Titanium Dioxide Nanoparticles Induce Mitochondrial Dynamic Imbalance and Damage in HT22 Cells

Zhao, Han; Chen, Liang; Zhong, Guisheng; Huang, Yina; Zhang, Xulai; Chu, Cenfeng; Chen, Lin; Wang, Ming

doi:https://doi.org/10.1155/2019/4607531

Journal of Nanomaterials

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Abstract Introduction Materials and Methods Results Discussion Conclusions Data Availability Conflicts of Interest Acknowledgments Supplementary Materials References Copyright Related Articles

Research Article | Open Access

Volume 2019 | Article ID 4607531 | https://doi.org/10.1155/2019/4607531

Titanium Dioxide Nanoparticles Induce Mitochondrial Dynamic Imbalance and Damage in HT22 Cells

Han Zhao,^1,2Liang Chen,¹Guisheng Zhong,³Yina Huang,^1,2Xulai Zhang,⁴Cenfeng Chu,³Lin Chen,^1,2and Ming Wang^1,2

Academic Editor: Enrico Bergamaschi

Received28 Aug 2018

Revised09 Jan 2019

Accepted16 Jan 2019

Published30 Apr 2019

Abstract

Mitochondria, as dynamic organelles, are precisely regulated by fusion and fission. The dynamic balance of fusion and fission controls mitochondrial morphology and their subcellular location and function. Exposure to titanium dioxide nanoparticles (TiO₂ NPs) may cause serious health problems. However, how TiO₂ NPs affect the mitochondrial dynamics remains unclear. In the present study, we investigated the changes of mitochondrial dynamics in the TiO₂NPs-treated HT22 cells by confocal and stimulated emission depletion (STED) microscopy. The confocal images demonstrated obvious changes in the average length and density of the mitochondria after TiO₂ NPs treatment, while STED images further obtained the nanoscale submitochondrial structures of the mitochondria under TiO₂ NPs insult. The fluorescence intensity distributions suggested that mitochondria fragmented in the TiO₂ NPs-treated cells. TiO₂ NPs treatment caused mitochondrial dynamic imbalance due to the imbalanced expression of dynamin-related protein 1 (Drp1) and optic atrophy 1 (Opa1). Furthermore, we examined the levels of oxidative stress and mitochondrial membrane potential (MMP) and the generation of adenosine triphosphate (ATP), which revealed the damage of mitochondria under TiO₂ NPs exposure. Meanwhile, the significant changes of expressions of B-cell lymphoma 2-associated X protein (Bax), B-cell lymphoma 2 (Bcl-2), cytochrome c (Cyt C), and caspase 9 demonstrated that TiO₂ NPs treatment activated the mitochondrial-related apoptosis pathway. These cellular events can be largely prevented via cell incubation with mitoTEMPO, a mitochondria-targeted superoxide scavenger. Our results confirm that TiO₂ NPs targeted the mitochondria, inducing mitochondrial dynamic imbalance and damage in HT22 cells. Our study provides an insightful understanding of the mechanisms underlying TiO₂ NPs cytotoxicity.

1. Introduction

Titanium dioxide nanoparticles (TiO₂ NPs) have been increasingly used in various applications, such as food additives, sunscreen, cosmetics, toothpastes, and environmental decontamination [1–5]. Studies estimated that annual TiO₂ NPs production was between 5000 and 6400 tons [6, 7]. The expanding usage and the large amounts of TiO₂ NPs being produced raise the risk of environmental exposure. TiO₂ NPs may cause serious health problems. For example, TiO₂ NPs were reported to cause a clear epigenetic alteration in lung fibroblasts [8]. Even gestational exposure to TiO₂ NPs impaired placentation [9]. Previous studies indicated that TiO₂ NPs were able to target the central nervous system and impair the brain [10–14]. Our own work has demonstrated that TiO₂ NPs exposure could affect hippocampal synaptic plasticity, which indicated that hippocampus neurons were susceptible to TiO₂ NPs exposure [15]. It is worth noting that oxidative stress, which is caused by excessive accumulation of reactive oxygen species (ROS), is the main reason for the negative health effects of TiO₂ NPs [16, 17]. Given the fact that mitochondria are the major source of ROS in neurons, mitoTEMPO is specifically targeted to mitochondria and subsequently eliminates mitochondrial superoxide and protects mitochondrial function [18, 19].

Mitochondrial morphology is dynamically regulated by an opposing balance of fusion and fission [20]. In mammalian cells, mitochondrial fusion is mainly regulated by the inner mitochondrial membrane protein, optic atrophy 1 (Opa1) [21]. The dynamin-like guanosine triphosphatase (GTPase), mitofusion 1 (Mfn1), and mitofusion 2 (Mfn2) are involved in mitochondrial fusion [22]. Mitochondrial fission is controlled by dynamin-related protein 1 (Drp1) [23, 24], which is principally scattered in the cytoplasm and passes to the mitochondrial surface [25], inducing fission when overaccumulated around mitochondria. Meanwhile, mitochondrial fission protein 1 (Fis1) promotes the recruitment of Drp1 [26]. In addition, mitochondrial adaptors, such as mitochondrial fission factor (Mff) [27], mitochondrial dynamics proteins 49/51 (MID49/51) [28], and mitochondrial elongation factor 1 (Mef 1) [29], are involved in such process. Additionally, accumulating pieces of evidence indicate that mitochondrial fragmentation resulted from imbalanced fusion and fission and was associated with mitochondrial functional impairment and even cell destruction [30, 31]. However, whether and how TiO₂ NPs affect mitochondrial structure and function still need to be elucidated to better depict the cytotoxicity of TiO₂ NPs.

HT22 cells, derived from primary-cultured mouse hippocampal neurons [32], serve as a cell line of hippocampus neurons of the brain. In this study, we applied the stimulated emission depletion (STED) microscopy technique to study the structure of mitochondria in HT22 cells under TiO₂ NPs insult, since it has the advantage of higher resolution than the conventional confocal microscopy [33, 34].

2. Materials and Methods

2.1. TiO₂ NPs Preparation

oTiO₂ NPs from anatase(Cat. #637254, Sigma-Aldrich, St. Louis, MO, USA) were dispersed in 10 mL of sterile double-distilled water in a centrifuge tube; then, the stock suspensions were ultrasonically treated in a bath sonicator (40 kHz, 60 W) at room temperature for more than 30 minutes before being diluted with culture medium to the specified concentrations (0.032 μg/mL, 0.16 μg/mL, 0.8 μg/mL, 4 μg/mL, and 20 μg/mL). According to a previous study [35], we chose the moderate and even lower doses as suggested above. The TiO₂ NPs suspensions used for the characterization below were dissolved in double-distilled water.

2.2. Characterization

For transmission electron microscopy (TEM) analysis, TiO₂ NPs suspensions were prepared as above. TiO₂ NPs suspensions (0.8 μg/mL and 20 μg/mL, dissolved in double-distilled water) were drop-coated on carbon-coated copper grids. The sample suspensions on the grids were dried out in air before measurement. The tests were performed at an accelerating voltage of 200 kV using a JEOL-2010 TEM (Japan Electron Optics Laboratory, Tokyo, Japan).

