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Article

Synthesis of Chitosan-Coated Silver Nanoparticle Bioconjugates and Their Antimicrobial Activity against Multidrug-Resistant Bacteria

by
Surbhi Shinde
1,
Veronica Folliero
1,
Annalisa Chianese
1,
Carla Zannella
1,
Anna De Filippis
1,
Luigi Rosati
2,
Marina Prisco
2,
Annarita Falanga
3,
Avinash Mali
1,
Marilena Galdiero
1,
Massimiliano Galdiero
1,* and
Gianluigi Franci
4,5,*
1
Department of Experimental Medicine, University of Campania “Luigi Vanvitelli”, 80138 Naples, Italy
2
Department of Biology, University of Naples “Federico II”, 80126 Naples, Italy
3
Department of Agricultural Science, University of Naples “Federico II”, 80055 Naples, Italy
4
Department of Medicine, Surgery and Dentistry “Scuola Medica Salernitana”, University of Salerno, 84081 Baronissi, Italy
5
Department of Sanitary Hygiene and Evaluative Medicine U.O.C. Clinical and Microbiological Pathology, Ruggi D’Aragona Medical School of Salerno, University Hospital of S. Giovanni di Dio, 84131 Salerno, Italy
*
Authors to whom correspondence should be addressed.
Appl. Sci. 2021, 11(19), 9340; https://doi.org/10.3390/app11199340
Submission received: 12 May 2021 / Revised: 3 October 2021 / Accepted: 6 October 2021 / Published: 8 October 2021
(This article belongs to the Special Issue Natural Compounds with Antimicrobial and Immunomodulatory Activity)
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Versions Notes

Abstract

:
The increase in multidrug-resistant bacteria represents a true challenge in the pharmaceutical and biomedical fields. For this reason, research on the development of new potential antibacterial strategies is essential. Here, we describe the development of a green system for the synthesis of silver nanoparticles (AgNPs) bioconjugated with chitosan. We optimized a Prunus cerasus leaf extract as a source of silver and its conversion to chitosan–silver bioconjugates (CH-AgNPs). The AgNPs and CH-AgNPs were characterized using transmission electron microscopy (TEM), dynamic light scattering (DLS), Fourier transform infrared spectroscopy (FT-IR), ultraviolet–visible spectroscopy (UV–Vis), and zeta potential measurement (Z-potential). The cytotoxic activity of AgNPs and CH-AgNPs was assessed on Vero cells using the 3-[4.5-dimethylthiazol-2-yl]-2.5-diphenyltetrazolium bromide (MTT) cell proliferation assay. The antibacterial activity of AgNPs and CH-AgNPs synthesized using the green system was determined using the broth microdilution method. We evaluated the antimicrobial activity against standard ATCC and clinically isolated multisensitive (MS) and multidrug-resistant bacteria (MDR) Escherichia coli (E. coli), Enterococcus faecalis (E. faecalis), Klebsiella pneumonia (K. pneumoniae), and Staphylococcus aureus (S. aureus), using minimum inhibitory concentration (MIC) assays and the broth dilution method. The results of the antibacterial studies demonstrate that the silver chitosan bioconjugates were able to inhibit the growth of MDR strains more effectively than silver nanoparticles alone, with reduced cellular toxicity. These nanoparticles were stable in solution and had wide-spectrum antibacterial activity. The synthesis of silver and silver chitosan bioconjugates from Prunus cerasus leaf extracts may therefore serve as a simple, ecofriendly, noncytotoxic, economical, reliable, and safe method to produce antimicrobial compounds with low cytotoxicity.

