Silica nanoparticles induce oxidative stress, inflammation, and endothelial dysfunction in vitro via activation of the MAPK/Nrf2 pathway and nuclear factor-κB signaling

Abstract

Despite the widespread application of silica nanoparticles (SiNPs) in industrial, commercial, and biomedical fields, their response to human cells has not been fully elucidated. Overall, little is known about the toxicological effects of SiNPs on the cardiovascular system. In this study, SiNPs with a 58 nm diameter were used to study their interaction with human umbilical vein endothelial cells (HUVECs). Dose- and time-dependent decrease in cell viability and damage on cell plasma-membrane integrity showed the cytotoxic potential of the SiNPs. SiNPs were found to induce oxidative stress, as evidenced by the significant elevation of reactive oxygen species generation and malondialdehyde production and downregulated activity in glutathione peroxidase. SiNPs also stimulated release of cytoprotective nitric oxide (NO) and upregulated inducible nitric oxide synthase (NOS) messenger ribonucleic acid, while downregulating endothelial NOS and ET-1 messenger ribonucleic acid, suggesting that SiNPs disturbed the NO/NOS system. SiNP-induced oxidative stress and NO/NOS imbalance resulted in endothelial dysfunction. SiNPs induced inflammation characterized by the upregulation of key inflammatory mediators, including IL-1β, IL-6, IL-8, TNFα, ICAM-1, VCAM-1, and MCP-1. In addition, SiNPs triggered the activation of the Nrf2-mediated antioxidant system, as evidenced by the induction of nuclear factor-κB and MAPK pathway activation. Our findings demonstrated that SiNPs could induce oxidative stress, inflammation, and NO/NOS system imbalance, and eventually lead to endothelial dysfunction via activation of the MAPK/Nrf2 pathway and nuclear factor-κB signaling. This study indicated a potential deleterious effect of SiNPs on the vascular endothelium, which warrants more careful assessment of SiNPs before their application.

Introduction

Nanotoxicology is an emerging field of research as a response to an exponential growth in the development and production of engineered nanoparticles (NPs) worldwide. The interactions of NPs with biological systems, as well as their environmental and human health effects, have not been fully explored.¹ There is concern that research on the possible health risks of NPs is not keeping pace with the rapid growth in the number of NP products entering the industry and market. Due to their special physicochemical features, NPs’ biological behavior may differ from that of larger particles. Previous research has shown that nanoscale particles are more toxic than fine particles or bulk materials with the same chemical composition.^2,3

Silica NPs (SiNPs) are among the top five commonly used nanomaterials listed in nanotechnology consumer products by the Woodrow Wilson International Center for Scholars.⁴ They have recently been extensively utilized in biomedical and biotechnological fields for biomolecule detection, diagnosis, imaging, drug delivery, gene therapy, and photodynamic therapy.^5,6 As a consequence, human exposure to SiNPs continues to increase in environmental, occupational, and medial settings. Therefore, the environmental and health impact of SiNPs deserve great concern. However, toxicological studies on SiNPs are far behind the speed of their application. Malvindi et al pointed out that SiNPs had good biocompatibility when used in a reasonable concentration range (up to 2.5 nM).⁷ However, as they are smaller than cellular organelles, it is increasingly recognized that SiNPs could penetrate the cytomembrane, deposit in mitochondria or even the nucleus, and eventually lead to cell death.^8–11 It has been confirmed that NPs can systemically translocate to the circulation from the lung.¹² Subsequently, translocated particles could mediate cardiovascular effects through direct interaction with vasculature, blood, and the heart. The cardiovascular toxicity of NPs has gradually drawn attention. However, related research is limited, and controversial reports exist.¹³

Endothelial dysfunction is believed to induce pathological changes in the cardiovascular system, and has been considered as a predictor and an initiating event of atherosclerosis and its complications.^14,15 As a biological barrier between circulating blood and the vessel wall, vascular endothelia are extremely important for the maintenance of vascular function and of homeostasis.¹⁶ For SiNPs, based on their access to systemic and coronary circulations under inhalation exposure and their wide application for diagnostics or drug delivery through intravenous injection, there would be quite a large probability for them to influence vascular reactivity by directly interacting with the vascular endothelium. A concentration-dependent cytotoxicity of SiNPs on endothelial cell line EA.hy926 has been previously reported.¹⁷ There is evidence that SiNPs can induce reactive oxygen species (ROS), impairment of proliferative activity, inflammation, and cell death on vascular endothelial cells.^18–20 Our previous study confirmed that SiNPs caused deoxyribonucleic acid (DNA) damage via the Chk1-dependent G₂/M-checkpoint signaling pathway on endothelial cells.²¹ However, understanding of the molecular mechanisms involved in the cytotoxicity of SiNPs on endothelium is still limited.

Based on these issues, a toxicity evaluation of SiNPs on endothelial cell injury and dysfunction was conducted in vitro with human umbilical vein endothelial cells (HUVECs), which have been used as a reference for in vitro studies of endothelial cell function. A series of evaluations, including cell viability, membrane injury, oxidative stress, nitric oxide (NO) release, and inflammatory mediators in HUVECs after exposure to SiNPs were investigated in vitro. Moreover, to understand the observed molecular mechanism of SiNP-induced oxidative stress, in vitro assays were conducted focusing on MAPK cascades, nuclear factor (NF)-κB, and Nrf2.

Materials and methods

Chemicals and reagents

Tetraethyl orthosilicate and 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyl-tetrazolium bromide (MTT) were obtained from Sigma-Aldrich, USA. Fetal bovine serum and Dulbecco’s modified Eagle’s medium (DMEM) were purchased from Invitrogen, USA. A MiniBest universal ribonucleic acid (RNA) extraction kit, PrimeScript™ RT Master Mix (Perfect Real Time), and SYBR Premix Ex Taq™ II were obtained from Takara, Japan. All other chemicals used were of the highest purity and available from commercial sources.

