Chitosan Nanoparticles to Enhance the Inhibitory Effect of Natamycin on <i>Candida albicans</i>

Liu, Yaling; Cui, Xiaoming; Zhao, Liping; Zhang, Weifen; Zhu, Shourong; Ma, Jinlong

doi:https://doi.org/10.1155/2021/6644567

Journal of Nanomaterials

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Abstract Introduction Materials and Methods Results and Discussion Conclusions Data Availability Conflicts of Interest Acknowledgments References Copyright Related Articles

Research Article | Open Access

Volume 2021 | Article ID 6644567 | https://doi.org/10.1155/2021/6644567

Chitosan Nanoparticles to Enhance the Inhibitory Effect of Natamycin on Candida albicans

Yaling Liu,¹Xiaoming Cui,²Liping Zhao,²Weifen Zhang,^2,3,4Shourong Zhu ,¹and Jinlong Ma^2,3,4

Academic Editor: Antonio Vassallo

Received27 Oct 2020

Revised11 Mar 2021

Accepted13 Mar 2021

Published05 Apr 2021

Abstract

Fungal keratitis is a stubborn fungal infection that is widespread worldwide. It can even affect the health and life of a patient. At present, natamycin (NAT) is the first-line drug in the treatment of fungal keratitis, despite its disadvantages of clinical use, such as low drug bioavailability and poor water solubility. Herein, inspired by the adhesion properties of chitosan and its excellent drug loading and antifungal properties, we designed simple natamycin-chitosan nanoparticles (NAT-NPs) to investigate the feasibility of chitosan with NAT for eye treatment. Results showed that the NAT-NPs increased the antifungal effect of NAT due to the antifungal feature of chitosan NPs. Therefore, NAT-NPs are expected to become potential candidates for the treatment of fungal keratitis due to their high bacteriostasis.

1. Introduction

In recent years, the incidence of fungal keratitis has increased significantly due to the rise in vegetative corneal trauma, improper use of contact lenses, and widespread use of antibiotics and hormones [1–4]. Fungal keratitis typically occurs in autumn and affects mostly males and middle-aged and elderly farmers; most patients have a history of trauma and local medication. Fungal keratitis results in severe visual impairment, and its treatment is more difficult than other corneal infections [5, 6]. Although the gold standard for the treatment of fungal keratitis has not been identified [7, 8], experts believe that natamycin (NAT) is a tetraene polyene that is the most important agent in the management of fungal keratitis [9]. Its mechanism of action combines the hydrophobic part of the molecule with the ergosterol of the fungal cell membrane to form a polyene steroid complex through Van der Waal forces, thereby changing the permeability of the cell membrane. It then causes the failure of ions, nucleotides, and amino acids in fungal cells, disrupting the normal metabolism of cells and inhibiting fungi [10]. The current NAT formulation and dosage regimen consist of 5% (w/v) ophthalmic suspension instilled in the conjunctival sac at hourly or two-hourly intervals for several days. However, frequent dosing is required with high drug loading (DL) to maintain the drug levels within the therapeutic window, which can result in poor compliance in patients [11, 12].

The cell in the cornea is relatively special and features a lipid-water-lipid sandwich-layered structure. The poor water solubility of NAT hinders its penetration into deep corneal layers and the anterior chamber, which limits its use as monotherapy only for superficial keratitis [13, 14]. Moreover, the drug is removed from the ocular surface within a few minutes due to the rapid clearance of drug by fast tear turnover, blinking, and lacrimal drainage; these events are the main reason for the low drug bioavailability of less than 5% [15–18]. To improve the residence time in front of the eyes, chitosan (CTS), poly(acrylic acid) acid, alginic acid, pectin, hyaluronic acid, and lecithin have been used as adhesive materials; these compounds have shown promising results [19–26]. Ramish et al. developed 5-fluorouracil-loaded CTS-coated sodium alginate-CTS nanoparticles (NPs) for ophthalmic administration. The retention time in the anterior cornea area was prolonged, improving bioavailability [24]. Therefore, drugs may be carried with adhesive materials for solubility and adhesion time, which in turn increases drug bioavailability.