1. Introduction

Multidrug-resistant bacteria (MDR), also known as “superbugs”, represent a serious threat to our society. Over time, microorganisms are gaining resistance to the available antimicrobials, and there is an urgent need to develop innovative and effective antimicrobial approaches. To date, specific resistance has developed against most antibiotics [1]. There are two main problems that should be addressed: (i) the lack of new classes of antibiotics; (ii) the shortening window between the commercial use of new variants of old antibiotics and the outbreak of resistant bacterial strains [2]. In recent years, antibiotics have been given in high doses due to increasing drug resistance, and the resulting toxicity has focused the attention on the need to develop and define innovative and effective antimicrobial treatments [3,4].
In the last 20 years, the emergence of nanotechnology has been allowing for the development of new potential alternative antimicrobial agents to be used against bacterial infections and for drug delivery, in both in vitro and in vivo models [5,6]. Among the metal nanoparticles, silver nanoparticles are studied for their excellent antimicrobial properties, which are due to silver ions inhibiting bacterial DNA replication and damaging cytoplasmic membrane, which causes cell death after a decrease in ATP levels [6]. These observations suggest that nanoparticles can be effective against both Gram-positive and Gram-negative bacteria. There are many advantages of using silver nanoparticles (AgNPs) as antimicrobial agents: they have high antibacterial activity based on multiple mechanisms of action and can help in overcoming the resistance of microorganisms to conventional antibiotics [7]. In addition, AgNPs can be synthesized with simpler and cheaper methods using chemical reactions and biosynthesis [8]. In the study of Rozykulyyeva et al., Punica granatum AgNPs showed high antibacterial activity on different oral pathogens, such as Actinobacillus actinomycetemcomitans, Pseudomonas aeruginosa, E. faecalis, and S. aureus [9]. Likewise, Ying Loo et al. reported a high antibacterial effect of pu-erh tea AgNPs against E. coli, K. pneumoniae, Salmonella typhimurium, and Salmonella enteritidis, with minimum inhibitory concentrations (MICs) of between 7.8 and 3.9 μg/mL recorded [10].
AgNPs simultaneously act on cell wall and cell permeability, impair metabolic pathways, induce DNA damage, inhibit protein synthesis and function, and promote the formation of reactive oxygen species [6,11]. Nanoparticles can be synthesized using various mechanisms and chemical and physical methods. The most cost effective, ecofriendly, and nonhazardous methods for synthesizing nanoparticles are those characterized as green approaches or green nanoparticle synthesis [12].
Green synthesis of nanoparticles employs processes using natural materials and is more innovative and cheaper than previous strategies [13,14]. The widespread availability of biological resources and the simplicity of the methodology are key benefits promoting the popular use of green chemistry for metal nanoparticle synthesis [15,16]. Presently, phytonanotechnology has been presented as a new avenue for nanoparticle synthesis with applications in the biomedical and environmental fields [17].
The low toxicity, potential antimicrobial activity, and opportunity for green synthesis of nanoparticles herald a new era of their production. Natural components for AgNP production with improved antimicrobial properties have recently been proposed, with one example being chitosan [18,19,20]. Chitosan is a natural polysaccharide biopolymer which consists of two monosaccharides, GlcNAc and D-glucosamine (GlcN), linked together by β-(1→4) glycosidic bonds [21]. Researchers have determined that chitosan from sweet cherry (Prunus avium L.) can inhibit the growth of microorganisms [22,23]. The main properties of chitosan are its nontoxicity, biocompatibility, biodegradability, and hemostatic properties. Due to these effects, polyelectrolytes such as chitosan have been used in various ways to stabilize nanoparticles and to increase their antimicrobial properties upon successful formation of polymer–metal ion complexes [24]. Previous studies have shown that chitosan can stabilize nanoparticle surfaces and thereby modulate cytotoxicity. Moreover, AgNPs coated with chitosan demonstrated high efficiency in killing common Gram-positive and Gram-negative bacteria as well as some fungi [25].
Considering the importance of metal nanoparticle synthesis, especially those of silver synthesized using different plants, the aim of this study was to develop a method for green synthesis of silver nanoparticles (AgNPs) with stable chitosan-coated silver nanoparticles (CH-AgNPs) using Prunus cerasus leaf extracts. Investigation of their antimicrobial activity has focused on different Gram-positive and Gram-negative strains of bacteria, paving the way for the possibility for their translation into clinical settings as an alternative antimicrobial strategy.

2. Materials and Methods

2.1. Tested Microorganisms

E. coli (ATCC 11229), E. faecalis (ATCC 29212), K. pneumoniae (ATCC 10031), and S. aureus (ATCC 6538) were obtained from the American Type Culture Collection (ATCC, Manassas, VA, USA. The multidrug-resistant (MDR) clinical isolates and multisensitive (MS) clinical isolates were collected from the “Vanvitelli” University Hospital based in Naples. Bacteria were identified via MALDI-TOF MS (Bruker Daltonics, Bremen, Germany) and the antibiotic resistance patterns were evaluated using a BD Phoenix system (Becton Dickinson, USA). The antibiotic resistance profile of the ATCC bacterial strains and clinical isolates used in the study are reported in Table 1 and Table 2, respectively.

2.2. Preparation of Chitosan Solution

Chitosan solution was prepared by dissolving chitosan (from shrimp shells, ≥75% deacetylated, C3646) powder to 0.1% (m/v) in 1% aqueous acetic acid solution (A6283) with subsequent stirring to promote dissolution. All the reagents were analytical grade, purchased from Sigma-Aldrich and were used without further purification.

2.3. Preparation of Plant Extract and Synthesis of Silver Nanoparticles

Fresh leaves grown by a local farmer under biological growth conditions were collected and then washed thoroughly with tap water three times followed by double sterile distilled water to remove dust particles. After washing, 10 g of fresh plant leaves were boiled in 100 mL of sterile distilled water in a 500 mL Erlenmeyer flask for 20 min. The extract was separated from the leaves via decantation and then filtered with Whatman filter paper No. 1. Thereafter, 5 mL of leaf extract was diluted with 4.5 mL of double distilled water and treated with 0.5 mL of 1 mM silver nitrate salt (AgNO3, 99.8%, Sigma, St Louis, MO, USA). The color change reaction was observed, indicating pH 6. This color change is indicative of nanoparticle formation, and the reaction mixture was then stored at room temperature for 24 h in the dark. The reaction mixture was then lyophilized to obtain nanoparticles in powder form. The lyophilization process was carried out in a freezer at −55 °C for 24 h, followed by processing conditions at a chamber pressure of 1000 mbar for 24 h.
The Prunus cerasus plant materials were harvested from a local farmer in Caserta (Campania, Italy) and authenticated through molecular analysis of the internal transcribed spacer (ITS) region of nuclear ribosomal DNA (data not shown). No approvals were required for the study, which complied with all relevant regulations.

