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1. Introduction
Over the recent decades, various diseases from minor infections to severe cancer have persisted in posing serious worldwide health issues that urgently need prompt addressing [1]. To date, cancer is one of the most widely spread and diagnosed diseases worldwide and has been reported to be the leading cause of death in our modern society [2]. Current conventional treatments using synthetic generic drugs, surgery, radiation therapy, hormone therapy, and chemotherapy have proven ineffective in treating cancer [3, 4]. Microbial infections, on the other hand, are also now posing major health problems, especially in developing countries. Available synthetic antibiotics that are used against these microbial infections usually lead to antibiotic resistance after repeated use, hence rendering the drugs inadequate [5]. Hence, this demands that a renewed effort be made to seek new materials/agents which are cheap and are highly efficient in treating these diseases. Recent research advancements have focused on the production of nanocomposites or metal nanoparticles made with natural biomolecules (e.g., polymers) as potential alternative anticancer and antimicrobial modalities [6].
Silver nanoparticles (AgNPs) are one of the most researched metal nanoparticles and have been the subject of interest due to their remarkable physicochemical properties, particularly their large surface area, tunable size, and stability [7]. Their application has been greatly demonstrated in a range of fields such as pharmaceuticals, medicine, and biotechnology [7–9]. These NPs are particularly well known for their antimicrobial activity, which is said to be attributed to the electrostatic interaction that occurs between the negatively charged cell membrane of microorganisms and the positively charged AgNPs [10, 11]. The accumulation of these NPs on the cell membrane is believed to alter the membrane causing it to lose permeability which leads to cell death [12]. However, due to toxic chemical agents used when preparing these NPs which affect their biocompatibility and pose environmental problems, biosynthesized AgNPs have been the subject of research recently. The biosynthesis of AgNPs involves a simple one-pot synthesis approach in which silver salts are reduced to fabricate AgNPs using nontoxic and natural polymers such as bacterial biomass, chitosan, and carbohydrates (e.g., starch) as both reducing and stabilizing agents [13,14].
For this experiment, colloidal AgNPs were prepared using porous cowpea starch. Cowpea (Vigna unguiculata L. Walp) is an annual plant legume that is cultivated and consumed mostly in South America, Asia, and Africa. Cowpea seed grains predominantly consist of bioactive compounds such as starch (35.0–52.0%), proteins (27%), and phenolic compounds (including phenol acids, flavonoids, and tannins) [15, 16]. These bioactive compounds are of great benefit to humans due to their anticarcinogenic effects and antioxidant and anti-inflammatory properties [17, 18]. Starch is the major dietary source of carbohydrates [19, 20]. It is a readily available biopolymer that possesses aldehyde terminals with hydroxyl groups capable of reducing silver nitrate (AgNO3) to silver metal while simultaneously stabilizing the resulting NPs [7]. These hydroxyl groups further enable good shape, size, and dispersion tunability which in turn enhance the biodegradability and biocompatibility of the NPs [21]. In 2018, starch was officially accepted by all major regulatory agencies for use in various oral drug delivery systems [22, 23]. Porous starch, in particular, has an important role in drug delivery since it processes all the properties that an ideal drug/gene delivery system should have which includes, inertness, biocompatibility, bioadhesiveness, high drug loading capacity, and amenability to synthetic modification, e.g., addition of biodegradable targeting ligands such as folic acid, for targeted delivery [22]. In cowpea grains, starch is the most abundant carbohydrate, and when extracted, it is extremely small and porous which is an advantage in drug/gene delivery system design applications.
Hence, this study aims at investigating the antibacterial and anticancer profiles of cowpea-porous-starch-mediated AgNPs for potential application as anticancer drug delivery modalities or antimicrobial agents.
