Bioinorganic Chemistry and Applications

Bioinorganic Chemistry and Applications / 2021 / Article

Research Article | Open Access

Volume 2021 |Article ID 9920890 | https://doi.org/10.1155/2021/9920890

Hock Ing Chiu, Che Nurul Azieyan Che Mood, Nur Nadhirah Mohamad Zain, Muggundha Raoov Ramachandran, Noorfatimah Yahaya, Nik Nur Syazni Nik Mohamed Kamal, Wai Hau Tung, Yoke Keong Yong, Chee Keong Lee, Vuanghao Lim, "Biogenic Silver Nanoparticles of Clinacanthus nutans as Antioxidant with Antimicrobial and Cytotoxic Effects", Bioinorganic Chemistry and Applications, vol. 2021, Article ID 9920890, 11 pages, 2021. https://doi.org/10.1155/2021/9920890

Biogenic Silver Nanoparticles of Clinacanthus nutans as Antioxidant with Antimicrobial and Cytotoxic Effects

Academic Editor: Giuseppe Ciccarella
Received09 Mar 2021
Revised21 Apr 2021
Accepted03 May 2021
Published15 May 2021

Abstract

Silver nanoparticles (AgNPs) previously synthesised using leaf (AgNP-L) and stem (AgNP-S) extracts of Clinacanthus nutans (C. nutans) were tested to evaluate antimicrobial, antioxidant, and cytotoxicity activities. The AgNPs showed good inhibition against bacteria, but not fungi. The inhibition results showed the highest activity against Staphylococcus aureus (S. aureus) with 11.35 mm (AgNP-L) and 11.52 mm (AgNP-S), while the lowest inhibition was against Escherichia coli (E. coli) with 9.22 mm (AgNP-L) and 9.25 mm (AgNP-S) in the disc diffusion method. The same trend of results was noted in the well diffusion method. The IC50 of AgNP-L and AgNP-S in 2,2-diphenyl-1-picrylhydrazyl (DPPH) and 2,2′-azino-bis (3-ethylbenzothiazoline-6-sulfonic acid) (ABTS) assays was 417.05 μg/mL and 434.60 μg/mL, as well as 304.31 μg/mL and 326.83 μg/mL, respectively. Ferric reducing power (FRAP) assay showed that AgNP-L [872.389 μmol/L Fe(II)] and AgNP-S [612.770 μmol/L Fe(II)] exhibited significantly ( < 0.05) greater antioxidant activities than leaf extract (CNL) [152.260 μmol/L Fe(II)] and stem extract (CNS) [110.445 μmol/L Fe(II)] of C. nutans. The AgNPs were also proven to possess cytotoxic effects on the breast (MCF-7), cervical (HeLa), and colon (HT-29) cancer cells in a dose-dependent manner. AgNP-S and AgNP-L showed significantly ( < 0.05) higher cytotoxicity against MCF-7 (117.43 μg/mL) and HT-29 (78.47 μg/mL), respectively. In conclusion, the biosynthesised AgNPs from aqueous extract leaves and stem of C. nutans have demonstrated promising potential towards antioxidant, antimicrobial, and cytotoxicity activities.

1. Introduction

AgNPs are well known as effective antimicrobial agents against bacteria and fungi [14]. Therefore, they have been studied in bacterial applications, for instance, in the medical, cosmetics, food, and textile industries [58]. Various skin diseases caused by pathogenic microorganisms are treated with antibiotics. Commonly prescribed antibiotics include erythromycin, clindamycin, tetracycline, penicillin, and ciprofloxacin [9]. Due to the development of antibiotic resistance, researchers are keen to identify alternatives in the development of new antibacterial agents. The biosynthesis of AgNPs can overcome antibiotic resistance and reduce costs compared to conventional antibiotics [10].

Side effects have been observed in synthetic antioxidants such as butylated hydroxytoluene (BHT) and hydroxyanisole (BHA). Low doses of tested BHA appear to be toxic to Vero cells with mitochondrial function loss based on an MTT assay [11]. Several studies reported significant antioxidant activity of the C. nutans extract [12, 13]. Thus, the biocompatible C. nutans-derived AgNPs could be an alternative for synthetic antioxidants. AgNPs demonstrated inhibition of free radicals, such as reactive oxygen species (ROS) produced from metabolic reactions to prevent damage to tissues or cells [14, 15]. A previous study reported that the synthesised AgNPs using Costus afer aqueous leaf extract showed higher antioxidant activity compared to the leaf extract only [16]. AgNPs may, therefore, be a new/novel antioxidant agent with the ability to avoid side effects exhibited by synthetic antioxidants.

In addition to antibacterial and antioxidant properties, the plant-derived AgNPs are widely studied for their cytotoxic effects against cancer cells [17]. Cancer cells are formed from the transformation of normal cells over a number of stages. These could be based on interactions between genetics and external influences, such as physical, chemical, and biological carcinogens [18]. Drug resistance can occur even after chemotherapy treatment [19]. Therefore, alternative biocompatible and cost-effective chemotherapy drugs are needed. It is evident that plant-derived AgNPs have the potential to inhibit the proliferation of cancer cells [20, 21]. Additionally, cytotoxicity of AgNPs has been reported to induce apoptosis of cancer cells through mitochondrial damage and oxidative stress leading to cell death [22, 23]. The aim of this project is, therefore, to assess the antimicrobial, antioxidant, and cytotoxicity properties of C. nutans-derived AgNPs that were previously synthesised [13].

2. Materials and Methods

2.1. Materials

Glacial acetic acid, methanol, and sodium acetate were purchased from QReC, Selangor, Malaysia. DPPH, 2,4,6-tris(2-pyridyl)-1,3,5-triazine (TPTZ), ABTS reagent, 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) reagent, iron(II) sulphate (FeSO4.7H2O), and BHA were obtained from Sigma-Aldrich, Missouri, USA. Mueller Hinton Agar (MHA), Mueller Hinton Broth (MHB), Potato Dextrose Broth (PDB), Sabouraud Dextrose Agar (SDA), and commercial silver nanoparticles (C-AgNP) were acquired from Merck, Darmstadt, Germany. Gentamycin sulphate, nystatin, and hydrochloric acid (HCl) were provided by Biobasic, Ontario, Canada. Glycerol was obtained from System®, Selangor, Malaysia. Potassium persulphate was purchased from Acros Organics, New Jersey, USA. 0.25% Trypsin-EDTA, RPMI 1640, penicillin-streptomycin, foetal bovine serum (FBS), L-glutamine, and Dulbecco’s Modified Eagle Medium (DMEM) were acquired from Gibco®, New York, USA. 5-fluorouracil (5-FU) was purchased from Tokyo Chemical Industry, Tokyo, Japan. 3-(4,5-dimethylthiazol-2-yl)-5-(3-carboxymethoxyphenyl)-2-(4-sulfophenyl)-2H-tetrazolium (MTS) kit was provided by Promega, WI, USA. Phosphate buffer saline (PBS) was obtained from Invitrogen, New York, USA.

2.2. Synthesis of AgNPs

Synthesis of AgNP-S and AgNP-L from CNS and CNL, respectively, was conducted according to our previous published work [13].

2.3. Antimicrobial Activities of Synthesised AgNPs

The antimicrobial activities were tested using the disc and well diffusion methods in the presence of an inhibition region. Then, the broth-microdilution approach was used to achieve the minimum inhibitory concentration (MIC) and minimum bactericidal concentration (MBC).

