Journal of Nanoparticles
Volume 2016 (2016), Article ID 4694367, 13 pages
http://dx.doi.org/10.1155/2016/4694367

Research Article

Screening Antimicrobial Activity of Nickel Nanoparticles Synthesized Using Ocimum sanctum Leaf Extract

Chitra Jeyaraj Pandian,¹ Rameshthangam Palanivel,² and Solairaj Dhanasekaran²

¹Department of Biochemistry, Manonmaniam Sundaranar University, Tirunelveli, Tamil Nadu 627012, India
²Department of Biotechnology, Science Campus, Alagappa University, Karaikudi, Tamil Nadu 630 004, India

Received 19 October 2015; Accepted 15 February 2016

Academic Editor: Tapas Sen

Copyright © 2016 Chitra Jeyaraj Pandian 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.

Abstract.

Antimicrobial efficacy of nickel nanoparticles synthesized using leaf extract of Ocimum sanctum (NiGs) was investigated against pathogenic Gram-negative (E. coli, K. pneumoniae, and S. typhi), Gram-positive (B. subtilis, S. epidermidis) bacteria and fungi (C. albicans, C. tropicalis, A. fumigatus, A. clavatus, and A. niger). 100 µg/mL NiGs showed maximum antimicrobial activity against tested pathogens compared to leaf extract and antibiotics. E. coli (25 mm) and C. albicans (23 mm) exhibited higher zone of inhibition at 100 µg/mL NiGs. MIC, MBC, and MFC values of NiGs against all tested pathogens ranged between 25 and 50 µg/mL. Growth of bacterial and fungal cells (10⁵ cfu/mL) was completely inhibited at 50 µg/mL NiGs. E. coli and C. albicans have showed strong antimicrobial activity with 81% and 50% reactive oxygen species (ROS) production, 30 and 16 µg/mL protein leakage, and 95 and 82 U/L LDH leakages, respectively. Gram-negative bacteria and Candida species showed more sensitivity to NiGs at all concentrations tested (25–100 µg/mL) than Gram-positive bacteria and Aspergillus species, respectively. Microbial growth in the presence of NiGs and ascorbic acid confirmed the involvement of ROS in antimicrobial activity. Hence, NiGs induced ROS generation was attributed to the protein and LDH leakage from microbial membranes.

1. Introduction

Recent increase in microbial resistance to diverse antibiotics and uncertainties in health care cost lead to the emergence of more economical new methods to produce nanoparticles with specific physical, chemical properties and limited resistance [1]. The antimicrobial activities of nanoparticles have been attributed to their relatively smaller sizes and high amount of surface-area-to-volume ratio that facilitate interacting closely with membranes of viruses, fungi, and bacteria [2]. Antimicrobial activities of metal nanoparticles like Ag, Cu, Ni, and Co (and their oxides) have been previously reported [3]. Stabilizing and protective agents in chemical synthesis of nanoparticles interact chemically with the surface of nickel nanoparticles and modify their morphology, electronic and magnetic properties [4]. In recent years, there is an increasing emphasis on green synthesis of metal nanoparticles because of their application in utilization of nontoxic renewable chemicals and elimination of generated waste [5]. Polymeric nanoparticles like chitin nanoparticles were also found to be low cost biodegradable material for environmental protection [6]. But the plant-mediated nanoparticles synthesis is rapid, cost-effective, ecofriendly, and safe single step method for human therapeutic use [7]. Medicinal plant Ocimum sanctum has been found to be highly effective in different types of animal models for antimicrobial, immunomodulatory, antistress, anti-inflammatory, antipyretic, antiasthmatic, hypoglycemic, hypotensive, and analgesic activities [8]. O. sanctum leaves have been reported to show strong antifungal activities and antibacterial activity [9]. Earlier studies provide substantial evidence that nanoparticles produce reactive oxygen species (ROS) in bacterial cells and ROS accumulation intracellularly regulates apoptosis [10]. Oxidative stress-induced respiratory cells damage can be determined by measuring respiratory chain lactate dehydrogenase activity in microbial cells and nanoparticles enhance protein leakage by increasing membrane permeability [11]. In our previous work [12], we have synthesized and characterized nickel nanoparticles using leaf extracts of Ocimum sanctum with 1 mM of aqueous nickel nitrate. Antimicrobial activity of synthesized nickel nanoparticles was evaluated by various susceptibility assays on bacterial and fungal pathogens. The toxicity of NiGs was studied against Gram-negative (Escherichia coli, Klebsiella pneumoniae,and Salmonella typhi) and Gram-positive (Bacillus subtilis, Staphylococcus epidermidis) bacterial and fungal pathogens (Candida albicans, Candida tropicalis, Aspergillus fumigatus, Aspergillus clavatus,and Aspergillus niger). We also substantiate that NiGs induced reactive oxygen species formation destroys microbial cell membrane and its permeability leading to growth suppression and cell death.

2. Materials and Methods

2.1. Materials and Strains

O. sanctum leaves were collected from Karaikudi town, Tamil Nadu, India. Taxonomic identification was done by Department of Botany, Alagappa University, Karaikudi, Tamil Nadu, India.

Lyophilized cultures of Escherichia coli (MTCC 1682), Klebsiella pneumoniae (MTCC 8911), Salmonella typhi (MTCC 3224), Bacillus subtilis (MTCC 6133), Staphylococcus epidermidis (MTCC 7919), Candida albicans (MTCC 3018), Candida tropicalis (MTCC 6222), Aspergillus fumigatus (MTCC 2508), Aspergillus clavatus (MTCC 1323), and Aspergillus niger (MTCC 281) were procured from Microbial Type Culture Collection (MTCC) located in Indian Institute of Microbial Technology, Chandigarh, India. Mueller-Hinton agar media for bacteria and potato dextrose agar media for fungi were purchased from Hi-Media Laboratories, Mumbai, India. Nickel nitrate was purchased from SD Fine Chemicals Ltd., Mumbai, India. All other chemicals were purchased from Sigma-Aldrich, Mumbai, India.

