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Oxidative Medicine and Cellular Longevity
Volume 2013 (2013), Article ID 102741, 11 pages
Neuroprotective Effects of Hesperidin, a Plant Flavanone, on Rotenone-Induced Oxidative Stress and Apoptosis in a Cellular Model for Parkinson’s Disease
1Department of Biochemistry and Biotechnology, Faculty of Science, College Rd, Annamalai Nagar, Chidambaram, Tamil Nadu 608002, India
2Centre for Healthy Brain Ageing, School of Psychiatry, Faculty of Medicine, University of New SouthWales, Sydney 2031, Australia
3Department of Food Science and Nutrition, College of Agriculture and Marine Sciences, Sultan Qaboos University, P.O. Box 50, Muscat 123, Oman
4Neuropharmacology Group, MND and Neurodegenerative Diseases Research Centre, Australian School of Advanced Medicine, Macquarie University, Balaclava Road, North Ryde, Sydney, NSW 2109, Australia
Received 8 July 2013; Accepted 15 August 2013
Academic Editor: Tullia Maraldi
Copyright © 2013 Kuppusamy Tamilselvam 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.
Rotenone a widely used pesticide that inhibits mitochondrial complex I has been used to investigate the pathobiology of PD both in vitro and in vivo. Studies have shown that the neurotoxicity of rotenone may be related to its ability to generate reactive oxygen species (ROS), leading to neuronal apoptosis. The current study was carried out to investigate the neuroprotective effects of hesperidin, a citrus fruit flavanol, against rotenone-induced apoptosis in human neuroblastoma SK-N-SH cells. We assessed cell death, mitochondrial membrane potential, ROS generation, ATP levels, thiobarbituric acid reactive substances, reduced glutathione (GSH) levels, and the activity of catalase, superoxide dismutase (SOD) and glutathione peroxidase (GPx) using well established assays. Apoptosis was determined in normal, rotenone, and hesperidin treated cells, by measuring the protein expression of cytochrome c (cyt c), caspases 3 and 9, Bax, and Bcl-2 using the standard western blotting technique. The apoptosis in rotenone-induced SK-N-SH cells was accompanied by the loss of mitochondrial membrane potential, increased ROS generation, the depletion of GSH, enhanced activities of enzymatic antioxidants, upregulation of Bax, cyt c, and caspases 3 and 9, and downregulation of Bcl-2, which were attenuated in the presence of hesperidin. Our data suggests that hesperidin exerts its neuroprotective effect against rotenone due to its antioxidant, maintenance of mitochondrial function, and antiapoptotic properties in a neuroblastoma cell line.
Parkinson’s disease (PD) is the second most common neurodegenerative disorder after Alzheimer’s disease. It is characterised by the progressive loss of dopaminergic neurons in the substantia nigra pars compacta and subsequent depletion of dopamine in the striatum, the main projection area of the substantia nigra. Numerous studies using postmortem human tissues, animal models, and neuronal cell lines have reported the involvement of several pathological mechanisms responsible for the loss of dopaminergic neurons in PD, including elevated levels of iron, ubiquitin-proteasome system (UPS) dysfunction and impairment, altered calcium homeostasis, excitotoxicity, inflammation, oxidative stress, and release of apoptotic factors [1, 2].
Rotenone is a naturally occurring lipophilic compound exhibiting insecticide-like properties and is obtained from the roots of certain plants species (Derris and Lonchocarpus) . It is one of the common neurotoxic agents used to examine the development of PD in animal models  and induces similar toxicity in primary dopaminergic cultures derived from embryonic mouse mesencephalon , PC12 cells , and human neuroblastoma SH-SY5Y cells . It inhibits mitochondrial electron transfer chain (ETC) complex I, which enhances the formation of ROS and leads to modest depletion of ATP and mitochondrial dysfunction culminating in apoptotic cell death .
Current pharmacological therapies for PD are inadequate, and alternative strategies such as stem cell therapy, neurotransplantation, and deep brain stimulation are still in infant stage. There has been considerable interest in the development of neuroprotective drugs from natural origins as a therapeutic strategy for PD . Citrus fruits and their products are important sources of health-promoting constituents and are widely consumed around the world . Hesperidin is a naturally occurring flavanone that exists in citrus and other plants and can be isolated in large amounts from the peels of Citrus aurantium (bitter orange), Citrus sinensis (sweet orange), and Citrus unshiu (satsuma mandarin) . Hesperidin is reported to exert a wide range of pharmacological effects such as antioxidant, anti-inflammatory, antihypercholesterolemic, and anticarcinogenic properties . It has also been demonstrated that hesperidin can protect neurons against various types of insults associated with many neurodegenerative diseases . In this study, we investigated the neuroprotective effect of hesperidin on rotenone-induced cellular model for PD by analysing its effect on rotenone-mediated oxidative stress generation, mitochondrial dysfunction, and apoptosis in human neuroblastoma SK-N-SH cells.