2.3.1. Microorganisms

The antimicrobial activities were tested against Gram-negative bacteria: (1) ATCC 27853 Pseudomonas aeruginosa (P. aeruginosa) and (2) ATCC 25922 E. coli; Gram-positive bacteria: (1) ATCC 25923 S. aureus, (2) ATCC 12228 Staphylococcus epidermidis (S. epidermidis), and (3) ATCC 19615 Streptococcus pyogenes (S. pyogenes); and fungi: (1) CA 1395 Candida albicans (C. albicans) and (2) Candida glabrata (C. glabrata). The bacteria and fungi were obtained from the Microbiology Laboratory of Clinical Trial Complex, Advanced Medical and Dental Institute (AMDI), USM, and Infectomics Cluster, AMDI, USM, respectively. The strains were stored in 10% glycerol at −80°C until further use.

2.3.2. Preparation of Media

MHA was used for bacterial cultures. The MHA was autoclaved at 121°C for 15 min. Then, the media were poured into a sterile Petri dish (Bio-Rad, California, USA), and it was left to solidify for 24 h at room temperature to avoid contamination. The same protocol was applied for fungi with SDA as the media. The plates were labelled and stored at 4°C in a sealed plastic bag till further need and prewarmed in an incubator at 37°C prior to the experiment.

2.3.3. Preparation of Inoculum and Samples

A single colony was transferred from the stock culture to 10 mL of MHB and PDB for bacteria and fungi, respectively. The culture suspension was incubated at 37°C for 24 h. Dilution of the culture with either MHB or PDB was performed corresponding to 1-2 × 108 CFU/mL of the 0.5 McFarland’s standard using a UV-VIS spectrophotometer and measured at 600 nm. The absorbance should be at 0.1 equivalent to 108 CFU/mL concentration. Each sample (5 mg) was dissolved in 1 mL of distilled water (dH2O). A sonicator (WUC-A10H, Wise Clean, Sonic Wise, California, USA) was used to sonicate the samples for 15 min. Then, the samples were sterile filtered before further use.

2.3.4. Disc Diffusion Method

The procedure was carried out according to the Clinical and Laboratory Standards Institute (CLSI) (M02-A11). Briefly, the prepared inoculum solution was swabbed onto MHA and SDA with a sterile cotton swab. Next, sterile Whatman filter paper (6 mm) (Maidstone, UK) was added with 20 μL of tested samples. The positive controls were gentamicin and nystatin. The discs were gently pressed on the agar and incubated with bacteria and fungi at 37°C and 30°C for 24 and 48 h, respectively. A clear inhibition zone was measured and expressed in millimetre (mm).

2.3.5. Well Diffusion Method

A well of 6 mm in diameter was punctured using sterile pipette tips. Then, the inoculum solution was swabbed on the agar with a sterile cotton swab. Next, 20 μL of the sample was added to each well. The positive controls were gentamicin and nystatin. On the other hand, the negative control was dH2O. Diffusion of samples into the agar was conducted for 1 h. Then, bacteria were incubated on the plate at 37°C and fungi at 30°C. The inhibition zones were obtained after 24 h for bacteria and 48 h for fungi [24].

2.3.6. Broth-Microdilution Assay

A broth-microdilution assay was utilised to assess the MIC and MBC. The method described by the Clinical and Laboratory Standards Institute (CLSI) (M07-A9) was used, with certain modifications. A serial dilution (7.8125 μg/mL to 1000 μg/mL) of the sample was prepared in 96-well plates flat bottom. Each well contained a sample (20 μL) and inoculum suspension (180 μL). The positive and negative controls were gentamicin and dH2O, respectively. The plate was incubated at 37°C for 24 h. Every well was pipetted with MTT in PBS solution (50 μL, 0.5 mg/mL) after the incubation time. After that, the plate was incubated for 30 min. The appearance of a dark purple colour indicated the presence of live bacteria. To determine the MBC values, 10 μL from the wells without purple colour were streaked on MHA and incubated at 37°C for 24 h. After 24 h, the MBC was assessed to differentiate between bactericidal (no growth of bacteria on the plate) and bacteriostatic (bacteria growth on the plate) agents from the samples [25].

2.4. Antioxidant Activities

The antioxidant activities were determined using the DPPH, ABTS, and FRAP assays. Serial dilutions of twofold were performed (31.25, 62.5, 125, 250, and 500 μg/mL) for each sample from their stock solution (1000 μg/mL).

2.4.1. DPPH Radical Scavenging Assay

The radical scavenging DPPH method of antioxidant activity was adapted with some modifications from [26, 27]. Briefly, in a 96-well plate, samples (50 μL) and 0.2 mM DPPH in methanol (150 μL) were added. The plate was incubated for 30 min in the dark, and the absorbance was then measured at 517 nm with microplate readers. The calculation of the antioxidant activity was based on where Abcontrol is the DPPH solution absorbance while Absample is the DPPH solution with sample absorbance.

2.4.2. ABTS Radical Scavenging Assay

With some modifications, the ABTS radical scavenging assay was adapted from [28]. Briefly, the working solution of ABTS cation radical was prepared by mixing 7 mM ABTS solution and 2.45 mM potassium persulphate at 1 : 1 ratio, and this was kept at room temperature for 16 h in the dark. The working solution was diluted with ethanol, and the absorbance at 734 nm was measured using a microplate reader. Each well was pipetted with the sample (20 μL) and ABTS working solution (180 μL). In the dark, this mixture was incubated for 6 min at room temperature, and the absorbance was measured at a wavelength of 734 nm. As the positive control, the sample was compared with BHA. The ABTS radical scavenging calculation was based on where the absorbance of ABTS working reagent with ethanol is ODcontrol and the absorbance of ABTS working reagent with the sample is ODsample.

2.4.3. FRAP Assay

With some changes, the FRAP test was modified according to [29]. In brief, the acetate buffer (0.3 M, pH 3.6) was prepared by mixing 46.3 mL of sodium acetate (0.3 M), 3.7 mL of acetic acid (0.3 M), and 50 mL of dH2O. Then, a mixture of 0.010 M TPTZ solution in 0.040 M HCl, 0.020 M FeCl3, and acetate buffer in the proportion of 1 : 1 : 10 (v/v/v) was prepared for FRAP reagent. The test was performed using a 96-well plate, and 20 μL of samples was mixed in the dark at an ambient temperature with 180 μL FRAP reagent. After 30 min, the absorbance of the sample was measured at 593 nm using a microplate reader. The FeSO4.7H2O standard curve was constructed in the range of 31.25 to 2000 μmol/L, and the FRAP activity was calculated in μmol of ferrous equivalent per μg dry extract (μmol Fe(II)/μg sample).

2.5. Cytotoxicity Studies

The cytotoxicity tests against MCF-7, HT-29, and HeLa cancer cell lines were carried out on the basis of their percentage of viability after treatment.

2.5.1. Cell Lines and Culture Media

The cell lines HT-29, HeLa, and MCF-7 were obtained from the American Type Culture Collection (ATCC). In DMEM, HeLa cell lines were maintained, while HT-29 and MCF-7 were maintained in RPMI 1640. 1% (v/v) L-glutamine, 10% (v/v) FBS, and 1% (v/v) penicillin-streptomycin were applied to both media at 37°C in the carbon dioxide (CO2) incubator (Heraeus BB15, Thermo Scientific, Massachusetts, USA).

