Cytotoxicity and antibacterial activity of gold-supported cerium oxide nanoparticles
Received 26 June 2014
Accepted for publication 23 September 2014
Published 27 November 2014 Volume 2014:9(1) Pages 5515—5531
Checked for plagiarism Yes
Review by Single anonymous peer review
Peer reviewer comments 4
Editor who approved publication: Professor Lei Yang
K Suresh Babu,1,† M Anandkumar,1,† TY Tsai,2 TH Kao,2 B Stephen Inbaraj,2 BH Chen2,3
1Centre for Nano Sciences and Technology, Madanjeet School of Green Energy Technologies, Pondicherry University, Kalapet, India; 2Department of Food Science, 3Graduate Institute of Medicine, Fu Jen University, Taipei, Taiwan
†These authors contributed equally to this work
Background: Cerium oxide nanoparticles (CeO2) have been shown to be a novel therapeutic in many biomedical applications. Gold (Au) nanoparticles have also attracted widespread interest due to their chemical stability and unique optical properties. Thus, decorating Au on CeO2 nanoparticles would have potential for exploitation in the biomedical field.
Methods: In the present work, CeO2 nanoparticles synthesized by a chemical combustion method were supported with 3.5% Au (Au/CeO2) by a deposition-precipitation method. The as-synthesized Au, CeO2, and Au/CeO2 nanoparticles were evaluated for antibacterial activity and cytotoxicity in RAW 264.7 normal cells and A549 lung cancer cells.
Results: The as-synthesized nanoparticles were characterized by X-ray diffraction, scanning and transmission electron microscopy, and ultraviolet-visible measurements. The X-ray diffraction study confirmed the formation of cubic fluorite-structured CeO2 nanoparticles with a size of 10 nm. All synthesized nanoparticles were nontoxic towards RAW 264.7 cells at doses of 0–1,000 µM except for Au at >100 µM. For A549 cancer cells, Au/CeO2 had the highest inhibitory effect, followed by both Au and CeO2 which showed a similar effect at 500 and 1,000 µM. Initial binding of nanoparticles occurred through localized positively charged sites in A549 cells as shown by a shift in zeta potential from positive to negative after 24 hours of incubation. A dose-dependent elevation in reactive oxygen species indicated that the pro-oxidant activity of the nanoparticles was responsible for their cytotoxicity towards A549 cells. In addition, cellular uptake seen on transmission electron microscopic images indicated predominant localization of nanoparticles in the cytoplasmic matrix and mitochondrial damage due to oxidative stress. With regard to antibacterial activity, both types of nanoparticles had the strongest inhibitory effect on Bacillus subtilis in monoculture systems, followed by Salmonella enteritidis, Escherichia coli, and Staphylococcus aureus, while, in coculture tests with Lactobacillus plantarum, S. aureus was inhibited to a greater extent than the other bacteria.
Conclusion: Gold-supported CeO2 nanoparticles may be a potential nanomaterial for in vivo application owing to their biocompatible and antibacterial properties.
Keywords: cerium oxide nanoparticles, gold supported cerium oxide, cytotoxicity, antibacterial activity, cellular uptake, reactive oxygen species
Cerium oxide (CeO2) nanoparticles (NPs) have been studied recently for their antimicrobial activity,1,2 due to the redox nature of CeO2 whereby the oxidation state switches between Ce3+ and Ce4+ depending on the external environment. This redox nature of CeO2 NPs aids in inhibiting bacterial growth and scavenging free radicals.3 The antibacterial activity of CeO2 NPs not only depends on nanoparticle size but also on the medium in which they are dispersed, as well as other factors such as pH and salt concentration.1 When NPs are tested in vivo, it is necessary to evaluate their cytotoxicity effect because free radicals can affect both normal and abnormal cells.4 Accordingly, the cytotoxicity also refers to death of healthy cells, mainly caused by production of reactive oxygen species (ROS).4 However, CeO2 NPs, being natural ROS scavengers, can generate ROS in certain specific environments and damage cancer cells. Auffan et al5 reported a toxicity of 7 nm CeO2 NPs that involved damage to DNA in human fibroblasts, mainly due to oxidative stress caused by the interaction between redox CeO2 NPs and other organic molecules. The cytotoxicity of CeO2 NPs was also reported by Li et al6 who demonstrated a protective effect on bacteria during initial exposure to CeO2 NPs because of the scavenging effect of free radicals, yet prolonged exposure could result in generation of ROS leading to toxicity. This phenomenon can eventually extend to growth of normal cells or inhibition of cancer cells.
Metal NPs, like gold (Au) NPs, have several potential applications in the biomedical field, including antibacterial activity.7–9 Au NPs combined with antibiotics have been reported to show improved antibacterial activity compared with antibiotics alone.7 Use of Au NPs as an antibacterial agent is mainly due to their unique biocompatibility, which depends on their size, shape, and concentration, as well as the nature of their surface functionalization.5,10–12 Chen et al10 illustrated the size-dependent toxic effect of Au NPs in mice, with a size of 8–37 nm being more toxic and a size in the range of 3–100 nm being less toxic. Thus, combining the antibacterial activities of Au NPs and CeO2 NPs would be a novel approach for developing a nanomaterial with strong antibacterial activity. Although many researchers have employed a combination of Au and CeO2 in catalytic applications, few reports are available concerning the biomedical applications of such a combination. A previous study by Menchón et al13 demonstrated that Au-coated CeO2 NPs (Au/CeO2 NPs) had better ROS scavenging activity, biocompatibility, and peroxidase activity than CeO2 NPs. However, the antibacterial activity of Au/CeO2 NPs remains unexplored.
Several authors have demonstrated Lactobacillus plantarum to have good antibacterial activity owing to its intrinsic ability to produce several antimicrobial substances, such as organic acids, hydrogen peroxide, bacteriocins, or related compounds.14–16 Of these metabolites, bacteriocins are of particular interest because there have been several reports demonstrating their antimicrobial efficiency across a broad spectrum of microbes.17–19 Although many bacteria can produce bacteriocins, L. plantarum is chosen in this study due to its Generally Regarded As Safe status. Bacteriocins are proteinaceous antimicrobial compounds produced extracellularly during the stationary phase of bacterial culture.15,17 Bacteriocins produced by Lactobacillus species are known as “plantaricins”, and their stability varies depending on the specific physicochemical environment and Lactobacillus species used.14,19–21 In view of this, we intended to coculture each test bacteria with L. plantarum to evaluate the possible synergistic antibacterial effect by L. plantarum and as-synthesized CeO2 NPs or Au/CeO2 NPs. Presently, there are no reports available on determining the antibacterial efficacy of Au/CeO2 NPs in a coculture where the culture has more than one bacterial species. The present work focuses on the cytotoxic effects of Au NPs, CeO2 NPs, and Au/CeO2 NPs in normal cells and in lung cancer cells, as well as their antibacterial activity against Gram-positive and Gram-negative bacteria in both monoculture and coculture systems. In addition, the underlying mechanism of cytotoxicity and antibacterial activity is elucidated.