2.2. Synthesis and Characterization of Nanoparticles

Nickel nanoparticles were synthesized using the leaf extract of O. sanctum and characterized according to our previous study [12]. Chemical interaction of compounds present in Ocimum sanctum leaf extract with nanoparticles and morphology of NiGs were characterized by Fourier transform infrared (FTIR) spectroscopy and transmission electron microscope (TEM), respectively.

2.3. Dose-Dependent Antimicrobial Assay

Antibacterial and antifungal assays were performed with Mueller-Hinton (MH) agar and Sabouraud dextrose (SD) agar medium, respectively. Bacterial and fungal cultures were prepared to 0.5 McFarland standards prior to the assay. Antimicrobial activity of NiGs was evaluated by disc diffusion assay against the Gram-negative bacteria (E. coli, K. pneumoniae, and S. typhi), Gram-positive bacteria (B. subtilis, S. epidermidis), and fungi (C. albicans, C. tropicalis, A. clavatus, A. fumigatus, and A. niger). Pure microbial cultures were subcultured on nutrient agar and uniformly swabbed on individual plates. 20 μL of NiGs at different concentrations (25, 50, and 100 μg/mL) was impregnated to 6 mm filter paper discs, dried, and placed on the culture plate. Bacterial and fungal cultures were incubated at 37°C for 24 h and 48 h, respectively [13]. Antimicrobial activities were studied by the diameter of zone of inhibition. Deionized water (as control) and leaf extract were used to compare the antimicrobial activity of NiGs.

2.4. Minimum Inhibitory Concentration (MIC), Minimum Bactericidal Concentration (MBC), and Minimum Fungicidal Concentration (MFC) Assay

100 μL of NiGs in serially descending concentrations 200 to 1 μg/mL was added to microtitre plates with 100 μL MH broth for bacterial or 100 μL SD broth for fungal assays. Dilutions were done by twofold serial dilution and 100 μL of bacterial and fungal samples was inoculated to respective wells. Bacterial and fungal plates were incubated for 24 h and 48 h, respectively, at 37°C [13] and optical densities were determined at 600 nm using microplate reader. Antibiotics (amoxicillin (Amx) and nystatin (Nys)) were used to compare the bactericidal and fungicidal activity of NiGs.

MBC and MFC were determined by subculturing 2 μL of above MIC serial dilution after 24 h of incubation in respective wells containing 100 μL of broth per well. Bacterial and fungal colonies were quantified by further incubation for 24 h and 48 h, respectively, at 37°C. MBC and MFC were the lowest concentration of nanoparticles or antibiotics that prevented the growth of bacterial and fungal colonies on solid media, respectively [14].

2.5. Determination of Microbial Growth Kinetics in the Presence of NiGs

Microbial growth rate was observed by inoculating the microtitre plates with MH and SD broth containing 10⁵ colony forming units (cfu) per mL of bacterial or fungal pathogens, respectively, and loaded with varying concentrations of nanoparticles (0, 25, 50, and 100 μg/mL). The plates were incubated at 37°C and shaken at 180 rpm. After inoculation, the optical density (OD) at 600 nm [15] was serially monitored at every 3 h interval till 24 h and every 6 h interval till 48 h for bacterial and fungal pathogens, respectively.

2.6. Detection of Reactive Oxygen Species (ROS)

Reactive oxygen species produced in microbial cells were determined by 2′,7′ dichlorofluorescein diacetate (DCFDA). Intracellular esterase cleaves fluorescence based probe dichloro-dihydro-fluorescein diacetate (DCFH-DA) to polar impermeable nonfluorescent molecule that accumulates intracellularly and its subsequent oxidation yields highly fluorescent product 2′,7′ dichlorofluorescein (DCF) which was monitored by increase in fluorescence. 10⁵ cfu/mL bacterial and fungal pathogens were treated with 0, 25, 50, and 100 μg/mL NiGs and incubated at 37°C for 6 h and 24 h, respectively. After incubation, the cultures were centrifuged at 5000 rpm for 10 min at 4°C. The supernatant was treated with 100 μM DCFDA for 1 h and the ROS formed (fluorescence intensity of DCF) was determined at 488 nm excitation wavelength and 535 nm emission wavelength using fluorescence spectrophotometer [11].

2.7. Assaying the Effect of NiGs on Protein Leakage

Bradford method was performed to analyze the protein leakage in the microbial cells. The bacterial and fungal pathogens (10⁵ cfu/mL) were treated with 0, 25, 50, and 100 μg/mL NiGs for 6 h and 24 h, respectively. After incubation, the contents were centrifuged at 5000 rpm for 5 min and supernatant was collected. 200 μL of supernatant from each sample was mixed with 800 μL of Bradford reagent and incubated for 10 min in dark at 37°C. The optical density was determined at 595 nm with bovine serum albumin as standard [16].

2.8. Assaying the Effect of NiGs on Lactate Dehydrogenase (LDH) Activity

The cytoplasmic enzyme LDH release and cell membrane instability were studied as per the procedure reported by Arokiyaraj et al. (2014) [17]. 100 μL of supernatant from each microbial culture treated with different concentrations of NiGs (0, 25, 50, and 100 μg/mL) was added to the reaction mixture containing 0.5 mL of 100 mM pyruvate, 5 mg NADH in 20 mL of 500 mM potassium phosphate buffer, and pH 7.5 at 30°C. Absorbance () was recorded for 0.5 to 5 min and relative change in the absorbance per minute () was calculated at 340 nm using UV-visible spectrophotometer. LDH activity was expressed in international unit (U/L) which is the amount of enzyme that reduces 1 μM of NAD per min at specific temperature:

where TV is the total reaction volume, 1000 is the conversion of U/mL into U/L, is the light path in cm, is the absorptivity of NADH in mM, and SV is the sample volume in mL.

2.9. Determining the Effect of Antioxidant on Microbicidal Activity of NiGs

The involvement of free radicals formation by NiGs was confirmed using antioxidant ascorbic acid that acts as scavenger of free radicals [18]. MH and SD broth with 10⁵ cfu/mL bacterial and fungal samples were supplemented with 100 μg/mL NiGs and 10 mM ascorbic acid and were shaken at 180 rpm at 37°C. The growth rate at OD 600 nm was determined at regular intervals till 24 h and 72 h of incubation for bacterial and fungal pathogens, respectively.