2.5.2. Preparation of Cell Concentration and Subculture

The cells were used upon reaching 80% confluent. The old media were pipetted out and rinsed with 5 mL of PBS. Then, 0.5 mL of 0.25% Trypsin-EDTA was applied and incubated in a CO2 incubator for 3 min. A 15 mL centrifuge tube was used to contain the solution. 5 mL of fresh media was then applied, and the mixture was centrifuged for 5 min at 1000 rpm (Heraeus Megafuge 16, Thermo Scientific, Massachusetts, USA). The supernatant was removed, and the pellets in 1 mL of complete media were resuspended. 50 μL of suspension was added to 50 μL of Trypan Blue and placed into a slide counter using an automated cell counter TC10 (Bio-Rad, Richmond, California) to count the total cells. At concentrations of 1 × 104 cells/well (HT-29), 5 ×  103 cells/well (MCF-7), and 1 × 104 cells/well (HeLa), the cells were seeded. The residual suspension was subcultured into a new flask and incubated for further use at 37°C in a CO2 incubator.

2.5.3. Cell Viability Using MTS Assay

In a 96-well plate, HT-29 (1 × 104 cells/well), MCF-7 (5 × 103 cells/well), and HeLa (1 × 104 cells/well) were seeded. The old media were pipetted out after 24 h and replaced with sample-containing media (12.5, 25, 50, 100, and 200 μg/mL). The untreated cells were used as control. The samples used were AgNP-L, AgNP-S, CNL, CNS, C-AgNP, and 5-Fu as the positive control. Then, after 72 h of incubation time, an MTS reagent (20 μL) was added to each well. The plates were then incubated for a further 4 h in the CO2 incubator again. A microplate reader was used to measure the absorbance at 490 nm. The cell viability (%) was calculated using where ODsample is the sample absorbance of the treated cells, and ODcontrol is the absorbance of the untreated cells.

2.6. Statistical Analysis

All of the above experiments were conducted in triplicate and expressed as mean ± standard deviation (SD). One-way variance analysis (ANOVA) and Tukey’s honest significant difference (HSD)/Dunnett’s t-test were used for the statistical analysis. The difference was considered statistically significant if  < 0.05.

3. Results and Discussion

3.1. Antimicrobial Activities

Gram-positive bacteria [Staphylococcus epidermidis (SE), Staphylococcus aureus (SA), and Streptococcus pyogenes (SE)], Gram-negative bacteria [Pseudomonas aeruginosa (PA) and Escherichia coli (EC)], and fungi [Candida glabrata (CG) and Candida albicans (CA)] were used to assess the antimicrobial activity of AgNPs. To screen for the presence of antimicrobial activity, the disc and well diffusion method was conducted. The microdilution of the broth was then carried out to obtain the values of MIC and MBC. Staphylococcus and Streptococcus are common bacteria genera present on the human skin [30], while S. epidermidis, S. aureus, and P. aeruginosa are among the normal “resident” bacteria on human skin. Skin disease can occur when the resident microorganism transforms into pathogenic forms under certain conditions [31, 32]. S. aureus is one of the main pathogenic bacteria which can cause various illnesses from minor skin infections to life-threatening diseases. P. aeruginosa can lead to dermatitis and even deeper soft-tissue infections [33]. C. albicans is the most virulent among other Candida species [34].

The inhibition zones of the AgNPs against pathogenic microorganisms are shown in Tables 1 and 2. The concentrations used in the experiments were fixed for all samples at 1000 μg/mL. Table 1 summarises the antimicrobial activity against microorganisms using the disc diffusion method. Samples AgNP-L and AgNP-S showed antimicrobial activity compared to plant extracts as there was a presence of inhibition zones after 24 h of incubation. Based on the results of the disc diffusion method, AgNP-L and AgNP-S showed the highest activities against S. aureus with 11.35 mm and 11.52 mm, respectively. However, both AgNPs demonstrated the lowest activity levels against E. coli with inhibition zones at 9.22 mm (AgNP-L) and 9.25 mm (AgNP-S). The inhibition zones of AgNPs (AgNP-L and AgNP-S) were significantly higher than the plant extracts (CNL and CNS). Interestingly, both AgNPs showed the highest activity against S. aureus with inhibition zones of 18.29 mm (AgNP-L) and 17.24 mm (AgNP-S) in the well diffusion method (Table 2). Coincidentally, both also displayed the lowest activity against E. coli with inhibition zones of 12.83 mm and 13.41 mm, respectively. There were no inhibition zones noted in samples using the aqueous plant extract (CNL and CNS). Despite showing higher antimicrobial activity against the pathogenic microorganisms, the AgNPs showed significant antimicrobial activity inhibiting the growth of the pathogenic microorganisms. However, no activity was observed when AgNPs and plant extracts were tested on fungi (C. albicans and C. glabrata).


SamplesInhibition zone (mm)
Gram-positive bacteriaGram-negative bacteriaFungi
SASESPECPACACG

CNL0.000a0.000a0.000a0.000a0.000a0.000a0.000a
CNS0.000a0.000a0.000a0.000a0.000a0.000a0.000a
AgNP-L11.350 ± 0.243b11.597 ± 0.311b10.260 ± 0.125b9.220 ± 0.433b10.073 ± 0.280b0.000a0.000a
AgNP-S11.517 ± 0.519b10.153 ± 0.232c10.493 ± 0.345b9.247 ± 0.081b10.000 ± 0.305b0.000b0.000a
C-AgNP0.000a0.000a0.000a0.000a0.000a0.000b0.000a
dH2O0.000a0.000a0.000a0.000a0.000a0.000b0.000a
Gentamycin21.957 ± 0.486c25.543 ± 0.440d22.967 ± 0.799c21.840 ± 0.155c17.530 ± 0.521cNDND
NystatinNDNDNDNDND17.367 ± 0.136c21.200 ± 0.200b

ND = not determined.

SamplesZone of inhibition (mm)
Gram-positive bacteriaGram-negative bacteriaFungi
SASESPECPACACG

CNL0.000a0.000a0.000a0.000a0.000a0.000a0.000a
CNS0.000a0.000a0.000a0.000a0.000a0.000a0.000a
AgNaP-L18.290 ± 0.303b16.987 ± 0.652b13.913 ± 0.311b12.830 ± 0.607b14.160 ± 0.436b0.000a0.000a
AgNaP-S17.237 ± 0.123c17.000 ± 0.146b13.730 ± 0.191b13.413 ± 4.500b14.140 ± 4.500b0.000a0.000a
C-AgNaPs0.000a0.000a0.000a0.000a0.000a0.000a0.000a
Gentamycin27.81 ± 0.206d31.84 ± 0.138c26.42 ± 0.678c24.45 ± 0.116c26.78 ± 0.102cNDND
dH2O0.000a0.000a0.000a0.000a0.000a0.000a0.000a
NystatinNDNDNDNDND26.267 ± 4.500b31.285 ± 5.511b

ND = not determined.
3.1.1. Broth-Microdilution Assay

Based on the antimicrobial activity using disc and well diffusion methods, the samples that produced inhibition zones (AgNP-L, AgNP-S, and gentamicin) were further used for the broth-microdilution assay to determine the MIC and the MBC. Based on the result of MBC, the bactericidal and bacteriostatic properties of the samples against pathogenic microorganisms can be determined. Bactericidal refers to the ability to kill microorganisms while bacteriostatic agents are able to inhibit microorganisms. Plates with no growth of bacteria indicate bactericidal properties while plates with bacteria growth indicate bacteriostatic abilities [25]. Table 3 shows the MIC and MBC values for the AgNPs. To determine the antimicrobial activity, the disc diffusion method was used because it is a simple and reliable method with a minimum cost [35]. However, MIC could not be determined because it requires a large range of concentrations and is not economic compared to disc or well diffusion. Therefore, to determine the MIC values, a broth-microdilution assay was carried out.


