SnO2-Doped ZnO/Reduced Graphene Oxide Nanocomposites: Synthesis, Characterization, and Improved Anticancer Activity via Oxidative Stress Pathway
Received 6 October 2020
Accepted for publication 30 November 2020
Published 8 January 2021 Volume 2021:16 Pages 89—104
Checked for plagiarism Yes
Review by Single anonymous peer review
Peer reviewer comments 3
Editor who approved publication: Professor Israel (Rudi) Rubinstein
Maqusood Ahamed,1 Mohd Javed Akhtar,1 MA Majeed Khan,1 Hisham A Alhadlaq1,2
1King Abdullah Institute for Nanotechnology, King Saud University, Riyadh 11451, Saudi Arabia; 2Department of Physics and Astronomy, College of Science, King Saud University, Riyadh 11451, Saudi Arabia
Correspondence: Maqusood Ahamed
King Abdullah Institute for Nanotechnology, King Saud University, Riyadh 11451, Saudi Arabia
Background: Therapeutic selectivity and drug resistance are critical issues in cancer therapy. Currently, zinc oxide nanoparticles (ZnO NPs) hold considerable promise to tackle this problem due to their tunable physicochemical properties. This work was designed to prepare SnO2-doped ZnO NPs/reduced graphene oxide nanocomposites (SnO2-ZnO/rGO NCs) with enhanced anticancer activity and better biocompatibility than those of pure ZnO NPs.
Materials and Methods: Pure ZnO NPs, SnO2-doped ZnO (SnO2-ZnO) NPs, and SnO2-ZnO/rGO NCs were prepared via a facile hydrothermal method. Prepared samples were characterized by field emission transmission electron microscopy (FETEM), energy dispersive spectroscopy (EDS), field emission scanning electron microscopy (FESEM), X-ray diffraction (XRD), ultraviolet-visible (UV-VIS) spectrometer, and dynamic light scattering (DLS) techniques. Selectivity and anticancer activity of prepared samples were assessed in human breast cancer (MCF-7) and human normal breast epithelial (MCF10A) cells. Possible mechanisms of anticancer activity of prepared samples were explored through oxidative stress pathway.
Results: XRD spectra of SnO2-ZnO/rGO NCs confirmed the formation of single-phase of hexagonal wurtzite ZnO. High resolution TEM and SEM mapping showed homogenous distribution of SnO2 and rGO in ZnO NPs with high quality lattice fringes without any distortion. Band gap energy of SnO2-ZnO/rGO NCs was lower compared to SnO2-ZnO NPs and pure ZnO NPs. The SnO2-ZnO/rGO NCs exhibited significantly higher anticancer activity against MCF-7 cancer cells than those of SnO2-ZnO NPs and ZnO NPs. The SnO2-ZnO/rGO NCs induced apoptotic response through the upregulation of caspase-3 gene and depletion of mitochondrial membrane potential. Mechanistic study indicated that SnO2-ZnO/rGO NCs kill cancer cells through oxidative stress pathway. Moreover, biocompatibility of SnO2-ZnO/rGO NCs was also higher against normal breast epithelial (MCF10A cells) in comparison to SnO2-ZnO NPs and ZnO NPs.
Conclusion: SnO2-ZnO/rGO NCs showed enhanced anticancer activity and better biocompatibility than SnO2-ZnO NPs and pure ZnO NPs. This work suggested a new approach to improve the selectivity and anticancer activity of ZnO NPs. Studies on antitumor activity of SnO2-ZnO/rGO NCs in animal models are further warranted.
Keywords: ZnO nanocomposites, improved anticancer activity, better selectivity, reactive oxygen species, caspase-3, breast cancer
According to a World Health Organization (WHO) report, cancer is the second leading cause of death worldwide.1 It has also been estimated that the total number of cancer cases will be doubled by year 2030 from 12.4 million new cases reported in 2008.2 In spite of the incredible effort to treat cancer, a lot needs to be done in cancer therapy. Recent cancer chemotherapies often fail to provide a complete anticancer response due to the development of drug resistance or their inability to efficiently differentiate between cancerous and noncancerous cells.3 This indiscriminate action normally leads to systemic toxicity in the human body.