TiO₂ NPs suspensions were added to a disposable low volume cuvette (50 μL). The average size distribution and zeta potential of TiO₂ NPs were detected by dynamic light scattering (DLS) using a Zetasizer Nano ZS90 (Malvern Instruments, Malvern, Worcestershire, UK).

2.3. Cell Culture

HT22 cells were from AllCells (Shanghai Biological Technology Co. Ltd., Shanghai, China). We carried out some experiments in the BE(2)C cell line, which is a human neuroblastoma cell line. The cells were planted in Dulbecco’s minimum essential medium (DMEM), added with 10% (/) fetal bovine serum (FBS, qualified, Gibco, Australia origin) at 37°C in a 5% (/) CO₂ incubator. The cells of experimental groups were treated with corresponding concentrations of TiO₂ NPs.

2.4. MitoTEMPO Incubation

MitoTEMPO (2-(2,2,6,6-tetramethylpiperidin-1-oxyl-4-ylamino)-2-oxoethyl)triphenylphosphonium chloride (10 μM, Sigma-Aldrich) was preincubated in cells 1 hour before being stimulated with/without 20 μg/mL of TiO₂ NPs to eliminate the mitochondrial ROS. The experiments consist of four groups (control, TiO₂ NPs, TiO₂ NPs+mitoTEMPO, and mitoTEMPO).

2.5. Confocal Imaging

Cells were cultured with/without TiO₂ NPs for 24 h. The culture medium was wiped off, the cells were washed 3 times with phosphate-buffered saline (PBS), and then the cells were incubated with 500 nM MitoTracker® Red CMXRos (Invitrogen, Pleasanton, CA, USA) at 37°C for 30 min in a 5% (/) CO₂ incubator. The solution was removed, the cells were washed with PBS 3 times, and then the mitochondrial morphology was analyzed with a confocal microscope (ZEISS LSM710, Carl Zeiss, Oberkochen, Germany). NIH ImageJ software (Scion Corporation, Frederick, MD, USA) was used to quantify and measure the fluorescent signals of mitochondrial length and density [36].

2.6. STED Imaging

For submitochondrial structure imaging, STED super-resolution light microscopy was applied. Cells were prepared in the same way for confocal imaging. The cells were incubated with 500 nM MitoTracker® Red CMXRos (Invitrogen) at 37°C for 30 min in the 5% (/) CO₂ incubator. The solution was removed, and the remaining cells were washed with PBS 3 times. A Leica TCS SP8 STED 3x microscope (Leica Microsystems) equipped with a white light pulse laser (WLL2), STED laser (775 nm), oil immersion 100x/NA 1.4 objective lens (HC PL APO CS2, Leica), and TCS SP8 time-gated system was used. Images were acquired in both confocal mode and STED mode with resolution at the same time. The obtained confocal and STED images were further deconvolved with the Huygens Professional software (Scientific Volume Imaging). NIH ImageJ software (Scion Corporation, Frederick, MD, USA) was used to measure the intensity of mitochondrial fluorescent signals. The images were rendered with pseudocolor to distinguish from images rendered only by confocal microscopy.

2.7. Western Blot Analysis

To compare the mitochondrial and cytoplasmic proteins, the Mitochondria Isolation Kit for Cultured Cells (Thermo Fisher Scientific, Waltham, MA) was used to obtain mitochondrial and cytoplasmic proteins. The concentrations of the proteins were estimated by the BCA assay (P0010, Beyotime, Shanghai, China). Then, samples were diluted to the same concentration and boiled in water for 10 min before they were stored at −20°C. Sample proteins were added to 12% sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) gels at 120 V. The separated proteins on the gel were transferred to 0.45 μm polyvinylidene difluoride (PVDF) membranes (Millipore, Billerica, MA, USA) at 300 mA for 45 min. Then, the membranes were incubated with 10% (/) fat-free milk at room temperature for 1 h. The blots were initially incubated overnight at 4°C with the following primary antibodies: anti-extracellular-regulated protein kinases 1/2 (erk1/2) (#9102s, Cell Signaling Technology, Danvers, MA, USA), anti-phospho-erk1/2 (#4376s, Cell Signaling Technology), anti-Drp1 (611113, BD Biosciences, San Diego, CA, USA), anti-opa1 (612606, BD Biosciences), anti-COXIV (ab14744, Abcam, Cambridge, MA, USA), anti-glyceraldehyde-3-phosphate dehydrogenase (GAPDH) (AB2302, Millipore), anti-Cyt C (sc-7159, Santa Cruz Biotechnology Inc., Dallas, TX, USA), anti-caspase 9 (AC062, Beyotime), anti-Bcl-2 (AB112, Beyotime), and anti-Bax (AB026, Beyotime). The following are the secondary antibodies: anti-chicken immnunoglobins of yolk (IgY), HRP conjugate (G135, Promega Corp., Madison, WI, USA), anti-mouse immunoglobulin G (IgG), HRP conjugate (W4021, Promega Corp.), and anti-rabbit IgG, HRP conjugate (W4011, Promega Corp.). NIH ImageJ analysis software (Scion Corporation, Frederick, MD, USA) was used to analyze the density.

2.8. Measurement of Oxidative Stress Markers

To measure the oxidative activity, the levels of ROS, malondialdehyde (MDA), and glutathione (GSH) were evaluated. The experiments were carried out according to protocols provided by each assay kit (Beyotime). Each sample was measured using an automated microplate spectrophotometer (CLARIOstar, BMG LABTECH, Offenburg, Germany). The values of ROS, MDA, and GSH obtained for untreated cells were considered 100%.

2.9. Measurement of Mitochondrial Membrane Potential (MMP)

MMP was measured using rhodamine 123 (Rh-123) staining. Rh-123 (10 μM) was treated to HT22 cells and incubated at 37°C for 30 min. Rh-123 can enter the mitochondrial matrix and the fluorescence strength reflects mitochondrial transmembrane potential. When the excitation wavelength was 480 nm, the fluorescence was analyzed with a fluorescence microplate reader (CLARIOstar, BMG LABTECH, Offenburg, Germany). The values of MMP obtained for untreated cells were considered 100%.

2.10. Measurement of Cellular Concentration of ATP

The release of ATP was assessed using an ATP assay kit (S0026, Beyotime). First, excessive medium was removed. Then, HT22 cells were dissociated with lysis buffer at 4°C. The lysates were centrifuged at 12,000g for 5 minutes, and then the supernatants were collected. ATP concentration was measured using a microplate reader (CLARIOstar, BMG LABTECH, Offenburg, Germany). The values of ATP obtained for untreated cells were considered 100%.

2.11. Hoechst 33342/Propidium Iodide (PI) Analysis

TiO₂ NPs-induced cell death was detected by a Hoechst 33342/PI detection kit (Beyotime). HT22 cells were added with corresponding concentrations of TiO₂ NPs for 24 or 48 h. Firstly, 10 μL of Hoechst 33342 was put into the wells with a total medium of 1 mL (1 : 100) at 37°C for 10 min; then, 5 μL of PI diluted with a total of 1 mL of medium (1 : 200) was put into the wells for another 10 min at room temperature. Fluorescence was measured at both excitation wavelengths of 352 nm and 488 nm using a microscope (Olympus IX81, Tokyo, Japan). Image-Pro Plus 6.0 software (Media Cybernetics Inc., MD, USA) was used to count the cell numbers.