SamplesMIC (μg/mL)MBC (μg/mL)
SASESPPAECSASESPPAEC

AgNP-L250250250250125250250250250125
AgNP-S250250250125125250250250125125
Gentamicin31.2562.531.2562.512531.2531.2531.2562.5125

The MIC was performed in a 96-well plate and incubated at 37°C for 24 hours. The MTT reagent was used as an indicator after 24 h. The change in colour from purple to yellow was indicative of bacteria death [25]. The MIC of AgNP-L was reported at the concentration of 250 g/mL against S. aureus, S. epidermidis, S. pyogenes, and P. aeruginosa, and it was reported at 125 μg/mL against E. coli. As for S. aureus, S. epidermidis, and S. pyogenes, the MIC of AgNP-S was reported at the concentration of 250 μg/mL, and it was reported at 125 μg/mL for E. coli and P. aeruginosa. The AgNP-L MBC was the same as the bactericidal MIC due to the absence of bacterial growth at 250 μg/mL against S. aureus, S. epidermidis, S. pyogenes, and P. aeruginosa, and it was reported at 125 μg/mL against E. coli. In MIC, the MBC of AgNP-S also demonstrated the same concentration. There were no MIC and MBC for fungi because there were no inhibition zones using the disc or well diffusion methods.

From the results in Tables 1 and 2, AgNP-L and AgNP-S showed inhibition zones compared to plant extracts (CNL and CNS). Plant extracts at 1000 μg/mL showed no inhibition zones. Previous studies have investigated the antimicrobial activity of C. nutans. However, results showed insignificant activity against acne-inducing bacteria even at high concentrations (5 mg/mL) [36]. The C. nutans leaf extract showed important antimicrobial effects against E. coli and S. aureus, with MIC values of 12.5 mg/mL [37].

As for AgNPs, the result in Tables 1 and 2 suggests that Gram-positive bacteria possess better inhibition zones compared to Gram-negative bacteria. Similar results were found by [38] where S. aureus inhibited a higher zone than E. coli, thus suggesting the absorption and accumulation of AgNPs on the cell wall. Nevertheless, insignificant inhibition zones occurred against C. albicans and C. glabrata. In the AgNPs synthesis with Lantana camara L. leaves, Gram-positive (S. aureus; 28 mm) bacteria have a larger inhibition zone than Gram-negative bacteria (P. aeruginosa, 21 mm; and E. coli, 22 mm) using the well diffusion method.

The other mechanism is due to the size of AgNPs. The small size of AgNPs results in a large surface area to volume ratio, and this is important in antimicrobial activity against pathogenic bacteria. AgNPs are able to easily attach and penetrate the microorganisms compared to bigger particles [10]. In a comparative study, size-controlled AgNPs with 5 nm showed the lowest minimum inhibitory concentrations compared to 100 nm against E.coli, B. subtilis, and S. aureus [39].

A former study hypothesised that cell death is caused by high concentrations of positive potassium (K+) ions in the extracellular fluids as a consequence of bacterial cell damage by AgNPs [40]. The study also reported that the amount of proteins released by the bacterial cells increased with the concentration of AgNPs. Another study reported that silver ions interrupt the enzymes and proteins needed for adenosine triphosphate (ATP) production, thus disturbing the life cycle of the cell and leading to cell death [41]. On the other hand, a study by [42] reported that cell death could occur due to the interaction of silver with protein. AgNPs react with sulphur-containing amino acids with the abundance of sulphur-containing proteins within and outside the bacterial cell, thus influencing the viability of the bacterial cell. Furthermore, silver ions from the nanoparticles interact with phosphorus in deoxyribonucleic acid (DNA), resulting in the inactivation of DNA replication and the inhibition of enzyme functions [43, 44]. Transmission electron microscopy (TEM) analysis showed a big gap between the cytoplasm and cell wall of the E. coli after treatment with silver, thus confirming the presence of phosphorous as a primary component in DNA molecules [45].

3.2. Antioxidant Activities

Reactive oxygen species (ROS) released in excess during metabolic reactions in the human body cause cell damage [46]. ROS can cause the development of cancer, cardiovascular disease, inflammation, aging, and neurological diseases [47]. Antioxidants function as scavengers to the free radicals caused by ROS, which decreases the risk of chronic disease [48]. Antioxidant activity of AgNPs was analysed in serial concentrations of 31.25, 62.5, 125, 250, and 500 μg/mL using DPPH, ABTS, and FRAP assays. These three assays were chosen as they are simple and inexpensive and produce fast results.

3.2.1. DPPH, ABTS, and FRAP Assays

Figure 1(a) shows the effects of radical scavenging activity for CNL, CNS, C-AgNP, AgNP-L, and AgNP-S compared with the standard antioxidant BHA. Inhibitory activity against the DPPH radical was seen in the samples examined. The determined half-maximal inhibitory concentration (IC50) values for CNL and CNS were >500 μg/mL, 417.05 μg/mL (AgNP-L), 434.60 μg/mL (AgNP-S), and 40.97 μg/mL (BHA). The results showed that control (BHA) exhibited significantly higher values, while C-AgNP showed significantly lower IC50 values than CNL, CNS, AgNP-L, and AgNP-S. Based on the order of BHA > AgNP-L > AgNP-S > CNL > CNS > C-AgNP, the scavenging effects of samples on radical DPPH decreased.

It was discovered that each sample’s capacity to scavenge free radicals differed and increased in a dose-dependent manner. Therefore, the interaction between sample form and concentration had significantly affected CNL, CNS, C-AgNP, and control (BHA). There were no significant differences between CNL and CNS for all concentrations. The same goes for AgNP-L and AgNP-S. However, there was a significant difference between the plant extracts (CNL and CNS) and AgNPs (AgNP-L and AgNP-S). Both AgNPs were significantly higher compared to C-AgNP. It shows that AgNPs are more effective as antioxidant agents compared to C. nutans plant extracts at all concentrations.

A previous study showed that synthesised AgNPs using Cleistanthus collinus leaf extract inhibited DPPH by 43.5% at 1000 μg/mL [49]. The current synthesised AgNPs showed 51.39% (AgNP-L) and 49.94% (AgNP-S) at 500 μg/mL. Previous studies reported that AgNPs showed 51% of DPPH inhibition at 200 μg/mL for AgNPs synthesised with Cassia tora leaf extract [50] and 80% inhibition at 100 μg/mL for AgNPs synthesised from the leaf extract of Croton bonplandianum [51].