Cancer nanotechnology can play a crucial role in the diagnosis and treatment of cancer to improve human health.4 A growing number of studies demonstrated that certain types of metal oxide nanoparticles (NPs) can selectively kill cancer cells with low toxicity to their normal counterparts.5–8 Particularly, ZnO NPs showed great promise for cancer therapy. Due to unique physiochemical characteristics ZnO NPs have shown inherent selective toxicity against cancer cells while posing minimum effects to the normal cells.9–11 ZnO NPs induce apoptosis in cancer cells through the generation of ROS and depletion of mitochondrial membrane potential (MMP)12,13 Manipulation in intracellular ROS generation is a probable way to irreversibly damage cancerous cells selectively without applying much harm to normal cells. The ROS-generating potential of ZnO NPs is associated with its optical properties.14 Optical behavior of ZnO NPs can be tuned by several methods including metal ion doping and synthesis of ZnO-based nanocomposites.14,15
Alternatively, studies reported some degree of toxicity of ZnO NPs in a wide range of organisms such as bacterial, microalgae, yeast, protozoa, zebrafish, and mice.16–20 Hence, there is an urgent need to tailor ZnO NPs with improved selectivity and anticancer activity.21 Semiconductor tin oxide (SnO2) and reduced graphene oxide (rGO) have shown great potential for biomedical applications.5,22 SnO2 and rGO can also be applied to tune physicochemical properties of metal oxide NPs including ZnO.23,24
Keeping the above points in mind, we prepared SnO2-doped ZnO NPs/reduced graphene oxide nanocomposites (SnO2-ZnO/rGO NCs) with improved anticancer potential and higher biocompatibility as compared to pure ZnO NPs. Pure ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs were prepared through a facile hydrothermal method. Prepared samples were characterized by field emission electron microscopy (FETEM), energy dispersive spectroscopy (EDS), field emission scanning electron microscopy (FESEM), X-ray diffraction (XRD), ultraviolet-visible (UV-VIS) spectrometer, and dynamic light scattering (DLS) techniques. Anticancer activity of pure ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs was examined in human breast cancer (MCF-7) cells. Possible mechanism of anticancer potentials of SnO2-ZnO/rGO NCs was delineated through ROS pathway. Biocompatibility of prepared samples were investigated in human normal breast epithelial (MCF10A) cells. Breast cancer cell lines were chosen in the present study because female breast cancer is the most commonly diagnosed cancer and the third leading cause of cancer death globally after colorectal and lung cancer.2
Materials and Methods
Synthesis of ZnO NPs, SnO2-ZnO NPs, and SnO2-doped-ZnO/rGO NCs
GO was prepared from pure graphite powder (<150 μm, 99.99% trace metals basis) (Millipore-Sigma, St Louis, MO, USA) applying modified Hummers' protocol.25 The SnO2-doped ZnO/rGO nanocomposite were synthesized through a facile hydrothermal method. Firstly, 0.02 g of GO was dispersed into 20 mL of ethanol (C2H5OH) (Millipore-Sigma) and sonicated for three hours in an ultrasonic bath to get uniform GO suspension. Zinc acetate dihydrate (Zn(CH3COO)2.2H2O) (99.999% trace metals basis, Millipore-Sigma) (2 mM), tin (II) chloride dihydrate (SnCl2.2H2O) (≥99.995% trace metals basis, Millipore-Sigma) (0.1 mM), and polyethylene glycol (PEG) (Millipore-Sigma) (0.2 g) were mixed in 20 mL distilled water under continuous stirring for one hour at room temperature to get homogenous solution. Then, GO suspension was mixed with homogenous solution and stirred for one hour, and pH of solution was maintained at 9 by adding aqueous ammonia solution. Then, solution transferred into a 50 mL autoclave and heated at 160°C for 12 h. Finally, the grey precipitates were washed and dried at 50°C for 12 h to get SnO2-ZnO/rGO nanocomposites. SnO2-doped ZnO NPs was prepared in similar procedure without adding GO, and pure ZnO NPs was synthesized without addition of tin chloride and GO during hydrothermal process. A schematic diagram of SnO2-ZnO/rGO NCs synthesis is given in Figure 1.