2. Materials and Methods
Rotenone, hesperidin, thiobarbituric acid (TBA), phenazine methosulfate (PMS), nitroblue tetrazolium (NBT), 5,5-dithiobis(2-nitrobenzoic acid) (DTNB), 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT), 2,7-diacetyl dichlorofluorescein (DCFH-DA), rhodamine 123 (Rh-123), heat-inactivated fetal calf serum (FCS), Dulbecco’s modified Eagle’s medium (DMEM), glutamine, penicillin-streptomycin, EDTA, and trypsin were purchased from Sigma Chemicals Co., St. Louis, USA. Anti-Bcl-2, anti-Bax, caspase 3, caspase 9, and cytochrome c antibodies were obtained from Cell Signalling (USA) and β-actin antibodies were purchased from Santa Cruz Biotechnology, Inc., USA. ATP Bioluminescence Assay Kit HS II was purchased from Roche Molecular Biochemicals. Anti-mouse and anti-rabbit secondary antibodies were purchased from Genei, Bangalore, India.
2.2. Cell Culture
The SK-N-SH neuroblastoma cell line was obtained from the National Centre for Cell Science (NCCS) Pune, India. Cells were grown in (DMEM) 12 (1 : 1), supplemented with 2 mM glutamine, penicillin (100 U/mL), streptomycin (100 U/mL), gentamicin (100 μg/mL), and 10% (vol/vol) heat-inactivated fetal bovine serum (FBS) (Sigma Chemicals Co, St Louis, USA), and the medium was changed every two days. Cells were maintained at 37°C in CO2 incubator in a saturated humidity atmosphere containing 95% air and 5% CO2. Rotenone and hesperidin were dissolved in fresh DMSO (0.05%) prior to each experiment. Hesperidin was added 4 h prior to rotenone treatment.
In Experiment I, cells were incubated with different concentrations of rotenone (2.5, 5, 50, 100, and 200 nM) for 24 h, and MTT assay was performed to detect IC50 value of rotenone. In Experiment II, cells were pretreated with different concentrations of hesperidin (2.5, 5, 10, 20, and 40 μg) for 4 h and then incubated with rotenone (effective dose) for 24 h. The effective dose of hesperidin was used to identify potential neuroprotective effects against rotenone toxicity.
2.3. MTT Assay
The proliferation of cells treated with various concentrations of rotenone and hesperidin was determined by the MTT assay based on the detection of mitochondrial dehydrogenase activity in living cells [14, 15]. MTT was added to each well, and the plates were incubated at 37°C for 4 h. Afterwards, the cells were centrifuged for 10 min, and the supernatant was removed, 200 μL of DMSO was added into each well, and absorbance was measured in a microplate reader (Molecular Devices, CA, USA) at 595 nm.
2.4. Determination of Intracellular ROS Generation
The formation of ROS was measured by using a nonfluorescent probe, 2,7-diacetyl dichlorofluorescein (DCFH-DA) that can penetrate into the intracellular matrix of cells, where it is oxidized by ROS to form fluorescent dichlorofluorescein (DCF) . The percentage of ROS was estimated in the control, hesperidin, and rotenone-treated SK-N-SH neuroblastoma cells. Briefly, an aliquot of the isolated cells cells/mL was made up to a final volume of 2 mL in normal PBS (pH 7.4). Then, 1 mL aliquot of cells was taken to which 100 μL DCFH-DA (10 μM) was added and incubated at 37°C for 30 min. Fluorescent measurements were made with excitation and emission filters were set at nm, and nm respectively (Shimadzu RF-5301 PC spectrofluorometer). All initial fluorescent values (time 0) were found to differ from each other by less than 5%. Results were expressed as percentage; increase in fluorescence was calculated using the formula [/()], and the fluorescence intensities at 0 and 30 min were measured.
2.5. Measurement of Intracellular ATP Levels
Cells were collected by centrifugation, and intracellular ATP was measured with a luminometer using an ATP Bioluminescence Assay Kit HS II (Roche Molecular Biochemicals) according to the manufacturer’s instructions.
2.6. TBARS Assay
SK-N-SH neuroblastoma cells were suspended in 130 mM KCl and 50 mM PBS containing 0.1 mL of 0.1 M dithiothreitol (DTT) and centrifuged at 20,000 g for 15 min (4°C). The supernatant was taken for biochemical estimation. The level of lipid peroxidation was determined by analysing TBARS as previously described . The pink-coloured chromogen formed by the reaction of 2-TBA with breakdown products of lipid peroxidation was measured.