2. Experimental
2.1. Materials
Human breast adenocarcinoma cells (MCF-7), human alveolar basal epithelial adenocarcinoma cells (A549), and human embryonic kidney cells (HEK293) were obtained from the Department of Biological Sciences at the University of KwaZulu Natal (Westville campus). Minimum Essential Medium (EMEM) containing Earle’s salts and L-glutamine, penicillin (500 units/ml)/streptomycin (5000 μg/ml), trypsin-versene, foetal bovine serum (FBS), benzolylated dialysis tubing (MWCO 12000 Da), and MTT were purchased from Sigma-Aldrich (St Louis, MO, USA). Mueller Hinton Broth (MHB) and Mueller Hinton Agar plates and microtiter plates were purchased from Bio-Rad Laboratories (Richmond, VA, USA). Microbank vials were purchased from Davies Diagnostic (SA). Bacterial cultures were obtained from Lancet Laboratories (SA). All other chemicals were of analytical grade and were supplied by Sigma-Aldrich (St Louis, MO, USA).
2.2. Methods
2.2.1. Starch Extraction
Starch extraction from the defatted flour was performed as described in [24] with slight modifications. Briefly, 100 g of cowpea starch was mixed with sodium borate buffer (12.5 mM, pH 10, 0.5% sodium dodecyl sulfate (SDS) (w/v) and 0.5% Na2S2O5 (w/v)) on a stirrer for 5 minutes, followed by 10 minutes’ centrifugation at 10,000×g to extract the proteins and recover the resultant residue. This was repeated 2X, and the resultant residue was washed 3X with distilled water and each time recovered by centrifugation. Thereafter, the residue was resuspended in distilled water and left overnight stirring to further extract the protein from the starch. Afterward, the starch slurry was filtered by passing through multilayers of cheesecloth and, thereafter, through a 250 μm sieve. This was then centrifuged at 10,000×g for 10 minutes, and thereafter, the brown layer formed on top of the starch layer was scraped with a spatula. Then, the starch was resuspended in water and centrifuged again, and this was repeated until all the brown particles were removed from the starch.
2.2.2. Preparation of Starch-Formulated/-Mediated AgNPs
AgNPs were prepared as previously described [25]. Briefly, 1.0 g of starch was mixed with 100 ml of deionized water and heated to 60°C on a hotplate with gentle stirring. Thereafter, 10 ml of starch solution was added with stirring to 50 ml of 1 mM AgNO3 solution, and the reaction process was carried out in dark for 3 hours until a clear brown colour was evident which indicated the formation of the AgNPs. Finally, the resultant AgNP solution was then dialyzed to remove excess unreacted by-products against 18 M Ohm water for 24 hours using a dialysis tube size of MWCO 12,000 Dalton. Different concentrations of AgNPs were prepared by adjusting the AgNO3 concentration.
2.2.3. Characterization of the Synthesized Nanoparticles
(1) UV Spectroscopy, TEM, SEM, ZetaPotential, and FTIR Spectroscopy. The formation of AgNPs was spectroscopically verified by using a UV-visible (vis) spectrophotometer (Cary 60 UV-Vis). The morphology and size of the AgNPs were determined using a JEOL JEM-1010 Transmission Electron Microscope with a Megaview III camera and iTEM UIP software (Tokyo, Japan) accessed from the University of Kwa-Zulu Natal (UKZN) (Westville Campus, South Africa). A FEI XL30 Scanning Electron Microscope accessed from the UKZN was used to evaluate the shape of the starch. The zeta potential was determined using a Zeta Sizer (Anton Paar, Particle analyser, Litesizer 500). The conjugation of the functional groups on starch and AgNPs was investigated using a Spectrum 100 FTIR spectrophotometer (PerkinElmer Co., Ltd., MA, USA) accessed from UKZN (Westville Campus, South Africa).
2.2.4. Bacterial Cultures and Maintenance
Four bacteria were used and divided into Gram-negative (Escherichia coli ATCC 25922 and Klebsiella pneumoniae ATCC 31488) and Gram-positive (Listeria monocytogenes and Staphylococcus aureus ATCC 25923) strains. Bacterial cultures were maintained as previously described [26]. Initially, all bacterial cultures were plated out, verified using the Gram-staining procedure, and stocked in microbank vials using 50% glycerol. Then, when needed, these were grown in MHB for 24 hours at 37°C, and the absorbance of bacterial cells was adjusted to the MacFarland Standard of 0.5 which corresponds to 108 CFU/ml and the density measured was at a wavelength of 600 nm [27, 28].
