Figure 10). The retardation of protein infiltration to the GCAC microcapsules shown in Figure 11 may be ascribed to the transport hindrance caused by the denser network structure of the genipin cross-linked membrane. The effects of genipin cross-linking variables on the permeability of the GCAC microcapsules were also investigated, and no statistically significant differences on the membrane cutoffs were detected within the tested ranges (data not shown). The above findings indicated that the covalent cross-linking treatment by genipin modulated the diffusion kinetics of the permeants but did not alter the membrane MWCO cutoffs.
3.5. Sustained Release of Encapsulated BSA
The permeability characteristics of the chitosan-based microcapsules were further examined by the release profiles of the encapsulated BSA. As shown in Figure 12, prolonged release of BSA from both the AC and GCAC microcapsules was evidenced. As well, the genipin cross-linked membrane delayed the release of BSA for an appreciable period of time. Specifically, the cumulative percentage of BSA released from the GCAC and AC capsules was 38.1% and 55.5% in the first 1 hour, respectively. Thereafter, these numbers increased to 46.8% versus 69.5% in 2 hours, and 70.4% versus 76.7% in 4 hours, and both above 95% after 12 hours (Figure 12). This delay in BSA release, which was consistent with the results obtained from the BSA ingress experiments, could be a result of transport obstruction in the GCAC membranes generated by the genipin-chitosan cross-links.
Additionally, the loss of stability of the encapsulated protein is one of the concerns regarding protein immobilization and drug delivery. In the present research, the stability of microencapsulated BSA was further examined by the integrity change reflected in their chromatographs. One can see in Figure 13 that the entrapped BSA in both AC and GCAC microcapsules showed a peak equivalent to the standard protein in terms of retention time and peak shape. The presence of some large molecules with molecular weights higher than the BSA standard was also detected at earlier elution time in the chromatographs of both BSA-containing microcapsules, and a higher amount of these unknown molecules was found inside the GCAC microcapsules. These large molecules, present in the GCAC microcapsules in a greater quantity, may likely arise from the BSA-chitosan complex, the genipin cross-linked BSA, or other impurities. Although the integrity of the encapsulated BSA was confirmed by HPLC, whether the genipin treatment would affect the enclosed proteins need further investigation.
3.6. In Vitro Degradation by Lysozyme
HMW FTIC-dextran (2000 KD) was encapsulated as a tracer to study the enzymatic degradation of microcapsule membrane in vitro. Being a large polymer in this size, this fluorescent probe should indefinitely be withheld inside the intact microcapsules and could not spread out unless the membranes became defected. A universal enzyme lysozyme was used in this study to decompose microcapsule membranes, and the leaching of encapsulated dextran induced by corrosion and degradation of the microcapsule membranes was examined. Exposure of the fluorescent tracer-loaded APA microcapsules to lysozyme (15 g/mL) resulted in an increase in the media’s fluorescence, proportional with incubation time ( Figure 14(a)) and reaching the intensity of 243 and 503 at day 3 and 7, respectively. With 10 times more concentrated lysozyme, the leaking of FITC-dextran occurred more rapidly, from 9, 272, to 513 at time 0, day 1 and day 3, respectively (Figure 14(b)). Conversely, leaking of encapsulated dextran from the AC and GCAC microcapsules was negligible (Figures 14(a) and 14(b)) under the same challenging condition, with membrane integrity preserved over the 7-d experimental period (data not shown). We further extended the test period to 30 days. Significant deterioration of microcapsule membranes began in the third week when using more concentrated lysozyme (150 g/mL). As shown in Figure 14(c), fluorescence leakage from the AC microcapsules intensified from 31, 68 to 136 on Days 7, 14 and 21, respectively. The enzyme actions on the GCAC mcirocapsules were much less as evidenced by significant reduced liberation of the enclosed FITC-dextran, with the fluorescence maintained below 40 for the first 2 weeks and reaching a plateau of 66 from Day 19. This indicated the preservation of the GCAC membrane integrity under this offending condition. Exposure to highly concentrated lysozyme (15 mg/mL) caused considerable leaking of FITC-dextran from the AC mcirocapsules, with the intensity escalating from 207, 440 to 582 at the end of the 2nd, 3rd and 4th week, respectively. In contrast, leaking of the fluorescent marker from the GCAC microcapsules remained insignificant for the first 24 days (intensity 100). Pronounced leaking was detected since Day 28, however the intensity in the challenging media remained less than half as for the AC mcirocapsules (Figure 14(d)). This finding suggested that although deterioration of the GCAC membranes occurred at higher lysozyme concentrations and extended time periods, the covalently cross-linked membrane showed stronger resistance to enzyme degradation compared to the noncross-linked AC membrane.
3.7. Resistance of Microcapsules to Simulated Gastrointestinal Fluids
Oral administration is one of the most preferred routes for therapeutic delivery. However, most macromolecules are susceptible to rapid degradation by the GI impediments , for example, the pH fluctuates from below 2 in the stomach to higher than 7 in the intensity, and the strong proteolytic enzymatic actions exist in the stomach and duodenum . Various encapsulation systems have been proposed in order to target therapeutics absorption from the lower colon and ileum [109–114]. In particular, covalent cross-linking is an effective means to improving chemical and proteolytic resistance to the GI environments [56, 59, 115–119]. In this study, we investigated the resistance of the GCAC microcapsules to the simulated GI conditions by sequential incubation with the simulated gastric fluid (SGF, pH 1.2) and the intestinal fluid (SIF, pH 7.5). Results show that the microcapsules remained physically intact in the SGF. After subjected to the SIF, microcapsules with high degree of cross-linking (genipin cross-linking at 20) appeared robust and largely retained spherical morphology after 1 week of interaction (Figures 15(a)–15(e)). For those with low cross-linking extent (cross-linked at 4), substantial membrane deterioration occurred (Figures 15(f)–15(j)). These indicated that the extent of microcapsule membrane degradation and tolerance to the GI impediments could be regulated to suit different oral applications, for instance, sustained release of drugs to different GI absorption sites, by controlling the degree of cross-linking, which could be achieved by manipulating the chitosan-genipin reaction variables  in this membrane and other microcapsule systems [20, 26, 27, 120].
This paper characterizes the structure and physical properties of the genipin cross-linked alginate-chitosan (GCAC) microcapsules. Results showed that the covalent cross-linked microcapsule membrane possessed strong membrane stability and potent resistance to a number of constraints including mechanical stress, calcium sequestration, enzyme degradation, and GI impediments. Results also demonstrated that the GCAC membrane excluded the infiltration of 70 KD FITC-dextran, while allowing for permeation of bovine serum albumin. These findings suggested that covalent cross-linking by genipin provides considerable improvement in the microcapsule strength and resistance while maintaining the permeability characteristics. Further development of this preparation may permit its use in various biomedical applications.
The authors would like to acknowledge the financial support from Canadian Institutes of Health Research (CIHR). Postgraduate scholarships from Natural Sciences and Engineering Research Council (NSERC) of Canada, Fonds Quebecois de la Recherche sur la Nature et les Technologies (FQRNT), and Greville Smith McGill Major to Chen are appreciated. The authors want to thank L. Mongeon, J Laliberte, H. Vali, R Cohen, TJ Rebello, and B Lawuyi for experimental assistance, and T. Haque for proofreading the manuscript.
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