2.7. SOD Activity Assay
Superoxide dismutase (SOD) activity was assayed by the method based on the inhibition of the formation of (NADH-PMS-NBT) complex as previously described .
2.8. Catalase Activity Assay
Catalase (CAT) activity was assayed by the decomposition of hydrogen peroxide as previously described . A decrease in absorbance due to H2O2 degradation was monitored at 240 nm for 1 min.
2.9. Glutathione Peroxidase Activity Assay
The activity of glutathione peroxidase (GPx) was assayed spectrophotometrically as previously described . Briefly, a known amount of enzyme preparation was allowed to react with hydrogen peroxides (H2O2) and GSH for a specified time period. The GSH content remaining after the reaction was measured.
2.10. Estimation of Glutathione
The total GSH content was measured by the method as previously described . This method was based on the development of a yellow colour, when 5,5-dithiobis (2-nitrobenzoic acid) was added to compound containing sulfhydryl groups.
2.11. Changes in Mitochondrial Transmembrane Potential ()
The change inin different treatment groups was observed microscopically and determined fluorometrically using the fluorescent dye rhodamine 123 (Rh-123) as previously described . Briefly, after incubation with treatment compounds for 24 h, 1 μL of fluorescent dye Rh-123 (5 m mol/l) was added to the cells and returned to the incubator for 15 min . The cells were then washed with PBS, observed under fluorescence microscope, and estimated by using blue filter (450–490 nm) (Olympus BX60 fluorescence microscope). Polarized mitochondria emit orange-red fluorescence, and depolarized mitochondria emit green fluorescence. The fluorescence intensity was measured at 535 nm using FLUOstar OPTIMA fluorometer (Durham, NC, USA).
2.12. Western Blotting
Briefly, cells seeded in 6-well plates were harvested and washed with PBS. Cells were lysed in 100 μL lysis buffer containing 20 mM Tris-Hcl, pH 7.4, 150 mM NaCl, 1 mM EDTA, 30 μg/mL aprotinin, and 1 mM phenylmethylsulfonyl fluoride and subjected to 12.5% polyacrylamide gel electrophoresis. A total volume of 30 μg of protein was loaded per lane. The separated proteins were blotted onto a PVDF membrane by semidry transfer (Bio-Rad). After blocking with 5% nonfat milk in TBS, the membranes were then incubated with various antibodies: Bcl-2, Bax, caspases 3 and 9, cytochrome c, and β-actin. The following dilutions were used for Bcl-2 and Bax (1 : 500), cytochrome c, caspases 3 and 9 (1 : 1000), and β-actin (1 : 2000). After primary antibody incubation, the membranes were incubated with secondary antibody at a concentration of 1 : 2000. Then, the membranes were washed with Tris-buffered saline and 0.05% Tween 20 thrice for 10 min interval; after extensive washes in TBST, the bands were visualized by treating the membranes with 3,3′-diaminobenzidine tetrahydrochloride (western blot detection reagent, Sigma, USA). Densitometry was performed using “Image J” analysis software.
2.13. Data Analysis
Statistical analysis was performed using one-way analysis of variance followed by Duncan’s multiple range test (DMRT) using Statistical Package for the Social Science (SPSS) software package version 12.0. Results were expressed as mean ± SD for four experiments in each group. values were considered significant.
3.1. Effect of Hesperidin on Rotenone-Induced Cell Death
Rotenone treatment (2.5, 5, 50, 100, and 200 nM for 24 h) of SK-N-SH cells induced a dose-dependent reduction in cell proliferation, with approximately 50% proliferation observed at 100 nM (Figure 1(a)). Hesperidin dose dependently (0.5, 5, 10, 20, and 40 μg) attenuated the changes in cell proliferation induced by 100 nM rotenone (Figure 1(b)), with approximately 85% protection following treatment with 20 μg hesperidin after 24 h.
3.2. Effect of Hesperidin on Rotenone-Induced ROS Formation
Figures 2(a) and 2(b) indicate the levels of TBARS and GSH in rotenone-treated SK-N-SH cells incubated with and without hesperidin. Rotenone treatment (100 nM) significantly increased the levels of TBARS parallel to decreased levels of GSH in SK-N-SH cells compared with nontreated cells. Pretreatment with hesperidin (20 μg) to rotenone-treated cells significantly decreased the levels of TBARS and increased GSH levels significantly, compared to cells treated with rotenone alone. Figures 2(c), 2(d), and 2(e) elucidate the activities of SOD, catalase and GPx in rotenone-treated SK-N-SH cells incubated with and without hesperidin. Compared with untreated cells, rotenone (100 nM) treatment increased SOD, catalase and GPx activities in SK-N-SH cells (Figures 2(c), 2(d), and 2(e)). Pretreatment with hesperidin significantly decreased the activities of SOD, catalase, and GPx, compared to cells treated with rotenone alone.
