Skip to main content

Antibacterial Activity of In Situ Prepared Chitosan/Silver Nanoparticles Solution Against Methicillin-Resistant Strains of Staphylococcus aureus



Investigation of new effective drugs against the methicillin-resistant strains of Staphylococcus aureus (MRSA) is an urgent issue of modern medicine. Antiseptics as an alternative of antibiotics are strong, sustained, and active preparations against resistant strains and do not violate microbiocenosis.

Materials and Methods

The activity of in situ prepared chitosan-Ag nanoparticles (Ag NPs) solution with different component ratio was tested against MRSA isolated from patients. Ag NPs were synthesized via chemical reduction method using green chemistry approach. In order to improve antimicrobial activity and dispersibility of Ag NPs, surface modification of Ag NPs by cetrimonium bromide (CTAB) was performed.

Ag NPs and chitosan-Ag NPs solution were characterized using X-ray diffraction, transmission electron microscopy, infrared spectroscopy, and spectrophotometric measurements.

Results and Conclusions

The results of XRD, FTIR, UV–Vis, and TEM measurements confirmed the chemical composition of chitosan and Ag NPs and their high purity.

Chitosan-AgNPs solutions have shown their superior antimicrobial efficacy compared to its pure forms. At the same time, in situ preparation of chitosan-Ag NPs solution (chitosan powder 6.0 μg/ml, Ag/CTAB NPs) was not possible due to the precipitation of the components. This result is very promising and may be considered as an effective solution in fighting against drug-resistant bacteria.


Infections remain a major cause of morbidity and mortality worldwide despite the presence of a significant number of antibiotics and antiseptics. In moderate and severe infections, antibiotic therapy is usually initiated empirically before obtaining results of bacteriological examination. Constant use of antibiotics created favorable conditions for the selection and multiplication of antibiotic-resistant microorganisms [22]. High prevalence of multidrug resistance to agents of all infectious processes is documented nowadays [6]. The most notorious multidrug-resistant bacterium is methicillin-resistant Staphylococcus aureus (MRSA) [9]. The pathogen is responsible for a broad spectrum of human and animal diseases ranging from the skin infections to such severe disorders as pneumonia, endocarditis, and septicemia, and these infections may impact human health [32]. Analysis of etiological causes of infections in patients with inadequate therapy revealed that therapy was inadequate in 32.6% cases of MRSA-based infections [12] and associated with 3–4 billion US dollars in annual health care costs [32].

Investigation of new effective drugs against the MRSA is an urgent issue of modern medicine. Antiseptics as an alternative of antibiotics are strong, sustained, and active preparations against resistant strains and do not violate microbiocenosis. Overcoming these problems requires new and innovative preparations. The approach of combining different mechanisms of antibacterial action by designing hybrid nanomaterials provides a new paradigm in the fight against resistant bacteria [18]. Metals, such as copper and silver, are extremely toxic to bacteria at exceptionally low concentrations. Due to biocidal activity, metals have been widely used as antimicrobial agents in a multitude of applications related to agriculture, healthcare, and the industry in general. Unlike other antimicrobial agents, metals are stable under conditions currently found in the industry allowing their use as additives [19].

The antimicrobial properties of silver have been known from antiquity, and increasing antibiotic resistance of bacteria and the ineffectiveness of synthetic antibiotics against some bacterial strains have led to the reemergence of interest in silver, silver salts, silver compounds, and nanocrystalline silver as antibacterial agents. Silver nanoparticles (Ag NPs) have significant antibacterial and antifungal effect [26]. Ag NPs show synergism with other antibiotics and antiseptics (ceftazidime, streptomycin, kanamycin, polymyxin) [25, 38]. But J. Jains showed that chloramphenicol decreases antibacterial effect of Ag NPs solution [16].

The main disadvantages that limit the use of Ag NPs are their easy aggregation, the uncontrolled release of silver ions, and their cytotoxicity potential [40]. Combination of Ag NPs with natural agents, such as chitosan, propolis, clays, or zeolites [33, 35], provides additional effects. The combination of polymers and nanosilver may synergistically improve their antimicrobial effects, and the use of in situ synthesis methods allows its incorporation into the polymer matrix attaining uniform distributions and avoiding aggregation [28].