2.2.5. Antibacterial Activity of the Porous-Starch-Formulated/-Mediated AgNPs
Antibacterial activity of porous starch-mediated AgNPs was assessed against Gram-negative and Gram-positive bacterial strains by agar disk diffusion assay as previously described [29]. Initially, the required nutrient media for all bacterial strains were prepared from Mueller Hinton agar, and 100 μl inoculums of each tested bacterial culture were swabbed onto agar plates and incubated at 37°C for 30 minutes. Thereafter, different concentrations of AgNPs sample solutions (1, 5, and 10 Molar) were pipetted onto 5.5 mm sterile Whatman No. 1 filter paper disks and then placed on the surface of the bacteria-treated plates. After a 24 hours’ incubation period at 37°C, the diameter of the zone of inhibition was measured. Control disks with starch only (10 Molar) served as the negative control, whilst those with antibiotic ciprofloxacin (10 Molar) served as the positive control. All tests were carried out in triplicate.
2.2.6. Determination of MIC
Microtiter plates were used to evaluate the MIC values for AgNP sample solutions with bacteria activity. Briefly, on the microplates, serial dilutions ranging from 0.1 to 500 μg/ml of each concentration of AgNPs were performed. Then, inoculums of bacterial cultures (100 μl) were added to each well except the sterility controls, and then, the plates were incubated at 37°C for 24 hours. Following this, 50 μl of 2 μg/ml growth indicator p-iodonitrotetrazolium was added to each well and the incubation continued for 30 minutes. Starch was used as a negative control; MHB was used as a sterility control, and MHB + test bacteria served as the growth control. Growth was indicated by violet-coloured suspensions, while growth inhibition was indicated by colourless suspensions [29].
2.2.7. Cell Culture and Maintenance
Cells were grown at 37°C and 5% CO2, in 25 cm2 flasks with a sterile medium (EMEM) with (FBS 10% v/v, medium, streptomycin sulphate (100 μg/ml), and penicillin G (100 U/ml)). These were then subcultured when necessary [30].
2.2.8. Cytotoxicity Profile Study
To determine the cytotoxic activity of the AgNPs and the starch on selected cell lines, an MTT assay was used [2,30]. Briefly, cell lines HEK293 (human embryonic kidney), A549 (human alveolar basal epithelial adenocarcinoma), and MCF-7 (human breast adenocarcinoma) were trypsinised and seeded at densities of 1.62 × 106, 1.93 × 106, and 1.72 × 106 cells/well, respectively, in 96-well plates and incubated for 24 hours at 37°C. After incubation, old media were replaced with new media (0.3 ml), AgNPs and starch solutions prepared at different concentrations of 4, 7, 11, 15, and 19 Molar were added, and the cells were incubated for a further 48 hours at 37°C. Then, the old medium was replaced with fresh medium+10% MTT solution (5 mg/ml in PBS) and then incubated for 4 hours at 37°C. The medium + MTT solution was then removed, and cells were washed with PBS (2 × 0.3 ml) followed by treatment with DMSO (0.3 ml). Absorbance measurements were recorded at 570 nm. Cell viability was related to the control of untreated cells (100%). The average absorbance values were converted into percentage cell viability, using the following equation:
IC50 values were determined by nonlinear regression based on the percentage cell viability vs. concentration of samples (μg/ml) plots (Figure S1), and these values represented the sample concentration needed to kill 50% of the tested cells.