Materials and methods
Cerium nitrate hexahydrate (Ce(NO3)3⋅6H2O, 99.9%, Sigma-Aldrich, St Louis, MO, USA), glycine (NH2⋅CH2COOH, Fisher Scientific, Mumbai, India), chloroauric acid (HAuCl4, Loba Chemie, Mumbai, India), and sodium borohydride (NaBH4, Sigma-Aldrich) were used for synthesis of both CeO2 and Au-impregnated CeO2 nanoparticles.
RAW 264.7 macrophage cells and A549 human lung adenocarcinoma epithelial cells were obtained from the Taiwan Food Industry Development Research Institute (Hsinchu, Taiwan) and their corresponding cell culture media, Dulbecco’s Modified Eagle Medium (DMEM) and Roswell Park Memorial Institute (RPMI)-1640 medium, respectively, were supplied by HyClone (Logan, UT, USA). Hank’s Balanced Salt Solution and fetal bovine serum were also sourced from HyClone, while 2.5% trypsin-ethylenediamine tetraacetic acid and penicillin-streptomycin were from Invitrogen (Carlsbad, CA, USA). Dimethyl sulfoxide and chemical reagents such as sodium bicarbonate and 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) were supplied by Sigma-Aldrich. Ethanol (95%) was obtained from the Taiwan Tobacco and Wine Bureau (Tainan, Taiwan). A fluorescence dye, ie, 5-(and 6-)-chloromethyl-2,7-dichlorodihydro fluorescein diacetate, from Molecular Probes (Eugene, OR, USA) was used for measuring intracellular ROS formation by a microplate spectrofluorometer (SpectraMax®, Molecular Devices, CA, USA). The Versa Max enzyme-linked immunosorbent assay (ELISA) reader was from Molecular Devices, the carbon dioxide incubator (SCA-165DS) was from Astec (Fukuoka, Japan), the inverted microscope (TS100) was from Nikon (Tokyo, Japan), and the 4BC-24 model laminar flow hood was from Jau-Hsin Co (Taipei, Taiwan).
Of the four pathogens chosen for antibacterial study, two Gram-negative bacterial strains, Escherichia coli O157:H7 (TWC 01) and Salmonella enteritidis SE 01, were obtained from clinical patients in Taiwan, and two Gram-positive bacterial strains, Bacillus subtilis (ATCC 27689) and Staphylococcus aureus (ATCC 10832) were obtained from the American Type Culture Collection (Manassas, VA, USA). L. plantarum TW10, a probiotic bacterium cocultured with each test bacteria for assessing a possible synergistic antibacterial effect with synthesized NPs, was isolated from Taiwanese pickled cabbage. Microbiological media, ie, tryptic soy broth and Lactobacilli MRS (Man-Rogosa-Sharpe) broth were sourced from Difco (Detroit, MI, USA). Commercial antibiotics (ampicillin and vancomycin) were purchased from Sigma-Aldrich. A Shel Lab incubator (model 1535, Sheldon Manufacturing Inc, Cornelius, OR, USA) was used to incubate the NPs with bacterial cells. The bacterial concentration was measured as a function of optical density at 600 nm using an ELISA reader from Thermo Fisher Scientific (Waltham, MA, USA). The optical density was calibrated using McFarland turbidity standard number 0.5 obtained from bioMérieux Clinical Diagnostics (March L′ Étoile, France).
Synthesis of CeO2 NPs
CeO2 NPs were synthesized by a combustion method with glycine as an oxidizer based on simple propellant chemistry. The stoichiometric amounts of cerium nitrate and glycine as shown below (Eq. 1) were dissolved in double-distilled water and mixed until a transparent solution was obtained. The mixture was kept over a hot plate for combustion and the resulting NPs were then centrifuged at 5,000 rpm for 30 minutes, followed by washing with double-distilled water three times to remove any unreacted nitrate and glycine, and drying in an oven overnight to obtain a pale yellow-colored product.
Synthesis of Au NPs
Au NPs were synthesized by the reduction of Au salt with sodium borohydride. NaBH4 solution was added dropwise to 0.5 g of HAuCl4 in water to maintain a molar ratio of HAuCl4:NaBH4 at 1:0.43 with stirring for 4 hours. The resulting suspension was then centrifuged at 7,000 rpm for 30 minutes, washed three times with double-distilled water, and dried in an oven at 100°C for 12 hours to obtain Au NPs.
Synthesis of Au-impregnated CeO2 NPs
Au NPs were impregnated onto the surface of CeO2 NPs using a deposition-precipitation method. First, 0.06 g of HAuCl4 was added to 1 g of CeO2 NPs in water and the solution was stirred and heated at 100°C until a dry powder was formed. The powder obtained was then redispersed in distilled water and NaBH4 solution (molar ratio of HAuCl4:NaBH4 at 1:0.43) was added dropwise to obtain a purple-colored precipitate, which was centrifuged, washed three times with double-distilled water, and dried in a hot air oven overnight to obtain CeO2 NPs coated with 3.5% Au.
Characterization of NPs
X-ray diffraction studies were performed in a diffractometer (Ultima IV, Rigaku Corporation, The Woodlands, TX, USA) using Cu Kα radiation with a scanning rate of 2° per minute and a step size of 0.02° for CeO2, Au/CeO2, and Au NPs in the 2θ range of 25°–40°. Particle size was determined by the Scherrer’s equation (Eq. 2) assuming a Gaussian shape for the peaks.
where d is the mean crystallite size (nm), k is Scherrer’s constant (0.9), β is the full width half maximum, and θ is the diffraction angle.