2.10. Statistical Analysis

All the experiments were performed in triplicate and the data were expressed as the mean ± standard deviation (SD). Error bars represent standard deviations of duplicate experiments.

3. Results and Discussion

3.1. Synthesis and Characterization of NiGs

NiGs were synthesized using O. sanctum leaf extract and the physiochemical properties were characterized (FTIR and TEM) and reported in our previous work [12].

The FTIR spectrum of NiGs in our previous study [12] evidenced the presence of functional groups such as O–H stretching carboxylic acid, C–N or C–C triple bond, N–H bend primary amines, C–C stretch aliphatic amines, and C–N rock in alkanes indicating the interaction of metabolites and proteins in the O. sanctum leaf extract with the NiGs. These interacting biological molecules could have been involved in the formation and stabilization of NiGs in aqueous medium. This is in concurrence with the findings by Mallikarjuna et al. [19] who have reported that the amino acid residues or proteins in O. sanctum leaf extract can strongly bind to silver nanoparticles, preventing its agglomeration and hence stabilizing the nanoparticles.

TEM micrograph of the NiGs in our previous study [12] showed that the shape of the NiGs was almost spherical and the distribution of the particles was narrow. The diameter of the sample ranged between 12 and 36 nm and shows a certain extent of particles agglomeration [12]. Our study is in good agreement with previous study by Govindasamy et al. [20] and Wang et al. [21] who have reported that the varied shape (irregular polygonal, cylindrical, and spherical) of nickel nanoparticles with particle agglomeration is due to magnetic interaction and polymer adherence between the particles, respectively.

3.2. Antibacterial and Antifungal Activity of NiGs

In disc diffusion assay, the suppression of bacterial growth was determined in Petri plates loaded with 25–100 μg/mL NiGs after 24 h at 37°C (Figure 1(a) and Table 1). Zone of inhibition was not observed in control plates loaded with deionized water while leaf extract has showed higher growth inhibition. Diameter of inhibition zone ranged from 15.3 to 25.1 mm, 9.5 to 23.3 mm, 8 to 20.2 mm, 7.1 to 19.5 mm, and 5.2 to 18.6 mm in E. coli, K. pneumoniae, S. typhi, B. subtilis, and S. epidermidis, respectively, with increase in NiGs concentration from 25 to 100 μg/mL. It is evident from Figure 1(a) that size of inhibition zone increases linearly with increase in NiGs concentration (25–100 μg/mL).

Table 1: Zone of inhibition (mean ± SD) of NiGs against bacterial and fungal pathogens.

Zone of inhibition (mm)

Bacteria
Leaf extract
NiGs (µg/mL)

25
50
100

E. coli
9.0 ± 0.2
15.3 ± 0.3
19.2 ± 0.5
25.1 ± 0.1

K. pneumoniae
7.8 ± 0.9
9.5 ± 0.5
18.1 ± 0.7
23.3 ± 0.7

S. typhi
5.8 ± 0.3
8.0 ± 1.4
18.3 ± 0.3
20.2 ± 0.3

B. subtilis
5.2 ± 0.5
7.1 ± 0.8
16.5 ± 0.2
19.5 ± 0.5

S. epidermidis
3.9 ± 0.6
5.2 ± 0.3
16.0 ± 0.8
18.6 ± 0.9

Fungi
Leaf extract
NiGs (µg/mL)

25
50
100

C. albicans
7.8 ± 0.1
14.5 ± 0.4
18.2 ± 0.7
23.1 ± 0.4

C. tropicalis
5.2 ± 0.6
12.4 ± 0.8
14.4 ± 0.2
21.6 ± 0.9

A. clavatus
4.5 ± 0.3
10.4 ± 0.1
14.3 ± 0.1
18.7 ± 0.5

A. fumigatus
3.7 ± 0.4
8.5 ± 0.3
10.7 ± 0.9
15.5 ± 0.6

A. niger
2.5 ± 0.1
6.2 ± 0.5
7.5 ± 0.5
12.4 ± 0.1

(a)

(b)

Figure 1: Zone of inhibition of (a) bacterial and (b) fungal pathogens treated with NiGs.

The presence of inhibition zone in Figure 1(b) confirmed the antifungal activity of NiGs. The size of inhibition zone differed with the type of fungal pathogen and concentration of NiGs. Maximum antifungal activity was observed at 100 μg/mL NiGs for C. albicans (23.1 mm), C. tropicalis (21.6 mm), A. clavatus (18.7 mm), A. fumigatus (15.5 mm), and A. niger (12.4 mm). Zone of inhibition was not observed in plates loaded with deionized water for tested fungal pathogens. Leaf extract showed minimal antifungal activity with inhibition zone diameter of 7.8, 5.2, 4.5, 3.7, and 2.5 mm for C. albicans, C. tropicalis, A. clavatus, A. fumigatus, and A. niger, respectively. Maximum antimicrobial activity was observed at 100 μg/mL NiGs for all tested pathogens at lower concentrations (25, 50 μg/mL). Therefore it is clear from the data that the antibacterial and antifungal activities are dose-dependent.

Disc diffusion study of NiGs confirmed that bacterial and fungal growth inhibition was dose-dependent with maximum activity at 100 μg/mL and it could be due to the release of nickel ions from NiGs that increased membrane permeability and ROS generation leading to cell death. This observation is in good agreement with the earlier antibacterial reports for zinc oxide nanoparticles at 2 to 12 mM concentration [22] and for silver nanoparticles at concentration 10 to 150 μM [14, 23].

3.3. Minimum Inhibitory Concentration (MIC) and Minimum Microbicidal Concentration (MBC/MFC)

MIC of NiGs was studied to determine the lowest concentration that could completely inhibit visible growth of bacterial and fungal pathogens. Antimicrobial activity of NiGs in terms of MIC, MBC, and MFC is shown in Table 2. Both inhibitory and bactericidal concentrations of leaf extract were found to be 100 μg/mL for Gram-positive bacteria (B. subtilis and S. epidermidis) and Aspergillus species (A. clavatus, A. fumigatus, and A. niger) while 50 μg/mL was observed for Gram-negative bacteria (E. coli, K. pneumonia, and S. typhi) and Candida species (C. albicans and C. tropicalis).