CTS is a polycationic biopolymer with unique physical-chemical (e.g., thermal stability and pH sensitivity), biological (e.g., antimicrobial activity), and mechanical (e.g., film forming) properties [27]. The nontoxic nature of the polymer permits its use for biomedical applications, while its antimicrobial, antifungal, and wound healing features lead to research of further possible uses [28, 29]. The positive charge that the CTS shell carries can bind to the negatively charged corneal surface to increase the residence time of a drug in front of the cornea [30]. In addition, CTS has good inhibitory activity against Escherichia coli, Staphylococcus aureus, and Candida albicans [31]. For example, Bhatta et al. developed natamycin-embedded lecithin-CTS adhesion NPs by CTS crosslinking [32]; the bioavailability of the drug on the eye was found to significantly increase, facilitating its penetration into the inner layers. However, the enhanced antifungal effect of CTS on NAT is unclear; so, further investigations without liposomes are needed.

In this article, CTS and TPP were used as wrappers to wrap NAT into NAT-NPs to enhance the inhibitory effect of NAT on C. albicans (Figure 1). These NAT-NPs were characterized by their , , , , and . In vitro release exhibited sustained release of for 12 h with an initial burst release of in the first hour. The IC50 and zone of inhibition of NAT-NPs showed stronger antifungal activity than NAT against C. albicans. We also found that the antifungal feature of CTS-NPs made a remarkable contribution to the excellent antifungal effect of NAT-NPs. Thus, sodium tripolyphosphate/CTS-NPs are expected to become potential candidates for the treatment of fungal keratitis due to their high bacteriostasis.

2. Materials and Methods

2.1. Materials

CTS (, ) was obtained from Hai Debei Marine Biotechnology Company (Jinan, People’s Republic of China). TPP () was purchased from Yantai Far Eastern Fine Chemical Co., Ltd. (Shandong, People’s Republic of China). Dimethyl sulfoxide (DMSO; ) was purchased from Damao Chemical Reagent Factory. Pimaricin (NAT; ) was purchased from Shanghai Yuanye Bio-Technology Co., Ltd. (Shanghai, People’s Republic of China). Tween-80 was purchased from Hengxing Reagents Co., Ltd. (Tianjin, People’s Republic of China).

Liquid Sabouraud medium and Sabouraud agar were purchased from Hopebio Qingdao Hope Bio-Technology Co., Ltd. (Qingdao, People’s Republic of China). TTC was purchased from BBI Life Sciences. C. albicans (Robin Berkhout ATCC® 18804) was purchased from Credible Leads to Incredible. A digital display vernier caliper was purchased from Senda Tools Co., Ltd. (Zhejiang, People’s Republic of China).

2.2. Preparation of NAT-NPs

NAT-loaded NPs were prepared by ionic gelation [33]. The fabrication of NAT-NPs is illustrated in Figure 1. First, we dissolved NAT in DMSO under ultrasound conditions in a warm water bath to prepare a 1 mg/mL NAT solution. CTS was solubilized in aqueous 1% (v/v) acetic acid at a concentration of 1% (w/v). TPP was solubilized in deionized water at a concentration of 1% (w/v). The NAT-NPs suspensions were obtained by injecting water-diluted TPP solutions into the mixture with different volumes of NAT solution injected into water-diluted CTS solutions. All processes were carried out under magnetic stirring at 500 rpm. The volume ratio of CTS to TPP was 5 : 1, whereas the volume ratios of NAT to CTS and TPP were 1 : 20, 1 : 12, 2 : 15, 1 : 6, 1 : 4, and 1 : 3. Blank NPs (without drug) were prepared following the same procedure. The prepared NPs were preserved after dialysis. The NAT-NPs suspensions were dialyzed against deionized water at room temperature for 48 h using a membrane with an MWCO of 3500 Da (Spectrum Laboratories Inc., USA).

2.3. Particle Size and PDI

The size distribution and zeta potential of NPs were determined by photon correlation spectroscopy with a Zetasizer Nano ZS Zen 3600 (Malvern Instruments, Inc.). Size distribution analysis and PDI were performed at 25°C. The zeta potential was measured by electrophoretic light scattering using a disposable zeta cuvette. All measurements were performed in triplicate, and results are presented as .