2.4. Synthesis of Silver Chitosan Nanoparticles

A 5 mL volume of leaf extract solution was combined with 3 mL of 1% chitosan solution (dissolved in acetic acid solution). Further, the reaction mixture was allowed to mix for 30 min and 1 mL of 1 mM silver nitrate (Sigma-Aldrich, St Louis, MO, USA) solution was added dropwise to the reaction mixture while it was magnetically stirred at 70 °C. Then, the reaction mixture was incubated for an additional 2 h. The mixture changed from colorless to light yellow within 30 min and, finally, to dark yellowish brown after the completion of the reaction. This change in color indicates the formation of chitosan-coated silver nanoparticles (CH-AgNPs). The synthesis process was monitored by visual observation of the color change and agglomeration within a certain period of time (24–48 h). Furthermore, to obtain CH-AgNP powder, the mixture was lyophilized after 48 h of reaction. The reaction was treated at −55 °C for 24 h and subjected to a chamber pressure of 1000 mbar for the next 24 h. The dried powder was designated as CH-AgNPs and stored for further study.

2.5. UV–Vis Spectroscopy

The optical properties of CH-AgNPs were observed using a UV–Vis spectrophotometer. After the addition of leaf extracts to silver nitrate solution the spectra were taken and a blank (distilled water) was used as reference for baseline correction. The results were recorded with the Analytik Jena Specord 210 Plus190 (UV–Vis) at 1100 nm. The spectrophotometer used synthetic quartz spectrophotometer cells (190–2500 nm, path length 10 mm, volume 1.75 mL). The measurements were collected at a wavelength range of between 200 and 800 nm at 1 nm resolution.

2.6. Dynamic Light Scattering and Zeta Potential

The size of AgNPs and CH-AgNPs was determined by dynamic light scattering (DLS) and the charge present on the surface of nanoparticles was determined using the Zetasizer Nanoseries (MALVERN Zetasizer Nano ZS, Malvern, UK). Zeta potentials were measured at 25 °C and obtained data were analyzed using Zetasizer software.

2.7. FT-IR Analysis

Nanoparticles in dried powder form were characterized by Fourier transform infrared spectroscopy (JASCO FT/IR-4100). Spectra were taken in the range of 400–4000 cm−1 at a resolution of 4 cm−1. The data from the FTIR reveal information about functional groups which are present in the nanoparticles.

2.8. Transmission Electron Microscopy Analysis

For determining the exact size and morphology of the AgNPs and CH-AgNPs, transmission electron microscopy (FEI Tecnai G2, TEM) was used. For analysis, 5 µL of AgNPs or CH-AgNPs was placed onto carbon-coated copper microgrids; excess solution was removed using filter paper, and the specimens were dried at room temperature. Staining was performed using UranyLess (EMS, Hatfield, PA, USA) for 2 min at room temperature; the grids were blotted on filter paper then washed with distilled water and air dried at room temperature. Further, TEM observation was performed using a FEI Tecnai G2 operating at 120 kV, with images captured by FEI TEM Imaging and Analysis (version 4.7 SP3).

2.9. Cytotoxicity Assay

In order to determine the efficacy and to provide biocompatibility of chitosan with AgNPs, we synthesized chitosan-coated silver nanoparticles and screened for their toxicity on Vero cell lines (ATCC® CCL-81™). The cytotoxicity of nanoparticles was evaluated using the 3-[4.5-dimethylthiazol-2-yl]-2.5-diphenyltetrazolium bromide (MTT) (Sigma-Aldrich, M2128) assay, based on the reduction of the yellowish MTT to the insoluble and dark blue formazan by viable and metabolically active cells [26]. Vero cells were cultured in Dulbecco’s modified Eagle’s medium (DMEM), 2 mM glutamine, 100 µg/mL penicillin, 0.1 mg/mL streptomycin, and 10% fetal calf serum in a 5% CO2 in incubator, seeded at 5 × 103 cells/well in 96-well plates and incubated for 24 h at 37 °C in 5% CO2. AgNPs and CH-AgNPs were tested at 50 µg/mL concentration followed by 2-fold dilution. After 24 h of incubation, 100 μL of MTT solution was added to cells and incubated for 3 h at 37 °C in 5% of CO2. Further MTT solution was removed and 100 μL dimethyl sulfoxide (DMSO) was added followed by incubation for 10 min at room temperature to dissolve the formazan crystals. Finally, the absorbance was measured at 540 nm and the data were analyzed. The experiment was corroborated by comparison to an untreated control (cells not treated with any compound).