Table 2: MIC, MBC, and MFC (mean ± SD) of NiGs against bacterial and fungal pathogens.

Bacteria
Leaf extract (µg/mL)
Amoxicillin (µg/mL)
NiGs (µg/mL)

MIC
MBC
MIC
MBC
MIC
MBC

E. coli
50 ± 0.3
50 ± 0.1
25 ± 0.3
50 ± 1.3
25 ± 0.3
25 ± 2.4

K. pneumoniae
50 ± 0.1
50 ± 0.0
50 ± 2.0
50 ± 0.1
25 ± 2.8
25 ± 0.7

S. typhi
50 ± 1.0
100 ± 0.8
50 ± 0.4
100 ± 0.0
25 ± 0.2
25 ± 1.6

B. subtilis
100 ± 0.5
100 ± 1.3
50 ± 1.7
100 ± 0.2
50 ± 0.2
50 ± 0.2

S. epidermidis
100 ± 0.2
100 ± 0.6
50 ± 0.2
100 ± 0.1
50 ± 0.5
50 ± 0.1

Fungi
Leaf extract (µg/mL)
Nystatin (µg/mL)
NiGs (µg/mL)

MIC
MFC
MIC
MFC
MIC
MFC

C. albicans
50 ± 0.2
50 ± 0.4
50 ± 0.1
50 ± 2.1
25 ± 1.4
50 ± 0.0

C. tropicalis
50 ± 0.1
100 ± 0.1
50 ± 0.7
100 ± 0.8
25 ± 0.7
50 ± 0.1

A. clavatus
100 ± 2.5
100 ± 0.9
50 ± 0.0
100 ± 1.2
50 ± 2.5
50 ± 0.5

A. fumigatus
100 ± 0.0
100 ± 1.3
100 ± 0.3
100 ± 0.0
50 ± 1.0
50 ± 1.2

A. niger
100 ± 0.9
100 ± 0.2
100 ± 1.0
100 ± 0.3
50 ± 0.8
50 ± 0.6

25 μg/mL NiGs were the minimum inhibitory concentration against all bacterial pathogens. 25 μg/mL NiGs showed bactericidal activity against E. coli, K. pneumonia, and S. typhi while 50 μg/mL NiGs exhibited bactericidal activity against B. subtilis and S. epidermidis. This data is comparable with the antibiotic amoxicillin which showed inhibitory activity at 50 μg/mL for all bacterial pathogens and bactericidal activity of 100 μg/mL for S. typhi, B. subtilis, and S. epidermidis. 25 μg/mL amoxicillin has showed bactericidal activity against E. coli, K. pneumoniae, S. typhi, B. subtilis, and S. epidermidis. Therefore the minimum inhibitory concentration (25 μg/mL) and minimum bactericidal concentration (50 μg/mL) of NiGs were much lower than the antibiotics.

Among fungal pathogens maximum sensitivity was observed in C. albicans and C. tropicalis has showed MIC and MFC of NiGs at 25 and 50 μg/mL, respectively. Minimum inhibitory and fungicidal concentration of NiGs were found to be 50 μg/mL for A. clavatus, A. fumigatus, and A. niger. MIC and MFC of antibiotic nystatin were observed at 50 and 100 μg/mL for most of the fungal pathogens tested. Gram-positive bacteria, A. clavatus, A. fumigatus, and A. niger, have showed MIC, MBC, and MFC of NiGs at 50 μg/mL. But Gram-negative bacteria, C. albicans and C. tropicalis, have showed higher sensitivity to NiGs at lower concentration (25 μg/mL). S. typhi and C. tropicalis recorded higher MBC and MFC (100 μg/mL), respectively, for both leaf extract and antibiotics. Higher antimicrobial activity was observed in NiGs than antibiotics and leaf extract for all the tested pathogens. No significant antibacterial and antifungal activities were observed at NiGs concentrations less than 25 μg/mL. Gram-negative bacteria and Candida species showed relatively higher sensitivity to all tested antimicrobial agents (NiGs, antibiotics, and leaf extract) than Gram-positive bacteria and Aspergillus species, respectively. It is clear from the results that NiGs have enhanced inhibitory, bactericidal, and fungicidal activities.

Higher MIC and MBC values of NiGs in Gram-positive (B. subtilis and S. epidermidis) pathogens than in Gram-negative bacteria (E. coli, K. pneumonia and S. typhi) are due to thick peptidoglycan layer in Gram-positive bacteria that have defended the easy penetration of nanoparticles through the cell membrane. Similarly, Arokiyaraj et al. [17] also reported higher MIC values of green synthesized silver nanoparticles (25 μg/mL) against Gram-positive bacteria than Gram-negative bacteria (6.25 μg/mL). Higher MIC and MFC values of NiGs in A. clavatus, A. fumigatus, and A. niger than in C. albicans, C. tropicalis in the present study are due to spore producing and filamentous nature of Aspergillus species (A. clavatus, A. fumigatus, and A. niger) that decreased fungi’s sensitivity to NiGs. This observation is in agreement with previous reports [13] on antimicrobial properties of biosynthesized silver nanoparticles against S. aureus, S. epidermidis, E. coli, A. niger, and C. albicans. Enhanced MIC, MBC, and MFC of NiGs compared to antibiotics and leaf extract are due to nickel nanoparticle’s larger surface to volume ratio and its penetration to cell membrane. This observation confirmed the earlier findings on antifungal activity [24] and antibacterial activity [25] of silver nanoparticles against C. albicans and of E. coli, respectively.

