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Logo of jbcThe Journal of Biological Chemistry
 
J Biol Chem. 2012 July 13; 287(29): 24460–24472.
Published online 2012 May 30. doi:  10.1074/jbc.M112.382226
PMCID: PMC3397871

trans-(−)-ϵ-Viniferin Increases Mitochondrial Sirtuin 3 (SIRT3), Activates AMP-activated Protein Kinase (AMPK), and Protects Cells in Models of Huntington Disease*

Abstract

Huntington disease (HD) is an inherited neurodegenerative disorder caused by an abnormal polyglutamine expansion in the protein Huntingtin (Htt). Currently, no cure is available for HD. The mechanisms by which mutant Htt causes neuronal dysfunction and degeneration remain to be fully elucidated. Nevertheless, mitochondrial dysfunction has been suggested as a key event mediating mutant Htt-induced neurotoxicity because neurons are energy-demanding and particularly susceptible to energy deficits and oxidative stress. SIRT3, a member of sirtuin family, is localized to mitochondria and has been implicated in energy metabolism. Notably, we found that cells expressing mutant Htt displayed reduced SIRT3 levels. trans-(−)-ϵ-Viniferin (viniferin), a natural product among our 22 collected naturally occurring and semisynthetic stilbenic compounds, significantly attenuated mutant Htt-induced depletion of SIRT3 and protected cells from mutant Htt. We demonstrate that viniferin decreases levels of reactive oxygen species and prevents loss of mitochondrial membrane potential in cells expressing mutant Htt. Expression of mutant Htt results in decreased deacetylase activity of SIRT3 and further leads to reduction in cellular NAD+ levels and mitochondrial biogenesis in cells. Viniferin activates AMP-activated kinase and enhances mitochondrial biogenesis. Knockdown of SIRT3 significantly inhibited viniferin-mediated AMP-activated kinase activation and diminished the neuroprotective effects of viniferin, suggesting that SIRT3 mediates the neuroprotection of viniferin. In conclusion, we establish a novel role for mitochondrial SIRT3 in HD pathogenesis and discovered a natural product that has potent neuroprotection in HD models. Our results suggest that increasing mitochondrial SIRT3 might be considered as a new therapeutic approach to counteract HD, as well as other neurodegenerative diseases with similar mechanisms.

Keywords: AMP-activated kinase (AMPK), Energy Metabolism, Huntington Disease, Natural Products, Sirtuins

Introduction

Huntington disease (HD)3 is an autosomal dominant, progressive neurodegenerative disorder characterized by psychiatric manifestations, cognitive decline, and movement abnormalities (1). The causative gene mutation for HD is an unstable CAG trinucleotide repeat sequence encoding a polyglutamine tract in the huntingtin (Htt) protein resulting in neuronal dysfunction and neuronal death predominantly in the striatum and cortex (2). Neither the normal function of Htt nor the mechanism whereby polyglutamine expansion results in selective loss of striatal neurons is fully understood, although impaired energy metabolism (3), oxidative stress (4), excitotoxicity (5), and transcriptional dysregulation (6) are implicated. Cells expressing polyglutamine-expanded full-length or N-terminal fragments of Htt exhibited increased oxidative stress and mitochondrial dysfunction (7). Abnormalities in mitochondrial function have been observed in postmortem HD brains (810) and cells from HD patients (11, 12). In addition, mitochondrial respiration and ATP production are significantly impaired in striatal cells expressing mutant Htt (13). More recent data suggest that mitochondrial dysfunction is a key event mediating mutant Htt-induced neurotoxicity (14).

SIRT3, a sirtuin family member, is located to mitochondria and is highly expressed in metabolically active tissues including brain (15). Consistent with its expression pattern and mitochondrial localization, deletion of SIRT3 in mice leads to striking hyperacetylation of mitochondrial proteins (16). These hyperacetylated proteins include key energy metabolic enzymes as well as antioxidant enzymes, such as Mn-SOD. The hyperacetylation results in dysfunction of these enzymes, eventually leading to mitochondrial dysfunction. Therefore, compounds that increase mitochondrial SIRT3 would improve mitochondrial function and might have therapeutic potential for HD.