In recent years, the efficiency of green chemistry methods for synthesis of metallic NPs has increased significantly [1]. Plant extracts are often used as reducing, stabilizing, and capping agents [23] providing cost-effective and environmentally benign methods for NPs synthesis. Among plant extracts, ginger extract is of great scientific interest thanks to its chemical and biological properties [8]. Leaf extract of ginger has already been used for synthesis of silver NPs [37]; however, the produced particles had a rather wide particle size distribution (10–100 nm). Ginger rhizome is widely used as a spice and a folk medicine; its extract contains specific phenolic compounds: gingerol and its derivatives, a number of bioactive phenolic and non-phenolic constituents [31]. These compounds exhibit a broad spectrum of activities including antimicrobial, antifungal, and antiviral ones. Rhizome ginger extract seems to be a very promising substratum for development of bioactive and biocompatible nanoparticles, because it demonstrates also antioxidant and anti-inflammatory properties.

Chitin and chitosan are promising materials for medical applications due to their bacteriostatic/bactericide properties and biocompatibility with human tissues [20]. Chitosan is a derivative of chitin, which can be obtained by chitin deacetylation. Both of them contain same monomers, N-acetyl-2-amino-2-deoxy-D-glucopyranose and 2-amino-2-deoxy-D-glucopyranose, which differ in the proportion of acetylated and deacetylated monomers. Chitosan is a promising material for forming composites with different substances, including metal nanoparticles such as Ag and Cu [33]. On the other hand, сetrimonium bromide (CTAB) can stabilize nanoparticles in solution and decrease the toxicity of some nanoparticles, such as ZnO, TiO2, and Ni [17]. But the data about antibacterial activities of CTAB-NPs complex are limited [7].

The purpose of this research is to find optimal ratio of chitosan and Ag NPs, modified by CTAB for solution composition (chitosan/Ag) that would be active against MRSA clinical strains.



Silver nitrate, L-ascorbic acid, and cetrimonium bromide (C16H33)N(CH3)3Br (CTAB) were purchased from Sigma-Aldrich and used as received. Ginger (Zingiber officinale, Zingiber acae) rhizome was purchased in a local supermarket (Poznan, Poland). Chitosan 200 kDa, deacetylation degree 82% was purchased from CJSC “Bioprogress” (Russia, Moscow) and used without further purification. Ultrapure water (resistivity > 17 MΩcm− 1) from a GZY-P10 water system was used throughout the experiments. All media and disks with antibiotics were purchased from Hi Media (India).

In Situ Preparation of Chitosan/Ag NPs Solutions

To prepare the chitosan/Ag solutions in situ, Ag NPs were synthesized and modified at first.

Synthesis of Ag NPs

Ag NPs were synthesized via chemical reduction method using green chemistry approach. Following this approach, we used ginger (Zingiber officinale) extract as a surfactant and ascorbic acid (vitamin C) as a reducing agent. To prepare ginger rhizome extract, 250 g of rhizome was washed thoroughly with distilled water and then cut into small pieces. Chopped ginger rhizome was kept in a water-ethanol solution (250 ml, 1:1 ratio) for 5 days (at room temperature, in dark place). Then, supernatant was vacuum filtered (through a Whatman filter paper) and stored (at 4 °C). To synthesize Ag NPs, silver nitrate (840 mg) was dissolved in water (20 ml) and ginger rhizome extract (20 ml) was added. Then, a mixture of solution of L-ascorbic acid (10%, 10 ml) and ginger extract (20 ml) was drop added to the silver nitrate solution under magnetic steering. The reaction mixture turned dark. Then, it was heated (60 °C, 1.5 h) under reflux. Then, freshly synthesized Ag NPs were washed with water, until pH reached 7, using centrifugation (4000 rpm, 30 min).

In order to improve antimicrobial activity and dispersibility of Ag NPs, surface modification of Ag NPs by CTAB, which is well-known due to its surface-active and antiseptic properties, was performed [17]. Typically, the dispersion of Ag NPs (3 ml, 76.4 mg/ml) was mixed with CTAB solution (20 ml, 6.7 mg/ml) and sonicated (3 h). Then, supernatant was collected for UV–Vis measurements and Ag NPs were washed with water, using centrifugation (4000 rpm, 30 min), three times. Content of CTAB in the supernatant was determined using the spectrophotometric technique (UV–Vis) by monitoring the intensity of the 190-nm peak. Adsorptivity of Ag NPs (in mg/g) towards CTAB was calculated from the difference between the initial CTAB content in the solution and its content in the supernatant after interaction with the sample. The adsorptivity and CTAB loading content were calculated from the following equations:

Adsorptivity (mg/g) = (weight of CTAB in solution − weight of CTAB in supernatant)/(weight of Ag NPs),

CTAB loading content (%) = (1 − (weight of Ag NPs)/(weight of CTAB loaded Ag NPs)) × 100%.