The antimicrobial activity (MIC) of NiGs was compared with the previously reported antimicrobial studies of silver nanoparticles (Table 3). NiGs showed better antimicrobial activity when compared to silver nanoparticles of similar particle size. Antimicrobial effectiveness of green synthesized metal nanoparticles depends on particle dosage, treatment time, and synthesis methods [14]. This could be the reason for higher antimicrobial activity of NiGs than silver nanoparticles. Variation in antimicrobial activity of antimicrobial activity of NiGs compared to silver nanoparticles of similar size could be mainly attributed to the differences in experimental conditions, shape, and crystal quality of the nanoparticles as reported in earlier study by Pang et al. [26].

Table 3: Comparison of the antimicrobial activity of NiGs with silver nanoparticles.

Organism
Antimicrobial effect (MIC)
Size (silver nanoparticles)
Ref. (silver nanoparticles)

NiGs (size: 12–36 nm) (present study)
Silver nanoparticles

E. coli
25 µg/mL
75 µg/mL
21 nm
[2]

K. pneumoniae
25 µg/mL
11 µg/mL
11–75 nm
[34]

S. typhi
25 µg/mL
75 µg/mL
21 nm
[2]

B. subtilis
50 µg/mL
70 µg/mL
20 nm
[35]

S. epidermidis
50 µg/mL
31.25 µg/mL
10–50 nm
[36]

C. albicans
25 µg/mL
0.5 mg/mL
10–30 nm
[37]

C. tropicalis
25 µg/mL
0.84 mg/L
25 nm
[38]

Aspergillus sp.
50 µg/mL
40 µg/mL
18 nm
[39]

A. fumigatus
50 µg/mL
8 µg/mL
20 nm
[40]

A. niger
50 µg/mL
75 µg/mL
20 nm
[41]

3.4. Growth Curves of Microbial Cells Treated with Different Concentrations of NiGs

Bacterial growth curves in Figure 2 clearly demonstrated the inhibition of bacterial growth at all tested concentrations of NiGs (25–100 μg/mL). Culture medium without NiGs has not shown any inhibition of growth and also reached stationary phase after 24 h. However, complete inhibition was obtained at 50 and 100 μg/mL NiGs for both Gram-positive (B. subtilis and S. epidermidis) and Gram-negative bacteria (E. coli, K. pneumonia, and S. typhi). 25 μg/mL NiGs could slightly inhibit growth of bacteria but were not sufficient to outpace the reproduction of bacterial cells. From the results, it is evidenced that the bactericidal activity of NiGs increased with increasing NiGs concentration. NiGs showed faster inhibition of growth in E. coli, K. pneumonia, and S. typhi than B. subtilis and S. epidermidis. Maximum inhibition was observed in E. coli at 100 μg/mL NiGs.

Figure 2: Growth curves of bacterial cells exposed to different concentrations of NiGs.

Inhibitory effects of NiGs on the growth and reproduction of fungal pathogens with respect to concentration are shown in Figure 3. In the absence of NiGs, growth of both tested Candida species (C. albicans and C. tropicalis) and Aspergillus species (A. clavatus, A. fumigatus, and A. niger) reached exponential phase rapidly. However when exposed to 25 μg/mL NiGs, growth lagged for longer hours (9 h and 24 h for bacterial and fungal pathogens, resp.). Further increasing NiGs concentration to 50 μg/mL suppressed the fungal growth while 100 μg/mL NiGs completely inhibited the growth of fungal pathogens. 100 μg/mL NiGs showed maximum inhibition in C. albicans while the effect was less at lower concentrations (25, 50 μg/mL). Therefore, complete growth inhibition of bacterial pathogens was at 50 μg/mL NiGs while at 100 μg/mL for fungal pathogens.

Figure 3: Growth curves of fungal cells exposed to different concentrations of NiGs.

Faster inhibition of growth and reproduction of bacterial and fungal pathogens at 100 μg/mL than 25 and 50 μg/mL NiGs is due to the availability of few nanoparticles and nickel ions for inhibition. Decreased antimicrobial activity at lower NiGs concentration is due to the availability of few NiGs for growth inhibition as discussed by Sawai [27] for antibacterial activities of metallic oxide (ZnO, MgO, and CaO) powders against S. aureus and E. coli. Microbicidal activity of NiGs is also due to the electrostatic interaction between positively charged nickel ions and negatively charged microbial cell membranes. These observations are in concurrence with earlier antimicrobial study [16] of zinc oxide nanoparticles against S. enterica and C. albicans.

3.5. NiGs Induced Reactive Oxygen Species (ROS) Generation

Reactive oxygen species (ROS) are the natural byproducts of the metabolism [28]. Induction of ROS synthesis leads to the formation of highly reactive radicals that destroy the cells [29] by damaging cell membranes, proteins, DNA, and intracellular system [11]. Figures 4(a) and 4(b) showed continuous generation of ROS in bacterial and fungal pathogens at all tested concentrations of NiGs. ROS generated by NiGs was concentration-dependent that increased with the increasing NiGs concentration from 25 to 100 μg/mL. NiGs at 100 μg/mL generated nearly three times higher ROS in E. coli, K. pneumoniae, S. typhi, B. subtilis, and S. epidermidis than at lower concentration (25 μg/mL). E. coli and K. pneumoniae have showed 81 and 71% ROS generation, respectively, while S. epidermidis has showed minimal (50%) generation of ROS at 100 μg/mL NiGs.

(a)

(b)

Figure 4: Formation of ROS in (a) bacterial and (b) fungal cells exposed to different concentrations of NiGs.

Similarly ROS generation at 100 μg/mL NiGs was two times higher than in lower concentration (25 μg/mL) for all tested fungal pathogens. ROS generation was not observed in both bacterial and fungal control plates without NiGs. Among fungal pathogens treated with NiGs, C. albicans and C. tropicalis showed maximum ROS production while A. niger recorded minimal (32%) production of ROS. Therefore, ROS generation was dependent on NiGs concentration and maximum ROS production was observed in Gram-negative bacteria (65% to 80%) and in Candida species (47 to 50%).

Increased generation of ROS from bacterial and fungal cells treated with NiGs at all varying concentrations is due to the reaction of NiGs with water forming ROS (hydrogen peroxide H₂O₂) that damages membrane proteins and permeability. Similar destruction of bacteria due to H₂O₂ generated by titanium oxide nanoparticles-biofilm interfaces was earlier discussed by Thirunavukkarasu et al. (2014) [30].