SiNP preparation and characterization

SiNPs in aqueous suspension were prepared using the Stöber method by the College of Chemistry, Jilin University, People’s Republic of China (PRC). Before use, the particles were isolated by centrifugation (12,000× g, 15 minutes), washed three times with deionized water, and then dispersed in 50 mL of deionized water sterilized by autoclave (0.1 MPa, 120°C, 20 minutes). The size and distribution of SiNPs were assessed by transmission electron microscopy (JEM2100; JEOL, Japan) and ImageJ software. Dynamic light scattering was employed using a Zetasizer (Nano ZS90; Malvern, UK) to examine the hydrodynamic sizes and zeta potential of SiNPs in different dispersion media. The stock suspensions of SiNPs were sonicated for 5 minutes through a sonicator (160 W, 20 kHz, 5 minutes; Bioruptor UDC-200, Belgium) before addition to DMEM or distilled water in order to minimize their aggregation. Meanwhile, inductively coupled plasma atomic emission spectrometry (ICP-AES) (Agilent 720, USA) was used for purity detection, and gel-clot limulus amebocyte lysate (LAL) assay for endotoxin measurement in SiNP suspensions, purchased from Zhan Jiang Bokang Marine Biological (PRC).

Cell culture

HUVECs were obtained from the Cell Resource Center, Shanghai Institutes for Biological Sciences, PRC. Cells were cultured in DMEM supplemented with 10% fetal bovine serum at 37°C in a 5% CO₂ humidified incubator.

Cell morphology

After the 24-hour exposure to SiNPs at concentrations of 12.5, 25, 50, and 100 μg/mL, the morphology of HUVECs was observed by using an optical microscope (Olympus IX81, Japan).

Cell-viability assay

The cytotoxicity of SiNPs was determined using the MTT assay as previously described.²² Briefly, cells were seeded in 96-well plates, with approximately 1×10⁴ cells per well. After overnight incubation, the old culture medium was discarded. In order to eliminate the possible reaction between SiNPs and serum in old culture medium, cells were treated by twice rinsing in fresh culture media without serum. Then, the cells were incubated in fresh culture media without serum but containing various concentrations of SiNPs for 24 hours at 37°C: 12.5, 25, 50 and 100 μg/mL. Controls were supplied with an equivalent volume of media without SiNPs or serum. Ultimately, absorbance was measured at 490 nm using a microplate reader (SpectraMax M5; Molecular Devices, USA).

Lactate dehydrogenase-release assay

The release of intracellular lactate dehydrogenase (LDH) into culture medium is an indicator of irreversible cell death due to cell-membrane damage. To determine the effect of SiNPs on the cell membrane, LDH release was assessed using a commercial LDH kit (Jiancheng, PRC) according to the manufacturer’s protocols. Briefly, cells were cultured in 24-well plates, with approximately 8×10⁴ cells per well. After 12 hours of growth, cells were treated by SiNPs at concentrations of 12.5, 25, 50, or 100 μg/mL for 24 hours at 37°C. The supernatants were collected, 100 μL cell medium was used for LDH-activity analysis, and absorbance at 440 nm was measured by an ultraviolet-visible spectrophotometer (Beckman DU-640B, USA). The amount of LDH released is expressed as LDH activity (U/L) in culture media.

SiNP uptake

The amount of SiNPs existing in cells was determined using ICP-AES. Briefly, HUVECs were exposed to SiNPs for 24 hours, subsequently washed with phosphate-buffered saline (PBS), and trypsinized. Cell density was determined with a hemocytometer. The cell suspensions were centrifuged at 1,500× g for 5 minutes. In total, 5 mL cell lysate containing HNO₃ and H₂O₂ (3:1) was added in cell pellets to dissolve SiNPs. Lastly, SiNPs that entered cells were measured by detecting the intracellular silicon content using ICP-AES.

Intracellular ROS measurement

The production of intracellular ROS was measured using the 2′,7′-dichlorofluorescein diacetate (DCFH-DA) (Beyotime, PRC) as an oxidation-sensitive probe. Briefly, HUVECs were treated with various concentrations of SiNPs for 24 hours. Then, the cells were incubated with PBS containing 10 mM DCFH-DA for 30 minutes in a CO₂ incubator. After incubation, the cells were washed with PBS. DCF fluorescence was observed using a flow cytometer (Becton-Dickinson, USA) and a laser scanning confocal microscope (LSM 710; Zeiss, Germany) by capturing images at 400× magnification.

Assessment of oxidative damage

In addition to the analysis of ROS levels, the malondialdehyde (MDA) content was measured as an end product of lipid peroxidation, which was carried out using commercially available kits (Jiancheng) according to the manufacturer’s instructions. Briefly, after exposure to SiNPs for 24 hours, HUVECs were washed once with ice-cold PBS and lysed in ice-cold radioimmunoprecipitation assay lysis buffer (Ding-Guo, PRC) for 30 minutes. After the lysates were centrifuged at 12,000× g, 4°C for 10 minutes, the supernatants were collected for measurement of the production of MDA. The protein concentrations of these extracts were determined by performing the bicinchoninic acid protein assay (Pierce, USA). The defense systems against free radical attack were assessed by the measurement of both the activities of superoxide dismutase (SOD) and glutathione peroxidase (GSH-Px), using the corresponding commercial kit from Nanjing Jiancheng Bioengineering Institute (Jiancheng).