2.2.9. Apoptosis Studies
To further evaluate the cell viability profile of the synthesized NPs, an apoptosis study was conducted as previously described [31]. At the onset, the HEK293, A549, and MCF-7 cells with densities of 1.62 × 106, 1.93 × 106, and 1.72 × 106 cells/well, respectively, were seeded into 12-well plates and incubated for 24 hours at 37°C. After incubation, AgNP and starch solutions of 10 Molar were separately added into the cells and then incubated for a further 24 hours at 37°C. Thereafter, the old media were removed, and the cells were washed with PBS (100 μl) and then stained with 10 μl of acridine orange/ethidium bromide (AO/ETBR) dye (100 μg ml−1 acridine orange and 100 μg ml−1 ethidium bromide). Finally, a fluorescent microscope (OLYMPUS) at ×200 magnification was used to study the morphological changes in the cells. The apoptotic index was calculated as follows:
2.2.10. Statistical Analysis
Antibacterial activity, cytotoxicity, and apoptosis studies were performed in triplicate, and the results were expressed as mean ± standard deviation (S.D). Data were analysed by one-way ANOVA and Tukey’s multiple comparison test to compare between the groups. Statistically significant values are indicated by
3. Results and Discussion
3.1. Synthesis and Characterization
3.1.1. Synthesis and UV Spectroscopy Analysis
Metal nanoparticles are well known for their unique properties, particularly optical, as a result of surface plasmon resonance (SPR) [32]. Hence, the formation of the synthesized AgNPs was verified by observing colour change and UV-vis spectroscopy. The AgNPs prepared by mixing starch extracted from cowpea with AgNO3 solution were successfully synthesized. This was indicated by the colour change of the reaction mixture from a colourless solution to a brown solution (Figures 1(a) and 1(b)). The colour change can be attributed to the reduction of silver ions (Ag+) from silver nitrate into AgNPs by active biomolecules present in the starch extract [7]. The colour of AgNPs is due to the excitation of SPR arising due to the collective oscillation of free conduction electrons induced by an interacting electromagnetic field [33, 34]. Starch is said to peak between 200 nm and 250 nm [35]; hence, the peak at 230 nm showed its presence. Furthermore, the characteristic absorption band of AgNPs is known to range between 400 nm and 500 nm [36, 37]. The absorption observed at 423 nm (Figure 1(c)), thus, confirmed the successful preparation of AgNPs by the starch extract.
[figures omitted; refer to PDF]
3.1.2. FTIR Spectroscopy Analysis
To identify the major functional groups present on the starch extract surface and their participation in the coating and stabilization of the AgNPs, FTIR analysis was carried out (Figure 2). Even though the mechanism of the reduction of silver ions to AgNPs is not exactly understood but postulated, comparing the FTIR spectra of the starch extract and that of the synthesized AgNPs results may shed some light with regards to whether the formulation was successful or not. Figure 2 shows the spectra of cowpea starch extract (a) and AgNPs formed with cowpea starch extract (b). From this, it can be seen that the spectrum of the starch extract matches very well with that of the synthesized AgNPs with a slight shift in peak positions and a decrease in intensity. The starch extract in Figure 2(a) showed characteristic intensity peaks at 3272 cm−1 assigned to O-H of alcohols from phenols, 2333 cm−1 and 2114 cm−1 assigned to C=C-C alkyne groups, 1635 cm−1 assigned to the N-H amine group, and 1151 cm−1, 1079 cm−1, and 1019 cm−1 assigned to C-O-H and C-O carbonyl functional groups [38, 39]. The presence of these functional groups in Figure 2(b) as well, especially the O-H hydroxyl groups which are attributed to polyphenols and have previously been reported to present a deterministic part in the silver ions reduction to AgNPs, confirms the successful formulation and capping of AgNPs by the starch extract [40, 41]. Moreover, the decrease in peak intensity of these functional groups observed in Figure 2 is said to indicate the binding of the extract’s bimolecular components such as glycogen or cellulose polysaccharide polymers on the surface of the AgNPs [42]. It is postulated that these polysaccharide polymers act as surfactants and capping agents that bind to the NPs by either their cysteine residues or by their free amine groups providing colloidal stability and preventing aggregation [42, 43]. Additionally, previous studies have reported that biomolecules such as alkynes, alcohols, amines, and phenols all have a strong capacity to interact with metal salts to aid their reduction to NPs [44–46]. From these findings, it can be deduced that the AgNPs were successfully synthesized and stabilized using cowpea porous starch extract as corroborated by the previous literature.
[figures omitted; refer to PDF]
3.1.3. TEM, SEM, and Zeta Potential Analysis
Nanoparticle stability is usually determined by shape, particle size, and surface charge (zeta potential) [2]. TEM analysis was able to give a clear morphology and size of AgNPs, while the morphological property of cowpea starch extract was analysed using SEM. Biosynthesized AgNPs appeared spherical with a uniform distribution, ranging from 40–70 nm as depicted in Figures 3(a) and 3(b)), while cowpea porous starch extract appeared spherical, granular, and polygonal in shape as depicted in Figures 3(c) and 3(d). These findings correlate with a previous study reported in [47]. Previous studies have shown that the diameter of plasma membrane pores of most cells ranges from 50–75 nm in size, and thus, the synthesized AgNPs having this size range are significant because it means they would be able to extravasate through the cell membrane of the cancer cells via an endocytosis-mediated mechanism [48]. The synthesized AgNPs displayed good stability as indicated by a zeta (Ω) potential measurement of −23.9 ± 1.02 mV (Figure 3(e)). According to previous research, good stability is shown by Ω potential values that are greater than +25 mV or less than −25 mV [49, 50]. Thus, it can be concluded that these findings are in good agreement with the known literature.