3.6. Effect of NiGs on Protein Leak from Microbial Cell Membranes

Figures 5(a) and 5(b) showed the enhanced leakage of intracellular proteins from microbial membranes into the extracellular medium at varying concentrations of NiGs (25, 50, and 100 μg/mL). No significant protein leakage from bacterial and fungal cells was detected in control. Protein leakage from NiGs treated bacterial and fungal cells increased with NiGs concentration from 25 to 100 μg/mL for a contact period of 6 h and 24 h, respectively, with maximum leak at 100 μg/mL NiGs.

(a)

(b)

Figure 5: Leakage of proteins from (a) bacterial and (b) fungal cells exposed to different concentrations of NiGs.

At 100 μg/mL NiGs, the amount of protein leakage was up to 30, 27, 24, 19, and 14 μg/mL (Figure 5(a)) for E. coli, K. pneumoniae, S. typhi, B. subtilis, and S. epidermidis, respectively. Protein leakage from E. coli, K. pneumoniae, S. typhi, B. subtilis, and S. epidermidis membranes ranged from 19 to 26, 15 to 24, 14 to 23, 10 to 16, and 8 to 12 μg/mL, respectively, at 25–50 μg/mL NiGs. The results suggested that NiGs could accelerate leakage of protein from bacterial cytoplasm and highest leakage (30 μg/mL) was observed in E. coli.

Similarly, elevated protein leakage was observed in all tested fungal pathogens treated with NiGs (Figure 5(b)). Protein leakage from C. albicans, C. tropicalis, A. clavatus, A. fumigatus, and A. niger ranged from 11 to 16, 11 to 15, 9 to 13, 8 to 13, and 5 to 11 μg/mL, respectively, at 25–100 μg/mL NiGs. C. albicans has showed highest protein leakage (16 μg/mL) compared to other fungal pathogens.

A similar phenomenon of ROS induced oxidative stress-induced leakage of cellular contents from microbial cell membranes treated with zinc oxide nanoparticles and silver nanoparticles was discussed elsewhere [11, 31].

3.7. Effect of NiGs on Lactate Dehydrogenase (LDH) Activity

The effect of NiGs on lactate dehydrogenase, an important cytoplasmic enzyme, is represented in Figures 6(a) and 6(b). Significantly higher leakage of intracellular LDH into extracellular medium was observed in both bacterial (43–95 U/L) (Figure 6(a)) and fungal (48–82 U/L) (Figure 6(b)) cells treated with NiGs than control group. LDH leakage into extracellular medium increased with increase in NiGs concentration from 25 to 100 μg/mL. The LDH leakage from E. coli, K. pneumoniae, S. typhi, B. subtilis, and S. epidermidis in the absence of NiGs (control) was 55, 52, 45, 36, and 32 U/L, respectively. However the cells treated with 25–100 μg/mL NiGs showed higher LDH leakage ranging from 69 to 95, 64 to 89, 56 to 83, 47 to 79, and 43 to 72 U/L for E. coli, K. pneumoniae, S. typhi, B. subtilis, and S. epidermidis. The maximum LDH leakage (95 U/L) was observed in E. coli compared to other bacterial pathogens.

(a)

(b)

Figure 6: LDH leakage of (a) bacterial and (b) fungal cells exposed to different concentrations of NiGs.

LDH activity of C. albicans, C. tropicalis, A. clavatus, A. fumigatus, and A. niger at 25–100 μg/mL NiGs was found to be 69–95, 64–89, 56–83, 47–79, and 43–72 U/L, respectively, when compared with their respective control (55, 52, 45, 36, and 32 U/L). Increase in LDH leakage with increase in NiGs concentration suggested that the NiGs enhanced the leakage of intracellular LDH.

Enhanced leakage of proteins from NiGs treated bacterial and fungal cell membranes into culture medium is due to generation of free radicals from NiGs surface that induced membrane damage and leaked membrane and cellular proteins as discussed elsewhere [32].

3.8. Effect of Antioxidant on Microbicidal Activity of NiGs

The involvement of ROS in antimicrobial activity of NiGs was confirmed by using antioxidant ascorbic acid to scavenge the ROS produced by NiGs. The protective activity of 10 mM ascorbic acid was observed (Figures 7(a) and 7(b)) against microbicidal activity of NiGs against tested pathogens. Pathogens treated with 100 μg/mL NiGs (Figures 3 and 4) have not showed any growth due to ROS formation. However, in the presence of ascorbic acid both bacterial and fungal pathogens exhibited growth similar to the control (Figures 3 and 4). Growth curves of bacterial and fungal pathogens in Figures 7(a) and 7(b) confirmed that ascorbic acid was able to protect the cells completely from toxicity of NiGs. It is evidenced from the study that ROS was involved in the microbicidal activity of NiGs and ascorbic acid prevented this antimicrobial activity by scavenging the generated ROS. Growth curves of all tested bacterial and fungal pathogens in the presence of 100 μg/mL NiGs and 10 mM ascorbic acid were similar to the control and this is due to the free radical scavenging activity of ascorbic acid.

(a)

(b)

Figure 7: Effect of ascorbic acid on (a) bactericidal and (b) fungicidal activity of NiGs.

3.9. Mechanism of Antimicrobial Activity of NiGs

Figure 8 summarizes the interaction of NiGs with microbial cells. The antimicrobial activity of nickel nanoparticles relies on generation of ROS and release of nickel ions Ni (II). Diffusion and endocytosis of NiGs followed by nickel nanoparticle’s accumulation in cell membrane alter membrane permeability and destroy membrane proteins. NiGs react with water forming ROS that penetrate the cell membrane causing protein disruption and cell membrane damage with subsequent leakage of cellular contents. Dissolution of Ni (II) ions and free radicals interrupt electron transport in the microbial cell resulting in cell death. These observations are in good agreement with earlier reports [19, 33] for antimicrobial activity of silver nanoparticles.