The reaction of DPPH towards antioxidants occurs through a hydrogen atom donor and electron transfer [52]. The synthesised AgNPs would be rich in hydrogen after adding the free radical (DPPH). Accordingly, the colour change from purple to yellow is a result of the conversion of free radical DPPH• (2,2-diphenyl-1-picrylhydrazyl radical) to non-free radical DPPH-H (2,2-diphenyl-1-picrylhydrazine). This is due to the transfer of hydrogen from AgNPs to free radicals in developing stable products [51]. The conjugation of biocompounds to silver ions has caused DPPH radical scavenging [53]. Therefore, biosynthesised AgNPs have potential as antioxidative agents. Although DPPH assay is simple and easy, it has its limitations. Samples that react rapidly with peroxyl radicals may either react slowly or not at all towards DPPH [52]. Therefore, the samples were further analysed using ABTS and FRAP assays.

Figure 1(b) demonstrates the antioxidant activity dependent on the ABTS radical scavenging assay. AgNPs with IC50 antioxidant activity of 304.31 μg/mL (AgNP-L) and 326.83 μg/mL (AgNP-S) are lower than CNL and CNS IC50 (>500 μg/mL). The IC50 for BHA is less than 31.25 μg/mL, and for C-AgNP, it is recorded at 341.81 μg/mL. The ABTS radical scavenging inhibition of all tested samples shows a dose-dependent manner. The reduction of free radicals is significantly increased at higher concentrations. The results obtained, however, also show that the sample reduction of ABTS•+ is significantly lower than BHA ( < 0.05). Based on the data, CNL has a higher activity for each concentration and is significantly different ( < 0.05) from CNS. AgNP-L and AgNP-S also showed significantly different ( < 0.05) results at every concentration, with AgNP-L possessing higher activity of ABTS scavenging compared to AgNP-S.

The ABTS assay defines how efficient antioxidants are at scavenging ABTS and forming the ABTS radical 2,2′-azino-bis(3-ethylbenzothiazoline-6-sulphonic acid (ABTS•+). Antioxidants serve as agents for donating hydrogen. The blue/green colour of ABTS•+ is produced from the reaction of ABTS with a strong oxidising agent (potassium persulphate) which produces radical cations [54].

From the calibration curve (y = 0.0017x + 0.0451; R2 = 0.9992), the FRAP values were calculated and expressed as mM Fe(II) per μg of the sample (μmol/L Fe(II)/μg sample). The calibration curve was determined using (FeSO4.7H2O). Figure 1(c) shows the antioxidant activity results based on the FRAP assay. The FRAP activity of all tested samples increased in a dose-dependent manner. There was no significant difference ( < 0.05) between CNL and CNS. However, the difference between plant extracts and AgNPs (AgNP-L and AgNP-S) was significant ( < 0.05), with AgNP-L showing higher activity compared to AgNP-S. At the highest concentration of AgNPs (500 μg/mL), the antioxidant activity of AgNP-L was found to be 872.389 μmol/L Fe(II) and AgNP-S [612.770 μmol/L Fe(II)] compared to the plant extracts with 110.445 μmol/L Fe(II) (CNL) and 152.260 μmol/L Fe(II) (CNS), respectively.

The FRAP assay is based on the principle of reducing antioxidants from ferric 2,4,6-tripyridyltriazine (Fe(III)-TPTZ) to ferrous (Fe(II)-TPTZ) complexes. Antioxidants act as electron donors. The colour of the end product (Fe(II)-TPTZ) is blue, and the antioxidant capacity is directly proportional to the colour intensity [55, 56].

3.3. Cytotoxicity Activities

Figure 2(a) shows the percentage of viability for MCF-7 after treatment with different samples. All samples showed a reduction in viable cells as the concentrations of samples increased. The IC50 was observed at 117.43 μg/mL for AgNP-S whereas the values were more than 200 μg/mL for CNL, CNS, AgNP-L, and C-AgNP. When the maximum sample concentration (200 μg/mL) was used, cell viability using plant extract was higher: CNL (77.05%) and CNS (72.10%) compared to synthesised AgNPs; AgNP-L (57.24%) and AgNP-S (26.47%). AgNP-L and AgNP-S showed lower cell viability compared to C-AgNP (83.27%). All samples tested showed a significant difference from untreated cells (control) ( < 0.05) at 100 and 200 μg/mL concentrations. Both AgNP-L and AgNP-S demonstrated a substantial difference from the control at the lowest concentration (12.5 μg/mL). AgNP-S showed the lowest cell viability compared to other samples (CNL, CNS, AgNP-L, and C-AgNP).

Figure 2(b) shows the percentage viability of HT-29 after treatment. All samples showed a decrease in cell viability when the concentrations increased. The IC50 for AgNP-L was 78.47 μg/mL, while the CNL, CNS, AgNP-S, and C-AgNP were more than 200 μg/mL. The IC50 for 5-Fu was less than 12.5 μg/mL. At the maximum concentration (200 μg/mL), the viabilities of AgNP-L (22.44%) and AgNP-S (74.00%) were higher than those of the plant extracts which were CNL (73.91%) and CNS (78.82%). Both AgNP-L and AgNP-S showed lower viability compared to C-AgNP (65.61%). All the samples examined showed a significant difference (< 0.05) from the control at concentrations of 50, 100, and 200 μg/mL. AgNP-L displayed a higher sensitivity relative to AgNP-S as AgNP-L showed a large difference as compared to the control at the lowest concentration (12.5 μg/mL).

Figure 2(c) shows the percentage of viable HeLa after treatment. The IC50 for AgNP-L is 175.35 μg/mL while IC50 for CNL, CNS, AgNP-S, and C-AgNP were more than 200 μg/mL and 5-Fu was less than 12.5 μg/mL. At the highest concentrations of samples used (200 μg/mL), the cytotoxic effects of AgNP-L (43.87%) and AgNP-S (54.33%) were higher compared to plant extracts which were CNL (87.72%) and CNS (90.23%). Both AgNP-L and AgNP-S showed higher cytotoxicity activity compared to C-AgNP (79.75%). All the samples analysed showed substantial variations at concentrations of 100 and 200 μg/mL. AgNP-L demonstrated a significant difference relative to AgNP-S, which was not significant at the lowest concentration of 12.5 μg/mL.

The MTS assays were used to determine the viability of the cancer cells (MCF-7, HT-29, and HeLa) after treating with samples. MTS solution is based on tetrazolium salt which measures the mitochondrial dehydrogenase activity of viable cells. The cell produces a dark purple formazan product when tetrazolium salt is cleaved by active mitochondria. Therefore, it can be used to measure the viability of the cells since the reaction only occurs in active living cells. If the cells die, they lose the ability to convert MTS into formazan [57]. The determined values are based on the formation of colours and are directly proportional to the number of cells that are viable.

Based on the findings shown, both AgNP-L and AgNP-S have produced higher cytotoxicity effects compared to plant extracts (CNL and CNS). The antiproliferative activities are categorised into four groups according to the values of IC50: ≤20 μg/mL (active), >20–100 μg/mL (moderately active), >100–1000 μg/mL (weakly active), and >1000 μg/mL (inactive) [58]. According to the National Cancer Institute (NCI), a crude extract is considered active for anticancer activity if it has an IC50 of less than 20 μg/mL [59]. Thus, the AgNPs were in the group weakly active as the IC50 value of AgNP-L was more than 200 μg/mL (MCF-7), 78.47 μg/mL for HT-29, and 173.35 μg/mL for HeLa. Also, the IC50 of AgNP-S was 117.43 μg/mL (MCF-7) and more than 200 μg/mL (HT-29 and HeLa). Furthermore, in previous experiments, it was discovered that AgNPs were not cytotoxic to 3T3-L1, a normal mouse embryonic fibroblast [22].