Structural analysis was carried out using scanning electron microscopy (SEM; model S-3400N, Hitachi, Tokyo, Japan). Electron microscopic images were recorded after coating the sample with carbon. Energy dispersive X-ray analysis was carried out for identification as well as quantification of Au on the surface of the CeO2 NPs. Both particle size and the surface morphology of the samples obtained were imaged by transmission electron microscopy (model JEM 2100F, JEOL Ltd, Tokyo, Japan). The samples were prepared by dropping a diluted solution of each nanoparticle type on a 150-mesh copper TEM grid (Ted Pella Inc, Redding, CA, USA) and vacuum-drying for one hour. Optical studies of the NPs obtained were carried out using an ultraviolet-visible spectrophotometer (model Lambda 650S, Perkin Elmer, Boston, MA, USA) in the scan range of 300–700 nm, with data collection at a resolution of 1 nm. Surface charge measurements for CeO2 NPs and Au/CeO2 NPs were carried out using a nanoparticle analyzer (model SZ-100, Horiba, Kyoto, Japan). The study samples were prepared by dispersing the NPs in double-distilled water at a concentration of 1 mg/mL and monitoring at regular intervals over a period of 48 hours.
Normal RAW 264.7 macrophage cells were cultured in DMEM containing 10% fetal bovine serum, 100 U/mL penicillin, and 100 μg/mL streptomycin, while the A549 human lung cancer cells were cultured in RPMI-1640 medium containing 5% fetal bovine serum, 100 U/mL penicillin, and 100 μg/mL streptomycin. The cultured cells were then incubated at 37°C under 90% humidity and 5% CO2 for 2–3 days. When cell density had reached 80% confluence, the cells were washed twice with phosphate-buffered saline (pH 7.4), and 1 mL of 0.05% trypsin-ethylenediaminetetraacetic acid was added, followed by shaking for a few minutes. The cells were then viewed under the microscope. Next, fresh medium was added to neutralize and harvest the cells, followed by centrifugation at 1,000 rpm for 5 minutes. Fresh medium was then added again to the supernatant for cell suspension, mixed with 10 mL of culture medium, and 0.2 mL of cell suspension was collected for MTT assay.
The cytotoxicity of Au NPs, CeO2 NPs, and Au/CeO2 NPs was determined by seeding 0.2 mL of cell suspension in a 96-well plate with each well containing 1.5×104 RAW 264.7 cells or 4,000 A549 cells. After incubation for 24 or 48 hours to enable attachment of cells to the bottom, the medium in the wells was replaced with fresh medium containing nine different concentrations of each type of nanoparticle (0.001, 0.01, 0.1, 1.0, 10, 50, 100, 500, and 1,000 μM) and incubated for 24 or 48 hours. The medium was then removed and 180 μL of reagent mixture containing MTT (5 mg/mL in phosphate-buffered saline) and Hank’s Balanced Salt Solution at a ratio of 1:9 (v/v) was added to each well. The well plate was then incubated for another 4 hours at 37°C and 5% CO2 to allow exponential cell growth. Upon incubating with the MTT reagent mixture, the tetrazolium ring in MTT was cleaved by mitochondrial dehydrogenase in metabolically active cells and eventually the pale yellow water-soluble tetrazolium salt was changed into a purple water-insoluble formazan derivative. The MTT solution was then removed and total mitochondrial activity was determined by dissolving the formazan crystals in 150 μL of dimethyl sulfoxide followed by shaking for 15 minutes and measuring the absorbance at 570 nm using an ELISA reader. Prior to measurement of absorbance, the plate reader was calibrated to zero using culture medium without cells. The relative cell viability in a percentage compared with the control wells was calculated using the formula: [ABS]NP/[ABS]CTL ×100, where [ABS]CTL and [ABS]NP denote absorbance measured in wells without and with NPs, respectively. To reduce artifacts arising from background MTT absorbance, the percentage cell viability data were obtained by subtracting the background absorbance at 690 nm from the test absorbance measurement at 570 nm.
Intracellular ROS production and uptake of NPs by cells
The formation of intracellular ROS was determined by measuring the oxidative transformation of the nonfluorescent reagent, CM-H2DCFDA, to a highly fluorescent compound, ie, dichlorofluorescein. Initially, cells were seeded in a 96-well plate at a density of 2×103 cells per well in 100 μL of medium. After 24 hours of incubation at 37°C and 5% CO2, the cells were treated separately with various concentrations (0.001, 0.01, 0.1, 1, 10, 50, 100, 500, and 1,000 μg/mL) of CeO2 NPs and Au/CeO2 NPs for 24 or 48 hours, washed three times with phosphate-buffered saline, and incubated with 10 μM CM-H2DCFDA for one hour at 37°C. The cells were then washed, and dichlorofluorescein was measured immediately using a microplate spectrofluorometer at an excitation and emission wavelength of 490 nm and 545 nm, respectively, with cells not exposed to NPs used as the control.
For the cellular uptake study, A549 human lung cancer cells were incubated with CeO2 NPs or Au/CeO2 NPs for 48 hours. After incubation, a portion of the cells was collected in a tube, centrifuged at 1,000 rpm for 10 minutes, and washed twice with phosphate-buffered saline. Next, 1.5 mL of 4% paraformaldehyde and 2.5% glutaraldehyde was added to fix the cells, followed by post-fixing with 1% osmium tetroxide, washing three times with phosphate-buffered saline, and sequentially washing with 30%, 50%, 70%, 90%, and 100% alcohol as well as 100% acetone for dehydration. The cell pellet was further treated with different ratios (3:1, 1:1, 1:3, 0:1) of 100% acetone/Spurr’s resin for 2 hours each and polymerized in an oven for cutting of an ultrathin section, which was then mounted on a carbon-coated grid for recording of TEM images.
The antibacterial activity of freshly prepared Au NPs, CeO2 NPs, and Au/CeO2 NPs along with commercial antibiotics, ie, ampicillin and vancomycin, was evaluated against four selected pathogens, ie, E. coli O157:H7 (TWC 01), S. enteritidis SE 01, B. subtilis (ATCC 27689), and S. aureus (ATCC 10832) by microbroth dilution tests. After an initial 20-minute thawing of frozen bacterial strains in ice, the test bacteria was subcultured aerobically in 5 mL of tryptic soy broth overnight, followed by centrifugation at 5,000 g for 10 minutes and suspension of the pellet in 10 mL of phosphate-buffered saline (pH 7.2). The optical density of each bacterial suspension was then adjusted to obtain 108 colony forming units (CFU)/mL by using McFarland turbidity standard number 0.5. From the stock solution of each nanoparticle type, nine different concentrations of 6, 12, 23, 47, 93, 186, 372, 744, and 1,488 μM were prepared in bacterial suspension at 108 CFU/mL. Likewise, the same concentrations were prepared separately for the commercial antibiotics, ampicillin and vancomycin. Subsequently, 200 μL of each concentration was put into a polystyrene tray containing 96 wells so that each well contained a bacterial concentration of 2×107 CFU/mL. The bacterial inoculum containing NPs was then incubated at 37°C for 16 hours. After incubation, the optical density of each well was determined at 600 nm using an ELISA reader. Optical density-concentration curves were obtained for relative comparison of bacterial inhibition as a function of NP/antibiotic concentration. For antibacterial activity in the test bacteria cocultured with L. plantarum TW10, a 50:50 (v/v) ratio of L. plantarum to each test bacteria was prepared after subculturing in Lactobacilli MRS broth and tryptic soy broth, respectively. The bacterial concentration was then adjusted to 108 CFU/mL, and the remaining procedure was the same as described above.