In Situ Preparation of Chitosan/Ag NPs Solutions

To obtain chitosan/Ag NPs solutions, 200 kDa chitosan (1 g) was dissolved in 2% acetic acid (100 ml) at room temperature during 24 h to form 1% chitosan solution. Two samples of Ag NPs were used in experiments—pure Ag NPs and Ag NPs-CTAB.

Physicochemical Characterization of Ag NPs and Chitosan

Powder X-ray diffraction (XRD) studies were conducted on an Empyrean diffractometer (PANalytical), using Cu Kα radiation (1.54 Å), a reflection-transmission spinner (sample stage), and PIXcel 3D detector, operating in the Bragg–Brentano geometry. The 2Theta scans were recorded at room temperature at angles ranging from 10° to 95° with a step size of 0.007°, in continuous scan mode.

Transmission electron microscopy (TEM) measurements were performed using a JEM-ARM-200F transmission electron microscope operating at an accelerating voltage of 200 kV.

The infrared spectra were obtained using a Tensor 27 (Bruker Optics) spectrometer equipped with a global source and MCT detector. Samples were prepared using potassium bromide as a matrix material and were mixed in proportions of 1 mg of sample to 200 mg KBr. Pellets were prepared using the standard technique under a pressure of 10 ton/cm2 with a barrel of 16 mm in diameter. The measurements were performed at room temperature. For each spectrum, 512 scans in the spectral range of 4000–400 cm− 1 were taken with a resolution of 4 cm− 1. The data were processed using the Opus software package.

Spectrophotometric measurements (UV–Vis) were performed using UV/VIS/NIR Spectrometer Lambda 950 (Perkin Elmer) at wavelengths 200–800 nm with water as referred solution.

Microbiological Tests

Bacterial Culture

Bacterial cultures were collected from the region of the middle nasal meatus and from the throat of the 70 inpatients by use of sterile cotton-tipped wire swabs. The specimens were transported immediately to the laboratory in transport media and then inoculated on blood agar. Bacterial cultures were identified morphologically and biochemically by standard laboratory procedures according to the Manual of Methods for General Bacteriology in the bacteriological laboratory of Sumy State University. We isolated 50 Staphylococcus aureus strains. Each culture underwent Gram staining and was tested for production of catalase, free coagulase, yellow pigment, mannitol fermentation, growth on high salt concentration, and lipase production on egg yolk agar medium (Hi Media, Mumbai).

Antimicrobial Susceptibility Testing

Antibiotic susceptibility tests were performed on all S. aureus isolates to determine their antibiotic resistance profiles. The Kirby-Bauer disk diffusion method was used to assess the antibiotic susceptibility of the isolates. Antimicrobial susceptibility testing was carried out on Muller-Hinton agar against azithromycin, levofloxacin, clarithromycin, ciprofloxacin, and methicillin (National Committee for Clinical Laboratory Standards, 1999). Fresh overnight cultures were prepared and used in tests. Standard strain of S. aureus ATCC 25923 was used as control. An aliquot (100 μL) from each isolate suspension was spread plated on Mueller Hinton agar. Antibiotic discs were gently pressed onto the inoculated Mueller Hinton agar to ensure intimate contact with the surface, and the plates were incubated aerobically at 37 °C for 18–24 h. Inhibition zone diameters were measured. Clinical strains were categorized as susceptible and resistant according to evaluation criteria developed by the Clinical and Laboratory Standards Institute (CLSI) guidelines [24]. The strains of Staphylococcus aureus which were found to be resistant to methicillin were screened as MRSA.

Determination of Minimum Inhibitory Concentrations of Chitosan-Ag NPs Solutions

Antimicrobial activities of chitosan solution, Ag NPs, and chitosan-Ag NPs solutions were determined according to the recommendations of NCCLS (1999) by the use of a broth macrodilution method. We determined the minimum inhibitory concentration (MIC) for test solutions against each methicillin-resistant Staphylococcus aureus (a total of 10 MRSA strains). The tube with the lowest concentration that completely inhibits visual growth of bacteria (no turbidity) was considered as the MIC.

Briefly, at the beginning, seven concentrations of pure Ag NPs and Ag/CTAB NPs were prepared using nutrient broth with the 2-fold serial dilution method. There were three identical rows of every type of Ag NPs dilution. Then, in every tube of each row, we added 1, 2, or 3 ml of 1% chitosan solution. Final concentration of chitosan and Ag NPs in tested tubes is shown in Table 1.