[figures omitted; refer to PDF]
3.1.4. Antibacterial Activity Study
The antibacterial activity of the synthesized porous-starch-mediated AgNPs of different Molar (M) concentrations (1 M, 5 M, and 10 M) was investigated against Gram-negative bacteria (E. coli and K. pneumoniae) and Gram-positive bacteria (L. monocytogenes and S. aureus) using the disc diffusion method. Figure 4 shows that AgNPs exhibited good antimicrobial activity against both Gram-positive and Gram-negative bacteria. No antimicrobial activity was displayed by the starch; this was expected since starch has never been reported to have any antimicrobial activity [51]. The antimicrobial activity observed in both bacterial strains is said to be due to the released silver cations from AgNPs which behave as bactericidal agents. Even though the main antibacterial activity mechanism of the AgNPs is not yet known, researchers have postulated that the AgNPs bind onto the bacteria’s cell surface and interact with the phosphorous and sulphur moieties on the cell membrane leading to metabolism failure which ultimately causes bacterial lysis or apoptosis [52]. This postulation has led to the proposal of several possible AgNP’s antibacterial activity mechanisms. These include interference of key metabolic pathways, interference of transcription and translation of protein, and disruption of cell wall synthesis [53]. Hence, it is said that the bacterial growth inhibition not only affects structural constituents but also affects biochemical constituents as well involving enzyme deactivation, cell physiology impairment, and strong ionic charge interaction between silver ions and cell membrane components leading to a synergistic effect against the bacteria causing its death [53, 54].
[figures omitted; refer to PDF]
Figure 4 further shows that AgNPs exhibited higher antimicrobial activity against Gram-negative E. coli (18 ± 0.5 mm) over Gram-positive L. monocytogenes (6 ± 0.4 mm) after treatment with 10 M AgNP solution. The activity differences can be credited to the diverse properties of each bacterial strain which ultimately constitutes to its mechanism of inhibition [13, 55]. In particular, Gram-positive bacteria are said to have a thick cell wall composition that is hard to be penetrated easily, while Gram-negative bacteria, on the other hand, possess an easily penetrable thin cell wall [11, 56]. The findings are in good agreement with previous reports [11, 55, 57–60]. From Figure 4, it is also observed that both the 1 M and 5 M AgNP solutions did not exhibit any microbial activity in all bacteria except in E. coli, whereas the 10 M exhibited good zones of inhibitions in all bacterial strains tested. When the zones of inhibitions were compared with ciprofloxacin (standard antibiotic drug), it was established that the 10 M AgNP solution was as strong as the antibiotic drug against the Gram-negative bacterial strains, while the opposite was true with the Gram-positive bacterial strains. Overall, between the three AgNP concentrations tested, the 10 M showed to be very effective against a range of tested bacterial strains. Table 1 shows in detail the inhibition zones of the AgNPs as measured with a Vernier caliper, as well as the respective minimum inhibitory concentrations which ranged from 5 to 16 mg/l. The lower MIC indicated that the NPs were more potent; hence, a less amount is needed to achieve the desired effect [51, 61]. Previous reports investigating the antimicrobial activity of biosynthesized AgNPs have reported a similar MIC range [55, 62–65]; hence, these findings are in good agreement. In general, the findings suggested these AgNPs as good potential antibacterial agents.