Precautions against endotoxin contamination
Care was taken to exclude the potential influence of endotoxin on the observed outcomes of the cytotoxicity and antibacterial experiments. Given that water is the most common source of endotoxin contamination in the laboratory, ultrapure water from a Millipore filtration system was used for all antibacterial experiments. Further, before use, all glasswares were washed thoroughly with warm water after soaking overnight in a 1% solution of alkaline detergent and autoclaving. We also used nitrile gloves and carried out all experiments in a laminar flow hood to avoid any potential influence of endotoxin on the observed cytotoxicity and antibacterial activity.
Results and discussion
Figure 1 shows the X-ray diffraction patterns for the Au NPs, CeO2 NPs, and Au/CeO2 NPs. The spectra obtained matched the International Centre for Diffraction Data card number, ie, 01-073-6318 and 03-065-2870 for the cubic fluorite structure of CeO2 NPs and the cubic structure of Au NPs, respectively. A broader peak corresponded to formation of NPs, and the average crystallite size of the CeO2 NPs was found to be 9.3 nm from the Scherrer’s formula. However, for Au/CeO2 NPs, a weak and low intensity peak appeared, which corresponded to a (111) reflection plane (Figure 1). Consequently, the particle size for the Au in the Au/CeO2 NPs could not be obtained by calculation.22 In addition, the difficulty in identification and quantitative measurement of size was due to formation of fine and highly dispersed Au NPs on CeO2 surface during Au deposition carried out by impregnation method.
Figure 1 X-ray diffraction pattern for the as-prepared nanoparticles.
Scanning electron microscopy
The SEM images for CeO2 NPs and Au/CeO2 NPs in Figure 2A and B depict a sponge-like porous network structure for the CeO2 particles. The sponge-like structure observed on the SEM images is mainly due to the large volume of gas released during the combustion process involved in the synthesis of CeO2 NPs. Fundamentally, a typical combustion process involves a reaction between fuel and an oxidizer, resulting in generation of gas (as shown in Eq. 1), which eventually escapes to the nanoparticle surface, creating a network structure with high porosity. Upon impregnation, a fine dispersion of Au along with a few Au agglomerates occurred, as shown by bright white spots in Figure 2B. In addition, the presence of well dispersed Au NPs identified on SEM images was consistent with the X-ray diffraction results. Figure 2C and D shows the energy dispersive X-ray spectra for the CeO2-NPs and Au/CeO2 NPs, respectively. The presence of Au peaks in Figure 2D confirmed incorporation of Au in the Au/CeO2 NPs. The energy dispersive X-ray spectra also revealed deposition of a 3.26 weight percentage of Au on the CeO2 surface, and the observed drop in percentage Au loading compared with actual loading may reflect leaching of weakly bound Au NPs from the surface of the CeO2 NPs during the several washing steps involved in their synthesis.
Figure 2 Scanning electron microscopic images of CeO2 NPs (A) and Au/CeO2 NPs (B) along with their corresponding energy dispersive X-ray spectra (C, D).
Transmission electron microscopy
The TEM images for CeO2, Au/CeO2, and Au NPs are shown in Figure 3A–C. A network-based structure was observed for CeO2 which can be attributed to the typical nature of the synthesis process. This network structure was mainly due to the large volume of gas released during formation of the NPs by a combustion process, as shown in the SEM images described above. Upon impregnation, Au NPs were deposited on the surface of the CeO2 NPs, which showed a nearly spherical shape and the average particle size of the CeO2 NPs was found to be 9.7 nm. In spite of its wider size distribution, the average Au size was calculated to be less than 5 nm. When Au was prepared in the absence of CeO2 NPs, the observed Au NP size was found to be higher (>15 nm), indicating the significant role of the CeO2 NP surface as a support for Au NPs.
Figure 3D shows the ultraviolet-visible spectra for CeO2 and Au/CeO2 NPs, with an inset depicting an enlarged view of the Au peak for Au NPs. As CeO2 absorbs strongly in the ultraviolet region, broad absorption of Au/CeO2 starting from 430 nm was observed, which was mainly due to the charge transfer transition between the O 2p and Ce 4f bands.23 Cerium in CeO2 NPs exists in two oxidation states, namely +3 and +4, exhibiting a characteristic absorption band at 253 nm and 270–340 nm, respectively.24 Pure Au NPs showed a localized surface plasmon resonance (LSPR) band around 522 nm. However, upon coating of Au NPs on the surface of CeO2 NPs, a new absorption band appeared at 567 nm, which corresponded to the LSPR of the Au NPs.25 Obviously, the bare CeO2 NPs did not show any LSPR and thus formation of the new band in Au/CeO2 NPs should be due to the LSPR of the Au NPs. Moreover, the LSPR band for Au NPs (522 nm) and Au/CeO2 NPs (567 nm) appeared at different wavelengths due to variation in the refractive indices between CeO2 (2.2) and Au (0.47) NPs, which is consistent with the observation made by Zhu et al.26 Although a sharp surface plasmon peak is expected for Au NPs, a broader absorption peak appeared, owing to the absence of capping agent.