2.4. Morphological Characteristics by Transmission Electron Microscopy (TEM)

The structure and topography of the NAT-NPs were examined by TEM analysis (CM30 electron microscope; Philips, Amsterdam, the Netherlands) at an acceleration voltage of 100 kV. One drop of the sample dispersion was carefully casted onto a clean copper grid. Extra solution was air-dried and directly observed under TEM without staining.

2.5. DL and EE

A measured amount of NAT-NPs formulation (6.5 mL) was centrifuged at a high speed (12,000 rpm for 30 min). Subsequently, the supernatant was collected and analyzed to determine the free NAT content, and the sediment was dried and weighed to estimate the DL and EE of NAT in NAT-NPs. The NAT content was determined by using a UV-visible light spectrophotometer (UV) at 303 nm, and a standard curve was obtained for NAT. DL (%) and EE (%) were calculated from the following equations:

2.6. FTIR and TGA Analyses

FT-IR analysis was conducted using an FT-IR Avater-360 spectrometer (PerkinElmer, Waltham, MA, USA), which scanned in the region of 4,000–400 cm^-1 for each spectrum at a resolution of 2 cm^-1. NAT-NPs, NAT, CTS, and TPP were mixed with KBr and compressed into pellets. The characteristic peaks of the FT-IR transmission spectra were documented.

Thermal characterizations were also performed by thermogravimetric (TGA) and differential thermal analyses (DTA) by using a TGA Q500 V20 Thermogravimetric Analyzer (TA Instruments, USA). TGA and DTA were carried out at 10°C/min from 0°C to 800°C at a flow rate of 60 mL/min and compared with NAT, CTS, TPP, and NAT-NPs.

2.7. In Vitro Drug Release Studies

NAT of the prepared NAT-NPs and free NAT was released in vitro at dissolution media at PBS (pH 7.4) at 37°C. In brief, NAT was dissolved in PBS, and NAT-NPs were dialyzed for 2 days. About 2 mL of NAT-NPs and NAT solution was immersed in 100 mL of dialyzed tube of PBS at 37°C and 100 rpm. About 1 mL of solution was removed at a predetermined time, and the same amount of buffer was immediately added. To increase NAT solubility, all samples were tested in an environment with and without Tween-80 plus 0.5% (v/v). The standard curve of NAT obtained from PBS buffer was used to calculate NAT release. All the experiments were performed in triplicate. The cumulative release rate () was calculated as follows: where and are the drug concentrations in released medium, is the volume of mediator removed, is the total amount of leaching medium, and and are the drug concentrations in the NPs and weight of the NPs, respectively.

3. In Vitro Antifungal Activity

3.1. MIC Assays

The influence of the NAT encapsulated NPs and free NAT on antifungal activity was evaluated in terms of MIC50. Sample tests were performed in 96-well plates with serial dilutions of NAT by adding known concentrations of the NP suspensions to liquid Sabouraud medium, as well as free NAT. A series of drug formations of.1, 4.2, 8.45, 16.9, 33.8, and 67.6 μM NAT was made in the medium. Some wells served as the growth control and sterility check. Cell suspensions of C. albicans were prepared in DMEM and adjusted to yield a final inoculum concentration of . The fungal suspension (100 μL) was added to each well, resulting in the desired final drug concentration and inoculum size. The microplates were incubated at 35°C for 24 h. Organism control and medium control were performed simultaneously to check growth inhibiting activity, organisms, and sterility of broth medium.

3.2. Inhibition Diameter Diffusion Experiment

The paper diffusion method was used to measure bacteriostatic diameter. A sterile cotton swab was dipped in the bacterial liquid, rotated, and squeezed inside the tube wall to remove the excess bacterial liquid and coated on the entire agar plate surface for three times, rotating the plate each time. Finally, a circle was applied along the edge of the plate. The surface dish cover was placed at room temperature for 3–5 min to make the surface slightly dry. Sterile forceps were used to paste the drug-containing paper flat on the surface of the plate, and the plate was placed in a 35°C incubator for 24 and 48 h within 15 min after being pasted. The bacteriostatic band was used to measure the bacteriostatic circle. The first group included NAT-NPs, free NAT, and PBS, whereas the second group included NAT-NPs, free NAT, and blank-NPs.