3.3. Effect of Hesperidin on Intracellular ROS Generation
The formation of intracellular ROS was measured in terms of fluorescence by DCF (Figures 3(a) and 3(b)). Addition of rotenone (100 nM) to cells caused a significant increase (~411%) in DCF fluorescence. Pretreatment of the cells with hesperidin (20 μg) lowered rotenone-induced free radical release as compared to rotenone-treated cells alone. No significant changes in ROS formation were detected in SK-N-SH cells treated with hesperidin alone.
3.4. Effect of Hesperidin on Rotenone-Induced ATP Depletion
Rotenone treatment (24 hr) depleted cellular ATP levels (% at 100 nM) (Figure 4). Pretreatment with hesperidin increased ATP levels significantly compared to rotenone only treated cells. No significant changes in ATP levels were detected in SK-N-SH cells treated with hesperidin alone.
3.5. Effect of Hesperidin on Mitochondrial Membrane Potential ()
Figures 5(a) and 5(b) show the mitochondrial membrane potential () measured by determining the red/green fluorescence ratio in the presence of Rh-123. Cells treated with 100 nM rotenone resulted in significant dissipation of. The average green fluorescence ratio was increased as a result of rotenone treatment as compared to untreated controls. Pretreatment with hesperidin to rotenone-treated cells displayed much higher red/green fluorescence, indicating a polarized state of mitochondrial membrane as compared to rotenone treatment alone.
3.6. Effect of Hesperidin on Apoptotic Markers
Rotenone treatment (100 nM) decreased the protein expression levels of antiapoptotic B-cell CLL/lymphoma 2 (Bcl-2) and increased the protein expression levels of proapoptotic Bcl-2-associated X protein (Bax) (Figures 5(a) and 5(b)). Hesperidin pretreatment (20 μg) attenuated the rotenone-induced reduction in Bcl-2 expression and increased expression of Bax (Figures 6(a) and 6(b)). We also examined the effect of hesperidin on the protein expression of cyt c and caspases 3 and 9. Treatment with rotenone (100 nM) for 24 h increased the expression of cyt c, caspases 3 and 9 at the protein level (Figures 7(a) and 7(b)). Hesperidin pretreatment significantly ameliorated the rotenone-mediated increase in cyt c, caspases 3 and 9 protein expression levels (Figures 7(a) and 7(b)).
Our results show that rotenone is cytotoxic to SK-N-SH neuroblastoma cells in line with previous studies. However, our group is the first to show that hesperidin can attenuate the toxic cascade in rotenone-treated cells. Reduction of the tetrazolium salt MTT to a blue formazan product is widely used for assessing cellular proliferation. The reduction is mainly catalyzed by dehydrogenases localized in the mitochondria of proliferating cells . Optimal mitochondrial function is a determinant of the proliferation and hence overall viability of these cells by playing a central role in regulating apoptotic cell death signalling by controlling cellular energy metabolism, contribution of reactive oxygen species (ROS) formation, and release of apoptotic factors into the cytosol . Data obtained from the MTT assay in the present study suggest a direct neuroprotective action of hesperidin against rotenone-mediated mitochondrial dysfunction.
Our data also demonstrate that rotenone treatment can stimulate the generation of intracellular ROS in SK-N-SH cells, as corroborated with previous studies [25, 26]. Inhibition of respiratory complex I by rotenone causes electrons to accumulate within respiratory chain components. These electrons can be added directly to oxygen molecules to produce [27, 28]. The mitochondria are the principle intracellular sources of ROS and also the major targets of oxidative stress . Hesperidin treatment significantly reduced ROS generation in rotenone-treated cells, which might be due to ROS scavenging property of hesperidin  and transition metal ions chelating properties . Additionally, other potential mechanisms such as the ability of hesperidin to enhance glutathione content could be involved in its protective effect on rotenone-induced oxidative stress generation.
When cells were incubated with rotenone, we found increased levels of TBARS, indicating overproduction of free radicals along with glutathione depletion, which is corroborated with previous studies . Our results show that the increase in the enzymatic activities of SOD, GPx, and CAT in neuroblastoma cells incubated with rotenone alone is likely due to a response towards increased ROS generation following rotenone treatment. Cassarino et al.  reported that complex I inhibition induces SOD activity in the brain tissue. Increment in GPx activity in rotenone alone treated cells indicated that there was an increase in the concentration of lipid peroxides and/or H2O2. Reduced GSH levels may also account for the increase in GPx activity .