Figure 1 A schematic diagram of SnO2-ZnO/rGO NCs synthesis.
Absorption spectra of prepared samples were recorded at the wavelength of 300–900 nm with a resolution of 0.5 nm (Shimadzu UV-1800 spectrometer, Reinach BL, Switzerland). Crystallinity and phase-purity were analyzed at powder X-ray diffraction (PXRD) (PanAnalytic X’Pert Pro, Malvern Instruments, UK) with Cu-Kα radiation (λ=0.15405 nm, at 45 kV and 40 mA). Structural characterization was further assessed through FETEM (JEM-2100F, JEOL, Inc., Tokyo, Japan). Elemental analysis was done by energy dispersive X-ray spectroscopy (EDS). Mapping of elemental distribution of SnO2-ZnO/rGO NCs was further done through FESEM (JSM-7600F, JEOL, Inc.). Hydrodynamic size and zeta potential in distilled water and culture medium were determined by DLS (ZetaSizer, Nano-HT, Malvern Instruments).
Cell Culture and Exposure Procedure
MCF-7 cells (ATCC HTB-22, ATCC, Virginia, USA) were cultured in DMEM (Invitrogen, Carlsbad, CA, USA) with 10% FBS and antibiotics (100 µg/mL streptomycin+100 U/mL penicillin). MCF10A (ATCC CRL-10317) cells were grown in mammary epithelial cell growth basal medium (MEBM) (Lonza Group Ltd, Basel, Switzerland) supplemented with mammary epithelial cell growth medium (MEGM) kit (Lonza Group Ltd) and 100 ng/mL cholera toxin. Cells were maintained in a humidified incubator under control conditions (37°C and 5% CO2). First, we exposed the cells with a range of concentrations (0–200 µg/mL) of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs for 24 h for cell viability assay. On the basis of cell viability results, we have chosen three moderate concentrations (10, 25, and 50 µg/mL) of these samples for further experiments. For microscopic study we have chosen one concentration (50 µg/mL) of prepared samples. In some experiments, cells were exposed to ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs with or without N-acetyl-cysteine (NAC) (2 mM) (Millipore-Sigma). Briefly, NPs/NCs were suspended in culture medium (DMEM+10% FBS) and diluted to desired concentration (0–200 µg/mL). Different dilutions of NPs were further sonicated utilizing sonicator bath at room temperature for 10 min at 40 W to avoid agglomeration of NPs/NCs before exposure to cells. Cells without NPs/NCs served as control in each experiment.
Cell viability was determined through MTT26 and NRU27 assays with some specific changes.28 Morphology of treated and control cells was grabbed through phase-contrast inverted microscope (Leica Microsystems, GmbH, Germany). Expression level of mRNA of caspase-3 gene (CASP3) was determined through real-time PCR (ABI PRISM, 7900HT Sequence Detection System) (Applied Biosystems, Foster City, CA, USA) according to the procedures described earlier.28,29 Colorimetric assay of caspase-3 enzyme was performed using BioVision kit (Milpitas, CA, USA). MMP was assayed using rhodamine-123 probe (Rh-123) (Millipore-Sigma).30 MMP level was quantitatively assayed through a microplate reader (Synergy-HT, BioTek Winooski, VT, USA) and intracellular images were grabbed using a DMi8 fluorescent microscope (Leica Microsystems). Intracellular level of ROS was assayed using 2ʹ-7ʹ-dichlorodihydrofluorescein diacetate (H2DCFDA, Millipore-Sigma) probe.8 ROS level was also determined both quantitatively (Microplate reader, Synergy-HT, BioTek) and qualitatively (DMi8 fluorescent microscope, Leica Microsystems). Fluorometric assay of intracellular hydrogen peroxide (H2O2) was done applying a commercial kit (MAK164 green fluorescence, Millipore-Sigma). Glutathione (GSH) level was quantified using Ellman’s method.31 Malondialdehyde (MDA), one of the end products of lipid peroxidation was estimated using procedures of Ohkawa et al.32 Glutathione peroxidase (GPx) enzyme activity was assayed applying methods of Rotruck et al.33 Procedures of Sinha were utilized to assay the catalase (CAT) enzyme activity34 Colorimetric assay of superoxide dismutase (SOD) enzyme was done using kit from Cayman Chemical Company (Michigan, OH, USA). Protein content was quantified using Bradford’s protocol.35 Brief description of each biochemical procedure with necessary steps is provided in supplementary information.