3.3. Statistical Analysis

Data were analyzed with Statistical Package for the Social Sciences version 16.0 software (SPSS Inc., Chicago, IL, USA). The experiments were carried out in triplicates, and values are expressed as the (SD). Student’s -test was conducted to determine significance. Statistical significance was considered at a probability level of .

4. Results and Discussion

4.1. Prepare and Characterization of NAT-NPs

The particle size is an important physical property of NPs that directly affects cellular uptake and biodistribution. Within a certain range, the smaller the particle size is, the better the penetration and absorption of the drug. A strong positive charge can penetrate both the cornea and the conjunctiva due to the positive surface charge and ability to enhance the passive diffusion of the drugs [34]. Therefore, the size and zeta potential of NAT-NPs were our primary concerns. The average diameter and PDI of the NAT-NPs prepared by the ion crosslinking method are shown in Figure 2 and Table 1. Given the different volume ratios of NAT/carrier, particle size and PDI were significantly different. In general, the particle size gradually increased with the increase in the NAT-to-carrier volume ratio. Considering particle size, PDI, and zeta potential, NAT-NPs were most appropriate when the ratios of NAT-to-carrier volume were 1 : 12 and 1 : 20.

The EE and DL of NAT-NPs are shown in Table 2. NAT-NPs had high drug encapsulation, which possibly led to the drug’s good therapeutic effect. Compared with the results of 1 : 20, the volume at 1 : 12 had higher EE. Thus, the volume at 1 : 12 was obtained for the following experiment. TEM images were also used to identify the structure of NAT-NPs and predict roughly spherical and subspherical particles (Figure 3(b)).

(a)

(b)

4.2. Fourier Transform Infrared Spectroscopy (FTIR) and TGA Analysis

FTIR was conducted to identify the structural composition of a substance or determine its chemical group by testing the characteristics of the molecular structure diagram. The FTIR spectra of CTS, NAT, and NAT-NPs are shown in Figure 4(a). The characteristic absorption bands of CTS appeared at 3500 and 3200 cm⁻¹, which were assigned to the -OH stretching and -NH bending vibration, respectively. The characteristic absorption bands of NAT appeared at 3260 (-NH), 1640 (C=C), 1163 (C-CO-C), and 1000 (-C-N) cm⁻¹. For the NAT-NP spectrum, features were observed in bands of 3260 (-NH), 3200 (-NH), and 1163 (C-CO-C) cm⁻¹ compared with CTS and NAT. These findings suggested an interaction between NAT and the nanocarrier and its successful encapsulation.

(a)

(b)

TGA and DTA analyses were carried out to determine sample stability and loss of weight in diverse temperatures to measure the physical and chemical changes of the NPs as a function of temperature. In Figure 4(b), the first event, observed from 50°C to 140°C (), should be linked to the volatilization of water molecules adsorbed on the NAT-NPs surface. NAT-NPs showed intensive weight loss (), which was attributed to the decomposition of the polymer starting from 240°C to 360°C. For CTS and NAT, weight loss appeared in the TG response from 260°C to 360°C () and in the TG response from 200°C to 520°C (), respectively. These TGA data showed some increase in thermal stability of NAT-NPs compared with NAT.

4.3. In Vitro Drug Release

The in vitro drug release of NAT-NPs and NAT in the simulated ocular circumstances (37°C, pH 7.4) was studied (Figure 5). A control group with 0.5% Tween-80 (v/v) was also established due to the poor water solubility of NAT. The NPs showed a two-step release pattern: one initial burst release within 2 h, followed by a second slow-release phase. The cumulative release of NAT freed from the NAT-NPs was 52.15% and 47.5% within 2 h with and without Tween-80, respectively. Some drug was adsorbed on the surface of NAT-NPs during the preparation, which explained the burst release within the first 2 h. More importantly, an initial burst release is beneficial in terms of antifungal activity as it helps achieve the therapeutic concentration of drug in a minimal period followed by constant release to maintain the sustained and controlled release of the drug. The cumulative releases of NAT were 64.32% and 58.54% within 12 h with and without Tween-80, respectively. There was no significant difference in NAT-NPs release between the two environments, but the NAT-NPs showed a stronger sustained release effect than free NAT.