Natural products and their synthetic derivatives are vital resources for the discovery of biologically active small organic molecules, and they exhibit numerous biophysical attributes that make them outstanding candidates for development of new drugs (17). Moreover, natural products are unique in terms of their chemical diversity when compared with most combinatorial chemical libraries (18, 19). Stilbenoids, constituting a class of resveratrol and its derivatives, naturally occur in several plant families, such as Cyperaceae, Dipterocarpaceae, Gnetaceae, and Vitaceae, and have recently been characterized chemically (20, 21). Among available stilbenoids, resveratrol has shown promise in treatment and prevention of neurodegenerative disorders, including Huntington disease (2224). However, recent work in HD transgenic mice demonstrated that resveratrol protected against peripheral deficits, but was not effective in the central nervous system in HD mice, probably due to instability of resveratrol (25). Moreover, concentrations of resveratrol required for neuroprotective actions were in the range of 10–100 μm (26).

To develop more potent neuroprotective agents from natural products, we have screened a unique collection of 22 stilbenic compounds that consists of naturally occurring resveratrol monomers and oligomers, as well as semisynthetic resveratrol derivatives. Here we demonstrate that one compound, trans-(−)-ϵ-viniferin (viniferin), preserves mitochondrial membrane potential and reduces reactive oxygen species (ROS) levels induced by mutant Htt. Moreover, viniferin increases mitochondrial SIRT3 levels, activates AMP-activated protein kinase (AMPK), and replenishes cellular NAD+ levels. The increased NAD+ leads to activation of SIRT3 deacetylase activity and enhances the antioxidant activity of target substrate Mn-SOD. SIRT3 is required for the neuroprotection of viniferin as inhibition of SIRT3 abolished the protection.

EXPERIMENTAL PROCEDURES

Compounds and Reagents

We purified a collection of 22 resveratrol monomers and oligomers from wild and cultivated Vitis spp. All compounds were characterized by comparison with their published electrospray mass spectrometry and 1H and 13C NMR data. Cell culture medium and supplements including DMEM, Neurobasal medium, fetal bovine serum (FBS), B-27, and N2 supplement were obtained from Invitrogen; tetramethyl rhodamine methyl ester (TRME), 5-(and-6)-chloromethyl-2′,7′-dichlorodihydrofluorescein diacetate, and acetyl ester (CM-H2DCFDA) were obtained from Molecular Probes (Eugene, OR); SsoFastTM EvaGreen® supermix was purchased from Bio-Rad; and nicotinamide and trichostatin A were obtained from Sigma. Antibodies were obtained from the following commercial sources: anti-active caspase-3 pAb (Promega, G7481); rabbit anti-Sirt3 (C terminus, Millipore, 07-1596); mouse β-actin (Sigma, A5441); mouse AMPK α1+α2 (Abcam, ab80039); phospho-AMPK (Cell Signaling, 2535); mouse anti-LKB1 (Santa Cruz Biotechnology, mouse mAb, Sc-32245); rabbit anti-LKB1 (Cell Signaling, 3047); phospho-LKB1 (Ser-428, Cell signaling, 3482); rabbit anti-Mn-SOD (Millipore, 06-984); mouse anti-Mn-SOD (Santa Cruz Biotechnology, Sc133254); and anti-acetyl lysine (Immunechem, ICP0380).

Cell Culture

Immortalized striatal precursor cells expressing normal Htt (STHdhQ7/Q7) or mutant Htt (STHdhQ111/Q111) were kindly provided by Dr. Marcy MacDonald and were prepared as described previously (27). The cells were maintained at 33 °C in DMEM containing 10% FBS, 400 μg/ml G418 (Invitrogen), in a humidified atmosphere of 95% air and 5% CO2.