Glutathione and glutamate cysteine ligase subunit-level estimation

Glutathione (GSH) levels were quantified using a commercial reduced GSH assay kit (Jiancheng), and the amount of GSH was expressed in terms of micromoles of GSH per gram of proteins. Glutamate cysteine ligase (GCL), also known as γ-glutamylcysteine synthetase, is the first rate-limiting enzyme in GSH synthesis, and has both catalytic (GCLC) and modifier (GCLM) subunits. Total GCLM and GCLC levels were quantified by real-time polymerase chain reaction (PCR) according to the methods mentioned in the following sections.

NO, NOS, and ET-1 measurement

NO content in cells was measured using a commercial kit (Jiancheng). Moreover, the messenger RNA (mRNA) expressions of inducible nitric oxide synthase (iNOS), endothelial NOS (eNOS), and ET-1 were quantified by real-time PCR. In brief, total RNA was isolated using the MiniBest universal RNA extraction kit according to the manufacturer’s protocol. Then, complementary DNA was synthesized using the PrimeScript RT Master Mix. To quantify relative mRNA levels of the genes in HUVECs, real-time PCR was performed using the SYBR Premix Ex Taq II following the manufacturer’s instructions on a Light-Cycler 480 instrument (Roche, Germany). All quantifications were performed with β-actin as an internal standard, and the relative amount of mRNA was calculated using the 2^−ΔΔCT method. Three independent experiments were used to determine the average fold changes for each target gene. The primer sets are listed in Table S1.

Quantification of mRNA levels of redox-and inflammation-related factors

The relative amount of redox related factors, including Nrf2 and its downstream genes, such as HMOX1, SOD2, CAT, GPX, GCLC, GCLM, NQO1, TXN1, and TXNRD1, were quantified using real-time PCR as mentioned earlier. Furthermore, inflammatory cytokines, including IL-1β, IL-6, IL-8, and TNFα, and ICAM-1, VCAM-1, and MCP-1, were also measured. The primer sets are listed in Table S1.

Western blot analysis

To analyze whether SiNPs influence the expression of cellular factors involved in the MAPK signaling pathway, we measured the protein levels of Nrf2, heme oxygenase (HO)-1, ERK, p38MAPK, JNK, and NF-κB in HUVECs by Western blot analysis after SiNP treatment for 24 hours. As an internal control, glyceraldehyde 3-phosphate dehydrogenase was also detected. Densitometric analysis of the Western blots was performed using Image Lab™ software (version 3.0; Bio-Rad, USA). The relative values of the samples were measured by normalizing all data to the respective control samples of each experiment.

Statistical analysis

Data are expressed as means ± standard deviations. Significance was determined by using one-way analysis of variance, followed by least significant difference tests to compare differences between groups. Differences were considered significant at P<0.05.

Results

Characterization of SiNPs

Prior to the study of toxicity, the characterization of SiNPs was examined. The morphology and average size of SiNPs were determined by transmission electron microscopy. As shown in Figure 1A, SiNPs had a near-spherical shape and were well dispersed, with an average diameter of 58 nm. Size distribution measured by ImageJ software showed approximately normal distribution (Figure 1B). Additionally, to investigate the possible effect of the dispersion medium on SiNPs, the hydrodynamic sizes and zeta potentials of SiNPs were measured either in DMEM after incubation at 37°C or in distilled water at room temperature at different time points, and these are summarized in Table 1. Owing to the van der Waals force and hydrophobic interaction with surrounding media, SiNPs generally had larger hydrodynamic size in dispersion media than their original size. The polydispersity index, an indicator of dispersion, showed SiNPs with good monodispersity in distilled water or DMEM. Zeta potential is a marker of colloidal stability. In general, when the absolute value of a zeta potential is higher than 30 mV, particles are not prone to aggregation or precipitation. All the results indicated that the SiNPs in dispersion media still possessed uniform shape along with relatively favorable dispersibility and stability. The major trace-metal impurities in SiNPs detected by ICP-AES are summarized in Table 2, suggesting that the purity of SiNPs was better than 99.9%. Additionally, the LAL assay indicated no detectable Gram-negative endotoxin on the SiNPs at concentrations of 0.65, 1.25, 2.5, 5, and 10 mg/mL, indicating SiNPs were endotoxin-free.

Figure 1.

Morphology and size distribution of SiNPs.

Notes: (A) TEM image: SiNPs had a near-spherical shape and good monodispersity, with an average diameter of 58 nm. (B) Size distribution measured by ImageJ software showed an almost normal distribution.

Abbreviations: SiNPs, silica nanoparticles; TEM, transmission electron microscopy; Std dev, standard deviation.

Table 1.

Hydrodynamic size, zeta potential, and PDI of SiNPs in distilled water or DMEM as dispersion medium at different time points

Time (hours)	Distilled water			DMEM
	Diameter (nm)	Zeta potential (mV)	PDI	Diameter (nm)	Zeta potential (mV)	PDI
0	106.33±1.23	−35.21±0.83	0.09±0.02	108.87±4.30	−31.83±4.78	0.08±0.02
3	102.67±1.28	−34.43±1.72	0.11±0.01	105.33±1.84	−32.90±3.51	0.10±0.01
6	105.13±0.91	−37.50±0.85	0.08±0.03	106.80±2.85	−35.50±1.31	0.09±0.03
12	108.93±1.28	−34.48±0.57	0.10±0.01	103.47±1.12	−30.30±1.99	0.10±0.01
24	106.37±2.14	−33.92±1.48	0.12±0.02	107.94±1.47	−30.33±1.35	0.11±0.02

Note: Data expressed as means ± standard deviation from three independent experiments.

Abbreviations: SiNPs, silica nanoparticles; PDI, polydispersity index; DMEM, Dulbecco’s modified Eagle’s medium.

Table 2.

Trace-metal impurity levels in SiNPs (μg/10 mg SiO₂)

Elements	Ca	Mg	Fe	Mn	Al	Cr
SiNPs	0.3354	0.0336	0.0202	0.0046	0.0061	0.0086

Abbreviation: SiNPs, silica nanoparticles.