In the present study, ATP levels were significantly reduced in rotenone-treated cells alone as compared to nontreated controls, which corroborates with previous studies [26, 33]. Since ATP is necessary for downstream events in the apoptotic cascade , the depletion of the intracellular ATP supply may not be expected to induce apoptosis. One study showed that both rotenone and 2-deoxyglucose caused similar ATP depletion. However, only rotenone exposure was toxic, suggesting that rotenone toxicity resulted from additional mechanisms such as oxidative damage [26, 35]. Similarly, mitochondrial ETC inhibitors such as rotenone deplete ATP and induce apoptosis, while oxidative phosphorylation inhibitors, which inhibit ATP synthesis without inhibiting the ETC, fail to induce apoptosis despite depleting ATP to the same extent as ETC inhibitors in dopaminergic neuronal cells. Therefore, intracellular ATP depletion per se is not sufficient for apoptosis induction. Rather, ROS production plays an essential role in apoptosis induced by mitochondrial ETC inhibition. Pretreatment with hesperidin partially attenuated rotenone-induced ATP deficiency.
It was reported by several groups that complex I inhibition by rotenone may result in the opening of mitochondrial permeability transition pores (PTP), which induces a specific conformational change of complex I and massive production of ROS [36–38]. Increased levels of ROS within the mitochondria are known to cause further mitochondrial membrane depolarization and further release of ROS. Due to rotenone treatment, mitochondrial membrane potential is reduced, leading to increased mitochondrial permeability and results in the enhanced release of cyt c from the mitochondria, which triggers activation of caspases 3 and 9 culminating with cell death . cyt c is not only an important electron carrier in the mitochondrial respiration chain, but also a death messenger in the cytosol, which forms apoptosome complexes with Apaf-1, dATP, and caspases 9 and 3 .
The efflux of the cyt c from the mitochondria is also regulated by BAD protein . In an apoptotic cell, BAD protein displaces Bax and binds to the antiapoptotic members Bcl-2 and Bcl-xL . Bax and Bcl-2 are involved in the regulation of caspase 3 mediated apoptosis . Numerous studies have shown that Bcl-2, as a negative regulator of cell death in the Bcl-2 family members, protects cells against apoptosis induced by various stimuli in a wide variety of cell types , whereas Bax is a positive regulator of cell death which promotes or accelerates cell death. It was reported that rotenone induces Bax expression in dopaminergic neuronal cell line MND9 . Elevations in proapoptotic proteins, such as Bax, are believed to stimulate mitochondrial generation of ROS and contribute to neuronal cell death in neurodegenerative diseases. Moreover, overexpression of Bcl-2 disrupts the proapoptotic proteins of Bax and prevents the mitochondrial release of cyt c, thereby inhibiting the activation of caspases and ultimately apoptosis [45, 46]. The ratio of Bcl-2 to Bax determines the survival or death of neurons following an apoptotic stimulus. Administration of hesperidin prevents the loss of, increases the mitochondrial permeability, and prevents the release of cyt c from the mitochondria, thereby inhibiting caspases 3 and 9, thus restoring the imbalance in the expression profiles of Bax and Bcl-2, and preventing cell death. Moreover, overexpression of Bcl-2 disrupts the proapoptotic proteins of Bax and prevents the mitochondrial release of cyt c, thereby inhibiting the activation of caspases, and apoptosis [45, 46].
Although the exact neuroprotective mechanism of action of hesperidin remains unclear, it is likely to demonstrate both antioxidant and cell signalling properties. Our data is in line with previous studies showing that hesperidin therapy could significantly attenuate ROS formation by reducing the levels of TBARS and restored antioxidant enzyme activity and GSH to physiological levels in the brain  and cultured PC12 cells . Another study showed that hesperidin treatment could reduce stress-induced anxiety, impaired locomotor activity, and mitochondrial dysfunction in mice by modulating the nitrergic pathway . Hesperidin also protected cortical neurons from ROS-mediated injury by activation of the prosurvival Akt and ERK1/2 signalling pathways . These pathways are involved in the inhibition of the release of proapoptotic proteins such as apoptosis signal-regulating kinase 1 (ASK1), BAD, and caspases 3 and 9, suggesting that the neuroprotective effects of hesperidin may be due to its effect on a yet unidentified receptor . Moreover, hesperidin can also protect against amyloid-beta- (Aβ-) associated neurotoxicity, and glutamate-induced excitotoxicity . A more recent study showed that hesperidin treatment could reduce cerebral damage due to induced stroke in the rat brain due to the reduction of free radicals and associated neuroinflammation . The results of our present study suggest that hesperidin attenuates neuronal damage induced by rotenone by reducing oxidative stress, mitochondrial dysfunction, and ameliorating apoptosis. These findings may have important implications in the use of hesperidin for the prevention of PD. However, further research involving various animal models and clinical trials is needed to validate hesperidin as a new therapeutic agent.