The disruption of the mitochondrial respiratory chain by AgNPs increases the production of ROS and DNA damage due to the interruption of ATP synthesis [60]. ROS are constantly being generated and eliminated in a biological system. The death of the cancer cell is hypothesised based on the excessive production of ROS (apoptosis) [61, 62]. The oxidative stress that induces apoptosis leads to the damage of cellular components in the cell [63]. Furthermore, the positive silver (Ag+) ion released by the dissolution of AgNPs causes cytotoxicity effects. Ag+ reacts with the thiol group of antioxidants such as glutathione and superoxide dismutase, thus leading to lipid peroxidation, oxidative stress, DNA damage, and cell death [64]. To conclude, the results indicate that AgNPs have cytotoxic effects against the cancer cell lines of MCF-7, HT-29, and HeLa.

4. Conclusions

Both Gram-positive and Gram-negative bacteria were inhibited by AgNP-L and AgNP-S, but the fungi response was negative. In addition, AgNP-L and AgNP-S showed the highest inhibition against S. aureus and lowest inhibition against E. coli. The results of these antimicrobial activities proved that AgNPs have the potential to be antimicrobial agents. In the DPPH, ABTS, and FRAP assays, AgNP-L and AgNP-S exhibited significantly greater antioxidant potency ( < 0.05) than plant extracts (CNL and CNS), which show promising potential for AgNPs as antioxidant agents. In the treatment of MCF-7, HT-29, and HeLa, both AgNP-L and AgNP-S demonstrated higher toxicity compared to CNL and CNS at similar concentrations. Furthermore, both AgNPs possessed a significant ( < 0.05) toxicity on all the cancer cells compared to the control. To conclude, the AgNPs have demonstrated potential as anticancer agents. However, more research is nseeded to support the potential for human cancer treatment. From all the studies conducted thus far, biologically synthesised AgNPs from C. nutans are simple and eco-friendly and have great potential to be applied as nanomedicine.

Data Availability

The data used to support the findings of this study are included within the article.

Conflicts of Interest

The authors declare that they have no conflicts of interest.

Acknowledgments

This study was supported by the Fundamental Research Grant Scheme (FRGS, Reference code: FRGS/1/2018/STG07/USM/02/9, Account code: 203.CIPPT.6711684) from the Ministry of Higher Education, Malaysia. Hock Ing Chiu would like to express his appreciation to USM for providing him USM Fellowship Scheme.