Table 1 Concentrations of chitosan and Ag NPs in experimental solutions

Test bacterial strains were grown in an appropriate broth, washed once in sterile saline, and diluted in distilled water. The bacterial concentration was standardized to an optical density of 0.08 at 600 nm (approximately 1.5 × 108 UFC/mL) using the McFarland scale. Then, 100 μl of S. aureus suspension was inoculated into tubes with Ag NPs, chitosan solution, and Ag NPs-chitosan solution. Tubes containing growth medium and tested samples without inoculums were used as controls. All tubes were incubated aerobically at 37 °C for 24 h. All the measures were triplicate.


Characterization of Ag NPs and Chitosan Used for In Situ Solution Preparation

A part of synthesized Ag NPs was modified by CTAB (Ag/CTAB NPs) (in order to improve bioactivity and stability of Ag NPs dispersions). The adsorptivity of Ag NPs towards CTAB was found to be 70.0 mg/g that corresponds to CTAB content in the sample of approximately 6.54%.

The results of XRD measurements of Ag NPs showed the presence of four sharp peaks at 38.15, 44.33, 64.48, 77.47, and 81.54 °2Theta (Fig. 1a). According to the American Mineralogist Crystal Structure Database (AMCSD) [5], these peaks were attributed to the silver. The wide peak within 12.00–21.06 °2Theta may be attributed to organic compounds which originated from synthesis (L-ascorbic acid and ginger). The XRD pattern of chitosan (Fig. 1a, inset) exhibits diffraction peaks at approximately 9 and 20 °2Theta, which are typical fingerprints of semicrystalline chitosan [5]. Crystallinity of chitosan is generated from hydrogen bonds between corresponding hydroxyl and N-acetyl groups. Each crystalline peak characterizes crystallographic structure, which is generated from parallel and antiparallel alignments of polymeric chains or sheets. Semicrystalline chitosan has amorphous and crystalline regions.

Fig. 1
figure 1

Characterization of Ag NPs and chitosan. a XRD patterns, b FTIR spectra, c UV–Vis absorbance spectrum of Ag NPs (water), d TEM image of Ag NPs

FTIR spectra of chitosan and Ag NPs are shown in Fig. 1b. The spectrum of chitosan shows broad and intensive bands at 3450–3200 cm− 1 (hydrogen-bonded OH stretching vibrations) overlapped with NH stretching bands, CH stretching band at 2783 cm− 1, and the band for amide I at 1652 cm− 1 (Fig. 1b). Bending vibrations of methylene and methyl groups are also visible at ν = 1375 cm− 1 and ν = 1426 cm− 1, respectively. Absorption in the range from 1160 to 1000 cm− 1 has been attributed to vibrations of CO group. The band located near ν = 1150 cm− 1 is related to asymmetric vibrations of CO in the oxygen bridge resulting from deacetylation of chitosan. The bands near 1080–1025 cm− 1 are attributed to νCO of the ring COH, COC, and CH2OH. The small peak at ~ 890 cm− 1 corresponds to wagging of the saccharide structure of chitosan [11, 13].

The FTIR spectrum of Ag NPs revealed several intensive peaks at 1226, 1366, 1636, 1714, 2851, 2924, and 3438 cm− 1. The latter were attributed to the H-bonded OH groups. The peaks at 1226 and 1366 cm− 1 are due to CO and CH bending vibrations; double peak at 1636 and 1714 cm− 1 point to a presence of C=C and C=O groups (stretching vibrations). The peaks at 2851 and 2924 cm− 1 are related to CH stretching vibrations [13]. The presence of organic groups on the Ag NPs surface are due to organic compounds used for their synthesis, L-ascorbic acid and ginger, which FTIR spectra are known [10]. If we compare the spectra of the latter with the Ag NPs one, one may notice that the double peak at 1636 and 1714 cm− 1 is inherent to the spectrum of L-ascorbic acid and blue-shifted. The most intensive ginger peaks situated within 1000–1200 cm− 1 (COC vibrations) are not intensively expressed in Ag NPs spectrum. Hence, L-ascorbic acid plays the predominant role in reduction of silver ions, transferring two electrons and transforming into dehydroascorbic acid [29]. The blue-shift of L-ascorbic acid peak position gives an evidence for the chemical bonding of this molecule on the Ag NPs surface.