2.12. Annexin V-Fluorescein Isothiocyanate and Propidium Iodide (Annexin V-FITC/PI) Staining

To further assess the effect of TiO₂ NPs on cell apoptosis, an Annexin V-FITC/PI assay was conducted. Cultured HT22 cells were collected 24 or 48 h after TiO₂ NPs exposure. Cells were then resuspended in binding buffer after washing with PBS. The cell suspensions were then treated with both Annexin V-FITC/PI at room temperature for 20 min in the dark. Cell suspensions were analyzed by a FACS Vantage flow cytometer (Becton Dickinson, CA, USA). The results were then analyzed using FlowJo software (FlowJo, OR, USA). Each quadrant indicated the different status of the cells. Q4 indicated surviving cells, Q3 indicated cells in early apoptosis, Q2 indicated cells in late-stage apoptosis, and Q1 indicated dead cells.

2.13. Mitochondrial Superoxide Assay

To monitor mitochondrial superoxide after TiO₂ NPs treatment, MitoSOX Red (5 μM, Invitrogen) was loaded into the cells that were treated with/without TiO₂ NPs for 24 h. After removing the culture medium and washing twice, the solution of MitoSOX Red diluted in HBSS/Ca/Mg was added into HT22 cells at 37°C for 10 min in the dark. The cells were washed twice with prewarmed HBSS/Ca/Mg to remove the excessive probes. To avoid saturation by excessive oxidation, all MitoSOX experiments were completed within 30 min of loading. Each sample was measured using an automated microplate spectrophotometer (CLARIOstar, BMG LABTECH, Offenburg, Germany). The excited wavelength of MitoSOX Red is 510 nm, and the emitted wavelength is 580 nm. The values of MitoSOX Red obtained for untreated cells were considered 100%. The images of MitoSOX Red and Hoechst33342 costaining were collected using a microscope (Olympus IX81, Tokyo, Japan). The intensity was subsequently analyzed by using NIH ImageJ software.

2.14. Statistical Analysis

All experiments were conducted at least three times. The statistical results are expressed as the error (SE). The data were analyzed with one-way analysis of variance followed by Bonferroni’s post hoc comparisons test using Origin Pro 8.0 (OriginLab Corporation, MA, USA). The differences were considered statistically significant when . The graphs were drawn using Origin Pro 8.0.

3. Results

3.1. Characterization of TiO₂ NPs

The particle size of the TiO₂ NPs was observed by TEM after dissolution in water. TiO₂ NPs were dispersed at a low concentration (0.8 μg/mL) and agglomerated at a high concentration (20 μg/mL) in the water (Figures 1(a) and 1(b)). According to DLS results, the -average of TiO₂ NPs in the water was nm (Figure 1(c)), which meant that the hydrodynamic diameter of TiO₂ NPs was much larger than the size revealed by TEM. The size distribution (PDI) was . The surface zeta potential of TiO₂ NPs (pH 7.86) was (Figure 1(d)), showing a negative surface charge in the water. The results were consistent with the findings in the previous study [37].

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3.2. TiO₂ NPs-Induced Mitochondrial Fragmentation

The mitochondrial morphology would change from normal to fragmented in pathological conditions. As shown in Figures 2(a) and 2(b), control cells showed normal mitochondria, while cells under TiO₂ NPs treatment showed fragmented mitochondrial structures, suggesting that the mitochondria were promoted to the fission state by TiO₂ NPs exposure. Mitochondrial density in whole cells was reduced in the TiO₂ NPs-treated groups compared with that in control cells (Figure 2(c)). Moreover, mitochondrial length was significantly shorter in the TiO₂ NPs-treated cell than that in control cells (Figure 2(d)). We found that mitochondrial fragmentation in the TiO₂ NPs-treated cells (20 μg/mL) could largely be prevented by mitoTEMPO incubation (Supplementary Figure 1). The similar results were shown in BE2C cell (Supplementary Figure 2).

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3.3. Submitochondrial Structures in Mitochondria

Compared with the length of the mitochondrial tubules shown in confocal microscopy, STED images further obtained the nanoscale submitochondrial structures of the mitochondria. Diffraction-limited confocal microscopy demonstrated that mitochondrial tubules were largely homogenously stained, and the mitochondrial tubules were shorter in the TiO₂ NPs-treated cells than in control cells (Figure 3(a)). Besides, the STED images showed the complex and lamellar submitochondrial structure in the control group and diffused and distributed submitochondrial structure in the TiO₂ NPs-treated groups, with short flaked and punctate spots (Figures 3(b) and 3(c)). Then, the fluorescence intensity distributions of submitochondrial structures along long axis of mitochondria show that the peaks of intensity were focused in the control group, but there were many peaks in the TiO₂ NPs-treated groups (Figures 3(d)–3(f)).

Figure 3

STED super-resolution microscopy revealed submitochondrial structures. (a) Confocal microscopy of mitochondria in control, 0.8 μg/mL, and 20 μg/mL groups. (b) STED super-resolution microscopy revealed submitochondrial structures of the same region using confocal microscopy. (c) Enlarged views of the white boxes in (b). (d–f) Averaged intensity distribution along the mitochondrial tubule sections in the corresponding red boxes in (c). Scale bars: 5 μm in (a) and (b); 1 μm in (c).

3.4. TiO₂ NPs Induced Imbalanced Expression of Mitochondrial Fission/Fusion Protein

Mitochondria and cytoplasmic proteins were independently isolated for Western blot analysis. As shown in Figure 4(a), Drp1 translocated to the mitochondria at a high concentration of TiO₂ NPs exposure, while Opa1 in mitochondria was decreased (Figure 4(b), ). For cytoplasmic proteins, there were no significant differences in Drp1 or Opa1 in the experimental groups (Figure 4(b), ). This demonstrated that TiO₂ NPs treatment in HT22 cells led to the accumulation of Drp1 to mitochondria while Opa1 was decreased, which may cause excessive mitochondrial fission. These results are consistent with the morphological changes of mitochondria. The imbalanced expression of dynamin-related protein 1 (Drp1) and optic atrophy 1 (Opa1) could largely be prevented by mitoTEMPO incubation (Supplementary Figure 3).

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3.5. ROS Generation and Oxidative Stress Levels

The induction of intracellular oxidation was measured using a 2,7-dichlorodihydrofluorescein diacetate (DCF-DA) probe to report ROS generation. Cells treated with TiO₂ NPs exhibited increased fluorescence intensity when compared to the control (Figure 5(a), ). Some other parameters connected with oxidative stress, such as the levels of MDA or GSH, were tested as well. MDA serves as a marker of lipid peroxidation. Its level determines the degree of damage to the membrane system. The results showed that MDA levels were significantly higher in the TiO₂ NPs-treated group than in the control group (Figure 5(b), ). GSH concentration directly reflects tissue antioxidant levels. There was a significant decrease in the level of GSH in the TiO₂ NPs-treated group compared to that in the control group (Figure 5(c), ). These results clearly indicated that the oxidative stress level was elevated in the TiO₂ NPs-treated cells. Furthermore, we examined oxidative stress (e.g., ROS, MDA, and GSH), which indicated that the oxidative stress under TiO₂ NPs exposure can be reversed by mitoTEMPO incubation (Supplementary Figure 4 A–C).