Table 1
Antibacterial activity and MIC of porous-starch-mediated AgNPs against various bacteria.
| Bacterial strains | Zone of Inhibition (mm) | |||||
| AgNP concentrations | Controls | |||||
| [1 M] | [5 M] | [10 M] | MIC [mg/l] | Starch [10 M] | Ciprofloxacin [10 M] | |
| (1) E. coli | 6 ± 0.3 | 11 ± 0.5 | 18 ± 0.5 | 12 | 0 | 21 ± 0.0 |
| (2) K. pneumoniae | 0 | 0 | 16 ± 0.2 | 16 | 0 | 20 ± 0.2 |
| (3) L. monocytogenes | 0 | 0 | 6 ± 0.4 | 5 | 0 | 20 ± 0.2 |
| (4) S. aureus | 0 | 0 | 8 ± 0.6 | 8 | 0 | 22 ± 0.3 |
aAmount of AgNPs in 100 μl of deionized water (mg/l): 1 M = 5.35 mg/l; 5 M = 26.75 mg/l; and 10 M = 53.5 mg/l. bData are presented as mean ± SD (n = 3). cZero (0) denotes no activity. dM denotes Molar.
3.1.5. Cell Viability/Cytotoxicity Profile Studies
(1) MTT Assay. The successful application of NPs in cancer therapy applications, particularly in gene delivery, largely depends on their toxicity; therefore, the determination of NPs’ cytotoxic profile is vital. The MTT assay which is based on the reduction of the tetrazolium salt, MTT, by living cells to form a blue formazan product which is spectroscopically quantified [30, 66] and reported as a measure of cell viability was employed to assess the cytotoxicity profiles of the synthesized AgNPs (test) against one mammalian noncancer cell line (HEK293) and two cancer cell lines (MCF-7 and A549). The cytotoxicity of porous starch (control) and AgNO3 was also evaluated for comparative studies. The cytotoxicity investigations were carried out at various increasing concentrations of 4, 7, 11, 15, and 19 M on the selected cells. Figure 5(a) shows that the AgNPs elicited moderate cytotoxicity profiles of 40% and 50% against MCF-7 and A549 cancer cells and a very low cytotoxicity profile of 15% against HEK293 cells at the highest dose tested, revealing that their cytotoxicity was cell-specific [67]. This could be due to the highest uptake of these AgNPs by these cells since they have an abnormally high metabolism rate, which leads to their high proliferation which, as a result, makes them more susceptible [68]. It has also been suggested that the cytotoxicity can be credited to the volume-large surface area ratio of AgNPs which enables them to enter the cancer cells easily leading to them to interact with the constituents of the cells and, hence, interrupt many cellular signalling pathways [69]. This disturbance is said to cause an increased influx in the reactive oxygen species (ROS) that lead to oxidative stress [70, 71]. Figure 5(a) further shows that the cytotoxicity of the AgNPs increased as the concentration increased, indicating its dose dependency in both cancer cells. The findings are in good agreement with the previous literature, which accounts for the concentration-dependent cytotoxicity of NPs [55, 67, 72, 73]. Furthermore, similar comparative studies were also conducted using AgNO3 and starch extract only. Figure 5(b) shows that significantly (
[figures omitted; refer to PDF]
Overall, between the test AgNPs and their AgNO3 counterpart, the test AgNPs exhibited low cytotoxicity with IC50 of41.7, 56.3, and 63.8 μg/ml on HEK293, MCF-7, and A549, respectively. The lower IC50 values indicated that the AgNPs were more potent; hence, a less amount is needed to achieve the desired effect, and it is less likely for these to have side effects [77]. From these findings, it can be deduced that these AgNPs were well tolerated by all cells tested even at the highest concentration tested. Furthermore, it can also be postulated that the inclusion of starch into the nanoparticles greatly improved their overall cytotoxicity and biocompatibility, thus indicating these AgNPs as great anticancer potential therapeutics.
(2) Apoptosis Assay. Generally, after the cells have been treated with potential toxicants (e.g., NPs), apoptosis (“programmed cell death”) can occur as a response to this external entity. [78]. During apoptosis, the cells undergo morphological changes that can be observed microscopically such as nuclear fragmentation and shrinkage of the cytoplasm. To capture these changes, a combination of fluorescence microscopy and AO/ETB double staining was used [31]. Figure 6 shows that the test AgNPs induced some level of apoptosis as determined by low apoptosis indices (AI) (<1.5) as seen in Table 2, and the apoptosis or morphological changes were most noticeable in the cancer cells (MCF-7 and A549) which appeared to have lost their usual shape and appeared round and shrunk, as compared to the control (HEK 293) (untreated cells) which did not show any morphological changes [79].