Cytotoxicity of SiNPs

To evaluate the possible toxicity of SiNPs on endothelial cells, cellular morphology and cell viability were determined after SiNP exposure to HUVECs for 24 hours. The morphological changes of HUVECs became gradually apparent as the dosage of SiNPs increased, and were characterized by cell-density reduction, irregular shape, and cellular shrinkage (Figure 2A). Changes in cellular morphology were directly reflected by cell viability. As indicated in Figure 2B, cell viability decreased remarkably, along with increased SiNP concentration. When cells were exposed to SiNPs at concentrations of 12.5, 25, 50, or 100 μg/mL, cell viability decreased to 92.93%, 81.24%, 42.68%, and 33.44%, respectively, which was significantly lower than that in the control group except for 12.5 μg/mL. Moreover, cell viability declined as time passed, suggesting a dose-and time-dependent effect of SiNP toxicity on HUVECs. Additionally, a significant difference in LDH release was observed when HUVECs were incubated with SiNPs for 24 hours compared with the control (Figure 2C). The LDH-leakage results showed that SiNPs induced injury to the cell membrane, which was strongly in accordance with the result for cell viability. A significant negative correlation was also observed between LDH leakage and MTT cell viability (R²=0.9559, Figure 2D).

Figure 2.

Cytotoxicity of HUVECs induced by SiNPs.

Notes: *P<0.05 versus control. Data presented as means ± SD of three identical experiments made in triplicate. (A) Morphological changes of HUVECs after exposure to SiNPs with various concentrations for 24 hours. Under observation by optical microscopy with 100× magnification, SiNPs induced cellular morphological changes, characterized by cell-density reduction, irregular shape, and cellular shrinkage. (B) Dose- and time-dependent cell-viability decline in HUVECs measured by MTT assay after 24 and 48 hours’ SiNP exposure. (C) Dose-dependent induction of LDH leakage to HUVECs after SiNP exposure for 24 hours. (D) A significant negative correlation between cell viability and membrane damage (LDH leakage) after 24 hours’ exposure to 12.5, 25, 50, and 100 μg/mL of SiNPs. The results indicated that SiNPs induced cytotoxicity in a dose- and time-dependent manner.

Abbreviations: HUVECs, human umbilical vein endothelial cells; SiNPs, silica nanoparticles; SD, standard deviation; MTT, 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide; LDH, lactate dehydrogenase.

Uptake of SiNPs by HUVECs

ICP-AES was applied for the investigation of cellular uptake of SiNPs. The number of internalized SiNPs was calculated via the silicon content in the lysis solution divided by the number of cells, providing a quantitative measurement of SiNP uptake. Results showed that after incubation with SiNPs for 24 hours, the average silicon content (μg) internalized by each 10⁶ cells was increased along with increased SiNP-exposure dosages, which were 0.12±0.04, 2.33±0.47, 5.46±0.85, 13.87±1.24, and 34.24±5.77 at control, 12.5, 25, 50, 100 μg/mL respectively, suggesting a clear dose-dependent increase in the uptake of the SiNPs by HUVECs.

Oxidative stress and damage triggered by SiNPs

To get a closer insight into cytotoxicity induced by SiNPs, the ROS level was determined by using DCFH-DA probe. As shown in Figure 3A, ROS production significantly increased after 24 hours of SiNP exposure. Furthermore, the fluorescence intensity was enhanced with the increase in the SiNP concentration, suggesting a significant increase in ROS production (Figure 3B). In the 100 μg/mL SiNP-treated group, the fluorescence intensity was significantly elevated (about 3.12-fold higher than that of control). Results demonstrated that SiNPs induced intracellular ROS generation increased in a dose-dependent manner. The overproduction of ROS would break down the balance of the oxidative/antioxidative system, resulting in lipid peroxidation, which is closely related to reduction of antioxidative capacity. Figure 3C shows that the intracellular level of MDA, an indicator of lipid peroxidation, was significantly increased in HUVECs exposed to SiNPs for 24 hours when compared to that in the control group. Furthermore, SiNPs inhibited the activity of GSH-Px (Figure 3E), and upregulated SOD activity (Figure 3D) and intracellular GSH content (Figure 3G) in HUVECs. In addition, the mRNA expressions of SOD, GSH-Px, and the GCL subunits GCLC and GCLM were measured. Significant change was confirmed in the mRNA expressions of SOD2 and GSH-Px, which was perfectly consistent with that in their activities (Figure 3F). Figure 3H showed that GCLC mRNA expression was upregulated by SiNPs, while the levels of GCLM mRNA were not altered. All these results revealed that SiNPs induced oxidative stress via ROS overproduction followed by disorder in the oxidant/antioxidant system and production of MDA.

Figure 3.

Oxidative stress and damage induced by SiNPs in HUVECs.

Notes: *P< 0.05 versus control. Data expressed as means ± SD from three independent experiments. HUVECs were treated with increasing concentrations of SiNPs for 24 hours, and then the fluorescence intensity of DCF was measured using laser scanning confocal microscopy and flow cytometry. The intracellular levels of ROS were significantly increased in a dose-dependent manner (A, B), and so was the production of MDA (C). SOD activity was increased, while GSH-Px levels decreased significantly in a dose-dependent way (D, E). Meanwhile, the relative mRNA expression of SOD2 and GSH-Px were measured by quantitative real-time PCR. Significant changes in their mRNA expressions were observed, which was consistent with the corresponding change in their activities (F). Additionally, GSH content increased, induced by SiNPs, and the relative mRNA expression of GCLC normalized to β-actin was upregulated, but there was no significant change in that of GCLM (G, H). In figure A the upper images were DCFH-DA staining under confocal microscopy. The lower images were DCFT-DA staining merged with optical morphology at the same visual field.