Cytotoxicity of Au, CeO2, and Au/CeO2 NPs
To investigate the therapeutic application of the synthesized NPs, the cytotoxicity of Au, CeO2, and Au/CeO2 NPs was evaluated by performing cell viability tests against normal RAW 264.7 macrophage cells and A549 human adenocarcinoma epithelial cells by MTT assay. In this study, a human lung cancer cell line was chosen because lung cancer is the leading cause of cancer deaths in Taiwan, while RAW 264.7 macrophages are widely used as a classic positive control representing normal cells and as a model cell line to represent osteoclasts. After incubating the NP-spiked cell culture for 24 or 48 hours, percentage cell viability was determined by measuring the cell survival rate relative to that of the control. Treatment of RAW 264.7 cells with CeO2 NPs for 24 and 48 hours and with Au/CeO2 NPs for 24 hours did not show any significant toxicity at any of the doses studied (0.001–1,000 μM, Figure 4). However, after 48 hours of treatment with Au/CeO2 NPs, a 13%–17% decrease in cell viability was observed at higher doses (50–1,000 μM), but no significant decline at a dose ≤10 μM. On the other hand, Au NPs at doses of 500 and 1,000 μM showed relatively greater toxicity towards RAW 264.7 cells, with the cell viability decreasing by 28.2% and 30.2%, respectively, after 24 hours of treatment, and by 37.8% and 40.3% after 48 hours of treatment, respectively (Figure 4). For A549 lung cancer cells, no significant toxicity occurred at Au NP and CeO2 NP doses ≤100 μM, or for Au/CeO2 NP doses ≤50 μM after 24 hours of treatment. However, by increasing the NP dose to 500 or 1,000 μM, the cell viability decreased to 86.6% and 76.9% for Au NPs, to 90.6% and 85.4% for CeO2 NPs, and to 81.1% and 70.6% for Au/CeO2 NPs, respectively (Figure 5). In addition, Au/CeO2 NPs resulted in a 12% decrease in cell viability even at a dose of 100 μM over a 24-hour incubation period. After prolonged incubation for 48 hours, the cytotoxicity towards A549 cells increased substantially for all the NPs, with Au/CeO2 NPs showing the strongest inhibitory effect, ie, 31.4%, 41.9%, and 51.0% for 100, 500, and 1,000 μM, respectively. Interestingly, both Au NPs and CeO2 NPs showed a similar inhibition at 500 μM (27.8% and 28.3%) and 1,000 μM (42.0% and 40.0%, Figure 5). The IC50 value was not determined because the inhibitory effect did not exceed 50% for any of the three types of NPs in the dose range tested (0.001–1,000 μM), with the exception of Au/CeO2 NPs at 1,000 μM.
Owing to their unique electronic properties, CeO2 NPs have an inherent tendency to exist in mixed valence states (Ce3+ and Ce4+) and switch between two different oxidation states via an oxidation-reduction cycle, thereby conferring antioxidant activity to these NPs.5,27 These dual oxidation states are mainly due to existing oxygen vacancies or defects created by the loss of oxygen and eventual reduction of Ce4+ to Ce3+. In the presence of ROS, Ce3+ undergoes oxidation initially and an autoregenerative mechanism reverts the oxidation state from Ce4+ back to Ce3+, thereby perpetuating the free radical scavenging activity.5,27 Moreover, it has been shown that CeO2 NPs are capable of mimicking superoxide dismutase activity with a catalytic rate constant exceeding that of a biological enzyme.28 These inherent material properties confer CeO2 NPs with well demonstrated cytoprotective ability in various normal mammalian or human cells. In several reports, CeO2 NPs have been shown to be nontoxic to murine insulinoma βTC-tet cells,29 human umbilical vein endothelial cells and human lung fibroblasts,30 RAW 264.7 macrophage cells,27 human breast epithelial cells,31 murine macrophages,32 and human colon cells.33 In contrast, several studies have demonstrated a cytotoxic effect of CeO2 NPs in normal cells, including human dermal fibroblasts5 and human peripheral blood monocytes,34 which was attributed to oxidative stress in the former and mitochondrial damage along with overexpression of apoptosis-inducing factor in the latter. In our study, Au/CeO2 NPs showed minimal toxicity (~15%–17%) towards normal RAW 264.7 macrophage cells (Figure 4), and thus CeO2 NPs and Au/CeO2 NPs can be deemed nontoxic because materials with cell viability >80% are usually considered cytocompatible.35 Based on the above discussion, both CeO2 NPs and Au/CeO2 NPs appear to protect RAW 264.7 cells by scavenging ROS and reducing oxidative stress after becoming localized inside the cells. In a toxicity study comparing three metal oxide NPs (CeO2, TiO2, and ZnO), Xia et al27 observed internalization of CeO2 NPs through LAMP-1-positive endosomal compartments in RAW 264.7 cells, suppression of ROS, and induction of cellular resistance to exogenous sources of oxidative stress. Hirst et al32 also demonstrated the protective effects of CeO2 NPs in J774A.1 murine macrophages in vitro and mouse tissue in vivo. Nevertheless, the toxicity of Au NPs can be dose-dependent, ie, Au NPs can be toxic at 500 and 1,000 μM, but possess no apparent toxicity at ≤100 μM (Figure 4). A similar outcome was demonstrated by Shukla et al,36 reporting >90% viability for RAW 264.7 cells after 48 hours of treatment with Au NPs at ≤100 μM, while no noticeable increase in proinflammatory cytokines such as tumor necrosis factor-α and interleukin-1β. Further, phagocytes such as macrophages and monocytes can react more strongly with microparticles than with NPs.37 For instance, Morishige et al38 did not observe any cytotoxicity towards THP-1 cells in the presence of 30–70 nm silica NPs, but 1,000 nm particles did have a cytotoxic effect. Thus, it may be postulated that the cytotoxicity of Au NPs at 500 and 1,000 μM may be attributable to the tendency of phagocytes like RAW 264.7 cells to agglomerate, resulting in higher cytotoxicity towards phagocytic RAW 264.7 cells.
Conversely, all the three types of as-synthesized NPs showed substantial cytotoxicity towards A549 lung cancer cells, with Au/CeO2 NPs having a greater inhibitory effect than Au NPs or CeO2 NPs for both the 24-hour and 48-hour treatments (Figure 5). While several studies have demonstrated their antioxidant behavior in normal cells, CeO2 NPs could also have cytotoxic effects in several types of cancer cells.39,40 For example, Tarnuzzer et al31 have shown CeO2 NPs to have a radioprotective effect in normal human CRL8798 breast cells but not in human MCF-7 breast cancer cells. Likewise, using CeO2 NPs codoped with yttrium and erbium, Babu et al30 noticed a cytoprotective effect in normal cells, such as human umbilical vein endothelial cells and human lung fibroblast cells (WI-38), but the viability of CRL-5803 lung cancer cells was decreased by 34% even at a dose of 100 nM.