2.10. Evaluation of Antibacterial Activity

MIC values of the nanoparticle suspensions were determined using the microdilution method, conducted in 96-well plates. The studies were performed in accordance with the Clinical and Laboratory Standards Institute (CLSI). Each substance was serially diluted to obtain concentrations in the range of 0.78 to 100 μg/mL. Ampicillin and vancomycin (ranging from 0.25 to 4 μg/mL) were used as a positive control for Gram-negative and Gram-positive bacteria, respectively. Untreated bacteria were used as negative control. Bacterial suspensions were adjusted to contain approximately 1 × 106 CFU/mL of bacteria. A volume of 50 µL of the inoculum was added to the wells, obtaining a concentration of 5 × 105 CFU/well. The plates were then incubated at 37 °C for 20 h.
Medium turbidity was measured using a microtiter plate reader (Sunrise, Tecan Austria GmbH, Austria) at 595 nm. MIC is the lowest concentration of a compound which causes 100% inhibition of microbial growth. All experiments were performed in triplicate, and values are reported as mean ± standard deviation.

2.11. Statistical Analysis

All analytical determinations were performed in triplicate, and the results are expressed as mean ± standard deviation. The statistical significance was assessed by GraphPad InStat 3 software (GraphPad Software, CA, USA), at a significance threshold value of p < 0.05.

3. Results

3.1. Characterization and Identification of CH-AgNPs

After mixing Prunus cerasus leaf extract with AgNO3 solution, we observed a color change from colorless to brown and yellowish brown, which indicates the formation of AgNPs and CH-AgNPs, respectively. The synthesis of AgNPs and CH-AgNPs were confirmed via UV–Vis spectroscopy analysis. UV–Vis spectra of nanoparticles were recorded in the range of 200–800 nm. UV–Vis spectra of AgNPs and CH-AgNPs exhibited a peak at 429 and 445 nm, respectively, which is mainly due to the surface plasmon resonance of nano forms of silver (Figure 1).
The second step in physicochemical characterization is the average particle size distribution by dynamic light scattering (DLS). The data highlighted that the average sizes of AgNPs and CH-AgNPs were 32.16 and 50 nm, respectively, with a polydispersity index of 0.2 (Figure 2a,b). The increase in CH-AgNP size is due to the chitosan coating AgNPs. We further investigated our biologically synthesized AgNPs and CH-AgNPs with surface charge definition via zeta potential analysis. The results indicate that AgNPs had a charge of −7.20 mV, while CH-AgNPs scored a value of 9 mV, with both measurements indicating the nanoparticles were stable (Figure 3a,b).

3.2. FT-IR Analysis of Biosynthesized CH-AgNPs

T-IR analysis of AgNPs and CH-AgNPs was performed in order to confirm the reduction of the molecular interaction and capping agent which is responsible for synthesizing and stabilizing the nanoparticles. This approach is generally used for qualitative analysis of nanostructures. FT-IR spectra of AgNPs shows peaks at 3280, 2856, 1527, 1295, 1017 and 823 cm−1 and a similar pattern for CH-AgNPs detected with peaks at 3178, 1653, 1509, 1381, 1278, and 1042 cm−1, respectively (Figure 4b,c). These peaks represent functional groups at different wavenumbers. The absorbance peak at 3280 cm−1 can be attributed to the vibrations of amino groups (N–H), which may be the presence of peptides, whereas the peak at 2856 cm−1 may be because of sym –CH3 stretching vibrations. However, the peak at 1527 cm−1 can be assigned to C=N stretching vibration, and the peak at 1295 cm−1 may be because of C–H deformation vibration. Similarly, the peak 1017 cm−1 can be assigned to C–O stretching vibration and peak at 823 cm−1 may be because of C–C skeletal vibration (Table 3). In case of CH-AgNPs, the peak at 3178 cm−1 is associated with amide group N–H stretching. The vibration peak shown at 1653 cm−1 can be assigned to C=C stretching vibrations. Moreover, a peak of 1509 cm−1 may be due to a broad amide II band. The peaks 1381, 1278, and 1042 cm−1 are assigned to C–H deformation vibration sym, C–H sym deformation vibration, and C–C skeleton vibration, respectively (Table 4).

3.3. Transmission Electron Microscopy (TEM) Analysis of Biosynthesized CH-AgNPs

Furthermore, TEM analysis confirmed that silver nanoparticles showed a spherical shape and polydisperse nature (Figure 5a,b). Interestingly, in the case of CH-AgNPs, the morphology of particles was spherical with a thin chitosan coating surrounding the silver core (Figure 5c,d). Moreover, a homogeneous distribution of the chitosan coating around the silver nanostructures was observed via TEM micrographs. The absence of aggregation was detected when nanoparticles were analyzed; this clearly indicates that nanoparticles were completely coated by a polymer. Indeed, AgNPs coated with chitosan showed a clear layer surrounding their core.

3.4. Evaluation of Cytotoxic Activity

One of the main goals of our study was the prospect of reducing the cellular toxicity of AgNPs and CH-AgNPs. In order to evaluate the chitosan contribution for this purpose, we investigated their effects on human cell lines. The MTT cell toxicity assay was performed against Vero cells treated with AgNPs and CH-AgNPs, respectively. Indeed, the data from the cell toxicity assay show that both the AgNPs and CH-AgNPs did not exhibit remarkable toxic effects in terms of Vero cell viability, even at the highest tested concentration of 50 μg/mL (Figure 6).