One-way ANOVA followed by Dunnett’s multiple comparison tests were applied for analysis of results. The p<0.05 was assigned as statistically significant.
Results and Discussion
Morphological and Microstructural Study
Morphology, particle size, and crystal structure of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs were determined by FETEM. Figure 2A showed that ZnO NPs were almost spherical shaped with size of 14 nm. It was noticed that the shape of nanoparticles remains same, but the size of NPs increases after SnO2 doping (19 nm) (Figure 2B) and rGO integration (29 nm) (Figure 2C). Increment of NP size after doping and rGO incorporation was also reported by other studies.15 Figure 2D–F showed the HRTEM of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs, respectively. These images depict the presence of ZnO, SnO2 and rGO with high quality lattice fringes without any distortion. The calculated interplanar spacing of adjacent lattice fringes of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs were 0.345 nm, 0.342 nm, and 0.340 nm that correspond to the (101) plane of hexagonal wurtzite structure of ZnO.36 The lattice fringes of SnO2 were 0.334 nm and 0.338 nm corresponding to the (110) planes of tetragonal phase of SnO2.23 The lattice fringes were in agreement with XRD spectra. TEM images were also suggested all grown particles were highly crystalline that confirm the incorporation of SnO2 and rGO into the crystalline matrix of ZnO without creating lattice defects. EDS spectra of prepared SnO2-ZnO/rGO NCs indicated the stoichiometric presence of Zn, Sn, O, and C without any impurities (Figure 3). The Cu peak came from copper grid of TEM. The SEM mapping of elemental distribution of SnO2-ZnO/rGO NCs showed uniform distribution of SnO2 and rGO in ZnO NPs (Figure 4).
Figure 2 (A–C) Low resolution TEM images and (D–F) high resolution TEM images of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs. Arrows represent rGO.
Figure 3 Elemental composition of SnO2-ZnO/rGO NCs assessed through EDS.
Figure 4 SEM elemental mapping of SnO2-ZnO/rGO NCs. (A) SEM image. (B) Zinc. (C) Tin. (D) Oxygen. (E) Carbon mapping.
Crystal structure, phase purity, and size of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs were also analyzed by XRD technique. The XRD spectra of all samples were presented in Figure 5A. The indexing of diffraction peaks represents the formation of single-phase hexagonal wurtzite ZnO according to JCPDS card number 36–1451. No clear diffraction peak of SnO2 indicated that homogeneous doping of SnO2 throughout the ZnO lattice and ionic radii of Zn (0.74°A) and Sn (0.71°A) are almost same.37 Absence of diffraction peak of rGO in XRD spectra of SnO2-ZnO/rGO NCs also indicate the uniform distribution of SnO2-ZnO NPs inhibited the restacking of rGO sheets.38 Besides, XRD spectra show narrow and sharp diffraction peaks depicting excellent crystallinity of prepared samples. Crystallite size of synthesized samples were determined corresponding to highest intensity peak (101) by Scherrer’s formula and provided in Table 1. Results showed that crystallite size increases from 15 nm to 31 nm after SnO2 doping and rGO integration, which was well matched with to size calculated from TEM. We further noticed slight shifting of XRD peaks toward a lower value as compared to pure ZnO (Figure 5B). This shifting also indicates successful integration of SnO2 and rGO into ZnO NPs. Figure 5C represent XRD spectra of prepared rGO, which shows intense reflection planes (002) and (100).24
Table 1 Structural and Optical Properties
Figure 5 (A) XRD spectra of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs. (B) XRD spectra of same samples in the diffraction region of 28–38. (C) XRD spectra of rGO.