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Considering that mitochondria are vital ROS formation organelles, we further tested mitochondrial ROS generation in HT22 cells. The MitoSOX Red probe was used to detect the mitochondrial superoxide levels. The intensity of the MitoSOX Red fluorescence is proportionate to the abundance of the superoxide. To determine whether the application of mitoTEMPO attenuates TiO₂ NPs-mediated mitochondrial ROS overproduction, HT22 cells were exposed with/without TiO₂ NPs in the absence or presence of mitoTEMPO. Cells were pretreated with mitoTEMPO for 1 h before the addition of TiO₂ NPs. A significantly increased MitoSOX Red intensity was detected in the TiO₂ NPs-treated group in the absence of mitoTEMPO, while the TiO₂ NPs-induced elevation of the mitochondrial superoxide was markedly attenuated by mitoTEMPO (Figure 6). The application of mitoTEMPO itself did not alter mitochondrial superoxide production (Figure 6). Similar results were shown in the BE2C cell (Supplementary Figure 5).

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3.6. Loss of Mitochondrial Membrane Potential and ATP

It is well known that ROS aggregation damages mitochondrial function. Mitochondrial function was further explored under TiO₂ NPs insult. The loss of MMP was assessed using a 5,5,6,6-tetrachloro-1,1,3,3-tetraethyl-imidacarbocyanine iodide (JC-1) assay kit, which showed that at a high concentration (20 μg/mL) of TiO₂ NPs, MMP was significantly reduced in the HT22 cells (Figure 5(d), ). The production of ATP was estimated with an ATP assay kit. It was found that TiO₂ NPs treatment significantly decreased ATP production at high concentrations (20 μg/mL) (Figure 5(e), ). Furthermore, we examined mitochondrial membrane potential and the generation of ATP, which showed that the damage of mitochondrial function under TiO₂ NPs exposure can be reversed by mitoTEMPO incubation (Supplementary Figures 4D and 4E).

3.7. TiO₂ NPs-Induced Cytotoxicity

Hoechst 33342/PI staining assays can distinguish dead cells. Hoechst 33342 can go across the cell membrane of normal cells and apoptotic cells showing blue fluorescence under ultraviolet light, while PI can go across the cell membrane of the necrotic cells to produce red fluorescence (Figures 7(a), 7(b), and 7(c)). With increasing concentrations of TiO₂ NPs, the red fluorescence became stronger, indicating a higher proportion of dead cells at both 24 and 48 h (Figure 7(d), ). Hoechst 33342/propidium iodide (PI) analysis suggested that mitoTEMPO incubation can reverse the ratio of dead cells (Supplementary Figure 6). Similar results were shown in BE2C cells (Supplementary Figure 7).

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Figure 7

Cytotoxicity induced by TiO₂ NPs treatment. (a–d) Cell death caused by TiO₂ NPs treatment in HT22 cells estimated by Hoechst 33342/PI staining. Typical fluorescence microscopy images of the control group and the groups treated with various concentrations of TiO₂ NPs: (a) Hoechst 33342 (blue); (b) PI (red); (c) merged. (d) The proportion of dead cells after being treated for 24 and 48 h (, , and ). (e) Apoptosis and necrosis caused by TiO₂ NPs treatment in HT22 cells. Representative flow cytometry data of TiO₂ NPs-treated HT22 cells showing the ratio of late apoptotic cells and early apoptotic cells in Q2 and Q3 for 24 h and 48 h. FITC: fluorescein isothiocyanate; PI: propidium iodide.

To quantify the apoptosis of HT22 cells after TiO₂ NPs treatment, Annexin V-FITC/PI double staining was conducted. The results showed an increase in apoptotic and necrotic cells when treated with TiO₂ NPs for 24 h (Figure 7(e)). The trend was similar when treated for 48 h (Figure 7(e)).

3.8. TiO₂ NPs-Induced Specific Expression of Mitochondrial-Related Apoptosis Proteins

To explore the underlying mechanisms responsible for apoptosis induced by TiO₂ NPs, the expression levels of Bcl-2, Bax, and caspase 9, as well as mitochondrial Cyt C were examined. As shown in Figure 8(a), there was a significant increase in the expression of caspase 9 and Bax, while a decrease of Bcl-2 and Cyt C in the TiO₂ NPs-treated HT22 cells can be found (Figure 8(b), ). The expression of p-ERK was increased in the TiO₂ NPs-treated cells (Figure 8(b), ). The significant changes of expressions of Bax, Bcl-2, Cyt C, caspase 9, and p-ERK caused by TiO₂ NPs treatment could largely be reversed by mitoTEMPO incubation (Supplementary Figure 8).

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Figure 8

Effects of TiO₂ NPs on apoptosis-related proteins. (a) Representative Western blot bands of apoptosis-related proteins in control cells and cells treated with TiO₂ NPs for 24 h. (b) Blot analysis of TiO₂ NPs-induced apoptotic protein expressions in HT22 cells ( and ). Bax: B-cell lymphoma 2-associated X protein; Bcl-2: B-cell lymphoma 2; COXIV: cytochrome c oxidase IV; Cyt C: cytochrome c; t-Erk: total extracellular-regulated protein kinases; p-Erk: phosphorylated extracellular-regulated protein kinases; GAPDH: glyceraldehyde-3-phosphate dehydrogenase; ERK1/2: extracellular-regulated protein kinases 1/2.

4. Discussion

Mitochondria have been conventionally studied by biochemical, genetic, and electron microscopic approaches. To investigate mitochondrial dynamics under TiO₂ NPs treatment, live-cell fluorescence microscopy was used as an indispensable tool to elucidate the mitochondrial dynamics. In this study, confocal microcopy was firstly used to observe the mitochondrial morphology. Though the mitochondrial tubules were largely homogenously stained in the sole confocal image, obvious differences in the length and density of the mitochondria were discovered in the cells after TiO₂ NPs treatment. STED was further employed to obtain the images of nanoscale submitochondrial structures of the mitochondria. As the appearance of fluorescence represents the location of the mitochondria, the normalized variance values represented the distribution of mitochondrial fragmentation. The more peak values in the TiO₂ NPs-treated group indicated more fragmentation. Other mitochondrial fluorescent stains could be used to label the mitochondria, such as tetramethylrhodamine methyl ester (TMRM) [34], rhodamine 123 [38], and 5,5,6,6-tetrachloro-1,1,3,3-tetraethylbenzimidazolylcarbocyanine iodide (JC-1) [39]. Here, we only explored the mitochondria itself. It is more persuasive to make a thorough inquiry of mitochondrial proteins, such as mitochondrial translocase of the outer membrane (TOM 20) complex [40], mitochondrial inner membrane organizing system (MINOS) [33], and voltage-dependent anion channel 1 (VDAC1), an outer mitochondrial membrane protein [41]. STED is a novel approach to explore the submitochondrial structures, providing a new method for deep investigations of nanoparticle toxicity in the future.