3.5. Evaluation of Antimicrobial Activity

We achieved a decrease in toxic properties of AgNPs and CH-AgNPs prepared from Prunus cerasus via the green synthesis method. They were then evaluated for their antibacterial activity. As a system model for the assay, we used two different species for both Gram-positive and Gram-negative bacteria (Figure 7a,b). Among Gram-positive bacteria, ATCC, MS, and MDR strains of E. faecalis and S. aureus were selected. In addition, we selected the Gram-negative bacteria ATCC, MS, and MDR strains of E. coli and K. pneumoniae. The antibacterial properties were evaluated using the microdilution method. The CH-AgNP have MICs ranging from 6.5 to 50 µg/mL and 12.5 to 25 µg/mL against the Gram-positive and Gram-negative strains, respectively. On the contrary, AgNPs have higher MICs as compared to CH-AgNPs; i.e., for Gram-positive strains, the MICs range from 100 to 12.5 µg/mL and for Gram-negative 50 to 12.5 µg/mL. The MIC of CH-AgNPs was significantly lower than that of bare AgNPs (p < 0.05). The MIC of CH-AgNP against Gram-negative bacteria ATCC, MDR, and MS strains was 12.5, 25, and 12.5 µg/mL, respectively. In the case of Gram-positive bacteria, E. faecalis ATCC, MDR, and MS strains have MICs of 6.5, 12.5, and 25 µg/mL, respectively. S. aureus ATCC 6538, MDR, and MS strains have MICs of 25 and 50 µg/mL, respectively. The high performance of CH-AgNP could be attributed to the presence of Ag+ and also positively charged groups in the chitosan structure. However, the Prunus cerasus leaf extract and chitosan solutions did not show any antimicrobial effect against bacteria.

4. Discussion

Although the use of silver and silver salts as antibacterial agents is an ancient method, silver nanoparticle (AgNP) fabrication has only recently been developed. Silver nanoparticles are well known for their antimicrobial activity, and there are also reports of their acute and chronic toxicity [36,37]. With this in mind, nanoparticles were obtained via green synthesis with the addition of compounds/peptides/chemical groups on their surfaces. This method is able to reduce toxicity to allow the application of nanoparticles in the treatment of human infectious diseases. Among the possible coatings, chitosan-coated silver nanoparticles have attracted significant attention in the biomedical field because of their unique biodegradable, biocompatible, nontoxic, and antimicrobial nature [38]. Many scientists have reported that chitosan has a strong affinity for metal ions as a result of a large number of amino and hydroxyl groups. In a study conducted by Nate et al. (2018), the role of the chitosan amino group was defined as being crucial for metal ion release and the formation of CH-AgNPs [39]. Plants represent the main source for NP synthesis. Several studies have demonstrated that the polyphenols present in plant extracts play a major role in the reduction of Ag+ ions [40]. In the present study, the antibacterial effect of CH-AgNPs prepared using Prunus cerasus leaf extract was assessed. The multitude of bioactive compounds present in Prunus cerasus makes it an excellent candidate for the synthesis of nanoparticles [41]. Moreover, the synthesis of metal nanoparticles using Prunus cerasus has not been explored to any great extent.
The results of UV–visible spectroscopy obtained in our study revealed a difference in size between AgNPs and CH-AgNPs. The CH-AgNPs were larger than uncoated AgNPs since layers of chitosan were observed to be wrapped around AgNPs, as in the work described by Lim et al. (2013) [42]. The zeta potential on the surface of nanoparticles indicates the particles are stable. Nanoparticles possessing higher negative or positive zeta potentials will tend to repel each other and do not form aggregates [43,44]. Our synthesized nanoparticles were found to be more stable than those previously reported in studies [45]. In the current study, the FT-IR analysis showed that numerous amino groups act as capping agents. The results clearly indicate that these identified amino groups are responsible for the interaction with the metal surface, acting as capping sites for AgNP stabilization [46]. From the results, it can be concluded that capping agents allow proteins to bind to AgNPs by the electrostatic attraction of negatively charged carboxylate groups present in the protein secreted by plants [47]. Many of the peaks observed in the IR spectra of AgNPs and CH-AgNPs are closely associated with flavonoids and terpenoids, suggesting the adsorption of these molecules on the nanoparticle surface. The presence of several functional groups can influence the reduction of metal ions into corresponding metal nanoparticles. Using TEM analysis, we observed the presence of polydisperse nanoparticles [45]. The TEM images clearly indicated a difference in average size, which were 32 and 50 nm for AgNPs and CH-AgNPs, respectively. The cytotoxicity of synthesized AgNPs and CH-AgNPs was screened in order to define the optimal concentrations for antimicrobial assays. The results reveal that CH-AgNPs did not show any relevant cytotoxicity against the Vero cell line for each tested concentration. We observed that CS-AgNPs at 312.5 μg/mL did not exhibit any cytotoxicity against L-929 fibroblast cells as has been previously reported [48]. The antibacterial potential of CH-AgNPs was evaluated against standard and clinically isolated Gram-positive and Gram-negative isolates. The CH-AgNPs efficiently inhibited bacterial growth compared to AgNPs. Our findings show that the MIC values of CH-AgNPs were lower than those of AgNPs. Within the same species, the coated nanoparticles exhibited a different effect between the various strains. A lower MIC value was recorded for the MDR strains. The stronger structural properties of the MDR strains could justify the lower MIC values recorded [49]. The present antimicrobial evaluation studies agreed with the reports of Asghar et al. 2020 [44]. Therefore, it could be assumed that the use of CH-AgNPs at their MIC value can effectively inhibit the growth of bacteria while not being toxic to normal cells. The mechanism of action for the antibacterial activity of chitosan might come from the contact-inhibitory mechanism between negatively charged teichoic acid in the peptidoglycan layer on the bacterial surface and the positively charged protonated amine moieties on the chitosan backbone [50]. Similar studies reported that the enhanced antibacterial activity of CH-AgNPs is due to the synergistic antibacterial potential of AgNPs with chitosan [51]. It is notable that metal NPs have more relevant bactericidal effects due to their high affinity with the active surface groups of microbial strains [52]. Similarly, it has been suggested that chitosan reacts with both the bacterial cell wall and the cell membrane [53].