Tet-Off PC12 cells expressing truncated mutant Htt N63-148Q were maintained as described previously (28). Mutant Htt was inducibly expressed when doxycycline was removed from the culture medium. Cells were differentiated in the presence of nerve growth factor (NGF, 50 ng/ml).

Neuroblastoma N2a cells were obtained from ATCC and cultured in DMEM+10% FBS medium. Mutant Htt (N63-148Q) was transfected by Lipofectamine 2000 (Invitrogen), and cell toxicity was determined by flow cytometry (FACSCalibur, BD Biosciences) 48 h after transfection.

Primary cortical neurons were prepared from embryonic day 18 pregnant C57/BL6 mice. Neurons were cultured in Neurobasal medium supplemented with B-27. Myc-tagged mutant Htt (N63-148Q) or normal htt (N63-16Q) was transfected by Lipofectamine 2000 (Invitrogen) at days in vitro 5; the transfection efficacy was ~5%. Neurons were fixed and stained for transgene expression by anti-Myc antibody and chromatin condensation by the dye Hoechst 33342 to determine the neuronal toxicity induced by mutant Htt.

Caspase3/7 Assay

Caspase3/7 activity was detected by a luminescence assay in 96-well plates. Cells were dissolved with 50 μl of Caspase-Glo® 3/7 Reagent (Promega, G8092) and gently mixed using a plate shaker at 300–500 rpm for 1 h. Then 100 μl of the mixture was transferred to a white-walled 96-well plate, 100 μl of medium with a corresponding concentration of compounds was used as a blank, and the luminescence intensity of each sample was measured in a luminometer (Fluoroskan Ascent FL, Thermo Scientific).

Intracellular ROS Measurements

Striatal cells were incubated with the fluorescent probe CM-H2DCFDA (1 μm) for 30 min in Krebs-Ringer-Hepes buffer supplemented with 5 mm glucose. Samples were analyzed using a flow cytometer (FACSCalibur). The mean fluorescence intensity of 10,000 cells was analyzed in each sample and corrected for autofluorescence from unlabeled cells.

Mitochondrial Potential Determination in Live Cells

Mitochondrial membrane potential was determined by using the fluorescent probe TRME. Striatal cells were incubated with TMRE for 1 h. Samples were analyzed by using a flow cytometer (FACSCalibur). The mean fluorescence intensity of 10,000 cells was analyzed in each sample and corrected for autofluorescence from unlabeled cells.

NAD+/NADH Assay

Intracellular NAD+ and NADH levels in striatal cells were measured with an NAD+/NADH assay kit (Abcam) according to the manufacturer's instructions. Briefly, 5 × 105 striatal cells were cultured in serum-free medium with or without viniferin for 24 h, and then the cells were washed with cold PBS and extracted with NADH/NAD extraction buffer by two freeze/thaw cycles (20 min on dry ice and then 10 min at room temperature). Total NAD (NADt) and NADH levels were detected in a 96-well plate, and color was developed and read at 450 nm. NAD+/NADH ratio was calculated as: (NADt − NADH)/NADH.

Mitochondrial Biogenesis

The mitochondrial copy numbers were calculated from the ratio of 12 S rRNA/18 S rRNA and Cox-2/cyclophilin A. The PCR primers for detecting the 12 S rRNA and Cox-2 gene of murine mitochondrial genome were designed on the basis of the GenBankTM nucleotide sequence. Each tube contained 15 ng of total DNA from the same extract as well as 10 μl of reaction mixture consisting of 2× SsoFastTM EvaGreen® supermix (1× final) and other pairs of the primers directed against either 18 S RNA or cyclophilin A (nuclear-encoding gene), with 0.5 μm primer in each case.