(a)

(b)

4.4. In Vitro Antifungal Activity of NPs

To assess the antifungal activity of NAT-NPs, the IC50 was determined (Figure 6 and Table 3). The IC50 of NAT-NPs showed stronger antifungal activity than free NAT against C. albicans. To further quantify the antifungal effect of NAT-NPs, we conducted an inhibition zone experiment. The zones of inhibition were defined as the maximum distances between the test disk and the fungal growth edge (recorded in millimeters). The zones of inhibition for NAT-NPs (24 h and 48 h) are shown in Figure 7(a-b) and Table 4, respectively. Whether at 24 or 48 h, the antifungal effect of NAT-NPs was much higher than that of NAT, which was consistent with the result of IC50. As expected, the zone of inhibition gradually decreased over time. We speculated that the reason for improving the antifungal effect of NAT-NPs was the increase in water solubility (increased bioavailability) of NAT and the antifungal effect of blank-NPs (CTS) themselves. To further verify the effect of blank-NPs on C. albicans, we compared the antifungal ability of NAT-NPs, blank-NPs, and NAT through the inhibition zone experiment Figure 7(c-d) and Table 5. CTS-NPs also presented considerable antifungal effects and were stronger than free NAT. Notably, the antifungal effect of NAT-NPs was far stronger than that of NAT and CTS. A synergistic effect may exist between NAT and CTS. These results may provide useful information for the facile application of NAT-NPs.

(a)

(b)

(a)

(b)

(c)

(d)

5. Conclusions

In this study, NAT-NPs exhibited good physicochemical properties and proved that NAT-NPs had a strong antifungal effect on C. albicans. The reason why NAT-NP had a stronger antifungal effect than NAT was related to the antifungal properties of CTS itself. CTS enhances NAT in the antifungal direction, making CTS an excellent carrier of NAT. Therefore, NAT-NPs is expected to be effective in clinical fungal keratitis due to its potent ability to inhibit fungi. Although the NPs formed in this paper demonstrated the slow-release effect of NAT-NPs and strong antifungal effects, further studies should be conducted to enable NAT-NPs to be applied earlier in clinical patients with fungal keratitis.

Data Availability

All the data of the study can be obtain by contacting with the corresponding author.

Conflicts of Interest

The author(s) declare(s) that they have no conflicts of interest.

Acknowledgments

The authors are indebted to the financial support from the National Natural Science Foundation of China (Nos. 81774125, 81973671), the Natural Science Foundation of Shandong Province (No. ZR2019BB071), and the Major Innovation and Technology Engineering Project of Shandong Province (No. 2019JZZY011106).