Abbreviations: HUVECs, human umbilical vein endothelial cells; SiNPs, silica nanoparticles; SD, standard deviation; DCF, dichlorofluorescein; ROS, reactive oxygen species; MDA, malondialdehyde; GSH-Px, glutathione peroxidase; PCR, polymerase chain reaction; mRNA, messenger ribonucleic acid; DA, diacetate; SOD, superoxide dismutase; GCLC, glutamate cysteine ligase – catalytic; GCLM, glutamate cysteine ligase – modifier.

Imbalanced NO/NOS in HUVECs caused by SiNPs

Results showed that SiNP treatment in HUVECs stimulated a rapid increase in NO content and iNOS mRNA levels, especially the high concentration of 50 or 100 μg/mL (Figure 4A and B). Interestingly, SiNPs produced a decline in eNOS and ET-1 mRNA levels (Figure 4B and C).

Figure 4.

NO/NOS systemic disorder and downregulated ET-1 mRNA expression mediated by SiNP exposure in HUVECs.

Notes: *P<0.05 versus control. Data presented as means ± SD, n=3. (A) Release of NO after SiNP exposure for 24 hours in HUVECs. (B) Real-time PCR assessment of mRNA levels for eNOS, iNOS, and ET-1 normalized to β-actin in HUVECs after 24 hours’ SiNP treatment.

Abbreviations: eNOS, endothelial nitric oxide synthase; iNOS, inducible NOS; SiNP, silica nanoparticle; HUVECs, human umbilical vein endothelial cells; SD, standard deviation; ET-1, endostatin 1; PCR, polymerase chain reaction; mRNA, messenger ribonucleic acid.

Inflammatory response induced by SiNPs

To further explore the effect of SiNPs on HUVECs at the molecular level, expressions of key inflammatory cytokines, adhesion molecules, and chemokines were detected. Results demonstrated that the expressions of mRNA for IL-1β, IL-6, IL-8, TNFα, ICAM-1, VCAM-1, and MCP-1 were all upregulated with SiNP exposure, indicating SiNP treatment produced a robust inflammation response in HUVECs (Figure 5). Of interest, ICAM-1 mRNA expression was only significantly upregulated by SiNPs with lower doses (12.5 or 25 μg/mL), but there was no obvious alteration at higher doses (50 or 100 μg/mL). These phenomena might be associated with the severe inhibition in cell viability mediated by SiNPs.

Figure 5.

Inflammatory response induced by SiNPs in HUVECs.

Notes: *P<0.05 versus control. Data presented as means ± SD, n=3. After exposure of HUVECs for 24 hours, SiNPs upregulated the endothelial gene expressions of inflammatory cytokines, including IL-1β, IL-6, IL-8, and TNFα, and adhesion molecules, such as ICAM-1, VCAM-1, and MCP-1, as recorded by quantitative real-time PCR.

Abbreviations: SiNPs, silica nanoparticles; HUVECs, human umbilical vein endothelial cells; SD, standard deviation; PCR, polymerase chain reaction; mRNA, messenger ribonucleic acid.

Activation of Nrf2, NF-κB, and MAPK signaling pathways

To understand the possible mechanism involved in SiNP-induced oxidative stress and injury in HUVECs, the Nrf2-mediated oxidative signaling pathway was investigated by performing quantitative real-time PCR and Western blot analysis. The mRNA expressions of Nrf2 and its key downstream genes tested were upregulated with SiNP exposure in HUVECs (Figure 6A). Consistent with this observation, SiNPs increased the protein expression of Nrf2 and HO-1 (Figure 6B). To further clarify the possible upstream oxidative signaling pathway involved in Nrf2 activation, leading to HO-1 induction, the activation of three key MAPKs – ERK, JNK, and p38 MAPK – was examined. Results demonstrated that expressions of the unphosphorylated forms of MAPKs were constant, regardless of SiNP exposure, whereas expressions of the phosphorylated forms of JNK and p38 MAPK were strongly induced by SiNPs, and that of ERK was suppressed (Figure 6B). Similarly, NF-κB in HUVECs was increased after exposure to SiNPs (Figure 6B).

Figure 6.

Redox-mediated Nrf2, NF-κB, and MAPK signaling pathway involved in SiNP cytotoxicity in HUVECs.

Notes: The mRNA expression of Nrf2 and its key downstream genes, including HMOX1, CAT, TXN1, TXNRD1, and NQO1, was measured through quantitative real-time PCR (A), and the protein levels of Nrf2, HO-1, NF-κB, ERK, JNK, p38 MAPK, and corresponding phosphorylated forms were measured through Western blot analysis (B). *P<0.05 vs control. Data presented as means ± SD, n=3.

Abbreviations: NF, nuclear factor; SiNP, silica nanoparticle; HUVECs, human umbilical vein endothelial cells; mRNA, messenger ribonucleic acid; PCR, polymerase chain reaction; HO, heme oxygenase; GAPDH, glyceraldehyde 3-phosphate dehydrogenase; SD, standard deviation.

Discussion

Nanomedicine, the use of nanotechnology for biomedical applications, has the potential to change the landscape of the diagnosis and therapy of many diseases. Along with the huge advancement in nanotechnology and material science, taking advantage of unique properties amenable for in vivo applications, SiNPs have emerged as a promising drug-delivery platform to realize the potential of nanomedicine.²³ Therefore, it is very likely for SiNPs to enter the bloodstream, and for endothelial cells to be exposed. Liu and Sun demonstrated that SiNPs can induce dysfunction of endothelial cells.²⁴ However, a complete understanding of how SiNPs interact with endothelial cells, particularly at the molecular level, remains unclear and poorly understood. Our findings demonstrated that direct exposure of HUVECs to SiNP-induced intracellular ROS generation led to oxidative stress, imbalance in redox status, and inflammation through the activation of Nrf2, MAPK, and NF-κB pathways, and subsequently to the dysfunction and injury of endothelial cells.