Prior to internalization and localization in cellular organelles, binding of NPs onto the cell membrane is the determining factor for their cellular uptake, which can be dependent upon the surface charge of both NPs and the cell surface.41 After binding of NPs to the cell membrane, uptake occurs via several mechanisms, such as pinocytosis or receptor-mediated endocytosis or phagocytosis.39,41 As shown in Figure 6, the positive zeta potentials of CeO2 NPs and Au/CeO2 NPs in freshly prepared solution (+41.5 mV and +55.6 mV, respectively) was shifted to negative in 24 hours (−24.2 mV and −8.5 mV) and further to −38.2 mV and −29.6 mV in 48 hours. Such switching of surface charge has been reported previously by Vincent et al42 who showed a shift in zeta potential from positive to negative following an increase in incubation time (over 4 days) and temperature (over 65°C). However, in our study, this charge shift was evident after 24 hours of incubation during the cytotoxicity test. Likewise, a negative mean zeta potential of −10.2 mV was reported for A549 cancer cells by Patil et al41 implying that only a few cationic sites are available for binding to negatively charged NPs. Obviously, negatively charged A549 cells should repel NPs of similar charge. Nonetheless, it is also possible that the negatively charged NPs may bind in clusters at cationic sites on A549 cells because of the repulsive force from a large pool of negatively charged sites on the cell surface, as pointed out by Patil et al.41 Asati et al43 also demonstrated efficient uptake of negatively charged polyacrylic acid-coated CeO2 NPs, with internalization into lysosomes and eventual cytotoxicity towards A549 cells. Accordingly, the negatively charged NPs may be clustered onto less populated and positively charged sites on the surface of the A549 cell via electrostatic interaction, which in turn may lead to localized neutralization of charge and subsequent cellular uptake by endocytosis.
Figure 6 Zeta potential of prepared CeO2 and Au/CeO2 solutions monitored at regular intervals for 48 hours.
The selective toxicity towards cancer cells may be explained on the basis of the unique pH-dependent antioxidant behavior of CeO2 NPs as proposed by Perez et al44 who found that their optimal antioxidant properties occurred at physiological pH, whereas their oxidase (pro-oxidant) activity occurred at acidic pH. In a later study, Asati et al43 postulated that internalization and localization of negatively charged CeO2 NPs in the lysosomes (an acidic environment) of A549 cells should switch off their antioxidant activity and turn on their oxidase activity. This phenomenon, known as the “Warburg effect”, occurs as a result of enhanced glycolysis and lactate production via activation of hypoxia inducible factor-1α caused by the elevated levels of ROS in tumor cells.35 Thus, in our study, the cytotoxicity of CeO2 NPs and Au/CeO2 NPs towards A549 cells may be ascribed to the pro-oxidant activity induced by their internalization and localization into the acidic environment found in lysosomes. Obviously, the NPs can produce ROS upon induction of oxidase activity, leading to oxidative stress and eventually apoptosis of A549 cells. In a similar study, Lin et al45 observed significant oxidative stress in A549 cells because of a reduction in glutathione and α-tocopherol levels, resulting in lipid peroxidation and subsequent damage to the cell membrane.
To further elucidate the inhibition mechanism in A549 cells, intracellular ROS production was measured using the same NP dose as that used in the cytotoxic study (0.001–1,000 μM). Figure 7A and B show the production of ROS in terms of fluorescence intensity as a function of NP dose after 24 and 48 hours of incubation, respectively. For both CeO2 NPs and Au/CeO2 NPs, generation of ROS increased in a dose-dependent manner, with a 2–3-fold increase when the incubation time increased from 24 hours to 48 hours. Compared with the control, generation of ROS increased after 24 hours by 45.3% for CeO2 NPs and by 44.1% for Au/CeO2 NPs, while relatively to a larger extent by 158.1% for CeO2 NPs and by 154.5% for Au/CeO2 NPs after 48 hours of treatment, indicating that the latter could induce more ROS production than the former, probably as a result of the ability of Au to prevent agglomeration of Au/CeO2 NPs. As mentioned before, although CeO2 NPs possess unique autoregenerative antioxidant activity, they can also behave as pro-oxidants depending on the compartment where they become localized inside the cell.5,27,34 Obviously, the tumor progression, invasion, metastasis, and the acidic tumor environment are closely interrelated.42 The difference between normal cells and cancer cells may also play a crucial role in determining the antioxidant or pro-oxidant behavior of CeO2 NPs.42 Accordingly, the ROS production observed in our study should be due to the pro-oxidant activity of CeO2, because A549 lung carcinoma cells have an inherently acidic environment resulting from upregulated glycolysis and increased lactic acid production. Nevertheless, Asati et al42 demonstrated that localization of CeO2 NPs in the cytoplasm induces low or no cytotoxicity, while internalization inside lysosomes results in profound toxicity to cells.
In order to verify cellular uptake of NPs and their intracellular localization, cells incubated with NPs for 48 hours were pelleted and TEM images were recorded (Figure 8A–L). It is evident from these images that both CeO2 NPs and Au/CeO2 NPs were internalized into A549 cancer cells, with NPs becoming agglomerated (Figure 8D, E, J, and K), probably because of the high NP dose used (1,000 μM). However, the size and shape of the NPs were clearly visible (Figure 8E and K) and seemed to be unchanged even after internalization. In addition, both types of NPs were predominantly localized inside the cytoplasmic matrix around the nucleus (Figure 8C and I). However, whether they were localized in the endoplasmic, vesicular, or cytosol compartments was difficult to distinguish from the TEM images. The localization of a high proportion of NPs in the cytoplasm should be the main reason for their cytotoxicity towards A549 cells only at higher doses (100–1,000 μM). It may also be inferred that, at high doses, a certain proportion of the NPs may penetrate into lysosomes to induce higher toxicity in an acidic environment. In addition, the substantial increase in oxidative stress caused by ROS production may lead to mitochondrial dysfunction, as seen in Figure 8F and L. Taken together, it may be postulated that the cytotoxicity in A549 cells may be caused by the pro-oxidant activity of CeO2 NPs or Au/CeO2 NPs, leading to oxidative stress and mitochondrial dysfunction.
Antibacterial activity of Au, CeO2 and Au/CeO2 NPs
The antibacterial activity of Au NPs, CeO2 NPs and Au/CeO2 NPs was evaluated using E. coli, S. enteritidis, B. subtilis, and S. aureus as test pathogens in both monoculture and coculture systems. For the coculture studies, a lactic acid bacterium, L. plantarum, reported to have antibacterial activity,15,20 was cocultured along with each test pathogen. The observed antibacterial efficiency of the NPs was also compared with that of two commercial antibiotics, ampicillin and vancomycin. Figures 9 and 10 show the changes in bacterial concentration resulting from exposure to the different types of NPs and antibiotics in the monoculture and coculture studies, respectively. The overlap of NP absorbance and bacterial optical density was eliminated by accounting for the optical density of the bacterial inoculum containing NPs at 0 hour. The NPs did not dramatically inhibit growth of the bacterial strains at a low dose, so the minimum inhibitory concentration was not determined. This is the reason why the serial dilution method was used to evaluate the inhibitory effects of the NPs on the bacteria tested.