Quantitative RT-PCR

The levels of PGC-1α mRNA and SIRT3 mRNA were detected by quantitative RT-PCR as follows. Total RNA from cultured cells was extracted with an RNeasy mini kit (Qiagen). cDNA was then reverse-transcribed and amplified by PCR with a Transcriptor reverse transcriptase kit (Applied Biosystems). Quantitative RT-PCR was carried out with the SsoFastTM EvaGreen® supermix in ABI 9700, and the results were normalized to β-actin.

Knockdown of SIRT3 in Striatal Cells

Stealth RNAi duplexes (Invitrogen) were designed to target mouse SIRT3 (NM_001177804.1; NM_ 022433.2). RNAi treatment of cells was as follows. 1 × 107 cells were collected and electroporated with 400 pm siRNA at 450 V, 600 microfarads. Then 106 cells/well were placed in 6-well plates. After 24 h of recovery in maintenance medium, cells were maintained in serum-free medium for 24 h and then assayed for toxicity or analyzed by Western blotting.

Immunoprecipitation

Cell extracts were prepared by resuspending PBS-washed cell pellets in 1 ml of Nonidet P-40 extraction buffer (50 mm Tris-HCl (pH 8.0), 150 mm NaCl, and 1% Nonidet P-40) supplemented with EDTA-free protease inhibitor mixture tablets (Roche Applied Science) with 10 mm nicotinamide and 5 μm trichostatin A. After incubation for 30 min on ice, nonextractable material was removed by centrifugation at 17,000 × g for 10 min at 4 °C, and the cleared supernatant fractions were subjected to immunoprecipitation.

Statistical Analysis

Data are expressed as means of triplicates ± S.D. from at least three independent experiments. Statistical significance was determined using a Student's t test, accepting a significance level of p < 0.05.

RESULTS

Viniferin Protects Neurons against Mutant Htt-induced Cell Toxicity

To develop small molecular compounds that have high potential to treat HD, we screened our unique collection of 22 stilbenic natural products and their semisynthetic derivatives in an inducible PC12 cell model that we have successfully used for compound screening (28). Among these 22 compounds, we identified six compounds that had protective activity in an inducible PC12 HD cell model. The EC50 ranged from 30 nm to 10 μm (Table 1). Viniferin was the most potent compound that exhibited consistent protection in different cell models of HD, including the transient transfection of mutant Htt N-terminal truncated form in N2a cells (Fig. 1A), immortalized striatal precursor cells expressing full-length huntingtin (Fig. 1B), as well as a primary neuronal model (Fig. 1, C and D). The neuroprotective effect of viniferin is specific to mutant Htt as viniferin had no effect on cell death in untransfected neurons (20 ± 4% in DMSO-untransfected neurons versus 15.6 ± 1.6% in viniferin-treated untransfected neurons).

TABLE 1
Structures and estimated EC50 of six protective compounds from 22 screened natural products
FIGURE 1.
Viniferin decreases mutant Htt toxicity in HD cell models. A, quantification of cell toxicity in N2a cells expressing mutant Htt with or without viniferin (V). #, p < 0.05 versus N63-16Q group, *, p < 0.05 versus vehicle (DMSO) group. ...

Viniferin Reduces Mutant Htt-mediated Oxidative Stress in Striatal Cells

The mitochondrion is the major site of superoxide formation, and the accumulation of superoxide is believed to contribute to oxidative damage associated with neurodegenerative disease (29). Cells expressing mutant Htt exhibited higher levels of ROS in response to withdrawal of trophic factors (serum deprivation). To determine whether viniferin could attenuate mutant Htt-induced accumulation of ROS, striatal cells were incubated in the absence or presence of 1 μm viniferin for 24 h prior to measurement of ROS levels. Intracellular ROS production was measured by fluorescence-activated cell sorting (FACS) with use of the fluorescent probe CM-H2DCFDA (30). Fig. 2A shows a representative image of intracellular ROS levels in striatal cells expressing wild-type Htt (STHdhQ7/Q7), mutant Htt (STHdhQ111/Q111), or STHdhQ111/Q111 cells treated with viniferin. Cells expressing mutant Htt had a greater increase in ROS levels in comparison with cells expressing wild-type Htt (Fig. 2, A and B). Viniferin treatment significantly reduced intracellular ROS accumulation in cells expressing mutant Htt (Fig. 2, A–C).