Kuppusamy Tamilselvam and Nady Braidy are the co-first authors.
Conflict of Interests
The authors of the paper do not have a direct financial relationship with the commercial identities mentioned in this paper that might lead to a conflict of interests.
The financial assistance by the Indian Council of Medical Research (ICMR, New Delhi, India) in the form of Senior Research Fellowship to Dr. K. Tamilselvam to carry out the above study is gratefully acknowledged. This work has also been supported by the National Health and Medical Research Council, the Curran Foundation (Australia), the Alzheimer’s Association, USA (Grant no. IIRG-08-89545), and by the Rebecca Cooper foundation (Australia). Dr. Nady Braidy is the recipient of an Alzheimer’s Australia Viertel Foundation Postdoctoral Research Fellowship from the University of New South Wales.
- W. Dauer and S. Przedborski, “Parkinson's disease: mechanisms and models,” Neuron, vol. 39, no. 6, pp. 889–909, 2003.
- V. Anantharam, E. Lehrmann, A. Kanthasamy et al., “Microarray analysis of oxidative stress regulated genes in mesencephalic dopaminergic neuronal cells: relevance to oxidative damage in Parkinson's disease,” Neurochemistry International, vol. 50, no. 6, pp. 834–847, 2007.
- P. Jenner, “Parkinson's disease, pesticides and mitochondrial dysfunction,” Trends in Neurosciences, vol. 24, no. 5, pp. 245–246, 2001.
- S. Przedborski and H. Ischiropoulos, “Reactive oxygen and nitrogen species: weapons of neuronal destruction in models of Parkinson's disease,” Antioxidants and Redox Signaling, vol. 7, no. 5-6, pp. 685–693, 2005.
- K. Radad, W.-D. Rausch, and G. Gille, “Rotenone induces cell death in primary dopaminergic culture by increasing ROS production and inhibiting mitochondrial respiration,” Neurochemistry International, vol. 49, no. 4, pp. 379–386, 2006.
- G. Wang, C. Qi, G.-H. Fan, H.-Y. Zhou, and S.-D. Chen, “PACAP protects neuronal differentiated PC12 cells against the neurotoxicity induced by a mitochondrial complex I inhibitor, rotenone,” FEBS Letters, vol. 579, no. 18, pp. 4005–4011, 2005.
- M. F. Molina-Jiménez, M. I. Sánchez-Reus, D. Andres, M. Cascales, and J. Benedi, “Neuroprotective effect of fraxetin and myricetin against rotenone-induced apoptosis in neuroblastoma cells,” Brain Research, vol. 1009, no. 1-2, pp. 9–16, 2004.
- J. T. Greenamyre, T. B. Sherer, R. Betarbet, and A. V. Panov, “Complex I and Parkinson's disease,” IUBMB Life, vol. 52, no. 3–5, pp. 135–141, 2002.
- M. Fukui, H. J. Choi, and B. T. Zhu, “Mechanism for the protective effect of resveratrol against oxidative stress-induced neuronal death,” Free Radical Biology and Medicine, vol. 49, no. 5, pp. 800–813, 2010.
- O. Benavente-Garcisa, J. Castillo, F. R. Marin, et al., “Uses and properties of citrus flavonoids,” Journal of Agricultural and Food Chemistry, vol. 45, pp. 4505–4515, 1997.
- A. Crozier, I. B. Jaganath, and M. N. Clifford, “Dietary phenolics: chemistry, bioavailability and effects on health,” Natural Product Reports, vol. 26, no. 8, pp. 1001–1043, 2009.
- M.-C. Chen, Y. I. Ye, J. I. Guang, and L. I. U. Jian-Wen, “Hesperidin upregulates heme oxygenase-1 to attenuate hydrogen peroxide-induced cell damage in hepatic L02 cells,” Journal of Agricultural and Food Chemistry, vol. 58, no. 6, pp. 3330–3335, 2010.
- J. Cho, “Antioxidant and neuroprotective effects of hesperidin and its aglycone hesperetin,” Archives of Pharmacal Research, vol. 29, no. 8, pp. 699–706, 2006.
- H. J. Park, D.-H. Shin, W. J. Chung et al., “Epigallocatechin gallate reduces hypoxia-induced apoptosis in human hepatoma cells,” Life Sciences, vol. 78, no. 24, pp. 2826–2832, 2006.
- T. Mosmann, “Rapid colorimetric assay for cellular growth and survival: application to proliferation and cytotoxicity assays,” Journal of Immunological Methods, vol. 65, no. 1-2, pp. 55–63, 1983.