Figure 8: Mechanism of antimicrobial activity of green synthesized nickel nanoparticles.

4. Conclusions

Green synthesis of nanoparticles provides more advancement in pharmaceutical and biomedical applications than chemical and physical methods due to their cost-effectiveness and ecofriendliness. To overcome the increasing drug resistance, public health problems, and adverse reactions, there is an utmost need to develop novel antimicrobial agents. Nickel nanoparticles were synthesized from leaf extract of O. sanctum and characterized as described in our previous study [12]. Among tested pathogens Gram-negative bacteria (E. coli, K. pneumonia, and S. typhi) and Candida species (C. albicans, C. tropicalis) showed higher growth inhibition and microbicidal activity when treated with NiGs than Gram-positive bacteria (B. subtilis and S. epidermidis) and Aspergillus species (A. clavatus, A. fumigatus, and A. niger), respectively. Enhanced antimicrobial activity of NiGs was attributed to the active formation of ROS that led to the loss of cellular proteins and LDH through damaged cell membrane resulting in cell death. In conclusion, the present study suggested that ROS generated from the surface of NiGs interacted and damaged the cell membranes resulting in leakage of cellular contents by cell disruption. This study reveals the potential of NiGs as an antimicrobial agent at 50 μg/mL and hence could be exploited as antimicrobial coatings on surface of materials for various environmental and biomedical applications.

Conflict of Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.

References

Q. A. Pankhurst, N. K. T. Thanh, S. K. Jones, and J. Dobson, “Progress in applications of magnetic nanoparticles in biomedicine,” Journal of Physics D: Applied Physics, vol. 42, no. 22, pp. 1–13, 2009.

J. R. Morones, J. L. Elechiguerra, A. Camacho et al., “The bactericidal effect of silver nanoparticles,” Nanotechnology, vol. 16, no. 10, pp. 2346–2353, 2005.

S. Ravikumar, R. Gokulakrishnan, and P. Boomi, “In vitro antibacterial activity of the metal oxide nanoparticles against urinary tract infectious bacterial pathogens,” Asian Pacific Journal of Tropical Disease, vol. 2, no. 2, pp. 85–89, 2012.

D. Liu, S. Ren, H. Wu, Q. Zhang, and L. Wen, “Morphology control in synthesis of nickel nanoparticles in the presence of polyvinylpyrrolidone (PVPK30),” Journal of Materials Science, vol. 43, no. 6, pp. 1974–1978, 2008.

A. R. Joseph and B. Viswanathan, “Synthesis of nickel nanoparticles with fcc and hcp crystal structures,” Indian Journal of Chemistry, vol. 50, pp. 176–179, 2010.

S. Dhananasekaran, R. Palanivel, and S. Pappu, “Adsorption of methylene blue, bromophenol blue, and coomassie brilliant blue by α-chitin nanoparticles,” Journal of Advanced Research, vol. 7, no. 1, pp. 113–124, 2016.

J. Huang, Q. Li, D. Sun et al., “Biosynthesis of silver and gold nanoparticles by novel sundried Cinnamomum camphora leaf,” Nanotechnology, vol. 18, no. 10, Article ID 105104, pp. 105104–105115, 2007.

L.-C. Chiang, L.-T. Ng, P.-W. Cheng, W. Chiang, and C.-C. Lin, “Antiviral activities of extracts and selected pure constituents of Ocimum basilicum,” Clinical and Experimental Pharmacology and Physiology, vol. 32, no. 10, pp. 811–816, 2005.

S. Jyoti, S. Satendra, S. Sushma, T. Anjana, and S. Shashi, “Antistressor activity of Ocimum sanctum (Tulsi) against experimentally induced oxidative stress in rabbits,” Methods and Findings in Experimental and Clinical Pharmacology, vol. 29, no. 6, pp. 411–416, 2007.

C. Pellieux, A. Dewilde, C. Pierlot, and J.-M. Aubry, “Bactericidal and virucidal activities of singlet oxygen generated by thermolysis of naphthalene endoperoxides,” Methods in Enzymology, vol. 319, pp. 197–207, 2000.

S.-H. Kim, H.-S. Lee, D.-S. Ryu, S.-J. Choi, and D.-S. Lee, “Antibacterial activity of silver-nanoparticles against Staphylococcus aureus and Escherichia coli,” Korean Journal of Microbiology and Biotechnology, vol. 39, no. 1, pp. 77–85, 2011.

C. J. Pandian, R. Palanivel, and S. Dhananasekaran, “Green synthesis of nickel nanoparticles using Ocimum sanctum and their application in dye and pollutant adsorption,” Chinese Journal of Chemical Engineering, vol. 23, no. 8, pp. 1307–1315, 2015.

S. C. Yen and M. D. Mashitah, “Characterization of Ag nanoparticles produced by White-Rot Fungi and Its in vitro antimicrobial activities,” The International Arabic Journal of Antimicrobial Agents, vol. 2, no. 3, pp. 1–8, 2012.

S. Gunalan, R. Sivaraj, and V. Rajendran, “Green synthesized ZnO nanoparticles against bacterial and fungal pathogens,” Progress in Natural Science: Materials International, vol. 22, no. 6, pp. 693–700, 2012.

I. Sondi and B. Salopek-Sondi, “Silver nanoparticles as antimicrobial agent: a case study on E. coli as a model for Gram-negative bacteria,” Journal of Colloid and Interface Science, vol. 275, no. 1, pp. 177–182, 2004.

G. Basak, D. Das, and N. Das, “Dual role of acidic diacetate sophorolipid as biostabilizer for ZnO nanoparticle synthesis and biofunctionalizing agent against Salmonella enterica and Candida albicans,” Journal of Microbiology and Biotechnology, vol. 24, no. 1, pp. 87–96, 2014.

S. Arokiyaraj, M. V. Arasu, S. Vincent et al., “Rapid green synthesis of silver nanoparticles from Chrysanthemum indicum L and its antibacterial and cytotoxic effects: an in vitro study,” International Journal of Nanomedicine, vol. 9, no. 1, pp. 379–388, 2014.