FIGURE 2.
Viniferin reduces ROS levels in cells expressing mutant Htt (STHdhQ111/Q111). A, representative CM-H2DCFDA-loaded cell images in indicated cells. Note the increased fluorescence in SThdhQ111/Q111 cells, and note that viniferin decreased the fluorescence ...

Viniferin Prevents Mitochondrial Dysfunction, Promotes Mitochondrial Biogenesis, and Attenuates PGC-1α Depletion in Striatal Cells Expressing Mutant Htt

Mutant Htt impaired mitochondrial function, as indicated by loss of mitochondrial membrane potential and lower NAD+/NADH ratios in cells expressing mutant Htt when compared with those expressing wild-type Htt (Fig. 3, A–D). To determine whether viniferin prevents mitochondrial dysfunction, cells expressing wild-type or mutant Htt were treated with 1 μm viniferin for 48 h and then loaded with the mitochondrial dye TRME, and changes in mitochondrial membrane potential were measured by FACS. Cells expressing mutant Htt exhibited lower mitochondrial membrane potential after serum withdrawal than did cells expressing wild-type Htt (Fig. 3A), and viniferin significantly attenuated the loss of mitochondrial potential that occurred in response to serum withdrawal in cells expressing mutant Htt (Fig. 3, B and C).

FIGURE 3.
Viniferin prevents mitochondrial membrane potential loss and promotes mitochondrial biogenesis in STHdhQ111/Q111 cells. A and B, histograms show that the peak of excitation of TMRE fluorescent dye shifted from the right in SThdhQ7/Q7 (Q7) cells (blue ...

To gain insight into the mechanism by which viniferin regulates energy metabolism, we measured intracellular NAD+/NADH levels. Consistent with our hypothesis, viniferin increased the NAD+/NADH ratio (Fig. 3D).

We also evaluated the role of viniferin in mitochondrial biogenesis. To measure mitochondrial DNA directly, we isolated total DNA and determined the relative copy number of mitochondrial DNA by a quantitative PCR assay of the mitochondrial DNA-encoded COX II and 12 S rRNA in striatal cells. Mutant Htt resulted in a significant reduction of mitochondrial DNA, indicating reduced mitochondrial biogenesis (Fig. 3, E and F). Viniferin treatment significantly increased the number of mitochondrial DNA copies, indicating increased mitochondrial biogenesis (Fig. 3, E and F).

PGC-1α, a potent transcriptional coactivator, is the major regulator of mitochondrial biogenesis (31). It has been reported that mutant Htt interrupts PGC-1α transcription and results in decreased PGC-1α levels (3133); therefore, we next determined the effect of viniferin on PGC-1α levels. As we predicted, PGC-1α mRNA levels in SThdhQ111/Q111 cells were significantly lower than were levels in SThdhQ7/Q7 cells (Fig. 3G). Viniferin ameliorated the impairment of PGC-1α expression in HD cells (Fig. 3G).