Optical properties of all prepared samples were examined through optical absorption study. Absorption spectra of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs, indicates SnO2 doping and rGO integration shifted the absorption edge of ZnO toward higher wavelength (Figure 6A). The band gap energy (Eg) for ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs were determined by Tauc’s formula.36
Figure 6 (A) optical absorption spectra of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs. (B) Tauc’s plot (αhν)2 vs (hν) of the same samples.
αhν = A(hν-Eg)1/2
where hν is the photon energy and A is the constant that does not depend on photon energy. The band gap energy (Eg) was determined by the extrapolation of linear portion of (αhν)2 vs hν curve to photon energy (hν) axis corresponding to α=0 (Figure 6B). The band gap values are provided in Table 1, which represent a decrement in band gap of ZnO NPs after SnO2 doping and rGO integration (3.30 eV-3.18 eV). It is reported that band gap energy of ZnO NPs could be tuned by doping metals oxides and/or integration of other semiconducting materials. Our results are in agreement with previous studies.39–41 Band gap tuning of ZnO NPs might be useful in cancer therapy. Tuning of band gap of semiconductor NPs might increase the threshold of ROS generation and oxidative stress in cancer cells through the generation of higher holes (h+) and electrons (e−) on the surface of NPs.8,42
Dynamic Light Scattering Study
It is important to assess the colloidal stability and surface charge of NPs in physiological media to understand the interaction of NPs with biological systems. DLS was applied to examine the hydrodynamic size and zeta potential of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs in distilled water and culture medium (Table 2). Hydrodynamic size of these samples in distilled water and culture medium were in the range of 55 nm to 96 nm, which were around three-to-five times higher than those of powder size calculated from TEM and XRD. Higher hydrodynamic size could be due to the agglomeration of particles in aqueous suspension and also reported in earlier studies.5,8,43 Zeta potential data showed that particles surface charge were ranging from 25–30 eV in distilled water and culture medium (DMEM+FBS). Zeta potential data suggested that colloidal suspension of prepared NPs and NCs were fairly stable. The higher value of zeta potential (positive or negative), the greater is the colloidal stability of nanoscale materials.44,45 Positive surface charge of prepared NPs and NCs under physiological medium provides favorable condition for their interaction with cancerous cells, which frequently carry negative surface charge.45
Table 2 Dynamic Light Scattering Characterization
Anticancer potential of ZnO NPs can be further improved by tuning of its physicochemical properties.3 In this study, we tried to enhance the cytotoxic potential of ZnO NPs against cancer cells through SnO2 doping and integration of rGO to prepare ZnO nanocomposites. Cytotoxicity of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs in breast cancer MCF-7 cells was assessed through MTT, NRU, and morphological examination. MCF-7 cells were exposed to different concentrations (0–200 µg/mL) of these samples for 24 h. MTT results demonstrated that all three samples were found to reduce cell viability in a dose-dependent manner in the concentration range of 10–200 µg/mL (Figure 7A). Furthermore, we observed that cytotoxicity of SnO2-ZnO/rGO NCs were significantly higher in comparison to pure ZnO NPs. MTT cell viability data were utilized to calculate the IC50s of prepared samples in MCF-7 cells. IC50s for ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs were 54.61, 38.73, and 27.86 µg/mL, respectively (Figure S1 and Table S1 of supplementary information). NRU data on cell viability was according to MTT results (Figure 7B). Figure 7C demonstrated that cell morphology after exposure to 50 µg/mL of ZnO, SnO2-ZnO, and SnO2-ZnO/rGO for 24 h. These images suggested that a significant number of cell death occurs (rounded morphology and low cell density) after exposure to ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs compared to controls. Similar to cell viability results, cell death induced by SnO2-ZnO/rGO NCs were greater than those of SnO2-ZnO NPs and pure ZnO NPs. Cytotoxic potential of ZnO NPs against different types of cancer cell lines has also been reported by other investigators.46–48 For example, a recent study reported anticancer activity of ZnO NPs against human small-cell lung cancer in an orthotopic mouse model.10
Apoptosis (a form of programmed cell death) might be stimulated by various internal or external factors such as injury, stress, starvation, and known apoptotic agents.49 ZnO NPs induce apoptosis in cancer cells through caspase-activation and MMP depletion.12,13 Caspase-3 is a protease that is present in mitochondria and critically involved in apoptotic pathway.50 Apoptotic response of prepared samples was determined by measuring the regulation of caspase-3 gene and MMP level in MCF-7 cells. Figure 8A showed that in comparison to control, ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs upregulated the mRNA expression level of the CASP3 gene in a dose-dependent manner (10–50 µg/mL). To confirm the mRNA data, we further examined the activity of caspase-3 enzyme (protein level). Results showed that activity of caspase-3 enzyme was dose-dependently higher in ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs treated groups compared to control group (Figure 8B). Moreover, effect of SnO2-ZnO/rGO NCs on activation of the caspase-3 gene was significantly higher than those of pure ZnO NPs.