- S. Karthikeyan, G. Kanimozhi, N. R. Prasad, and R. Mahalakshmi, “Radiosensitizing effect of ferulic acid on human cervical carcinoma cells in vitro,” Toxicology In Vitro, vol. 25, no. 7, pp. 1366–1375, 2011.
- W. G. Niehaus Jr. and B. Samuelsson, “Formation of malonaldehyde from phospholipid arachidonate during microsomal lipid peroxidation,” European Journal of Biochemistry, vol. 6, no. 1, pp. 126–130, 1968.
- P. Kakkar, B. Das, and P. N. Viswanathan, “A modified spectrophotometric assay of superoxide dismutase,” Indian Journal of Biochemistry and Biophysics, vol. 21, no. 2, pp. 130–132, 1984.
- H. Aebi, “Catalase in vitro,” Methods in Enzymology, vol. 105, no. C, pp. 121–126, 1984.
- J. T. Rotruck, A. L. Pope, H. E. Ganther, A. B. Swanson, D. G. Hafeman, and W. G. Hoekstra, “Selenium: biochemical role as a component of glatathione peroxidase,” Science, vol. 179, no. 4073, pp. 588–590, 1973.
- G. L. Ellman, “Tissue sulfhydryl groups,” Archives of Biochemistry and Biophysics, vol. 82, no. 1, pp. 70–77, 1959.
- N. Rajendra Prasad, A. Karthikeyan, S. Karthikeyan, and B. Venkata Reddy, “Inhibitory effect of caffeic acid on cancer cell proliferation by oxidative mechanism in human HT-1080 fibrosarcoma cell line,” Molecular and Cellular Biochemistry, vol. 349, no. 1-2, pp. 11–19, 2011.
- J. L. York, L. C. Maddox, P. Zimniak, T. E. McHugh, and D. F. Grant, “Reduction of MTT by glutathione S-transferase,” BioTechniques, vol. 25, no. 4, pp. 622–624, 1998.
- M. F. Beal, “Energetics in the pathogenesis of neurodegenerative diseases,” Trends in Neurosciences, vol. 23, no. 7, pp. 298–304, 2000.
- Y. Moon, K. H. Lee, J.-H. Park, D. Geum, and K. Kim, “Mitochondrial membrane depolarization and the selective death of dopaminergic neurons by rotenone: protective effect of coenzyme Q10,” Journal of Neurochemistry, vol. 93, no. 5, pp. 1199–1208, 2005.
- T. B. Sherer, R. Betarbet, C. M. Testa et al., “Mechanism of toxicity in rotenone models of Parkinson's disease,” Journal of Neuroscience, vol. 23, no. 34, pp. 10756–10764, 2003.
- J. F. Turrens, A. Alexandre, and A. L. Lehninger, “Ubisemiquinone is the electron donor for superoxide formation by complex III of heart mitochondria,” Archives of Biochemistry and Biophysics, vol. 237, no. 2, pp. 408–414, 1985.
- J. St-Pierre, J. A. Buckingham, S. J. Roebuck, and M. D. Brand, “Topology of superoxide production from different sites in the mitochondrial electron transport chain,” Journal of Biological Chemistry, vol. 277, no. 47, pp. 44784–44790, 2002.
- G. Fiskum, R. E. Rosenthal, V. Vereczki et al., “Protection against ischemic brain injury by inhibition of mitochondrial oxidative stress,” Journal of Bioenergetics and Biomembranes, vol. 36, no. 4, pp. 347–352, 2004.
- S. V. Jovanovic, S. Steenken, M. Tosic, B. Marjanovic, and M. G. Simic, “Flavonoids as antioxidants,” Journal of the American Chemical Society, vol. 116, no. 11, pp. 4846–4851, 1994.
- V. Gaur and A. Kumar, “Hesperidin pre-treatment attenuates NO-mediated cerebral ischemic reperfusion injury and memory dysfunction,” Pharmacological Reports, vol. 62, no. 4, pp. 635–648, 2010.
- D. S. Cassarino, C. P. Fall, R. H. Swerdlow et al., “Elevated reactive oxygen species and antioxidant enzyme activities in animal and cellular models of Parkinson's disease,” Biochimica et Biophysica Acta, vol. 1362, no. 1, pp. 77–86, 1997.
- X.-X. Li, G.-R. He, X. Mu et al., “Protective effects of baicalein against rotenone-induced neurotoxicity in PC12 cells and isolated rat brain mitochondria,” European Journal of Pharmacology, vol. 674, no. 2-3, pp. 227–233, 2012.