The UV–Vis absorbance spectrum of the Ag NPs dispersed in water (Fig. 1c) revealed the asymmetric peak at approximately 387 nm. The peak within 387–420 nm is known as the characteristic peak for Ag NPs and is usually attributed to the surface plasmon resonance effect [30]. The asymmetry of this peak (plateau) may be ascribed to fast precipitation of Ag NPs. The peak at approximately 264 nm is also known for Ag NPs and is usually related to transition of electrons to higher energy states running in Ag NPs [38]. From the other hand, UV–Vis spectrum of L-ascorbic acid also revealed a peak at 255 nm [4]. Hence, the peak at 264 nm in Ag NPs spectrum may be considered as red-shifted peak of L-ascorbic acid confirming the presence of these chemically bonded molecules on Ag NPs surface.

It is interesting that UV–Vis spectrum of Ag/CTAB NPs (Fig. 1c, blue line) revealed a symmetric peak at 417 nm. This confirmed that the stability of Ag NPs in water was improved due to surface modification by CTAB molecules.

TEM measurements revealed that Ag NPs have roundish shape and the majority of them are 10–12 nm in size (Fig. 1d).

Antibacterial Activities of the In Situ Prepared Chitosan/Ag NPs Solutions Against Methicillin-Resistant Strains of Staphylococcus aureus

MIC of pure Ag NPs and Ag/CTAB NPs against 100% MRSA was 9.6 μg/ml. The lowest concentrations have shown lesser activities (Table 2). Chitosan solution demonstrates antibacterial activities with MIC 6 μg/ml against 100% clinical strains of MRSA. Among them, 60% of strains had MIC 3.3 and 5 μg/ml chitosan solution.

Table 2 Antibacterial activity of pure Ag NPs to multi-resistant strains of S. aureus

The inhibitory effect of the chitosan-Ag NPs solution against MRSA is presented in Fig. 2a. It was found that chitosan-Ag NPs solution showed superior antimicrobial efficacy compared to its pure forms. At the same time, in situ preparation of chitosan-Ag NPs/CTAB solution (chitosan 6.0 μg/ml, Ag/CTAB NPs) was not possible due to the precipitation of the components: formation of gray-black ring agglutination and separation of the components into two phases. Antibacterial activity could not be evaluated in this case. Taking into account the unexpected result of chitosan and CTAB mixing and the lowest antibacterial activity of Ag NPs-CTAB (see Fig. 2b), we concluded that Ag NPs surface modification by CTAB is not promising. The presence of CTAB molecules on Ag NPs surface improved the stability of water dispersions, however significantly decreased antimicrobial activity and caused solution precipitation.

Fig. 2
figure 2

The percentage of sensitive strains of MRSA after treatment. Chitosan-Ag NPs solution (a) and chitosan-AgNPs-CTAB solution (b). 3.3, 5, and 6 μg/ml—these are the concentrations of chitosan in solution


Toxicity refers to any harmful impacts on an organism during exposure to nanoparticles and their salts. If the aim is to sterilize or disinfect a specific organism, toxicity may be interpreted as a positive result (antibacterial, antiviral) [15]. The current fundamental need in nanotechnology is the development of eco-friendly and reliable methods for synthesis of metallic nanoparticles. We have affirmed the use of biological reducing agents that are natural, low-cost, and ecofriendly materials for producing silver nanoparticles, to avoid the presence of risky and toxic solvents [37]. The use of Ag NPs as therapeutic agents is limited because of their cytotoxicity against mammalian cells. Several factors can have impact on the effect of Ag NPs against microorganisms, such as size, shape, stability, and concentration of Ag NPs [4].

In our research, we obtained Ag NPs with size of 5–18 nm. It is one of the most fundamental parameters affecting the optical [39], antimicrobial [27], and antiviral properties of Ag NPs [21]. Smaller particles display greater antibacterial activity. Some studies revealed that the NPs greater than 10 nm accumulate on the cellular surface and compromise cellular permeability; however, NPs smaller than 10 nm penetrate into the bacteria, affecting DNA and the enzymes leading to cellular death [14]. It is interesting to note that although the majority of the results proved that the hypothesis of toxicity increases with decreased particle size, there are also experimental data showing that smaller NPs were either less toxic or had no size-dependent toxicity [15]. There are many studies which showed the antimicrobial activity of the Ag NPs with the range of their size from 3 to 100 nm [19].