References

D. He, J. Hao, B. Zhang et al., “Pathogenic spectrum of fungal keratitis and specific identification of Fusarium solani,” Investigative Ophthalmology & Visual Science, vol. 52, no. 5, pp. 2804–2808, 2011.
View at: Publisher Site | Google Scholar
P. K. Shukla, M. Kumar, and G. B. Keshava, “Mycotic keratitis: an overview of diagnosis and therapy,” Mycoses, vol. 51, no. 3, pp. 183–199, 2008.
View at: Publisher Site | Google Scholar
P. A. Thomas, “Fungal infections of the cornea,” Eye (London, England), vol. 17, no. 8, pp. 852–862, 2003.
View at: Publisher Site | Google Scholar
T. Sirikul, T. Prabriputaloong, A. Smathivat, R. S. Chuck, and A. Vongthongsri, “Predisposing factors and etiologic diagnosis of ulcerative keratitis,” Cornea, vol. 27, no. 3, pp. 283–287, 2008.
View at: Publisher Site | Google Scholar
F. Mellado, T. Rojas, and C. Cumsille, “Fungal keratitis: review of diagnosis and treatment,” Arquivos Brasileiros de Oftalmologia, vol. 76, no. 1, pp. 52–56, 2013.
View at: Publisher Site | Google Scholar
M. Srinivasan, “Fungal keratitis,” Current Opinion in Ophthalmology, vol. 15, no. 4, pp. 321–327, 2004.
View at: Publisher Site | Google Scholar
N. V. FlorCruz, I. V. Peczon, and J. R. Evans, “Medical interventions for fungal keratitis,” Cochrane Database of Systematic Reviews, vol. 2, article CD004241, 2012.
View at: Publisher Site | Google Scholar
N. V. FlorCruz and I. V. Peczon, “Medical interventions for fungal keratitis,” Cochrane Database of Systematic Reviews, vol. 1, article CD004241, 2008.
View at: Publisher Site | Google Scholar
Y. F. Li, J. Jin, Q. Guo, Y. M. Ha, and Q. P. Li, “Complexation of synthetic CDM-AM copolymer with natamycin and carbendazim to improve solubility and fungicidal activity,” Carbohydrate Polymers, vol. 125, pp. 288–300, 2015.
View at: Publisher Site | Google Scholar
U. B. Kompella, A. C. Amrite, R. Pacha Ravi, and S. A. Durazo, “Nanomedicines for back of the eye drug delivery, gene delivery, and imaging,” Progress in Retinal and Eye Research, vol. 36, pp. 172–198, 2013.
View at: Publisher Site | Google Scholar
D. Gulsen and A. Chauhan, “Ophthalmic drug delivery through contact lenses,” Investigative Ophthalmology & Visual Science, vol. 45, no. 7, pp. 2342–2347, 2004.
View at: Publisher Site | Google Scholar
J. Kim, A. Conway, and A. Chauhan, “Extended delivery of ophthalmic drugs by silicone hydrogel contact lenses,” Biomaterials, vol. 29, no. 14, pp. 2259–2269, 2008.
View at: Publisher Site | Google Scholar
T. Bourcier, A. Sauer, A. Dory, J. Denis, and M. Sabou, “Fungal keratitis,” Journal Français d'Ophtalmologie, vol. 40, no. 9, pp. e307–e313, 2017.
View at: Publisher Site | Google Scholar
G. G. Müller, N. Kara-José, and R. S. . Castro, “Antifúngicos em infecções oculares: drogas e vias de administração,” Revista Brasileira de Oftalmologia, vol. 72, no. 2, pp. 132–141, 2013.
View at: Publisher Site | Google Scholar
P. W. Morrison and V. V. Khutoryanskiy, “Advances in ophthalmic drug delivery,” Therapeutic Delivery, vol. 5, no. 12, pp. 1297–1315, 2014.
View at: Publisher Site | Google Scholar
D. R. Janagam, L. Wu, and T. L. Lowe, “Nanoparticles for drug delivery to the anterior segment of the eye,” Advanced Drug Delivery Reviews, vol. 122, pp. 31–64, 2017.
View at: Publisher Site | Google Scholar
R. Herrero-Vanrell, M. Vicario de la Torre, V. Andrés-Guerrero, D. Barbosa-Alfaro, I. T. Molina-Martínez, and I. Bravo-Osuna, “Nano and microtechnologies for ophthalmic administration, an overview,” Journal of Drug Delivery Science and Technology, vol. 23, no. 2, pp. 75–102, 2013.
View at: Publisher Site | Google Scholar
A. Urtti, “Challenges and obstacles of ocular pharmacokinetics and drug delivery,” Advanced Drug Delivery Reviews, vol. 58, no. 11, pp. 1131–1135, 2006.
View at: Publisher Site | Google Scholar
S. L. Fialho and A. da Silva-Cunha, “New vehicle based on a microemulsion for topical ocular administration of dexamethasone,” Clinical & Experimental Ophthalmology, vol. 32, no. 6, pp. 626–632, 2004.
View at: Publisher Site | Google Scholar