References

  1. 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. View at: Publisher Site | Google Scholar
  2. M. K. Rai, S. D. Deshmukh, A. P. Ingle, and A. K. Gade, “Silver nanoparticles: the powerful nanoweapon against multidrug-resistant bacteria,” Journal of Applied Microbiology, vol. 112, no. 5, pp. 841–852, 2012. View at: Publisher Site | Google Scholar
  3. M. Amin, S. Hameed, A. Ali et al., “Green synthesis of silver nanoparticles: structural features and in vivo and in vitro therapeutic effects against Helicobacter pylori induced gastritis,” Bioinorganic Chemistry and Applications, vol. 2014, Article ID 135824, 11 pages, 2014. View at: Publisher Site | Google Scholar
  4. S. Rajeshkumar and C. Malarkodi, “In vitro antibacterial activity and mechanism of silver nanoparticles against foodborne pathogens,” Bioinorganic Chemistry and Applications, vol. 2014, Article ID 581890, 10 pages, 2014. View at: Publisher Site | Google Scholar
  5. X. Chen and H. J. Schluesener, “Nanosilver: a nanoproduct in medical application,” Toxicology Letters, vol. 176, no. 1, pp. 1–12, 2008. View at: Publisher Site | Google Scholar
  6. F. Zhang, X. Wu, Y. Chen, and H. Lin, “Application of silver nanoparticles to cotton fabric as an antibacterial textile finish,” Fibers and Polymers, vol. 10, no. 4, pp. 496–501, 2009. View at: Publisher Site | Google Scholar
  7. S. Kokura, O. Handa, T. Takagi, T. Ishikawa, Y. Naito, and T. Yoshikawa, “Silver nanoparticles as a safe preservative for use in cosmetics,” Nanomedicine: Nanotechnology, Biology and Medicine, vol. 6, no. 4, pp. 570–574, 2010. View at: Publisher Site | Google Scholar
  8. E. Antony, S. Gunasekaran, M. Sathiavelu, and S. Arunachalam, “A review on use of plant extracts for gold and silver nanoparticle synthesis and their potential activities against food pathogens,” Asian Journal of Pharmaceutical and Clinical Research, vol. 9, pp. 18–23, 2016. View at: Publisher Site | Google Scholar
  9. P. D. Gupta, R. Babu, and P. V. Deshmukh, “Antibacterial activity of 6 Indian medicinal plants against bacterial pathogens isolated from various skin ailments,” Asian Journal of Experimental Biological Sciences, vol. 4, pp. 336–344, 2013. View at: Google Scholar
  10. M. Rai, A. Yadav, and A. Gade, “Silver nanoparticles as a new generation of antimicrobials,” Biotechnology Advances, vol. 27, no. 1, pp. 76–83, 2009. View at: Publisher Site | Google Scholar
  11. V. Labrador, P. Fernández Freire, J. M. Pérez Martín, and M. J. Hazen, “Cytotoxicity of butylated hydroxyanisole in Vero cells,” Cell Biology and Toxicology, vol. 23, no. 3, pp. 189–199, 2007. View at: Publisher Site | Google Scholar
  12. H. W. Chong, K. Rezaei, B. L. Chew, and V. Lim, “Chemometric profiling of Clinacanthus nutans leaves possessing antioxidant activities using ultraviolet-visible spectrophotometry,” Chiang Mai Journal of Science, vol. 45, pp. 1519–1530, 2018. View at: Google Scholar
  13. S. N. A. Mat Yusuf, C. N. A. Che Mood, N. H. Ahmad, D. Sandai, C. K. Lee, and V. Lim, “Optimization of biogenic synthesis of silver nanoparticles from flavonoid-rich Clinacanthus nutans leaf and stem aqueous extracts,” Royal Society Open Science, vol. 7, 2020. View at: Publisher Site | Google Scholar
  14. T. Sivakumar, D. Gajalakshm, V. K. Subramania, and K. Palanisamy, “Tuber extract mediated biosynthesis of silver nanoparticles and its antioxidant, antibacterial activity,” Journal of Biological Sciences, vol. 15, no. 2, pp. 68–77, 2015. View at: Publisher Site | Google Scholar
  15. A.-R. Phull, Q. Abbas, A. Ali et al., “Antioxidant, cytotoxic and antimicrobial activities of green synthesized silver nanoparticles from crude extract of Bergenia ciliata,” Future Journal of Pharmaceutical Sciences, vol. 2, no. 1, pp. 31–36, 2016. View at: Publisher Site | Google Scholar
  16. E. E. Elemike, O. E. Fayemi, A. C. Ekennia, D. C. Onwudiwe, and E. E. Ebenso, “Silver nanoparticles mediated by Costus afer leaf extract: synthesis, antibacterial, antioxidant and electrochemical properties,” Molecules, vol. 22, pp. 1–20, 2017. View at: Publisher Site | Google Scholar
  17. N. Hanan, H. Chiu, M. Ramachandran et al., “Cytotoxicity of plant-mediated synthesis of metallic nanoparticles: a systematic review,” International Journal of Molecular Sciences, vol. 19, no. 6, p. 1725, 2018. View at: Publisher Site | Google Scholar
  18. S. Lokina, A. Stephen, V. Kaviyarasan, C. Arulvasu, and V. Narayanan, “Cytotoxicity and antimicrobial activities of green synthesized silver nanoparticles,” European Journal of Medicinal Chemistry, vol. 76, pp. 256–263, 2014. View at: Publisher Site | Google Scholar
  19. F.-S. Liu, “Mechanisms of chemotherapeutic drug resistance in cancer therapy—a quick review,” Taiwanese Journal of Obstetrics and Gynecology, vol. 48, no. 3, pp. 239–244, 2009. View at: Publisher Site | Google Scholar
  20. S. Z. L. Ghozali, V. Lim, and N. H. Ahmad, “Biosynthesis and characterization of silver nanoparticles using Catharanthus roseus leaf extract and its proliferative effects on cancer cell lines,” Journal of Nanomedicine & Nanotechnology, vol. 6, no. 4, Article ID 1000305, 2015. View at: Publisher Site | Google Scholar
  21. E. S. Al-Sheddi, N. N. Farshori, M. M. Al-Oqail et al., “Anticancer potential of green synthesized silver nanoparticles using extract of nepeta deflersiana against human cervical cancer cells (HeLA),” Bioinorganic Chemistry and Applications, vol. 2018, Article ID 9390784, 12 pages, 2018. View at: Publisher Site | Google Scholar
  22. F. Yakop, S. Aisyah, A. Ghafar et al., “Silver nanoparticles Clinacanthus Nutans leaves extract induced apoptosis towards oral squamous cell carcinoma cell lines,” Artificial Cells, Nanomedicine, and Biotechnology, vol. 46, pp. S131–S139, 2018. View at: Publisher Site | Google Scholar
  23. K. Z. Khor, J. Joseph, F. Shamsuddin, V. Lim, E. J. Moses, and N. Abdul Samad, “The cytotoxic effects of moringa oleifera leaf extract and silver nanoparticles on human kasumi-1 cells,” International Journal of Nanomedicine, vol. 15, pp. 5661–5670, 2020. View at: Publisher Site | Google Scholar
  24. P. Manivasagan, J. Venkatesan, K. Senthilkumar, K. Sivakumar, and S. K. Kim, “Biosynthesis, antimicrobial and cytotoxic effect of silver nanoparticles using a novel Nocardiopsis sp. MBRC-1,” BioMed Research International, vol. 2013, Article ID 287638, 9 pages, 2013. View at: Publisher Site | Google Scholar
  25. M. A. Ansari, H. M. Khan, A. A. Khan et al., “Evaluation of antibacterial activity of silver nanoparticles against MSSA and MRSA on isolates from skin infections,” Biology and Medicine, vol. 3, pp. 141–146, 2011. View at: Google Scholar
  26. Y. K. Yong, J. J. Tan, S. S. Teh et al., “Clinacanthus nutansExtracts are antioxidant with antiproliferative effect on cultured human cancer cell lines,” Evidence-Based Complementary and Alternative Medicine, vol. 2013, Article ID 462751, 8 pages, 2013. View at: Publisher Site | Google Scholar
  27. N. Muniyappan and N. S. Nagarajan, “Green synthesis of silver nanoparticles with Dalbergia spinosa leaves and their applications in biological and catalytic activities,” Process Biochemistry, vol. 49, no. 6, pp. 1054–1061, 2014. View at: Publisher Site | Google Scholar
  28. R. A. Khan, M. R. Khan, S. Sahreen, and M. Ahmed, “Evaluation of phenolic contents and antioxidant activity of various solvent extracts of Sonchus asper (L.) Hill,” Chemistry Central Journal, vol. 6, p. 12, 2012. View at: Publisher Site | Google Scholar
  29. Rockenbach, L. V. Gonzaga, V. M. Rizelio, A. E. d. S. S. Gonçalves, M. I. Genovese, and R. Fett, “Phenolic compounds and antioxidant activity of seed and skin extracts of red grape (Vitis vinifera and Vitis labrusca) pomace from Brazilian winemaking,” Food Research International, vol. 44, no. 4, pp. 897–901, 2011. View at: Publisher Site | Google Scholar
  30. Z. Gao, G. I. Perez-Perez, Y. Chen, and M. J. Blaser, “Quantitation of major human cutaneous bacterial and fungal populations,” Journal of Clinical Microbiology, vol. 48, no. 10, pp. 3575–3581, 2010. View at: Publisher Site | Google Scholar
  31. H. H. Kong, “Skin microbiome: genomics-based insights into the diversity and role of skin microbes,” Trends in Molecular Medicine, vol. 17, no. 6, pp. 320–328, 2011. View at: Publisher Site | Google Scholar