- Y. Eguchi, A. Srinivasan, K. J. Tomaselli, S. Shimizu, and Y. Tsujimoto, “ATP-dependent steps in apoptotic signal transduction,” Cancer Research, vol. 59, no. 9, pp. 2174–2181, 1999.
- M. Watabe and T. Nakaki, “ATP depletion does not account for apoptosis induced by inhibition of mitochondrial electron transport chain in human dopaminergic cells,” Neuropharmacology, vol. 52, no. 2, pp. 536–541, 2007.
- J. S. Isenberg and J. E. Klaunig, “Role of the mitochondrial membrane permeability transition (MPT) in rotenone-induced apoptosis in liver cells,” Toxicological Sciences, vol. 53, no. 2, pp. 340–351, 2000.
- W. Pei, A. K. F. Liou, and J. Chen, “Two caspase-mediated apoptotic pathways induced by rotenone toxicity in cortical neuronal cells,” The FASEB Journal, vol. 17, no. 3, pp. 520–522, 2003.
- A. Panov, S. Dikalov, N. Shalbuyeva, G. Taylor, T. Sherer, and J. T. Greenamyre, “Rotenone model of Parkinson disease: multiple brain mitochondria dysfunctions after short term systemic rotenone intoxication,” Journal of Biological Chemistry, vol. 280, no. 51, pp. 42026–42035, 2005.
- T. Kaufmann, S. Schlipf, J. Sanz, K. Neubert, R. Stein, and C. Borner, “Characterization of the signal that directs Bcl-xL, but not Bcl-2, to the mitochondrial outer membrane,” Journal of Cell Biology, vol. 160, no. 1, pp. 53–64, 2003.
- X. Jiang and X. Wang, “Cytochrome C-mediated apoptosis,” Annual Review of Biochemistry, vol. 73, pp. 87–106, 2004.
- E. Yang, J. Zha, J. Jockel, L. H. Boise, C. B. Thompson, and S. J. Korsmeyer, “Bad, a heterodimeric partner for Bcl-x(L), and Bcl-2, displaces Bax and promotes cell death,” Cell, vol. 80, no. 2, pp. 285–291, 1995.
- J. C. Reed, “Double identity for proteins of the Bcl-2 family,” Nature, vol. 387, no. 6635, pp. 773–776, 1997.
- S. J. Korsmeyer, “Bcl-2 initiates a new category of oncogenes: regulators of cell death,” Blood, vol. 80, no. 4, pp. 879–886, 1992.
- P. De Sarno, S. A. Shestopal, T. D. King, A. Zmijewska, L. Song, and R. S. Jope, “Muscarinic receptor activation protects cells from apoptotic effects of DNA damage, oxidative stress, and mitochondrial inhibition,” Journal of Biological Chemistry, vol. 278, no. 13, pp. 11086–11093, 2003.
- S. Desagher and J.-C. Martinou, “Mitochondria as the central control point of apoptosis,” Trends in Cell Biology, vol. 10, no. 9, pp. 369–377, 2000.
- I. Budihardjo, H. Oliver, M. Lutter, X. Luo, and X. Wang, “Biochemical pathways of caspase activation during apoptosis,” Annual Review of Cell and Developmental Biology, vol. 15, pp. 269–290, 1999.
- S. Kamisli, O. Ciftci, K. Kaya, et al., “Hesperidin protects brain and sciatic nerve tissues against cisplatin-induced oxidative, histological and electromyographical side effects in rats,” Toxicology and Industrial Health, 2013.
- H. J. Heo, D.-O. Kim, S. C. Shin, M. J. Kim, B. G. Kim, and D.-H. Shin, “Effect of antioxidant flavanone, naringenin, from citrus junos on neuroprotection,” Journal of Agricultural and Food Chemistry, vol. 52, no. 6, pp. 1520–1525, 2004.
- G. L. Viswanatha, H. Shylaja, K. S. Sandeep Rao, et al., “Hesperidin ameliorates immobilization-stress-induced behavioral and biochemical alterations and mitochondrial dysfunction in mice by modulating nitrergic pathway,” ISRN Pharmacology, vol. 2012, Article ID 479570, 8 pages, 2012.
- D. Vauzour, K. Vafeiadou, C. Rice-Evans, R. J. Williams, and J. P. E. Spencer, “Activation of pro-survival Akt and ERK1/2 signalling pathways underlie the anti-apoptotic effects of flavanones in cortical neurons,” Journal of Neurochemistry, vol. 103, no. 4, pp. 1355–1367, 2007.
- S. S. Raza, M. M. Khan, A. Ahmad et al., “Hesperidin ameliorates functional and histological outcome and reduces neuroinflammation in experimental stroke,” Brain Research, vol. 1420, pp. 93–105, 2011.