MMP level of cells is compromised under stressful condition and is an excellent indicator of apoptosis.51 Figure 8C showed that dose-dependent reduction in MMP level after exposure to ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs. Fluorescent microscopy data also indicated that brightness of Rh-123 probe decreases (indicator of MMP loss) in all three samples ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs compared to control (Figure 8D). Similarly, MMP loss caused by SnO2-ZnO/rGO NCs was significantly higher in comparison to pure ZnO NPs. Apoptosis mediated anticancer activity of ZnO NPs was also reported by other investigators. Duan et al observed the anticancer activity of ZnO NPs in human melanoma (A375) cells was mediated through MMP depletion and caspase activation.52 Another recent report also suggested that ZnO NPs induced caspase-dependent apoptosis in gingival squamous cell carcinoma cells mediated through the mitochondrial pathway.53
Intracellular ROS generation and oxidative stress have been suggested as a possible mechanism to eliminate cancer cells.54 Recent studies indicated that ZnO NPs destroy cancer cells through ROS generation.14,55 Oxidative stress generating potential of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs in MCF-7 cells were explored through measuring several markers of pro-oxidants and antioxidants. Figure 9A depicted that all three samples induce ROS generation dose-dependently. Fluorescent microscopic images also suggested that brightness of DCF probe (indicator of ROS generation) were higher in ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs treated cells than those of control cells (Figure 9B). Intracellular H2O2 level (Figure 9C) and MDA level (Figure 9D) were also significantly higher in ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs treated cells as compared to controls (p<0.05). Importantly, pro-oxidants generating potential of SnO2-ZnO/rGO NCs were significantly higher in comparison to pure ZnO NPs.
Cell possesses antioxidant defense systems to get rid of ROS by inducing antioxidant molecule GSH along with several antioxidant enzymes.56 GSH scavenge ROS and free radicals to protect cells from oxidative damage.57 Main antioxidant enzymes are GPx, SOD, and CAT. GPx is mainly responsible for removal of hydroperoxides, hence, it may protect membranes, lipids, and proteins from oxidation. SOD provides a first line of defense by converting highly reactive superoxide anion (O2•–) into H2O2. CAT further breaks H2O2 into water and molecular oxygen.58 Antioxidant defense potential of MCF-7 cells was assessed following exposure for 24 h to ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs. (Figure 10A–D) showed that all three samples reduced the GSH level and decreased the activity of several antioxidant enzymes (GPx, SOD, and CAT) in a dose-dependent manner. Again, effects of SnO2-ZnO/rGO NCs on antioxidant markers were significantly higher than those of pure ZnO NPs.
Possible Mechanism of Anticancer Activity
Higher ROS production that surpasses the antioxidant defense capacity of the cells causes oxidative stress that induces oxidative damage of cellular components such DNA, lipid, and proteins.9 Recent studies indicated that ROS generation induces enzyme deactivation, lipid peroxidation, and membrane damage, which are the core mechanisms accountable for anticancer activity of ZnO NPs.59,60 Hence, in this study, we further examined the role of ROS and oxidative stress in anticancer activity of SnO2-ZnO/rGO NCs in MCF-7 cancer cells. Cells were exposed for 24 h to 50 µg/mL of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs in the presence and absence of NAC. Figure 11A demonstrated that NAC significantly alleviated the ROS generation induced by ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs. We further found that NAC, efficiently reverted that cytotoxicity induced by ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs (Figure 11B). These results confirm that SnO2-ZnO/rGO NCs induced cytotoxicity in MCF-7 cancer cells was mediated through ROS generation. Altogether, our data suggested that SnO2-ZnO/rGO NCs-induced toxicity in MCF-7 cells might be caused by ROS generation via mitochondrial pathway.