A. J. Kora and J. Arunachalam, “Assessment of antibacterial activity of silver nanoparticles on Pseudomonas aeruginosa and its mechanism of action,” World Journal of Microbiology and Biotechnology, vol. 27, no. 5, pp. 1209–1216, 2011.

K. Mallikarjuna, G. Narasimha, G. R. Dillip et al., “Green synthesis of silver nanoparticles using Ocimum leaf extract and their characterization,” Digest Journal of Nanomaterials and Biostructures, vol. 6, no. 1, pp. 181–186, 2011.

R. Govindasamy, R. Jeyaraman, J. Kadarkaraithangam et al., “Novel and simple approach using synthesized nickel nanoparticles to control blood-sucking parasites,” Veterinary Parasitology, vol. 191, pp. 332–339, 2013.

X. S. Wang, X. Liu, L. Wen, Y. Zhou, Y. Jiang, and Z. Li, “Comparison of basic dye crystal violet removal from aqueous solution by low-cost biosorbents,” Separation Science and Technology, vol. 43, no. 14, pp. 3712–3731, 2008.

A. K. Suresh, D. A. Pelletier, and M. J. Doktycz, “Relating nanomaterial properties and microbial toxicity,” Nanoscale, vol. 5, no. 2, pp. 463–474, 2013.

H. F. Salem, K. A. M. Eid, and M. A. Sharaf, “Formulation and evaluation of silver nanoparticles as antibacterial and antifungal agents with a minimal cytotoxic effect,” Internation Journal of Drug Development and Research, vol. 3, pp. 293–304, 2011.

K.-J. Kim, W. S. Sung, B. K. Suh et al., “Antifungal activity and mode of action of silver nano-particles on Candida albicans,” BioMetals, vol. 22, no. 2, pp. 235–242, 2009.

W.-R. Li, X.-B. Xie, Q.-S. Shi, H.-Y. Zeng, Y.-S. Ou-Yang, and Y.-B. Chen, “Antibacterial activity and mechanism of silver nanoparticles on Escherichia coli,” Applied Microbiology and Biotechnology, vol. 85, no. 4, pp. 1115–1122, 2010.

H. Pang, F. Gao, and Q. Lu, “Morphology effect on antibacterial activity of cuprous oxide,” Chemical Communications, vol. 7, no. 9, pp. 1076–1078, 2009.

J. Sawai, “Quantitative evaluation of antibacterial activities of metallic oxide powders (ZnO, MgO and CaO) by conductimetric assay,” Journal of Microbiological Methods, vol. 54, no. 2, pp. 177–182, 2003.

W. Lin, Y.-W. Huang, X.-D. Zhou, and Y. Ma, “Toxicity of cerium oxide nanoparticles in human lung cancer cells,” International Journal of Toxicology, vol. 25, no. 6, pp. 451–457, 2006.

J. S. Kim, E. Kuk, K. N. Yu et al., “Antimicrobial effects of silver nanoparticles,” Nanomedicine: Nanotechnology, Biology, and Medicine, vol. 3, no. 1, pp. 95–101, 2007.

S. Thirunavukkarasu, R. Abdul, J. Chidambaram et al., “Green synthesis of titanium dioxide nanoparticles using Psidium guajava extract and its antibacterial and antioxidant properties,” Asian Pacific Journal of Tropical Medicine, vol. 7, no. 12, pp. 968–976, 2014.

M. Fang, J.-H. Chen, X.-L. Xu, P.-H. Yang, and H. F. Hildebrand, “Antibacterial activities of inorganic agents on six bacteria associated with oral infections by two susceptibility tests,” International Journal of Antimicrobial Agents, vol. 27, no. 6, pp. 513–517, 2006.

O. Choi and Z. Hu, “Size dependent and reactive oxygen species related nanosilver toxicity to nitrifying bacteria,” Environmental Science and Technology, vol. 42, no. 12, pp. 4583–4588, 2008.

K. Kenneth, Y. Wong, and L. Xuelai, “Silver nanoparticles—the real ‘silver bullet’ in clinical medicine,” Medicinal Chemistry Communications, vol. 1, pp. 125–131, 2010.

R. K. Chrakanth, C. Ashajyothi, A. K. Oli, and C. Prabhurajeshwar, “Potential bactericidal effect of silver nanoparticles synthesised from Enterococcus species,” Oriental Journal of Chemistry, vol. 30, no. 3, pp. 1253–1262, 2014.

S. Agnihotri, S. Mukherji, and S. Mukherji, “Size-controlled silver nanoparticles synthesized over the range 5–100 nm using the same protocol and their antibacterial efficacy,” RSC Advances, vol. 4, no. 8, pp. 3974–3983, 2014.

Y. S. Chan and M. D. Mashitah, “Biosynthesis of silver nanoparticles from Schizophyllum commune and In-vitro antibacterial and antifungal studies,” Journal of Physical Science, vol. 24, no. 2, pp. 83–96, 2013.

A. Nasrollahi, Kh. Pourshamsian, and P. Mansourkiaee, “Antifungal activity of silver nanoparticles on some of fungi,” International Journal of Nano Dimension, vol. 1, no. 3, pp. 233–239, 2011.

A. Panáček, M. Kolář, R. Večeřová et al., “Antifungal activity of silver nanoparticles against Candida spp.,” Biomaterials, vol. 30, no. 31, pp. 6333–6340, 2009.

C. Gao, Y. Xu, and C. Xu, “In Vitro activity of nano-silver against ocular pathogenic fungi,” Life Science Journal, vol. 9, no. 4, pp. 750–753, 2012.

A. Monir and S. Azar, “Antifungal activity of silver nanoparticles indifferent sizes against some pathogenic fungi,” Journal of Applied Chemical Research, vol. 8, no. 4, pp. 115–122, 2014.

J. Jain, S. Arora, J. M. Rajwade, P. Omray, S. Khandelwal, and K. M. Paknikar, “Silver nanoparticles in therapeutics: development of an antimicrobial gel formulation for topical use,” Molecular Pharmaceutics, vol. 6, no. 5, pp. 1388–1401, 2009.