Viniferin Ameliorates Mutant Htt-induced SIRT3 Decline

To further understand the molecular mechanisms underlying protection by viniferin, we focused on mitochondria. SIRT3 is a mitochondrial sirtuin that plays an important role in energy metabolism and mitochondrial function. Murine SIRT3 includes a long inactive isoform (about 37 kDa) and a short active isoform (about 28 kDa) (3436). Both isoforms were significantly reduced in cells expressing mutant Htt (SThdhQ111/Q111 cells) (Fig. 4A), and viniferin significantly increased the levels of both isoforms of SIRT3 protein in SThdhQ111/Q111 cells (Fig. 4B). To determine whether SIRT3 decrease is the cause or consequence of mitochondria depolarization, we did a time course study. Our results indicated that mutant Htt-expressing SThdhQ111/Q111 cells displayed mitochondrial depolarization before detectable SIRT3 decrease (Fig. 4, C and D), suggesting that the SIRT3 might represent a compensatory response to mitochondrial dysfunction. However, SIRT3 protein levels declined along with persistent mitochondrial dysfunction (Fig. 4C), viniferin preserved SIRT3 protein levels (particularly the 28-kDa active isoform), and this protection lasted longer than its analog resveratrol (Fig. 4, E and F).

FIGURE 4.
Viniferin increases levels of SIRT3 protein and its deacetylase activity. A and B, striatal cells expressing mutant Htt (STHdhQ111/Q111 (Q111)) exhibited lower SIRT3 protein levels than cells expressing normal Htt (STHdhQ7/Q7 (Q7)) at 24 h following serum ...

We then determined whether viniferin also altered the SIRT3 deacetylase activity by measuring the acetylated Mn-SOD, a SIRT3 substrate. We incubated cells with viniferin for 4 h and found that viniferin reduced acetylated Mn-SOD levels, indicating that viniferin increases SIRT3 deacetylase activity (Fig. 4G).

Viniferin Increases SIRT3-dependent AMPK Activation

AMPK is a ubiquitous heterotrimeric serine/threonine protein kinase, which functions as a fuel sensor. Importantly, activated AMPK stimulates ATP-generating catabolic pathways, such as cellular glucose uptake and fatty acid α-oxidation. AMPK activation also represses ATP-consuming processes to restore intracellular energy balance (37, 38). To gain insight into the mechanism by which viniferin protects mitochondrial function, we treated striatal cells expressing mutant Htt with viniferin for 30 min and analyzed the levels of activated AMPK by Western blotting. Viniferin robustly increased the levels of activated AMPK (phosphorylated AMPK) in SThdhQ111/Q111 cells, but total AMPK protein levels remained unchanged (Fig. 5A). This increase in AMPK activation in response to viniferin is more sensitive in SThdhQ111/Q111 cells as we only detected increased AMPK phosphorylation after treatment with high concentrations of viniferin in SThdhQ7/Q7 cells (data not shown). To determine whether activation of AMPK is due to increased SIRT3 mediated by viniferin, we blocked the increase of SIRT3 with SIRT3 siRNA, which abolished the AMPK activation induced by viniferin (Fig. 5B), suggesting that SIRT3 increase is upstream and is required for AMPK activation mediated by viniferin.

FIGURE 5.
Viniferin increases AMPK activation, and SIRT3 is required for viniferin-mediated AMPK activation. A, Western blotting of STHdhQ111/Q111 cells treated with viniferin (V) or vehicle DMSO. The upper panel shows representative blots, and the bottom panel ...

Viniferin Attenuates Mutant Htt-induced Hyperacetylation of LKB1

AMPK is allosterically activated by AMP and by phosphorylation at Thr-172 in the catalytic α-subunit, mainly by an upstream AMPK kinase, LKB1 (39, 40). Because LKB1 regulates AMPK activity (41), we first sought to determine whether LKB1 activity is altered by mutant Htt, and if so, whether viniferin modifies LKB1 activity, which is regulated by phosphorylation or acetylation. First, we measured the levels of phospho-LKB1 in cells expressing mutant Htt versus normal Htt and found that mutant Htt did not alter the levels of phosphorylated LKB1 (data not shown). Viniferin had no effect on LKB1 phosphorylation (data not shown). Remarkably, mutant Htt increased levels of acetylated LKB1, although total LKB1 levels were not altered in cells expressing mutant Htt (Fig. 6A). Viniferin significantly reduced acetylated LKB1 levels in striatal cells expressing mutant Htt (Fig. 6B). Because LKB1 is a substrate of SIRT3, to determine whether the increased acetylated LKB1 is due to the mutant Htt-induced decrease of SIRT3, we performed immunoprecipitation. SIRT3 interacts with LKB1, and viniferin did not alter this interaction (data not shown). Next, to determine whether SIRT3 mediated the effect of viniferin on LKB1 acetylation, we treated cells with SIRT3 siRNA. Inhibition of SIRT3 increased LKB1 acetylation and also abolished the effect of viniferin on the acetylation of LKB1 (Fig. 6C).