A. M. de Campos, A. Sánchez, R. Gref, P. Calvo, and M. J. Alonso, “The effect of a PEG versus a chitosan coating on the interaction of drug colloidal carriers with the ocular mucosa,” European Journal of Pharmaceutical Sciences, vol. 20, no. 1, pp. 73–81, 2003.
View at: Publisher Site | Google Scholar
M. Kassem, A. Abdelrahman, M. Ghorab, M. Ahmed, and R. Khalil, “Nanosuspension as an ophthalmic delivery system for certain glucocorticoid drugs,” International Journal of Pharmaceutics, vol. 340, no. 1-2, pp. 126–133, 2007.
View at: Publisher Site | Google Scholar
D. Owensiii and N. Peppas, “Opsonization, biodistribution, and pharmacokinetics of polymeric nanoparticles,” International Journal of Pharmaceutics, vol. 307, no. 1, pp. 93–102, 2006.
View at: Publisher Site | Google Scholar
A. A. Badawi, H. M. El-Laithy, R. K. El Qidra, H. El Mofty, and M. El dally, “Chitosan based nanocarriers for indomethacin ocular delivery,” Archives of Pharmacal Research, vol. 31, no. 8, pp. 1040–1049, 2008.
View at: Publisher Site | Google Scholar
R. C. Nagarwal, R. Kumar, and J. K. Pandit, “Chitosan coated sodium alginate-chitosan nanoparticles loaded with 5-FU for ocular delivery: In vitro characterization and in vivo study in rabbit eye,” European Journal of Pharmaceutical Sciences, vol. 47, no. 4, pp. 678–685, 2012.
View at: Publisher Site | Google Scholar
M. A. Kalam, “The potential application of hyaluronic acid coated chitosan nanoparticles in ocular delivery of dexamethasone,” International Journal of Biological Macromolecules, vol. 89, pp. 559–568, 2016.
View at: Publisher Site | Google Scholar
R. Sharma, M. Ahuja, and H. Kaur, “Thiolated pectin nanoparticles: Preparation, characterization and ex vivo corneal permeation study,” Carbohydrate Polymers, vol. 87, no. 2, pp. 1606–1610, 2012.
View at: Publisher Site | Google Scholar
H. Vaghari, H. Jafarizadeh-Malmiri, A. Berenjian, and N. Anarjan, “Recent advances in application of chitosan in fuel cells,” Sustainable Chemical Processes, vol. 1, no. 1, p. 16, 2013.
View at: Publisher Site | Google Scholar
S. A. Agnihotri, N. N. Mallikarjuna, and T. M. Aminabhavi, “Recent advances on chitosan-based micro- and nanoparticles in drug delivery,” Journal of Controlled Release, vol. 100, no. 1, pp. 5–28, 2004.
View at: Publisher Site | Google Scholar
J. Kumirska, M. X. Weinhold, J. Thöming, and P. Stepnowski, “Biomedical activity of chitin/chitosan based materials—influence of physicochemical properties apart from molecular weight and degree of N-acetylation,” Polymers, vol. 3, no. 4, pp. 1875–1901, 2011.
View at: Publisher Site | Google Scholar
X. Wang, S. Wang, and Y. Zhang, “Advance of the application of nano-controlled release system in ophthalmic drug delivery,” Drug Delivery, vol. 23, no. 8, pp. 2897–2901, 2016.
View at: Publisher Site | Google Scholar
O. M. Sharaf, M. S. Al-Gamal, G. A. Ibrahim et al., “Evaluation and characterization of some protective culture metabolites in free and nano-chitosan-loaded forms against common contaminants of Egyptian cheese,” Carbohydrate Polymers, vol. 223, article 115094, 2019.
View at: Publisher Site | Google Scholar
R. S. Bhatta, H. Chandasana, Y. S. Chhonker et al., “Mucoadhesive nanoparticles for prolonged ocular delivery of natamycin: in vitro and pharmacokinetics studies,” International Journal of Pharmaceutics, vol. 432, no. 1-2, pp. 105–112, 2012.
View at: Publisher Site | Google Scholar
F. Sonvico, A. Cagnani, A. Rossi et al., “Formation of self-organized nanoparticles by lecithin/chitosan ionic interaction,” International Journal of Pharmaceutics, vol. 324, no. 1, pp. 67–73, 2006.
View at: Publisher Site | Google Scholar
A. R. N. Pontillo and A. Detsi, “Nanoparticles for ocular drug delivery: modified and non-modified chitosan as a promising biocompatible carrier,” Nanomedicine (London, England), vol. 14, no. 14, pp. 1889–1909, 2019.
View at: Publisher Site | Google Scholar

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Copyright © 2021 Yaling Liu et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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