Keeping a balance of fusion and fission controls mitochondrial morphology and their subcellular location and function [42]. Once the balance is disturbed, it restricts mitochondrial movement, reduces energy production, increases oxidative stress, and promotes cell functional disorder and cell death [23, 43]. Additionally, accumulating evidence indicates that mitochondrial fragmentation resulted from an imbalanced fusion and fission and is associated with abnormal mitochondrial function and cell destruction [30, 31]. When apoptosis is induced, Drp1 leaves the cytosol and passes to the membrane of mitochondria [44]. In our study, p-Drp1 was increased after TiO₂ NPs exposure. Studies have reported that Drp1 has a critical effect on mitochondrial fragmentation, and excessive expression of Drp1 can cause mitochondrial fragmentation, while down expression slows the mitochondrial fragmentation and reduces cell damage [44, 45]. So, Drp1 plays a vital role in preserving the dynamic balance of mitochondria. In the current study, the change of mitochondrial morphology supports the observation that the expression of fusion/fission proteins was altered under TiO₂ NPs exposure, as normal control cells showed normal mitochondrial length, while TiO₂ NPs reduced the mitochondrial length. Our results demonstrate that TiO₂ NPs affect mitochondrial dynamics via the expression of fusion/fission proteins, leading to mitochondrial fragmentation.

Erk1/2 are widely expressed extracellular-regulated protein kinases that take part in regulating cell proliferation and differentiation, cell morphology maintenance, cytoskeleton construction, cell apoptosis, and cell carcinogenesis. A study has shown significant increases of phospho-ERK in neurodegenerative dopaminergic neurons [46]. The activation of ERK1/2 is involved in mitochondrial dynamic disorder by regulating Drp1 phosphorylation at Ser616 and Drp1 translocation [47]. The inhibition of ERK1/2 phosphorylation can protect mitochondrial morphology and dynamic balance [36]. Here, we explored the possibility of using the ERK protein in mitochondrial dynamic disorder induced by TiO₂ NPs. Western blot data demonstrated that the p-ERK expression was significantly increased in cells by high TiO₂ NPs exposure. Maybe, the p-ERK is involved in regulating Drp1 function, and ERK1/2 phosphorylation might promote Drp1 recruitment to mitochondria; then, the ERK-Drp1 signaling pathway could affect the mitochondria through fusion/fission balance to prevent excessive fission procedures.

Oxidative stress is the result of the overaccumulation of ROS and a deficient antioxidant defense [4, 48–50]. Oxidative stress could damage DNA, which could result in the loss of cell viability in the central nervous system [51, 52]. ROS participates in many cellular activities, including cell proliferation, cell growth, and cell apoptosis [53]. TiO₂ NPs treatment caused excessive ROS production and reduced antioxidant defense, resulting in cell death at last. The increased ROS accumulation may reduce the mitochondrial membrane potential [54–56]. Besides, the reduced mitochondrial membrane potential can trigger mitochondrial fragmentation [57]. Emerging evidence suggests that ROS accumulation may cause mitochondrial fragmentation through the alteration of mitochondrial dynamics [58]. Damage to the integrity of mitochondrial morphology leads to ROS accumulation and induces oxidative stress [59, 60]. Studies have also demonstrated that Drp1 has a vital role in TiO₂ NPs-induced ROS accumulation and mitochondrial membrane potential reduction [47]. So, in our study, Drp1 overexpression caused the imbalance of mitochondrial fission/fusion proteins, resulting in mitochondrial fragmentation, which further led to ROS accumulation and MMP collapse. Meanwhile, ROS accumulation and MMP collapse may in turn aggravate mitochondrial fragmentation. This interaction may lead to cell apoptosis under TiO₂ NPs exposure.

5. Conclusions

In summary, our study demonstrates that TiO₂ NPs exposure induced mitochondrial dynamic imbalance and damaged mitochondrial function, as evidenced by increased ROS production and reduced mitochondrial membrane potential and mitochondrial ATP production. This observation was accompanied by the increased cell apoptosis under TiO₂ NPs insult. These cellular events can be largely prevented via cell incubation with mitoTEMPO. Our findings demonstrate the effects of TiO₂ NPs on mitochondrial dynamics and partly illustrate the underlying mechanisms of TiO₂ NPs cytotoxicity.

Data Availability

The data used to support the findings of this study are available from the corresponding authors upon request.

Conflicts of Interest

The authors report no conflicts of interest in this work.

Acknowledgments

This work was supported by the National Natural Science Foundation of China (Grants 81870723, 81570915, and 81371503) and the National Basic Research Program of China (Grants 2012CB932502 and 2011CB504506).

Supplementary Materials

Supplementary 1. Supplementary Figure 1: mitoTEMPO reverses mitochondrial fragmentation caused by TiO₂ NPs exposure in HT22 cells. (A) Representative confocal images of mitochondria. (B) The average length of the mitochondria in entire cells and quantification of the size of mitochondria according to the grouped differently sized bins. cells/group. ( vs. the control group and vs. the TiO₂ NPs group.)

Supplementary 2. Supplementary Figure 2: mitoTEMPO reverses mitochondrial fragmentation caused by TiO₂ NPs exposure in BE2C cells. (A) Representative confocal images of mitochondria. (B) The average length of the mitochondria in entire cells and quantification of the size of mitochondria according to the grouped differently sized bins. cells/group. ( vs. the control group and vs. the TiO₂ NPs group.)

Supplementary 3. Supplementary Figure 3: mitoTEMPO largely prevents the imbalanced expression of Drp1 and Opa1 caused by TiO₂ NPs exposure in HT22 cells. (A) Representative Western blot bands of Drp1 and Opa1 from mitochondrial and cytoplasmic proteins. (B) The quantification of the expressions of Drp1 and Opa1 from mitochondrial and cytoplasmic proteins. ( vs. the control group and vs. the TiO₂ NPs group.) Drp1: dynamin-related protein 1; Opa1: optic atrophy 1; COXIV: cytochrome c oxidase IV; GAPDH: glyceraldehyde-3-phosphate dehydrogenase.

Supplementary 4. Supplementary Figure 4: mitoTEMPO reverses oxidative stress, mitochondrial membrane potential, and the production of ATP caused by TiO₂ NPs treatment in HT22 cells. (A) ROS levels, (B) MDA levels, (C) GSH levels, (D) MMP, (E) ATP production, and (F) MitoSOX Red intensity ( vs. the control group, vs. the control group, vs. the TiO₂ NPs group, and vs. the TiO₂ NPs group.) ROS: reactive oxygen species; MDA: malondialdehyde; GSH: reduced glutathione hormone; MMP: mitochondrial membrane potential; ATP: adenosine triphosphate.

Supplementary 5. Supplementary Figure 5: mitoTEMPO suppresses TiO₂ NPs-induced mitochondrial superoxide production in BE2C cells. (A) Representative images of MitoSOX Red (red) and Hoechst 33342 (blue) staining. (B) The statistics of the fluorescence intensity. (C) The fluorescence intensity of MitoSOX Red using an automated microplate spectrophotometer. ( vs. the control group, vs. the TiO₂ NPs group, and vs. the TiO₂ NPs group.)

Supplementary 6. Supplementary Figure 6: mitoTEMPO reverses the ratio of PI-positive cells in HT22 cells by Hoechst 33342/PI staining. (A) Typical fluorescence microscopy images of the control group, TiO₂ NPs group, TiO₂ NPs+mitoTEMPO group, and mitoTEMPO group. Upper row: Hoechst 33342 (red); middle row: PI (blue); bottom row: merged. (B) The proportion of PI-positive cells treated with TiO₂ NPs for 24 h. ( vs. the control group and vs. the TiO₂ NPs group.)