As mentioned earlier, the effects of chitosan on the stability and antimicrobial properties of the synthesized Ag NPs were evaluated. Prior to susceptibility testing, the synthesized nanoparticles were subjected to different methods of characterization to determine their purity. Our research showed that Ag NPs in concentration of 9.6 μg/ml are effective against 100% of MRSA strains and CTAB did not increase Ag NPs effectiveness.

It is known that chitosan has significant antibacterial activity against a broad spectrum of bacteria [2]. Despite this, some reports indicate that pure chitosan does not prevent severe infections [3]. There have been several publications that have reported various combinations of chitosan and silver with improved antimicrobial properties [11]. Silver-chitosan nanocomposites were proposed as coatings for biomedical-engineering and food-packaging applications and wound-dressing applications [2, 3]. But there are limited data about the antibacterial effect of chitosan-Ag NPs solution against MRSA [34]. Our data demonstrates that simple mixing of Ag NPs in chitosan solution can enhance antibacterial activity of both components. We get increase of all investigated substance antibacterial activities. MIC of chitosan was 3.3 μg/ml and pure Ag NPs MIC and Ag NPs with CTAB MIC were 1.2 and 2.4 μg/ml, respectively. Kaur et al. (2013) also reported antibacterial activity of silver/chitosan nanocomposites against S. aureus, in which they showed similar results [36], but they did not determine the MIC. This finding demonstrates effectiveness of chitosan-Ag NPs solution, but we did not see advantages of CTAB as an antibacterial agent. On the contrary, another study showed that Ag NPs stabilized with CTAB has pronounced antibacterial effect against S. aureus and Escherichia coli. Probably, in our experiment, chitosan links with CTAB that decreases Ag NPs effect for bacterial cells.


In this study, the activity of in situ prepared chitosan-Ag NPs solutions with different component ratios were tested against MRSA isolated from patients. Our results showed that simple mixing of the chitosan solution and Ag NPs reduces the minimal inhibition concentration of the substances into 2- and 4-folds (3.3 and 1.2 μg/ml), respectively. This result is very promising and may be considered as an effective solution in fighting against drug-resistant bacteria. It is also a progress in the direction towards personalized medicine. Future cytotoxicity study of chitosan-Ag NPs solution would give an answer about doses suitable for clinical use.


Ag NPs:

Silver nanoparticles


Acute respiratory infections


Cetrimonium bromide


Fourier transform infrared spectroscopy


Methicillin-resistant strains of Staphylococcus aureus


Transmission electron microscopy


Ultraviolet–visible spectroscopy


X-ray diffraction


  1. Abboud Z, Vivekanandhan S, Misra M, Mohanty A (2016) Leaf extract mediated biogenic process for the decoration of graphene with silver nanoparticles. Mater Lett 178:115–119

    Article  Google Scholar 

  2. Bangyekan C, Aht-Ong D, Srikulkit K (2006) Preparation and properties evaluation of chitosan-coated cassava starch films. Carbohydr Polym 63(1):61–71

    Article  Google Scholar 

  3. Burkatovskaya M, Castano A, Demidova-Rice T, Tegos G, Hamblin M (2008) Effect of chitosan acetate bandage on wound healing in infected and noninfected wounds in mice. Wound Repair Regen 16(3):425–431

    Article  Google Scholar 

  4. Cao X, Cheng C, Ma Y, Zhao C (2010) Preparation of silver nanoparticles with antimicrobial activities and the researches of their biocompatibilities. J Mater Sci 21(10):2861–2868

    Google Scholar 

  5. Downs R, Hall-Wallace M (2003) The American Mineralogist crystal structure database. Am Mineral 88:247–250

    Article  Google Scholar 

  6. Davies J, Davies D (2010) Origins and evolution of antibiotic resistance. Microbiol Mol Biol Rev 74:417–433

    Article  Google Scholar 

  7. Ghosh IN, Patil SD, Sharma TK (2013) Synergistic action of cinnamaldehyde with silver nanoparticles against spore-forming bacteria: a case for judicious use of silver nanoparticles for antibacterial applications. Int J Nanomedicine 8:4721–4731

    Google Scholar 

  8. Grzanna R, Lindmark L, Frondoza C (2005) Ginger—an herbal medicinal product with broad anti-inflammatory actions. J Med Food 8(2):125–132

    Article  Google Scholar 

  9. Hansra N, Shinkai R (2011) Cutaneous community-acquired and hospital-acquired methicillin resistant Staphylococcus aureus. Dermatol Ther 24:263–272