Currently, the cell uptake of NPs is an important issue in designing suitable cell-tracking and drug-carrier nanomaterial systems. Phagocytosis and nonphagocytic endocytosis were involved in the cellular uptake of NPs.^10,25 It is increasingly recognized that SiNPs can enter cells easily by endocytosis.^19,26 We also confirmed that SiNPs were internalized via the endocytic pathway,²⁷ and mainly accumulated in the cytoplasm.^27,28 Besides, the endothelial caveolae, clathrin-coated pits, and macropinocytosis were also involved.²⁹ Cellular or subcellular distribution of NPs has a serious influence on protein or gene expression, and cytotoxicity.³⁰ As indicated in Figure 2, SiNPs induced change in cell morphology, decline in cell viability, and loss of membrane integrity, indicated by LDH release, suggesting SiNPs did result in cytotoxicity in HUVECs. Meanwhile, the endothelial cytotoxicity mediated by SiNPs was increased in a dose- and time-dependent manner. This may be correlated with the amount of silicon taken up by HUVECs, since as the concentrations of SiNPs grew, more SiNPs localizing inside would initiate more deleterious cytotoxicity.

It has been suggested that NP–cell interactions may lead to oxidative stress and oxidant injury.³¹ NPs not only induce spontaneous ROS generation at the surface, owing to their chemical and surface characteristics, but also lead to free radical generation after their interaction with cellular constituents and components, eg, mitochondrial damage.³² Indeed, previous studies have reported oxidative stress as the toxic mechanism of SiNPs in various cell types.^33–35 Oxidative stress arises from a significant increase in concentrations of ROS to levels that are toxic to biomolecules like DNA, proteins, and lipids. Subsequently, the abnormal accumulation of intracellular ROS could induce oxidative stress and cause oxidative damage, followed by the production of lipid peroxidation and inhibition of antioxidant activities, resulting in cells failing to maintain normal physiological redox-regulated functions.

Our previous studies suggested oxidative stress induced by SiNPs is possibly mediated by ROS-dependent pathways in hepatocellular carcinoma cells in vitro.²⁷ In the present study, direct measurement of ROS, as well as the induction of MDA, activities of antioxidant enzymes (eg, SOD, GSH-Px), and GSH, provided strong evidence for the involvement of oxidative stress in SiNP-induced toxicity (Figure 3). MDA, one of the final products of lipid oxidation by free radicals and ROS, is commonly known as a marker of oxidative stress. Lipid peroxidation further gave rise to more free radicals, and then damage biomolecules and cause injury to the cell membrane and cytotoxicity in conjunction with ROS, as indicated by an increased level of LDH enzyme release and inhibition of cell viability (Figure 2). Notably, our results demonstrated an increase in either SOD activity or GSH content, inconsistent with some reports finding inhibition of SOD activity and depletion of reduced GSH once oxidative stress occurred. However, the elevated activities of antioxidant enzymes, like SOD and CAT, and a decrease in GSH level were involved in nickel NP-induced oxidative stress in human skin epidermal cells.³⁶ Meanwhile, the increased SOD activity was consistent with its upregulated expression in mRNA levels.

Research has demonstrated that GCL activity can be rapidly increased following exposure to oxidative stress due to an increase in GCL holoenzyme formation.³⁷ Increased expressions of GCLC and GCLM mRNA can be a direct marker of oxidative stress.³⁸ In our study, GCLC was transcriptionally upregulated by SiNPs, which may further increase GSH synthesis. Weldy et al observed increased levels in endothelial GCLC and GCLM as well as total GSH after diesel exhaust-particulate exposure.³⁹ This phenomenon might be correlated with exposure dosage, time, particle size, and other physicochemical properties of NPs, as well as cell type, etc.

NO plays a key role in endothelial function, and endothelial dysfunction is associated with and may contribute to an increased risk of cardiovascular events.⁴⁰ Furthermore, it is very critical in proinflammatory responses, and is overproduced in abnormal physiological conditions. ROS induced by SiNPs may trigger the generation of NO,³⁴ consistent with our data, as reflected in Figure 4. Similarly, Corbalan et al demonstrated that SiNPs penetrate the plasma membrane of endothelial cells and stimulate NO release in vitro.¹⁹ An increase in NO generation can also lead to higher microvascular permeability.⁴¹ Conversely, it has been postulated that the nanomechanics and cytoskeletal rearrangements in endothelial cells result in altered NO production,⁴² consistent with our observed morphological change induced by SiNPs, as shown in Figure 2. Consequently, the process of increased and prolonged NO production leads to depletion of enzymatic substrates and cofactors and uncoupling of eNOS eventually.⁴³ Uncoupled eNOS can generate superoxide anion radical, O₂⁻•,⁴⁴ which rapidly reacts with NO to produce peroxynitrite (ONOO⁻), and change the balance of [NO]/[ONOO⁻] unfavorably. Certainly, the generated ROS like O₂⁻• mediated by SiNPs could also be involved in the production of ONOO⁻ in the presence of NO. ONOO⁻ can further react with CO₂, lipids, etc, to yield the hydroxyl radical •OH and eventually oxidative stress. Another study by Corbalan et al also showed that SiNPs induced a low [NO]/[ONOO⁻] ratio in human platelets, consequently leading to platelet aggregation.⁴⁵ Our previous in vivo study suggested SiNPs could lead to endothelial NO/NOS system disorder followed by endothelial dysfunction.⁴⁶