Supplementary 7. Supplementary Figure 7: mitoTEMPO reverses the ratio of PI-positive cells in BE2C cells by Hoechst 33342/PI staining. (A) Typical fluorescence microscopy images of the control group, TiO₂ NPs group, TiO₂ NPs+mitoTEMPO group, and mitoTEMPO group. Upper row: Hoechst 33342 (red); middle row: PI (blue); bottom row: merged. (B) The proportion of PI-positive cells treated with TiO₂ NPs for 24 h. ( vs. the control group and vs. the TiO₂ NPs group.)

Supplementary 8. Supplementary Figure 8: mitoTEMPO prevents the changes of apoptosis-related proteins caused by TiO₂ NPs in HT22 cells. (A) Representative Western blotbands of apoptosis-related proteins. (B) Blot analysis of apoptotic protein expressions in HT22 cells. ( vs. the control group, vs. the control group, and vs. the TiO₂ NPs group.) Bax: B-cell lymphoma 2-associated X protein; Bcl-2: B-cell lymphoma 2; COXIV: cytochrome c oxidase IV; Cyt C: cytochrome c; t-Erk: total extracellular-regulated protein kinases; p-Erk: phosphorylated extracellular-regulated protein kinases; GAPDH: glyceraldehyde-3-phosphate dehydrogenase; ERK1/2: extracellular-regulated protein kinases 1/2.