    Article  Google Scholar 

  10. Hemmati K, Hesaraki S, Nemati A (2014) Evaluation of ascorbic acid-loaded calcium phosphate bone cements: physical properties and in vitro release behavior. Ceram Int 40(3):3961–3968

    Article  Google Scholar 

  11. Huang L, Dai T, Xuan Y, Tegos G, Hamblin M (2011) Synergistic combination of chitosan acetate with nanoparticle silver as a topical antimicrobial: efficacy against bacterial burn infections. Antimicrob Agents Chemother 55(7):3432–3438

    Article  Google Scholar 

  12. Ibrahim E, Sherman G, Ward S, Fraser V, Kollef M (2000) The influence of inadequate antimicrobial treatment of bloodstream infections on patient outcomes in the ICU setting. Chest 118:146–155

    Article  Google Scholar 

  13. Infrared spectroscopy—materials science, engineering and technology, book edited by TheophileTheophanides, ISBN 978-953-51-0537-4, Published: April 25, 2012 under CC BY 3.0 license // Chapter 2: Suédina M.L. Silva, Carla R.C. Braga, Marcus V.L. Fook, Claudia M.O. Raposo, Laura H. Carvalho, Eduardo L. Canedo Application of infrared spectroscopy to analysis of chitosan/clay nanocomposites. DOI:

  14. Inphonlek S, Pimpha N, Sunintaboon P (2010) Synthesis of poly (methyl methacrylate) core/chitosan-mixed-polyethyleneimine shell nanoparticles and their antibacterial property. Colloids Surf B: Biointerfaces 77(2):219–226

    Article  Google Scholar 

  15. Ivask A, Kurvet I, Kasemets K, Blinova I, Aruoja V, Suppi S (2014) Size-dependent toxicity of silver nanoparticles to bacteria, yeast, algae, crustaceans and mammalian cells in vitro. PLoS ONE 9(7):e102108

    Article  Google Scholar 

  16. Jain J, Arora S, Rajwade J (2009) Silver nanoparticles in therapeutics: development of an antimicrobial gel formulation for topical use. Mol Pharm 66(5):1388–1401

    Article  Google Scholar 

  17. Jin Y, Deng J, Liang J, Shan C, Tong M (2015) Efficient bacteria capture and inactivation by cetyltrimethylammonium bromide modified magnetic nanoparticles. Colloids Surf B Biointerfaces 136:659–665

    Article  Google Scholar 

  18. Kaur P., ChoudharyandA., Thakur R. Synthesis of chitosan-silver nanocomposites and their antibacterial activity.Int J Sci Eng Res 2013;4(4): 869–872

  19. Kon K, Rai M (2013) Metallic nanoparticles: mechanism of antibacterial action and influencing factors. J Comp Clin Path Res 2/1:160–174

    Google Scholar 

  20. Kumar M, Muzzarelli R, Muzzarelli C, Sashiwa H, Domb A (2004) Chitosan chemistry and pharmaceutical perspectives. Chem Rev 104(12):6017–6084

    Article  Google Scholar 

  21. Lara H, Ayala-Nuñez N, Ixtepan-Turrent L, Rodriguez-Padilla C (2010) Mode of antiviral action of silver nanoparticles against HIV-1. J Nanobiotechnol 8:1

    Article  Google Scholar 

  22. Levy S, Marshall B (2004) Antibacterial resistance worldwide: causes, challenges and responses. Nat Med Suppl 10(12):123–129

    Google Scholar 

  23. López-Miranda J, Vázquez M, Fletes N, Esparza R, Rosas G (2016) Biosynthesis of silver nanoparticles using a Tamarix Gallica leaf extract and their antibacterial activity. Mater Lett 176:285–289

    Article  Google Scholar 

  24. M100-S17 Vol. 27 No. 1 Replaces M100-S16 Vol. 26 No. 3 Performance standards for antimicrobial susceptibility testing; Seventeenth Informational Supplement

  25. Maqusood A, Mohamad S, Siddiqu M (2010) Silver nanoparticle applications and human health. Clin Chim Acta 411(23–24):1841–1848

    Google Scholar 

  26. Marambio-Jones, Hoek (2010) A review of the antibacterial effects of silver nanomaterials and potential implication for human health and the environment. Nanopart Res 12:1531–1551

    Article  Google Scholar 

  27. Morones J, Elechiguerra J, Camacho A (2005) The bactericidal effect of silver nanoparticles. Nanotechnology 16(10):2346–2353