[figure omitted; refer to PDF]Table 2
Apoptotic Indices of AgNPs, AgNO3, and starch in selected cell lines.
| Cell lines | Apoptotic Indices | |||
| Cells only | AgNPs | AgNO3 | Starch | |
| HEK293 | 0.0 | 0.00 | 0.01 | 0.00 |
| A549 | 0.0 | 0.10 | 0.19 | 0.02 |
| MCF-7 | 0.0 | 0.12 | 0.14 | 0.08 |
The apoptosis activity can be attributed to the prooxidant behaviour shown by AgNPs when inside cancer cells, due to the different redox and osmotic state of these cells [80]. It is believed that these AgNPs enter the cells via endocytosis and elicit their anticancer activity in a controlled release manner ultimately improving their bioavailability [81]. The difference between normal cells and cancer cells is said to contribute to reduced toxicity. It is postulated that the imbalance in the redox and osmotic state of cancer cells triggers the conversion AgNPs which further triggers the production of free radicals. This results in increased stress in the endoplasmic reticulum and disrupts the mitochondrial membrane which leads to mitochondrial proteins leakage which triggers apoptosis via caspase activation [82, 83]. These cellular disruptions then initiate damage to the DNA triggering cell cycle arrest which eventually leads to cell death. This is supported by the nonearly apoptotic cells which appeared light yellow and late apoptotic cells which appeared orange as seen in Figure 6. Hence, the data suggest that porous-starch-mediated AgNPs were able to alter the cell cycle in a dose-dependent manner which explains the observed link between cell death and cell growth inhibition.
4. Conclusions
This study investigated the antimicrobial and anticancer potential of porous-starch-mediated silver nanoparticles. These AgNPs were successfully synthesized using a porous starch extract from cowpea and were very stable. They all showed good antibacterial activity against four tested Gram-positive and Gram-negative bacterial strains. When tested on noncancer and cancerous cell lines, these AgNPs were well tolerated as indicated by a cell viability greater than 50% and low apoptotic indices (<0.2) at the highest dose tested.
Acknowledgments
The Durban University of Technology is acknowledged for the support.
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Abstract
Health issues involving inadequate treatment of diseases such as cancer and microbial infections continue to be the subject of much ongoing recent research. Biosynthesized silver nanoparticles (AgNPs) were characterized using Transmission Electron Microscopy (TEM), Zeta Sizer, Ultraviolet (UV), and Fourier Transform Infrared (FTIR) spectroscopy. Their antimicrobial activity was evaluated on selected Gram-positive and Gram-negative bacterial strains, using the disc diffusion and broth dilution assays. Cell viability profiles were evaluated using MTT (3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide) and apoptosis studies on selected human noncancer and cancer cells. The biosynthesized AgNPs were evaluated to be spherical clusters, with sizes between 40 and 70 nm. The absorption peak at 423 nm and the presence of polyphenols confirmed the synthesis and stabilization of these tested AgNPs. The AgNPs showed a good stability of −23.9 ± 1.02 mV. Good antimicrobial activity (6.0–18.0 mm) was seen on all tested bacteria at a minimum inhibitory concentration (MIC) ranging from 5 to 16 μg/ml, with the highest activity seen against Gram-negative Escherichia coli (18 ± 0.5 mm), and the lowest activity was seen against Gram-positive Listeria monocytogenes (6.0 ± 0.4 mm) after treatment with the AgNPs. These NPs showed a concentration-dependent and cell-specific cytotoxicity with low IC50 values (41.7, 56.3, and 63.8 μg/ml). The NPs were well tolerated by tested cells as indicated by a more than 50% cell viability at the high dose tested and low apoptotic indices (<0.2). These findings indicated that these biosynthesized AgNPs showed great potential as effective antibacterial agents and anticancer drug delivery modalities.
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Details
; Mellem, John 1
; Mbatha, Londiwe Simphiwe 1
1 Department of Biotechnology and Food Science, Faculty of Applied Sciences, Durban University of Technology, P.O Box 1334, Steve Biko Campus, Durban 4000, South Africa