References

H. Choi, E. Stathatos, and D. D. Dionysiou, “Sol-gel preparation of mesoporous photocatalytic TiO₂ films and TiO₂/Al₂O₃ composite membranes for environmental applications,” Applied Catalysis B: Environmental, vol. 63, no. 1-2, pp. 60–67, 2006.
View at: Publisher Site | Google Scholar
C. R. Esterkin, A. C. Negro, O. M. Alfano, and A. E. Cassano, “Air pollution remediation in a fixed bed photocatalytic reactor coated with TiO₂,” AICHE Journal, vol. 51, no. 8, pp. 2298–2310, 2005.
View at: Publisher Site | Google Scholar
T. Kaida, K. Kobayashi, M. Adachi, and F. Suzuki, “Optical characteristics of titanium oxide interference film and the film laminated with oxides and their applications for cosmetics,” Journal of Cosmetic Science, vol. 55, no. 2, pp. 219-220, 2004.
View at: Google Scholar
T. C. Long, N. Saleh, R. D. Tilton, G. V. Lowry, and B. Veronesi, “Titanium dioxide (P25) produces reactive oxygen species in immortalized brain microglia (BV2): implications for nanoparticle neurotoxicity,” Environmental Science & Technology, vol. 40, no. 14, pp. 4346–4352, 2006.
View at: Publisher Site | Google Scholar
T. Xia, M. Kovochich, and A. Nel, “The role of reactive oxygen species and oxidative stress in mediating particulate matter injury,” Clinics in Occupational and Environmental Medicine, vol. 5, no. 4, pp. 817–836, 2006.
View at: Publisher Site | Google Scholar
N. C. Mueller and B. Nowack, “Exposure modeling of engineered nanoparticles in the environment,” Environmental Science & Technology, vol. 42, no. 12, pp. 4447–4453, 2008.
View at: Publisher Site | Google Scholar
C. O. Robichaud, A. E. Uyar, M. R. Darby, L. G. Zucker, and M. R. Wiesner, “Estimates of upper bounds and trends in nano-TiO₂ production as a basis for exposure assessment,” Environmental Science & Technology, vol. 43, no. 12, pp. 4227–4233, 2009.
View at: Publisher Site | Google Scholar
N. A. Patil, W. N. Gade, and D. D. Deobagkar, “Epigenetic modulation upon exposure of lung fibroblasts to TiO₂ and ZnO nanoparticles: alterations in DNA methylation,” International Journal of Nanomedicine, vol. 11, pp. 4509–4519, 2016.
View at: Publisher Site | Google Scholar
L. Zhang, X. Xie, Y. Zhou et al., “Gestational exposure to titanium dioxide nanoparticles impairs the placentation through dysregulation of vascularization, proliferation and apoptosis in mice,” International Journal of Nanomedicine, vol. 13, pp. 777–789, 2018.
View at: Publisher Site | Google Scholar
J. Wang, G. Zhou, C. Chen et al., “Acute toxicity and biodistribution of different sized titanium dioxide particles in mice after oral administration,” Toxicology Letters, vol. 168, no. 2, pp. 176–185, 2007.
View at: Publisher Site | Google Scholar
J. Wang, Y. Liu, F. Jiao et al., “Time-dependent translocation and potential impairment on central nervous system by intranasally instilled TiO₂ nanoparticles,” Toxicology, vol. 254, no. 1-2, pp. 82–90, 2008.
View at: Publisher Site | Google Scholar
J. X. Wang, C. Y. Chen, H. W. Yu et al., “Distribution of TiO₂ particles in the olfactory bulb of mice after nasal inhalation using microbeam SRXRF mapping techniques,” Journal of Radioanalytical and Nuclear Chemistry, vol. 272, no. 3, pp. 527–531, 2007.
View at: Publisher Site | Google Scholar
J. Wang, C. Chen, Y. Liu et al., “Potential neurological lesion after nasal instillation of TiO₂ nanoparticles in the anatase and rutile crystal phases,” Toxicology Letters, vol. 183, no. 1-3, pp. 72–80, 2008.
View at: Publisher Site | Google Scholar
J. Wu, W. Liu, C. Xue et al., “Toxicity and penetration of TiO₂ nanoparticles in hairless mice and porcine skin after subchronic dermal exposure,” Toxicology Letters, vol. 191, no. 1, pp. 1–8, 2009.
View at: Publisher Site | Google Scholar
X. Gao, S. Yin, M. Tang et al., “Effects of developmental exposure to TiO₂ nanoparticles on synaptic plasticity in hippocampal dentate gyrus area: an in vivo study in anesthetized rats,” Biological Trace Element Research, vol. 143, no. 3, pp. 1616–1628, 2011.
View at: Publisher Site | Google Scholar
A. Nel, T. Xia, L. Madler, and N. Li, “Toxic potential of materials at the nanolevel,” Science, vol. 311, no. 5761, pp. 622–627, 2006.
View at: Publisher Site | Google Scholar
T. Xia, M. Kovochich, J. Brant et al., “Comparison of the abilities of ambient and manufactured nanoparticles to induce cellular toxicity according to an oxidative stress paradigm,” Nano Letters, vol. 6, no. 8, pp. 1794–1807, 2006.
View at: Publisher Site | Google Scholar
H. L. Liang, F. Sedlic, Z. Bosnjak, and V. Nilakantan, “SOD1 and MitoTEMPO partially prevent mitochondrial permeability transition pore opening, necrosis, and mitochondrial apoptosis after ATP depletion recovery,” Free Radical Biology & Medicine, vol. 49, no. 10, pp. 1550–1560, 2010.
View at: Publisher Site | Google Scholar
H. Hu and M. Li, “Mitochondria-targeted antioxidant mitotempo protects mitochondrial function against amyloid beta toxicity in primary cultured mouse neurons,” Biochemical and Biophysical Research Communications, vol. 478, no. 1, pp. 174–180, 2016.
View at: Publisher Site | Google Scholar
D. C. Chan, “Mitochondrial fusion and fission in mammals,” Annual Review of Cell and Developmental Biology, vol. 22, no. 1, pp. 79–99, 2006.
View at: Publisher Site | Google Scholar
C. Delettre, G. Lenaers, J. M. Griffoin et al., “Nuclear gene OPA1, encoding a mitochondrial dynamin-related protein, is mutated in dominant optic atrophy,” Nature Genetics, vol. 26, no. 2, pp. 207–210, 2000.
View at: Publisher Site | Google Scholar
T. Koshiba, S. A. Detmer, J. T. Kaiser, H. Chen, J. McCaffery, and D. C. Chan, “Structural basis of mitochondrial tethering by mitofusin complexes,” Science, vol. 305, no. 5685, pp. 858–862, 2004.
View at: Publisher Site | Google Scholar
I. Scott and R. J. Youle, “Mitochondrial fission and fusion,” Essays in Biochemistry, vol. 47, pp. 85–98, 2010.
View at: Publisher Site | Google Scholar
D. C. Chan, “Mitochondria: dynamic organelles in disease, aging, and development,” Cell, vol. 125, no. 7, pp. 1241–1252, 2006.
View at: Publisher Site | Google Scholar
E. Smirnova, L. Griparic, D. L. Shurland, and A. M. van der Bliek, “Dynamin-related protein Drp1 is required for mitochondrial division in mammalian cells,” Molecular Biology of the Cell, vol. 12, no. 8, pp. 2245–2256, 2001.
View at: Publisher Site | Google Scholar
Y. Yoon, E. W. Krueger, B. J. Oswald, and M. A. McNiven, “The mitochondrial protein hFis1 regulates mitochondrial fission in mammalian cells through an interaction with the dynamin-like protein DLP1,” Molecular and Cellular Biology, vol. 23, no. 15, pp. 5409–5420, 2003.
View at: Publisher Site | Google Scholar
H. Otera, C. Wang, M. M. Cleland et al., “Mff is an essential factor for mitochondrial recruitment of Drp1 during mitochondrial fission in mammalian cells,” The Journal of Cell Biology, vol. 191, no. 6, pp. 1141–1158, 2010.
View at: Publisher Site | Google Scholar
C. S. Palmer, L. D. Osellame, D. Laine, O. S. Koutsopoulos, A. E. Frazier, and M. T. Ryan, “MiD49 and MiD51, new components of the mitochondrial fission machinery,” EMBO Reports, vol. 12, no. 6, pp. 565–573, 2011.
View at: Publisher Site | Google Scholar
J. Zhao, T. Liu, S. Jin et al., “Human MIEF1 recruits Drp1 to mitochondrial outer membranes and promotes mitochondrial fusion rather than fission,” The EMBO Journal, vol. 30, no. 14, pp. 2762–2778, 2011.
View at: Publisher Site | Google Scholar
J. Grohm, N. Plesnila, and C. Culmsee, “Bid mediates fission, membrane permeabilization and peri-nuclear accumulation of mitochondria as a prerequisite for oxidative neuronal cell death,” Brain, Behavior, and Immunity, vol. 24, no. 5, pp. 831–838, 2010.
View at: Publisher Site | Google Scholar
J. Estaquier and D. Arnoult, “Inhibiting Drp1-mediated mitochondrial fission selectively prevents the release of cytochrome c during apoptosis,” Cell Death and Differentiation, vol. 14, no. 6, pp. 1086–1094, 2007.
View at: Publisher Site | Google Scholar
J. Liu, L. Li, and W. Z. Suo, “HT22 hippocampal neuronal cell line possesses functional cholinergic properties,” Life Sciences, vol. 84, no. 9-10, pp. 267–271, 2009.
View at: Publisher Site | Google Scholar
D. C. Jans, C. A. Wurm, D. Riedel et al., “STED super-resolution microscopy reveals an array of MINOS clusters along human mitochondria,” Proceedings of the National Academy of Sciences of the United States of America, vol. 110, no. 22, pp. 8936–8941, 2013.
View at: Publisher Site | Google Scholar
M. Ishigaki, M. Iketani, M. Sugaya et al., “STED super-resolution imaging of mitochondria labeled with TMRM in living cells,” Mitochondrion, vol. 28, pp. 79–87, 2016.
View at: Publisher Site | Google Scholar
H. Shi, R. Magaye, V. Castranova, and J. Zhao, “Titanium dioxide nanoparticles: a review of current toxicological data,” Particle and Fibre Toxicology, vol. 10, no. 1, p. 15, 2013.
View at: Publisher Site | Google Scholar
X. Gan, S. Huang, L. Wu et al., “Inhibition of ERK-DLP1 signaling and mitochondrial division alleviates mitochondrial dysfunction in Alzheimer’s disease cybrid cell,” Biochimica et Biophysica Acta (BBA) - Molecular Basis of Disease, vol. 1842, no. 2, pp. 220–231, 2014.
View at: Publisher Site | Google Scholar
S. Hussain, L. C. Thomassen, I. Ferecatu et al., “Carbon black and titanium dioxide nanoparticles elicit distinct apoptotic pathways in bronchial epithelial cells,” Particle and Fibre Toxicology, vol. 7, no. 1, p. 10, 2010.
View at: Publisher Site | Google Scholar
M. K. Miah, I. H. Shaik, U. Bickel, and R. Mehvar, “Effects of hepatic ischemia-reperfusion injury on the P-glycoprotein activity at the liver canalicular membrane and blood-brain barrier determined by in vivo administration of rhodamine 123 in rats,” Pharmaceutical Research, vol. 31, no. 4, pp. 861–873, 2014.
View at: Publisher Site | Google Scholar
B. Chazotte, “Labeling mitochondria with JC-1,” Cold Spring Harbor Protocols, vol. 2011, no. 9, 2011.
View at: Publisher Site | Google Scholar
C. A. Wurm, D. Neumann, M. A. Lauterbach et al., “Nanoscale distribution of mitochondrial import receptor Tom20 is adjusted to cellular conditions and exhibits an inner-cellular gradient,” Proceedings of the National Academy of Sciences of the United States of America, vol. 108, no. 33, pp. 13546–13551, 2011.
View at: Publisher Site | Google Scholar
H. Singh, R. Lu, P. F. G. Rodríguez et al., “Visualization and quantification of cardiac mitochondrial protein clusters with STED microscopy,” Mitochondrion, vol. 12, no. 2, pp. 230–236, 2012.
View at: Publisher Site | Google Scholar
L. M. Westrate, J. A. Drocco, K. R. Martin, W. S. Hlavacek, and J. P. MacKeigan, “Mitochondrial morphological features are associated with fission and fusion events,” PLoS One, vol. 9, no. 4, article e95265, 2014.
View at: Publisher Site | Google Scholar
A. Jahani-Asl, M. Germain, and R. S. Slack, “Mitochondria: joining forces to thwart cell death,” Biochimica et Biophysica Acta (BBA) - Molecular Basis of Disease, vol. 1802, no. 1, pp. 162–166, 2010.
View at: Publisher Site | Google Scholar
K. W. Young, L. G. P. Piñon, E. T. W. Bampton, and P. Nicotera, “Different pathways lead to mitochondrial fragmentation during apoptotic and excitotoxic cell death in primary neurons,” Journal of Biochemical and Molecular Toxicology, vol. 24, no. 5, pp. 335–341, 2010.
View at: Publisher Site | Google Scholar
S. Frank, B. Gaume, E. S. Bergmann-Leitner et al., “The role of dynamin-related protein 1, a mediator of mitochondrial fission, in apoptosis,” Developmental Cell, vol. 1, no. 4, pp. 515–525, 2001.
View at: Publisher Site | Google Scholar
J. H. Zhu, F. Guo, J. Shelburne, S. Watkins, and C. T. Chu, “Localization of phosphorylated ERK/MAP kinases to mitochondria and autophagosomes in Lewy body diseases,” Brain Pathology, vol. 13, no. 4, pp. 473–481, 2003.
View at: Google Scholar
Y. X. Gui, X. Y. Wang, W. Y. Kang et al., “Extracellular signal-regulated kinase is involved in alpha-synuclein-induced mitochondrial dynamic disorders by regulating dynamin-like protein 1,” Neurobiology of Aging, vol. 33, no. 12, pp. 2841–2854, 2012.
View at: Publisher Site | Google Scholar
E. Huerta-García, J. A. Pérez-Arizti, S. G. Márquez-Ramírez et al., “Titanium dioxide nanoparticles induce strong oxidative stress and mitochondrial damage in glial cells,” Free Radical Biology and Medicine, vol. 73, pp. 84–94, 2014.
View at: Publisher Site | Google Scholar
I. Iavicoli, V. Leso, L. Fontana, and A. Bergamaschi, “Toxicological effects of titanium dioxide nanoparticles: a review of in vitro mammalian studies,” European Review for Medical and Pharmacological Sciences, vol. 15, no. 5, pp. 481–508, 2011.
View at: Google Scholar
J. J. Stevens, B. Graham, E. Dugo, B. Berhaneselassie-Sumner, K. Ndebele, and P. B. Tchounwou, “Arsenic trioxide induces apoptosis via specific signaling pathways in HT-29 colon cancer cells,” Journal of Cancer Science & Therapy, vol. 9, no. 1, pp. 298–306, 2017.
View at: Google Scholar
J. A. Smith, S. Park, J. S. Krause, and N. L. Banik, “Oxidative stress, DNA damage, and the telomeric complex as therapeutic targets in acute neurodegeneration,” Neurochemistry International, vol. 62, no. 5, pp. 764–775, 2013.
View at: Publisher Site | Google Scholar
V. Freyre-Fonseca, N. L. Delgado-Buenrostro, E. B. Gutiérrez-Cirlos et al., “Titanium dioxide nanoparticles impair lung mitochondrial function,” Toxicology Letters, vol. 202, no. 2, pp. 111–119, 2011.
View at: Publisher Site | Google Scholar
B. Halliwell and J. M. Gutteridge, “Oxygen toxicity, oxygen radicals, transition metals and disease,” Biochemical Journal, vol. 219, no. 1, pp. 1–14, 1984.
View at: Publisher Site | Google Scholar
Y. Liu and D. R. Schubert, “The specificity of neuroprotection by antioxidants,” Journal of Biomedical Science, vol. 16, no. 1, p. 98, 2009.
View at: Publisher Site | Google Scholar
Y. Sagara, K. Ishige, C. Tsai, and P. Maher, “Tyrphostins protect neuronal cells from oxidative stress,” The Journal of Biological Chemistry, vol. 277, no. 39, pp. 36204–36215, 2002.
View at: Publisher Site | Google Scholar
S. Kumari, S. L. Mehta, and P. A. Li, “Glutamate induces mitochondrial dynamic imbalance and autophagy activation: preventive effects of selenium,” PLoS One, vol. 7, no. 6, article e39382, 2012.
View at: Publisher Site | Google Scholar
G. Benard, N. Bellance, D. James et al., “Mitochondrial bioenergetics and structural network organization,” Journal of Cell Science, vol. 120, Part 5, no. 5, pp. 838–848, 2007.
View at: Publisher Site | Google Scholar
S. Wu, F. Zhou, Z. Zhang, and D. Xing, “Mitochondrial oxidative stress causes mitochondrial fragmentation via differential modulation of mitochondrial fission-fusion proteins,” The FEBS Journal, vol. 278, no. 6, pp. 941–954, 2011.
View at: Publisher Site | Google Scholar
C. Mammucari and R. Rizzuto, “Signaling pathways in mitochondrial dysfunction and aging,” Mechanisms of Ageing and Development, vol. 131, no. 7-8, pp. 536–543, 2010.
View at: Publisher Site | Google Scholar
A. M. van der Bliek, Q. Shen, and S. Kawajiri, “Mechanisms of mitochondrial fission and fusion,” Cold Spring Harbor Perspectives in Biology, vol. 5, no. 6, 2013.
View at: Google Scholar