Au NPs did not have any significant inhibitory effect on the tested bacterial strains in either the monoculture or coculture studies. However, in the monoculture studies, both CeO2 NPs and Au/CeO2 NPs inhibited the growth of all tested pathogens, with the effects being higher for B. subtilis and S. enteritidis when compared with E. coli and S. aureus (Figure 9). Despite some inconsistency at the initial doses (6 and 12 μM), the percentage inhibition achieved by both NPs showed a dose-dependent increase for all types of bacteria. More specifically, following a rise in NP concentration from 0 to 1,488 μM, the antibacterial activity of CeO2 NPs and Au/CeO2 NPs increased by 52.3% and 69.6% for B. subtilis, by 40.9% and 45.7% for S. enteritidis, by 25.2% and 38.2% for E. coli, and by 12.4% and 24.2% for S. aureus, respectively, indicating that the inhibitory effect of the NPs was broad spectrum regardless of whether the bacteria were Gram-positive or Gram-negative (Figure 9). Compared with the antibiotics, ie, ampicillin and vancomycin, at 1,488 μM, the antibacterial efficiency of CeO2 NPs and Au/CeO2 NPs relative to ampicillin was 41.4% and 46.3% higher for S. enteritidis, 25.2% and 38.2% higher for E. coli, 12.6% and 24.6% higher for S. aureus, and 49.6% and 66.9% higher for B. subtilis, respectively. Whereas, the antibacterial efficiency of CeO2 NPs and Au/CeO2 NPs relative to vancomycin was 52.3% and 69.6% higher for B. subtilis, 54.2% and 60.6% higher for S. enteritidis, 30.5% and 46.2% higher for E. coli, and 12.8% and 24.9% higher for S. aureus, respectively. Taken together, the test pathogens inhibited by both NPs in the monoculture tests showed the following order: B. subtilis > S. enteritidis > E. coli > S. aureus. For further comparison, with a NP concentration of 1,488 μM, Au/CeO2 NPs had a greater antibacterial effect than CeO2 NPs for E. coli, S. enteritidis, B. subtilis, and S. aureus by 34%, 11%, 25%, and 49%, respectively. Of the two antibiotics, ampicillin was more efficient in inhibiting the growth of E. coli (100% at 372 μM) and S. enteritidis (93.0% at 47 μM) than vancomycin (82.7% and 75.4% for both bacteria at 1,488 μM), while vancomycin completely destroyed B. subtilis at a lower dose of 12 μM. Although ampicillin is a broad-spectrum drug, it failed to show pronounced antibacterial activity towards Gram-positive B. subtilis. Nevertheless, both antibiotics had high antibacterial activity towards S. aureus. The variation in inhibitory effect towards the different bacterial strains may be due to a difference in antibacterial action, as ampicillin irreversibly inhibits the activity of transpeptidase, an enzyme required for cell wall synthesis, while vancomycin acts by inhibiting cross-linking in the cell wall.
In bacterial systems cocultured with L. plantarum, S. aureus was retarded to a greater extent by both CeO2 NPs and Au/CeO2 NPs, followed by E. coli, B. subtilis, and S. enteritidis (Figure 10). This trend was the opposite to that observed in monoculture studies, in which both NPs showed the lowest anti-S. aureus activity, implying that coculture of L. plantarum with S. aureus could enhance the antibacterial activity of CeO2 NPs and Au/CeO2 NPs towards antibiotic-resistant S. aureus (Figures 9 and 10). In addition, inhibition of E. coli by CeO2 NPs increased by 20% compared with monoculture systems, but no significant change was noted for Au/CeO2 NPs. In contrast, the antibacterial activity towards S. enteritidis and B. subtilis dropped by 6% and 12.1% for CeO2 NPs, respectively, whereas a much higher inhibition (14.3% and 31.2%, respectively) was shown for Au/CeO2 NPs. Following an increase in NP concentration from 0 to 1,488 μM, the percent inhibition of S. aureus, E. coli, B. subtilis, and S. enteritidis by CeO2 NPs and Au/CeO2 NPs increased by 45.7% and 42.1%, 44.7% and 41.2%, 40.2% and 38.4%, and 34.9% and 31.4%, respectively (Figure 10). Compared to monoculture treatment without L. plantarum, the antibacterial efficiency of NPs towards Gram-positive and Gram-negative bacteria followed a reverse trend with S. aureus > B. subtilis for the former and E. coli > S. enteritidis for the latter.” Unlike the monoculture system, a uniform trend was observed for inhibition of all the bacteria by NPs and antibiotics in the presence of L. plantarum, in the following order: ampicillin > CeO2 NPs > Au/CeO2 NPs >> vancomycin. Of all the various treatments, NPs at 1,488 μM showed superior antibacterial activity when compared with vancomycin, with 32%–39% higher inhibition efficiency for CeO2 and 29%–37% higher inhibition efficiency for Au/CeO2. However, the inhibition efficiency of CeO2 NPs and Au/CeO2 NPs was 46.1% and 42.5% higher relative to ampicillin for E. coli, 37.5% and 33.7% higher for S. enteritidis, 79.7% and 51.2% higher for B. subtilis, and 47.5% and 43.8% higher for S. aureus, respectively. Thus, in the presence of L. plantarum, inhibition of S. aureus by ampicillin was greatly enhanced compared with the same treatment in monoculture systems.
It has been well documented that the antibacterial activity of CeO2 NPs depends mainly on the surface charge and oxidoreductive ability of the cerium atoms.46,47 According to zeta potential measurements, as shown in Figure 6, the surface charge on CeO2 NPs and Au/CeO2 NPs showed positive values of 41.5 mV and 55.6 mV, respectively, in freshly prepared solution. As mentioned earlier under results and discussion of cytotoxic study, the zeta potential shifted gradually from positive to negative with time, reaching −24.2 mV and −8.5 mV after 24 hours and −38.2 mV and −29.6 mV after 48 hours. Because the NP dispersion was prepared just before the start of the antibacterial experiments, this shift in surface charge over a 16-hour incubation period should be responsible for significant toxicity in both Gram-positive and Gram-negative bacteria. Also, the interaction of both NPs with Gram-negative bacteria might occur during the initial period of incubation when the surface charge of both NPs is positive, whereas a shift in the surface charge of the NPs to negative during the later period of incubation may favor a predominant interaction with Gram-positive bacteria. In a study dealing with the cytotoxicity of commercial CeO2 NPs in Gram-negative E. coli, rapid toxicity occurred upon adsorption of NPs on the cell membrane after one hour and remained constant until 5 hours.46 Upon adsorption via electrostatic interaction, the cerium atoms on NPs may undergo reduction from Ce4+ to Ce3+ on the cell surface, eventually leading to oxidative stress and cytotoxicity to bacteria.46,48 Further, the bacterial growth may also be affected by modification of nutrient transport on the outer cell membranes through alteration in membrane viscosity and corruption of specific ionic pumps.49 With regard to inhibition of E. coli by commercial CeO2 NPs, Thill et al46 pointed out that a direct spatial contact is essential for inducing cytotoxicity in bacteria.