5. Conclusions

The simple and rational exploitation of a green synthesis procedure was used to produce biogenic silver nanoparticles and silver nanoparticles conjugated with chitosan. On the basis of obtained results, the combination of chitosan with AgNPs against Gram-positive and Gram-negative bacteria offers a valuable contribution to nanomedicine. In vitro studies show that the chitosan-coated AgNPs exhibited substantial activity against ATCC, MS, and MDR strains. According to these findings, this nanoconjugate system may provide a frugal method for the development of a new generation of effective antibacterial agents. These outcomes open new avenues in the formulation of CH-AgNPs for in vivo studies in animal models in our future research.

Author Contributions

Conceptualization, M.G. (Massimiliano Galdiero) and G.F.; methodology, S.S., V.F., C.Z., A.C. and A.M.; validation, L.R., V.F. and C.Z.; formal analysis, A.F. and L.R.; investigation, resources, S.S., G.F. and M.P.; writing—original draft preparation, S.S, V.F. and C.Z.; writing—review and editing G.F. and A.D.F.; supervision, M.G. (Marilena Galdiero), G.F and M.G. (Massimiliano Galdiero); project administration, M.G. (Massimiliano Galdiero). All authors have read and agreed to the published version of the manuscript.

Funding

This research received no external funding.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable, no study involving humans was performed in this research.

Data Availability Statement

The data presented in this study are available on request from the corresponding author. The data are not publicly available since a public repository was not required for this project.

Conflicts of Interest

The authors declare no conflict of interest.