Upon analysis of endothelial gene expressions, we observed that SiNPs caused a decrease in eNOS mRNA levels while simultaneously upregulating iNOS mRNA expression, as reflected in Figure 4. It was demonstrated that a large amount of NO accumulation produced by iNOS overexpression in damaged tissue forms ONOO⁻.⁴⁷ Moreover, the inhibition of eNOS has been shown to impair microvascular barrier function, characterized by the increase in microvascular fluid and protein flux.^48,49 Simultaneously, the transcriptional regulation of iNOS is largely mediated by the transcription factor NF-κB, whereas the downregulation of eNOS possibly might be due to negative feedback caused by an increase in available NO, likely iNOS-derived.⁵⁰ It is becoming increasingly clear that an imbalance between NO and ET-1 is a characteristic of endothelial dysfunction and important in the progression of vascular disease. Numerous reports have demonstrated an increase in plasma ET-1 as well as its mRNA in the lung and heart after particle exposure.^51–53 However, a previous report showed a decline in ET-1 expression after diesel exhaust-particulate exposure.³⁹ Our observed downregulating effect of SiNPs on ET-1 expression in HUVECs might have been due to NO-mediated inhibition on EDN1 gene expression.⁵⁴

There is a growing body of evidence that SiNPs cause toxic and inflammatory effects due to their unique physicochemical profile.^55–57 At present, the regulatory mechanism regarding inflammation response mediated by SiNPs exposure is not totally understood. It has been confirmed that ROS generated by SiNPs trigger proinflammatory responses.^34,58 Moreover, inflammatory factors are capable of inducing activation of nicotinamide adenine dinucleotide phosphate (NADPH) oxidases and ROS production, subsequently resulting in oxidative stress and impairment in vascular reactivity.^59–61 TNFα plays an important role in the promotion of inflammatory response, IL-1β and IL-8 are important for regulation of inflammatory response, and IL-6 is crucial for induction of acute-phase reactions. Excessive production of any of these factors contributes to harmful inflammatory reactions. Strikingly, we observed that endothelial cells had dramatically increased response to SiNPs for the expressions of IL-1β, -6, and -8 and TNFα, suggesting a robust proinflammatory response occurred after SiNP treatment.

It has been reported that decreased viability of endothelial cells may result in the loss of endothelial cell integrity and an increase in vascular permeability, thus leading to an increase in the migration of monocytes and macrophages into vessels in vivo.^14,62 Monocyte migration and adhesion to endothelial cells are considered to be one of the early events in the initiation of atherosclerosis, which is caused by the upregulation of adhesion molecules in endothelial cells and the increased expression of chemokines.⁶³ SiNPs can significantly augment proinflammatory and procoagulant responses through CD40-CD40L-mediated monocyte–endothelial cell interactions.⁶⁴ VCAM-1 and ICAM-1 contributed to the inflammatory process by facilitating the adhesion of monocytes to endothelial cells. Exposure to SiNPs induces protein expression of ICAM-1 and VCAM-1.⁶⁵ Our data also indicated significantly upregulated mRNA expression in VCAM-1, while ICAM-1 only increased after 12.5 or 25 μg/mL SiNP exposure on HUVECs. Enhanced expression of ICAM-1 was provoked by several kinds of NPs, but varied. For instance, ZnO NPs significantly upregulate ICAM-1 expression at a dose greater than 10 μg/mL,⁶⁶ while such upregulation requires greater than 20 μg/mL for iron oxide NPs in endothelial cells.¹⁴ MCP-1 is known to exacerbate inflammation and has influence on the progression of atherosclerosis.⁶⁷ It can regulate the transmigration of adhered monocytes across the endothelial barrier into the subendothelial layer.⁶⁸ Despite belonging to macrophage-derived factor, MCP-1 mRNA expression in endothelial cells was significantly increased under SiNP exposure once the dosage was greater than 25 μg/mL. Our results suggest that SiNPs may have the potential to initiate monocyte recruitment, adhesion, and migration into the sub-endothelial layer of the intima, representing a considerable risk factor for promoting early events in the development of atherosclerosis.

The role of oxidative stress in inflammatory and endothelial dysfunction is still unclear, but it is a main research area in nanotoxicology. Oxidative stress could trigger the induction of the MAPK signaling pathway, and of transcription factors, such as Nrf2 and NF-κB. These transcription factors could induce mRNA expression of proinflammatory mediators, and finally cause inflammation and related diseases. Therefore, to further elucidate the molecular mechanism of the observed oxidative stress and related physiological alteration by SiNP exposure, the evaluation of toxicity needs to be focused on the oxidative stress-responding signal-transduction pathway (ie, the MAPK pathway) and transcription factors (ie, NF-κB and Nrf2).

Nrf2 has been recognized as a transcription factor that controls mechanisms of cellular defense response against oxidative stress. Under oxidative stress, Nrf2 is stabilized and translocated to the nucleus, where it can transactivate a large battery of antioxidant response element-regulated genes, including endogenous antioxidants (ie, SOD, CAT, GSH-Px, and Trx reductase [TrxR]), phase II detoxifying enzymes (ie, GCL, NAD[P]H:quinone oxidoreductase [NQO]-1, and HO-1), and transporters. The induction of Nrf2 and its downstream gene expression is an adaptive intracellular response to protect against NP-induced oxidative stress and related oxidative damage. For instance, SiNP exposure, which exerts toxic effects, alters the protein regulation of such antioxidant proteins as TrxR in human keratinocyte cells³⁰ and HO-1 in human endothelial cells¹⁷ or human bronchial cells.⁵⁸ Furthermore, human lung fibroblast cells could counteract the oxidative stress induced by SiNPs via the induction of enzymatic activities, such as CAT and GSH S-transferase, an enzyme that catalyzes reactions in order to detoxify peroxidized lipids.⁶⁹ As indicated in Figure 6A, SiNP-induced activation of Nrf2 was observed, which further triggered expressions of antioxidant genes, such as HO1, CAT, TXN1, TXNRD1, and NQO1, to restore oxidative homeostasis. In addition, the GCLC and GCLM genes also contain antioxidant-response elements within their 5′-promoter region, and can be transcriptionally regulated by the activation of Nrf2.^70–72 Therefore, the increase in GCLC mRNA expression might have been Nrf2-mediated, as well as the upregulated SOD mRNA expression referred to in Figure 3F.