    Article  Google Scholar 

  28. Murugadoss A, Prasad P, Ghosh S, Chattopadhyay A (2008) The antibacterial properties of a novel chitosan-Ag-nanoparticle composite. Int J Food Microbiol 124:142–146

    Article  Google Scholar 

  29. Mushran S, Agrawal M, Mehrotra R, Sanehi R (1974) Kinetics and mechanism of reduction of silver (I) by ascorbic acid. J Chem Soc Dalt Trans 14:1460

    Article  Google Scholar 

  30. Mulvaney P (1996) Surface plasmon spectroscopy of nanosized metal particles. Langmuir 12:788–800

  31. Nile SH, Park SW (2015) Chromatographic analysis, antioxidant, anti-inflammatory, and xanthine oxidase inhibitory activities of ginger extracts and its reference compounds. Ind Crop Prod 70:238–244

    Article  Google Scholar 

  32. Nair N, Biswas R, Götz F (2014) Impact of Staphylococcus aureus on pathogenesis in polymicrobial infections. Infect Immun 82(6):2162–2169

    Article  Google Scholar 

  33. Palza H (2015) Antimicrobial polymers with metal nanoparticles. Int J Mol 16(1):2099–2116

    Article  Google Scholar 

  34. Regiel A, Irusta S, Kyzioł A, Arruebo M, Santamaria J (2013) Preparation and characterization of chitosan-silver nanocomposite films and their antibacterial activity against Staphylococcus aureus. Nanotechnology 24(1):015101

    Article  Google Scholar 

  35. Regiel A, Kyziol A, Arruebo M (2013) Chitosan-silver nanocomposites—modern antibacterial materials. Chemik 67(8):683–692

    Google Scholar 

  36. Shameli K, Bin AM, Zargar M (2011) Synthesis and characterization of silver/montmorillonite/chitosan bionanocomposites by chemical reduction method and their antibacterial activity. Int J Nanomedicine 6(31):271–284

    Article  Google Scholar 

  37. Singh C, Sharma V, Naik P K, Khandelwal V, Singh H (2011) A green biogenic approach for synthesis of gold and silver nanoparticles using Zingiber Officinale. Dig J Nanomater Biostructures 6(2):535–542

  38. Singh R, Wagh P, Wadhwani S (2013) Synthesis, optimization, and characterization of silver nanoparticles from Acinetobacter calcoaceticus and their enhanced antibacterial activity when combined with antibiotics. Int J Nanomedicine 8:4277–4290

    Google Scholar 

  39. Siwach O, Sen P (2008) Fluorescence properties of Ag nanoparticles in water. Spectrochim Acta A Mol Biomol Spectrosc 69:659–663

    Article  Google Scholar 

  40. Wang X, Wang Z, Zhang J, Qi H, Chen J, Xu M (2016) Cytotoxicity of AgNPs/CS composite films: Ag NPs immobilized in chitosan matrix contributes a higher inhibition rate to cell proliferation. Bioengineered 7(5):283–290

Download references


The authors would like to thank Dr. Barbara Peplinska for TEM measurements and Dr. Zuzanna Pietralik for support in FTIR measurements.


No funding supported this research.

Availability of Data and Materials

The data of the current research will not be shared at this time because the current research is a part of a big project and their results are not published yet.

Author information

Authors and Affiliations



VH conceived of the research design and participated in the antibacterial research, manuscript preparation, and correction and discussion. OK participated in the XRD, FTIR, and UV–Vis discussion. OI participated in the Ag NPs manufacturing, TEM, manuscript design, and discussion. MP participated in the research and manuscript design, manuscript preparation and correction, and discussion. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Maksym Pogorielov.

Ethics declarations

Ethics Approval and Consent to Participate

We collected biological material from 70 patients. All procedures were taken after the written informed agreement according with national standards. All procedures and experiments were approved by the Bioethical Commission of Sumy State University. Contact details of Commission—tel./fax + 38(0542) 66–09-50, e-mail:

Consent for Publication

Not applicable.

Competing Interests

The authors declare that they have no competing interests.

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (, which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Holubnycha, V., Kalinkevich, O., Ivashchenko, O. et al. Antibacterial Activity of In Situ Prepared Chitosan/Silver Nanoparticles Solution Against Methicillin-Resistant Strains of Staphylococcus aureus. Nanoscale Res Lett 13, 71 (2018).

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI:


  • Chitosan
  • Silver nanoparticles
  • CTAB
  • MRSA
  • Antibacterial activity