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Copyright © 2019 Han Zhao et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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Journal of Nanomaterials

Titanium Dioxide Nanoparticles Induce Mitochondrial Dynamic Imbalance and Damage in HT22 Cells

Abstract

1. Introduction

2. Materials and Methods

2.1. TiO2 NPs Preparation

2.2. Characterization

2.3. Cell Culture

2.4. MitoTEMPO Incubation

2.5. Confocal Imaging

2.6. STED Imaging

2.7. Western Blot Analysis

2.8. Measurement of Oxidative Stress Markers

2.9. Measurement of Mitochondrial Membrane Potential (MMP)

2.10. Measurement of Cellular Concentration of ATP

2.11. Hoechst 33342/Propidium Iodide (PI) Analysis

2.12. Annexin V-Fluorescein Isothiocyanate and Propidium Iodide (Annexin V-FITC/PI) Staining

2.13. Mitochondrial Superoxide Assay

2.14. Statistical Analysis

3. Results

3.1. Characterization of TiO2 NPs

3.2. TiO2 NPs-Induced Mitochondrial Fragmentation

3.3. Submitochondrial Structures in Mitochondria

3.4. TiO2 NPs Induced Imbalanced Expression of Mitochondrial Fission/Fusion Protein

3.5. ROS Generation and Oxidative Stress Levels

3.6. Loss of Mitochondrial Membrane Potential and ATP

3.7. TiO2 NPs-Induced Cytotoxicity

3.8. TiO2 NPs-Induced Specific Expression of Mitochondrial-Related Apoptosis Proteins

4. Discussion

5. Conclusions

Data Availability

Conflicts of Interest

Acknowledgments

Supplementary Materials

References

Copyright

2.1. TiO₂ NPs Preparation

3.1. Characterization of TiO₂ NPs

3.2. TiO₂ NPs-Induced Mitochondrial Fragmentation

3.4. TiO₂ NPs Induced Imbalanced Expression of Mitochondrial Fission/Fusion Protein

3.7. TiO₂ NPs-Induced Cytotoxicity

3.8. TiO₂ NPs-Induced Specific Expression of Mitochondrial-Related Apoptosis Proteins