Effect of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs on Normal Human Mammary Epithelial (MCF10A) Cells
It is very important for anticancer drugs to have minimum or no effects on noncancerous normal cells. Benign nature of ZnO NPs against noncancerous normal cells have been reported previously.11,14,61 Hence, at the end of this study, we examined the effects of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs in normal breast cells (MCF10A). Cells were exposed to different concentrations (0–200 µg/mL) of these samples for 24 h. Figure 12A showed that ZnO NPs were not toxic to normal MCF10A cells up to 25 µg/mL concentration. However, cytotoxicity of pure ZnO NPs increases with increasing the concentrations from 50–200 µg/mL. In contrast, SnO2-ZnO/rGO NCs were not toxic to normal MCF10A cells even at a higher concentration (200 µg/mL). These results suggested that in comparison to ZnO NPs and SnO2-ZnO NPs, SnO2-ZnO/rGO NCs have greater biocompatibility toward normal cells and higher cytotoxicity toward cancer cells. As we observed that ROS generation due to SnO2-ZnO/rGO NCs exposure was the primary cause of killing of MCF-7 cancer cells. Hence, we further examined the ROS-generating potential of ZnO NPs, SnO2-ZnO NPs, and SnO2-ZnO/rGO NCs in MCF10A cells. As we can see that SnO2-ZnO/rGO NCs did not induce intracellular ROS generation in normal human mammary epithelial cells even at 200 µg/mL (Figure 12B). Consequently, SnO2-ZnO/rGO NCs showed improved anticancer activity and better biocompatibility compared to pure ZnO NPs. Possible mechanism of anticancer potential of SnO2-ZnO/rGO NCs is presented as a schematic diagram (Figure 13).
Figure 13 Possible mechanism of anticancer activity of SnO2-ZnO/rGO NCs.
In summary, SnO2-ZnO/rGO NCs were successfully synthesized by a simple hydrothermal procedure. XRD data confirmed the formation of single-phase of hexagonal wurtzite ZnO. HRTEM and SEM mapping showed homogenous distribution of SnO2 and rGO in ZnO NPs with high quality lattice fringes without any distortion. Band gap energy of SnO2-ZnO/rGO NCs decreases after SnO2 doping and rGO integration. The SnO2-ZnO/rGO NCs demonstrated strong anticancer activity against MCF-7 cells compared to pure ZnO NPs. The SnO2-ZnO/rGO NCs induced apoptosis in MCF-7 cancer cells through the upregulation of the caspase-3 gene and depletion of MMP. Mechanistic approach showed that SnO2-ZnO/rGO NCs kill breast cancer cells through ROS generation via mitochondrial pathway. Moreover, biocompatibility of SnO2-ZnO/rGO NCs was also greater in normal breast epithelia MCF10A cells than those of pure ZnO NPs. Overall our results provided a new approach to improve the selectivity and anticancer activity of ZnO in human breast cancer cells by tailoring its physicochemical properties. This work warrants further research on antitumor activity of SnO2-ZnO/rGO NCs in animal breast cancer models.
This work was supported by the National Plan for Science, Technology, and Innovation (MAARIFAH), King Abdulaziz City for Science and Technology, Kingdom of Saudi Arabia, under Award 13-NAN908-02.
All authors made substantial contributions to conception and design, acquisition of data, or analysis and interpretation of data; took part in drafting the article or revising it critically for important intellectual content; agreed to submit to the current journal; gave final approval of the version to be published; and agree to be accountable for all aspects of the work.
The authors report no conflicts of interest in this work.
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