To further clarify the possible upstream oxidative signaling pathway involved in Nrf2 activation, we examined MAPK, which is involved in cell survival against oxidative stress through the Nrf2 signaling pathway. The MAPK signaling pathway is classified into three components: ERK1/2, JNK, and p38 MAPK. As seen in Figure 6, SiNPs activated the MAPK signaling pathway via phosphorylation, especially p38 MAPK and JNK. The activation of MAPK signaling molecules could ultimately activate the transcription factor NF-κB,⁷³ suggesting that SiNP-induced upregulated NF-κB expression may occur via the MAPK-Nrf2 signaling pathway. It has been confirmed that the activation of NF-κB and induction of HO-1 via the p38-Nrf2 signaling pathway are involved in oxidative stress induced by ceria NPs,⁷⁴ the ERK-Nrf2 pathway in that by SiNPs in human bronchial epithelial cells,⁵⁸ the p38-Nrf2 pathway in the oxidative damage induced by TiO₂ NPs,^75,76 and the p53 pathway in oxidative stress by ZnO NPs.⁷⁷ Additionally, NF-κB is a known modulator of inflammation, and its activation is responsive to various oxidant stimuli. For the inflammatory process, NF-κB binds to cognate DNA sequences in the regulatory region of genes involved in inflammatory response, leading to release of immunorelated cytotoxic factors (eg, iNOS) and proinflammatory cytokines, as mentioned earlier through κB sites located in their promoter region,⁷⁸ implying the strike inflammation response induced by SiNPs in this study might have been related to NF-κB activation to some extent.

Conclusion

In summary, the present study demonstrated that SiNPs induced ROS generation and caused redox imbalance, oxidative stress, and NO/NOS system disorder, leading to oxidative damage and inflammation response, which consequently resulted in endothelial cytotoxicity and endothelial dysfunction via the MAPK-Nrf2 and NF-κB signaling pathways. Further studies on the mechanisms by which SiNPs induce the MAPK-Nrf2 signaling pathway are warranted to better understand NP-induced cytotoxicity by oxidative stress, as are studies with inhibitors and in vivo animal studies. All in all, our findings suggest that SiNP exposure could be a hazardous factor for vascular homeostasis, and more studies need to focus on SiNP exposure, adverse effects, and biological mechanisms in considering the safety of the application of NPs.

Supplementary material

Table S1.

Real-time PCR primer pairs

Gene name	Description	Primer sequence	Primer size (bp)
NFE2L2	F	ATTGCCTGTAAGTCCTGGTCAT	102
	R	GCTTTTGCCCTAAGTTCATCTC
HMOX1	F	CTTCTTCACCTTCCCCAACAT	109
	R	TTCTATCACCCTCTGCCTGACT
SOD2	F	CGTGACTTTGGTTCCTTTGAC	109
	R	AGTGTCCCCGTTCCTTATTGA
CAT	F	GCCTTTGGCTACTTTGAGGTC	124
	R	AACCCGATTCTCCAGCAAC
GPX	F	CCCAGTCGGTGTATGCCTTC	109
	R	CAGAGGGACGCCACATTCT
NQO1	F	AAGCCGCAGACCTTGTGATA	115
	R	GCAGCGTAAGTGTAAGCAAACT
TXN1	F	CATTTCCATCGGTCCTTACAG	248
	R	ACCCACCTTTTGTCCCTTCTTA
TXNRD1	F	CTCTTGGATAGGAGTTGGTGAA	126
	R	ATGGGCTTGAGACTGGTGACT
GCLC	F	CTCTGCCTATGTGGTGTTTGTG	119
	R	CATCTCTTTTCTGTGCTACCTTCA
GCLM	F	AGTTCCCAAATCAACCCAGAT	236
	R	TCAATAGGAGGTGAAGCAATGA
EDN1	F	GACATCATTTGGGTCAACACTC	121
	R	GGCATCTATTTTCACGGTCTGT
NOS3	F	AGCATCCCTACTCCCACCAG	101
	R	CCTCCCAGTTCTTCACACGA
NOS2	F	AAGCGGAGACCCAAGAGAAG	121
	R	TCGCAAAGAGGATGGTGACT
IL1B	F	CCTGCGTGTTGAAAGATGATAA	174
	R	CTGCTTGAGAGGTGCTGATGTA
IL8	F	CTGTGTGAAGGTGCAGTTTTG	83
	R	GGGTGGAAAGGTTTGGAGTAT
IL6	F	ACAGACAGCCACTCACCTCTTC	170
	R	ATCTTTTTCAGCCATCTTTGGA
TNF	F	TAGCCCATGTTGTAGCAAACC	136
	R	ATGAGGTACAGGCCCTCTGAT
CCL2	F	TCTGTGCCTGCTGCTCATAG	154
	R	CTTGCTGCTGGTGATTCTTCTA
ICAM1	F	GTTGCCTAAAAAGGAGTTGCTC	88
	R	GCACATTGGTTGGCTATCTTCT
VCAM1	F	TGGGAAAAACAGAAAAGAGGTG	238
	R	CTCAAAACTCACAGGGCTCAG
ACTB	F	TGACGTGGACATCCGCAAAG	205
	R	CTGGAAGGTGGACAGCGAGG

Abbreviation: PCR, polymerase chain reaction.