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Applsci 11 09340 g001 550
Figure 1. UV–Vis absorption spectra of synthesized AgNPs (429 nm) and CH-AgNPs (445 nm).
Figure 1. UV–Vis absorption spectra of synthesized AgNPs (429 nm) and CH-AgNPs (445 nm).
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Applsci 11 09340 g002 550
Figure 2. Particle size distribution of synthesized (A) silver nanoparticles (32.16 nm) and PDI (0.2), and (B) silver chitosan nanoparticles (50 nm) and PDI (0.2).
Figure 2. Particle size distribution of synthesized (A) silver nanoparticles (32.16 nm) and PDI (0.2), and (B) silver chitosan nanoparticles (50 nm) and PDI (0.2).
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Applsci 11 09340 g003 550
Figure 3. Zeta potential analysis of (A) AgNPs (−7.20 mV) and (B) CH-AgNPs (9 mV).
Figure 3. Zeta potential analysis of (A) AgNPs (−7.20 mV) and (B) CH-AgNPs (9 mV).
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Figure 4. FT-IR analysis of (A) AgNPs and (B) FT-IR analysis of silver chitosan nanoparticles.
Figure 4. FT-IR analysis of (A) AgNPs and (B) FT-IR analysis of silver chitosan nanoparticles.
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Figure 5. Transmission electron microscopy analysis of synthesized AgNPs (A,B) and CH-AgNPs (C,D).
Figure 5. Transmission electron microscopy analysis of synthesized AgNPs (A,B) and CH-AgNPs (C,D).
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Figure 6. MTT assay on Vero cells treated with different concentrations of AgNPs and CH-AgNPs for 24 h.—refers to the negative control, i.d. cells treated with DMSO; + indicates positive control that corresponds to cells not treated with any compound. * p < 0.05.
Figure 6. MTT assay on Vero cells treated with different concentrations of AgNPs and CH-AgNPs for 24 h.—refers to the negative control, i.d. cells treated with DMSO; + indicates positive control that corresponds to cells not treated with any compound. * p < 0.05.
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Figure 7. Antibacterial activity of nanoparticles against (A) a panel of Gram-negative bacteria: E. coli ATCC, E. coli MS, E. coli MDR, K. pneumoniae ATCC, K. pneumoniae MS, and K. pneumoniae MDR; (B) S. aureus ATCC, S. aureus MS, S. aureus MDR, E. faecalis ATCC, E. faecalis MS, and E. faecalis MDR. * p < 0.05.
Figure 7. Antibacterial activity of nanoparticles against (A) a panel of Gram-negative bacteria: E. coli ATCC, E. coli MS, E. coli MDR, K. pneumoniae ATCC, K. pneumoniae MS, and K. pneumoniae MDR; (B) S. aureus ATCC, S. aureus MS, S. aureus MDR, E. faecalis ATCC, E. faecalis MS, and E. faecalis MDR. * p < 0.05.
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Table
Table 1. Antibiotic resistance profile of the ATCC bacterial strains: S. aureus, E. faecalis, E. coli, and K. pneumoniae.
Table 1. Antibiotic resistance profile of the ATCC bacterial strains: S. aureus, E. faecalis, E. coli, and K. pneumoniae.
Antibiotic Resistance Profile of the ATCC Bacterial Strains
Staphylococcus aureus ATCC 6538
ANTIBIOTICSMIC (mg/L)INTERPRETATION
Fusidic acid ≤0.5S
Daptomycin0.25S
Erythromycin≤0.25S
Fosfomycin≤8S
Gentamicin≤0.5S
Linezolid2S
Levofloxacin≤0.12S
Oxacillin≤0.25S
Teicoplanin≤0.5S
Tetracycline≤1S
Tigecycline≤0.12S
Trimethoprim/sulfamethoxazole≤10S
Vancomycin≤0.5S
Penicillin≤0.03S
Rifampicin≤0.03S
Enterococcus faecalis ATCC 29212
Ampicillin≤2S
Gentamicin/syn≤500S
Imipenem≤1S
Linezolid2S
Teicoplanin≤0.5S
Tigecycline≤0.12S
Vancomycin2S
Cefuroxime≤64R
Escherichia coli ATCC 11229
Amikacin≤2S
Amoxicillin/clavulanate≤2S
Ampicillin≤8S
Cefepime≤1S
Cefotaxime≤1S
Ceftazidime≤1S
Cefuroxime4S
Ciprofloxacin≤0.25S
Ertapenem≤0.5S
Fosfomycin≤16S
Gentamicin≤1S
Imipenem≤0.25S
Levofloxacin≤0.5S
Meropenem≤0.25S
Piperacillin8S
Piperacillin/tazobactam≤4S
Tobramycin≤1S
Trimethoprim/sulfamethoxazole≤20S
Tigecycline≤0.5S
Klebsiella pneumoniae ATCC 10031
Ciprofloxacin≤0.25S
Fosfomycin≤16S
Ampicillin≤8S
Gentamicin≤1S
Trimethoprim/sulfamethoxazole≤20S
Amikacin≤2S
Amoxicillin/clavulanate≤2S
Cefepime≤1S
Cefotaxime≤1S
Ceftazidime≤1S
Ertapenem≤0.5S
Imipenem0.5S
Meropenem≤0.25S
Piperacillin/tazobactam≤4S
Colistin≤0.5S
Table
Table 2. Antibiotic resistance profile of the clinical isolates: S. aureus MS, S. aureus MDR, E. faecalis MS, E. faecalis MDR, E. coli MS, E. coli MDR, K. pneumoniae MS, and K. pneumoniae MDR.
Table 2. Antibiotic resistance profile of the clinical isolates: S. aureus MS, S. aureus MDR, E. faecalis MS, E. faecalis MDR, E. coli MS, E. coli MDR, K. pneumoniae MS, and K. pneumoniae MDR.
Antibiotic Resistance Profile of the Clinical Isolated Bacteria
Staphylococcus aureus MS
Fusidic acid ≤0.5S
Daptomycin0.25S
Erythromycin≤0.25S
Fosfomycin≤8S
Gentamicin≤0.5S
Linezolid2S
Levofloxacin≤0.12S
Oxacillin≤0.25S
Teicoplanin≤0.5S
Tetracycline≤1S
Tigecycline≤0.12S
Trimethoprim/sulfamethoxazole≤10S
Vancomycin≤0.5S
Penicillin≤0.03S
Fusidic acid ≤0.5S
Daptomycin0.25S
Erythromycin≤0.25S
Staphylococcus aureus MDR
Fusidic acid ≤0.5S
Daptomycin0.25S
Erythromycin>4R
Fosfomycin>64R
Gentamicin>8R
Linezolid2S
Levofloxacin≥8R
Oxacillin>2R
Teicoplanin≤0.5S
Tetracycline≤1S
Tigecycline≤0.12S
Trimethoprim/sulfamethoxazole20S
Vancomycin≤0.5S
Penicillin>0.25R
Rifampicin>2R
Enterococcus faecalis MS
Ampicillin≤2S
Gentamicin/syn≤500S
Imipenem≤2S
Linezolid2S
Teicoplanin≤0.5S
Tigecycline≤0.25S
Vancomycin2S
Cefuroxime≤64R
Enterococcus faecalis MDR
Ampicillin>8R
Gentamicin/syn≥500R
Imipenem>8R
Linezolid2S
Teicoplanin≤0.5S
Tigecycline>0.25R
Vancomycin2S
Cefuroxime≤64R
Escherichia coli MS
Amikacin≤2S
Amoxicillin/clavulanate≤2S
Ampicillin≤8S
Cefepime≤1S
Cefotaxime≤1S
Ceftazidime≤1S
Cefuroxime4S
Ciprofloxacin≤0.25S
Ertapenem≤0.5S
Fosfomycin≤16S
Gentamicin≤1S
Imipenem≤0.25S
Levofloxacin≤0.5S
Meropenem≤0.25S
Piperacillin8S
Piperacillin/tazobactam≤4S
Tobramycin≤1S
Trimethoprim/sulfamethoxazole≤20S
Tigecycline≤0.5S
Escherichia coli MDR
Amikacin>16R
Amoxicillin/clavulanate>32/2R
Ampicillin>8R
Cefepime>8R
Cefotaxime>4R
Ceftazidime>8R
Cefuroxime>8R
Ciprofloxacin>1R
Ertapenem≤0.25S
Fosfomycin≤16S
Gentamicin>4R
Imipenem≤0.25R
Levofloxacin>2R
Meropenem≤0.125S
Piperacillin>16R
Piperacillin/tazobactam>16/4R
Tobramycin>4R
Trimethoprim/sulfamethoxazole≤1/19S
Tigecycline1R
Klebsiella pneumoniae MS
Ciprofloxacin≤0.25S
Fosfomycin≤16S
Gentamicin≤1S
Trimethoprim/sulfamethoxazole≤20S
Amikacin≤2S
Ampicillin ≤8S
Amoxicillin/clavulanate≤2S
Cefepime≤1S
Cefotaxime≤1S
Ceftazidime≤1S
Ertapenem≤0.5S
Imipenem≤0.25S
Meropenem≤0.25S
Piperacillin/tazobactam≤4S
Colistin≤0.5S
Klebsiella pneumoniae MDR
Ciprofloxacin≥4R
Fosfomycin64S
Gentamicin≤1S
Trimethoprim/sulfamethoxazole≥320R
Amikacin≥64R
Amoxicillin/clavulanate≥32R
Ampicillin>8R
Cefepime≥64R
Cefotaxime≥64R
Ceftazidime≥64R
Ertapenem≥8R
Imipenem≥16R
Meropenem≥16R
Piperacillin/tazobactam≥128R
Colistin≤0.5S
Table
Table 3. FT-IR analysis of AgNPs.
Table 3. FT-IR analysis of AgNPs.
Sr No.FT-IR Peak (cm−1) at AgNPsFunctional GroupReferences
13280vibrations of amino groups (N–H)Liu et al. 2013 [26]
22856sym –CH3 stretching vibrationYang et al. 2000 [27]
31527C=N stretching vibrationNabedryk et al. 1986 [28]
41295C–H deformation vibrationYin et al. 2019 [29]
51017C–O stretching vibrationOngen et al. 2012 [30]
6823C–C skeletal vibrationBollino et al. 2017 [31]
Table
Table 4. FT-IR analysis of CH-AgNPs.
Table 4. FT-IR analysis of CH-AgNPs.
Sr No.FT-IR Peak (cm−1) at CH-AgNPsFunctional GroupReferences
13178amide group N–H stretchBen-Refael 2020 [32]
21653C=C stretching vibrationYe et al. 2007 [33]
31509broad amide II bandService et al. 2010 [34]
51278C–H sym deformation vibrationLi et al. 2015 [35]
61042C–C skeleton vibrationLiu et al. 2013 [26]
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Shinde, S.; Folliero, V.; Chianese, A.; Zannella, C.; De Filippis, A.; Rosati, L.; Prisco, M.; Falanga, A.; Mali, A.; Galdiero, M.; et al. Synthesis of Chitosan-Coated Silver Nanoparticle Bioconjugates and Their Antimicrobial Activity against Multidrug-Resistant Bacteria. Appl. Sci. 2021, 11, 9340. https://doi.org/10.3390/app11199340