  32. T. C. Scharschmidt and M. A. Fischbach, “What lives on our skin: ecology, genomics and therapeutic opportunities of the skin microbiome,” Drug Discovery Today: Disease Mechanisms, vol. 10, no. 3-4, pp. e83–e89, 2013. View at: Publisher Site | Google Scholar
  33. A. L. Cogen, V. Nizet, and R. L. Gallo, “Skin microbiota: a source of disease or defence?” British Journal of Dermatology, vol. 158, no. 3, pp. 442–455, 2008. View at: Publisher Site | Google Scholar
  34. F. L. Mayer, D. Wilson, and B. Hube, “Candida albicanspathogenicity mechanisms,” Virulence, vol. 4, no. 2, pp. 119–128, 2013. View at: Publisher Site | Google Scholar
  35. M. Balouiri, M. Sadiki, and S. K. Ibnsouda, “Methods for in vitro evaluating antimicrobial activity: a review,” Journal of Pharmaceutical Analysis, vol. 6, no. 2, pp. 71–79, 2016. View at: Publisher Site | Google Scholar
  36. M. T. Chomnawang, S. Surassmo, V. S. Nukoolkarn, and W. Gritsanapan, “Antimicrobial effects of Thai medicinal plants against acne-inducing bacteria,” Journal of Ethnopharmacology, vol. 101, no. 1-3, pp. 330–333, 2005. View at: Publisher Site | Google Scholar
  37. H. S. Yang, T. W. Peng, P. Madhavan, M. S. A. Shukkoor, and G. A. Akowuah, “Phytochemical analysis and antibacterial activity of methanolic extract of Clinacanthus nutans leaf,” International Journal of Drug Development & Research, vol. 5, pp. 349–355, 2013. View at: Google Scholar
  38. B. Paul, B. Bhuyan, D. D. Purkayastha, and S. S. Dhar, “Photocatalytic and antibacterial activities of gold and silver nanoparticles synthesized using biomass of Parkia roxburghii leaf,” Journal of Photochemistry and Photobiology B: Biology, vol. 154, pp. 1–7, 2016. View at: Publisher Site | Google Scholar
  39. 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. View at: Publisher Site | Google Scholar
  40. D. K. Tiwari, J. Behari, and P. Sen, “Time and dose-dependent antimicrobial potential of Ag nanoparticles synthesized by top-down approach,” Current Science, vol. 95, pp. 647–655, 2008. View at: Google Scholar
  41. M. Yamanaka, K. Hara, and J. Kudo, “Bactericidal actions of a silver ion solution on Escherichia coli, studied by energy-filtering transmission electron microscopy and proteomic analysis,” Applied and Environmental Microbiology, vol. 71, no. 11, pp. 7589–7593, 2005. View at: Publisher Site | Google Scholar
  42. R. Rawashdeh and Y. Haik, “Antibacterial mechanisms of metallic nanoparticles: a review,” Dynamic Biochemistry, Process Biotechnology and Molecular Biology, vol. 3, pp. 12–20, 2009. View at: Google Scholar
  43. 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. View at: Publisher Site | Google Scholar
  44. G. M. Sulaiman, W. H. Mohammed, T. R. Marzoog, A. A. A. Al-Amiery, A. A. H. Kadhum, and A. B. Mohamad, “Green synthesis, antimicrobial and cytotoxic effects of silver nanoparticles using Eucalyptus chapmaniana leaves extract,” Asian Pacific Journal of Tropical Biomedicine, vol. 3, no. 1, pp. 58–63, 2013. View at: Publisher Site | Google Scholar
  45. Q. L. Feng, J. Wu, G. Q. Chen, F. Z. Cui, T. N. Kim, and J. O. Kim, “A mechanistic study of the antibacterial effect of silver ions onEscherichia coli andStaphylococcus aureus,” Journal of Biomedical Materials Research, vol. 52, no. 4, pp. 662–668, 2000. View at: Publisher Site | Google Scholar
  46. D. Wu and A. I. Cederbaum, “Alcohol, oxidative stress, and free radical damage,” Alcohol Research & Health: The Journal of the National Institute on Alcohol Abuse and Alcoholism, vol. 27, pp. 277–284, 2003. View at: Publisher Site | Google Scholar
  47. L. A. Pham-Huy, H. He, and C. Pham-Huy, “Free radicals, antioxidants in disease and health,” International Journal of Biomedical Science, vol. 4, pp. 89–96, 2008. View at: Google Scholar
  48. J. K. Willcox, S. L. Ash, and G. L. Catignani, “Antioxidants and prevention of chronic disease,” Critical Reviews in Food Science and Nutrition, vol. 44, no. 4, pp. 275–295, 2004. View at: Publisher Site | Google Scholar
  49. R. Vennilaraj, K. Palanisamy, and S. Bitragunta, “Green synthesis of silver nanoparticles from Cleistanthus collinus leaf extract and their biological effects,” International Journal of Chemistry, vol. 34, no. 1, pp. 1103–1107, 2013. View at: Google Scholar
  50. A. Saravanakumar, M. Ganesh, J. Jayaprakash, and H. T. Jang, “Biosynthesis of silver nanoparticles using Cassia tora leaf extract and its antioxidant and antibacterial activities,” Journal of Industrial and Engineering Chemistry, vol. 28, pp. 277–281, 2015. View at: Publisher Site | Google Scholar
  51. V. Kumar, S. Mohan, D. K. Singh, D. K. Verma, V. K. Singh, and S. H. Hasan, “Photo-mediated optimized synthesis of silver nanoparticles for the selective detection of Iron(III), antibacterial and antioxidant activity,” Materials Science and Engineering: C, vol. 71, pp. 1004–1019, 2017. View at: Publisher Site | Google Scholar
  52. D. Huang, B. Ou, and R. L. Prior, “The chemistry behind antioxidant capacity assays,” Journal of Agricultural and Food Chemistry, vol. 53, no. 6, pp. 1841–1856, 2005. View at: Publisher Site | Google Scholar
  53. J. K. Patra and K. H. Baek, “Biosynthesis of silver nanoparticles using aqueous extract of silky hairs of corn and investigation of its antibacterial and anticandidal synergistic activity and antioxidant potential,” IET Nanobiotechnology, vol. 10, no. 5, pp. 326–333, 2016. View at: Publisher Site | Google Scholar
  54. R. L. Prior, X. Wu, and K. Schaich, “Standardized methods for the determination of antioxidant capacity and phenolics in foods and dietary supplements,” Journal of Agricultural and Food Chemistry, vol. 53, no. 10, pp. 4290–4302, 2005. View at: Publisher Site | Google Scholar
  55. S. B. Iloki-Assanga, L. M. Lewis-Luján, C. L. Lara-Espinoza et al., “Solvent effects on phytochemical constituent profiles and antioxidant activities, using four different extraction formulations for analysis of Bucida buceras L. and Phoradendron californicum Complementary and Alternative Medicine,” BMC Research Notes, vol. 8, pp. 396–409, 2015. View at: Publisher Site | Google Scholar
  56. I. F. F. Benzie and J. J. Strain, “The ferric reducing ability of plasma (FRAP) as a measure of “antioxidant power”: the FRAP assay,” Analytical Biochemistry, vol. 239, no. 1, pp. 70–76, 1996. View at: Publisher Site | Google Scholar
  57. Y. Liu, E. Neely, Z. Simmons, and J. R. Connor, “Adaptive endoplasmic reticulum stress alters cellular responses to the extracellular milieu,” Journal of Neuroscience Research, vol. 93, no. 5, pp. 766–776, 2015. View at: Publisher Site | Google Scholar
  58. Z. Baharum, A. Akim, Y. Taufiq-Yap, R. Hamid, and R. Kasran, “In vitro antioxidant and antiproliferative activities of methanolic plant part extracts of Theobroma cacao,” Molecules, vol. 19, no. 11, pp. 18317–18331, 2014. View at: Publisher Site | Google Scholar
  59. A. Ghasemzadeh, A. Nasiri, H. Jaafar, A. Baghdadi, and I. Ahmad, “Changes in phytochemical synthesis, chalcone synthase activity and pharmaceutical qualities of sabah snake grass (Clinacanthus nutans L.) in relation to plant age,” Molecules, vol. 19, no. 11, pp. 17632–17648, 2014. View at: Publisher Site | Google Scholar
  60. P. V. AshaRani, G. Low Kah Mun, M. P. Hande, and S. Valiyaveettil, “Cytotoxicity and genotoxicity of silver nanoparticles in human cells,” ACS Nano, vol. 3, no. 2, pp. 279–290, 2009. View at: Publisher Site | Google Scholar
  61. H.-U. Simon, A. Haj-Yehia, and F. Levi-Schaffer, “Role of reactive oxygen species (ROS) in apoptosis induction,” Apoptosis, vol. 5, no. 5, pp. 415–418, 2000. View at: Publisher Site | Google Scholar
  62. J. L. Martindale and N. J. Holbrook, “Cellular response to oxidative stress: signaling for suicide and survival,” Journal of Cellular Physiology, vol. 192, no. 1, pp. 1–15, 2002. View at: Publisher Site | Google Scholar
  63. M. J. Piao, K. A. Kang, I. K. Lee et al., “Silver nanoparticles induce oxidative cell damage in human liver cells through inhibition of reduced glutathione and induction of mitochondria-involved apoptosis,” Toxicology Letters, vol. 201, no. 1, pp. 92–100, 2011. View at: Publisher Site | Google Scholar
  64. S. Arora, J. Jain, J. M. Rajwade, and K. M. Paknikar, “Cellular responses induced by silver nanoparticles: In vitro studies,” Toxicology Letters, vol. 179, no. 2, pp. 93–100, 2008. View at: Publisher Site | Google Scholar

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