The difference in inhibitory effect between Gram-positive and Gram-negative bacteria may be due to variations in the membrane surface, surface charge density, and metabolic process. Of the two Gram-positive bacteria tested, B. subtilis was inhibited to a greater extent by both NPs than was S. aureus, which may be ascribed to a spore-forming tendency and the presence of a high content of hydrophilic proteins on the cell surface of the former.48 Inbaraj et al50 have recently shown that the hydrophilic nature of bacteria can influence the antibacterial activity of metal oxide NPs. Likewise, the extracellular polymeric substance produced by Gram-negative E. coli O157:H7 may block electrostatic interaction between NPs and the cell membrane, which in turn may decrease the inhibitory effect when compared with S. enteritidis. A similar phenomenon was observed by Zeyons et al49 and Inbaraj et al51 with regard to inhibition of extracellular polymeric substance-producing Synechocystis and E. coli O157:H7 by CeO2 NPs and Fe3O4 NPs, respectively. In addition, categorization of E. coli O157:H7 as “slightly charged in relative to S. enteritidis may also explain its lower antibacterial activity by both NPs.51 The relatively stronger antibacterial effect shown by Au/CeO2 NPs than by CeO2 NPs may be due to a better suspension being achieved by coating of Au onto CeO2. Biradar et al7 have recently demonstrated that incorporation of Au can enhance the antibacterial activity of commercial antibiotics when used as combination therapy against S. aureus, E. coli, Pseudomonas aeruginosa, and Klebsiella pneumoniae. However, in coculture studies, both CeO2 NPs and Au/CeO2 NPs exhibited a similar inhibitory effect against all tested bacteria, and the mechanism needs to be explored further (Figure 10). The Gram-positive L. plantarum used in the coculture experiment may have modulated the inhibitory effect of both NPs by masking the benefits of Au decoration over CeO2 NPs.
As mentioned in the previous section, bacteriocins alone or in combination with other metabolites produced during the L. plantarum culture experiment may be responsible for this modulating effect on the antibacterial activity of both NPs.18,21 Moreover, the low inhibitory effect of CeO2 NPs on E. coli O157:H7 and that of both NPs on S. aureus in the monoculture tests was substantially enhanced by coculture with L. plantarum. As pointed out by François et al15 and Sharif et al,20 L. plantarum can effectively inhibit the growth of E. coli and S. aureus. Similarly, a Lactobacillus species was shown to be effective against S. aureus in two other studies.14,17 Thus, by combining isolates from Lactobacillus species, the antibacterial activity of CeO2 NPs towards E. coli and S. aureus could be greatly enhanced.
While several studies have evaluated the toxicity of metal oxide NPs, mainly in mammalian cells, few studies have investigated the antibacterial effect of CeO2 NPs. Some studies have shown inconsistent results for bacterial inhibition by CeO2 NPs. For instance, Thill et al46 and Pelletier et al48 have observed substantial toxicity towards E. coli bacteria because of oxidative stress through direct adsorption of CeO2 NPs onto the cell surface. However, several authors have found very little toxicity under room lighting and at room temperature.6,52 This difference in NP toxicity can be dependent upon surface charge as well as the physicochemical environment.1,46,48 In previous studies, both Kartsonakis et al52 and Li et al53 observed a marked decrease in E. coli concentration upon illumination of CeO2 NPs in bacterial systems, with a minimum effect being noticed in a non-illuminated environment. Variations in pH, growth medium, particle size, and NP concentrations could alter the toxicity of CeO2 NPs towards bacteria. By comparing uncoated and coated NPs, Kartsonakis et al52 demonstrated that polypyrrole-coated and polyaniline-coated CeO2 NPs had a better inhibitory effect against E. coli. Nevertheless, for dextran-coated CeO2 NPs, a non-lethal response was shown by Shah et al1 under varying physical and chemical environments, including pH, aeration, salt concentration (MgSO4, CaCl2, and KCl), natural organic matter, and fructose. Thus, bacterial interactions with NPs depend on many factors, making elucidation of the mechanism of inhibition a complicated issue. Future mechanistic investigations involving detailed imaging experiments and molecular analysis could facilitate understanding of the toxicity of NPs towards various microorganisms.
In summary, the present work describes the synthesis of porous CeO2 NPs by a combustion method and subsequent support with Au using a deposition-precipitation method. As-prepared CeO2 NPs and Au/CeO2 NPs were tested for cytotoxicity towards normal RAW 264.7 macrophage cells and A549 lung cancer cells as well as their antibacterial activity towards Gram-positive and Gram-negative bacteria. Au-supported CeO2 NPs showed better biocompatibility with normal RAW 264.7 macrophage cells, but inhibited the growth of A549 adenocarcinoma epithelial cells. This outcome demonstrated better selectivity of Au/CeO2 NPs towards cancerous cells in a concentration-dependent manner than CeO2 NPs. Also, the antibacterial activity of CeO2 NPs and Au/CeO2 NPs towards various bacterial species such as E. coli, S. enteritidis, B. subtilis, and S. aureus suggests that, compared with pure Au, Au/CeO2 NPs exhibited a better antibacterial effect, while CeO2 NPs and Au/CeO2 NPs inhibited B. subtilis and S. enteritidis in preference to E. coli and S. aureus. In bacterial systems cocultured with L. plantarum, inhibition of S. aureus was greater with CeO2 NPs and Au/CeO2 NPs. Au-supported CeO2 NPs may be a potential nanomaterial for in vivo application owing to their biocompatible and antibacterial properties.
KSB acknowledges start-up grant support (PU/PC/Start-up Grant/2011-12/312) provided by Pondicherry University. The authors are grateful to the Central Instrumentation Facility, Pondicherry University, India, and to Professor Tzong Jwo Jang and Mr Yen-Sheng Wu in the Electron Microscope Laboratory, School of Medicine, Fu Jen University, Taipei, Taiwan, for transmission electron microscopy recordings and other characterizations. This study is also supported by a grant (NSC 101-2632-B-030-001-MY3) from the Ministry of Science and Technology, Taiwan.
The authors report no conflicts of interest in this work.
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