AMA Style

Shinde S, Folliero V, Chianese A, Zannella C, De Filippis A, Rosati L, Prisco M, Falanga A, Mali A, Galdiero M, et al. Synthesis of Chitosan-Coated Silver Nanoparticle Bioconjugates and Their Antimicrobial Activity against Multidrug-Resistant Bacteria. Applied Sciences. 2021; 11(19):9340. https://doi.org/10.3390/app11199340

Chicago/Turabian Style

Shinde, Surbhi, Veronica Folliero, Annalisa Chianese, Carla Zannella, Anna De Filippis, Luigi Rosati, Marina Prisco, Annarita Falanga, Avinash Mali, Marilena Galdiero, and et al. 2021. "Synthesis of Chitosan-Coated Silver Nanoparticle Bioconjugates and Their Antimicrobial Activity against Multidrug-Resistant Bacteria" Applied Sciences 11, no. 19: 9340. https://doi.org/10.3390/app11199340

APA Style

Shinde, S., Folliero, V., Chianese, A., Zannella, C., De Filippis, A., Rosati, L., Prisco, M., Falanga, A., Mali, A., Galdiero, M., Galdiero, M., & Franci, G. (2021). Synthesis of Chitosan-Coated Silver Nanoparticle Bioconjugates and Their Antimicrobial Activity against Multidrug-Resistant Bacteria. Applied Sciences, 11(19), 9340. https://doi.org/10.3390/app11199340

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