FIGURE 6.
Viniferin decreases mutant Htt-induced hyperacetylation of LKB1, and this action is SIRT3-dependent. A, cells expressing mutant Htt exhibit increased levels of acetylated LKB1. The left panel shows representative blots, and the right panel shows quantification ...

SIRT3 Is Required for Viniferin-mediated Neuroprotection against Mutant Htt

Viniferin induced SIRT3 expression and protected cells against mutant Htt-induced neurotoxicity. We then asked whether SIRT3 is a critical mediator of neuroprotection by viniferin. Striatal cells were treated with SIRT3 siRNA before viniferin treatment, and we found that SIRT3 siRNAs completely abolished the protective effects of viniferin on mutant Htt (Fig. 7, A and B), suggesting that SIRT3 is indeed the critical mediator of the neuroprotection of viniferin against mutant Htt.

FIGURE 7.
SIRT3 mediates the protective effects of viniferin on mutant Htt. A, STHdhQ111/Q111 cells were treated with SIRT3 siRNA (10 nm) or scrambled control RNA for 48 h and then collected and analyzed by Western blotting. Note that both the 37-kDa and the 28-kDa ...

DISCUSSION

Our data support a working model for viniferin shown in Fig. 8. Viniferin attenuates mutant Htt-induced depletion of mitochondrial SIRT3, a soluble protein that controls global mitochondrial protein acetylation levels. For example, SIRT3 deacetylates its substrate Mn-SOD and enhances its antioxidant activity; SIRT3 also deacetylates LKB1, resulting in activation of AMPK, and activated AMPK promotes mitochondrial biogenesis and homeostasis of energy metabolism, thereby protecting cells from mutant Htt-mediated mitochondrial dysfunction. Activation of AMPK leads to increased levels of cellular NAD+, which in turn activates SIRT3 and subsequently affects multiple pathways involved in energy metabolism. Our results demonstrate that the effect of viniferin on enhancing mitochondrial function is mediated through SIRT3.

FIGURE 8.
Diagram of the protective mechanism of viniferin. Viniferin counteracts mutant Htt-induced depletion of SIRT3 and facilitates its deacetylase activity. SIRT3 deacetylates its substrates Mn-SOD and then enhances its antioxidant activity. SIRT3 also deacetylates ...

SIRT3 has been shown to play important roles in various mitochondrial functions, such as maintaining basal ATP levels and regulating apoptosis and energy homeostasis (42). Human SIRT3 exists in two isoforms, a full-length protein (~44 kDa) and a shorter, active form (~28 kDa) lacking the N-terminal 142 amino acids (43). The molecular mass of mouse SIRT3 is controversial, however. Our data confirmed the presence of two forms of endogenous mouse SIRT3 (37 and 28 kDa).

Recent studies have indicated that neuronal SIRT3 protects cells against excitotoxicity (44). Notably, we found that mutant Htt depleted SIRT3 protein levels. Although the molecular mechanisms underlying this regulation remain to be investigated, our findings open a new avenue for therapeutic intervention for HD. In this study, we demonstrate that viniferin, a stilbene resveratrol dimer with a five-membered oxygen heterocyclic ring, increases SIRT3 protein levels and plays a neuroprotective role in HD at a range of 100 nm–1 μm. The preservation of SIRT3 protein levels by viniferin is not at the transcriptional level; it might result from enhancing protein translation or slowing down protein degradation. The role of SIRT3 in the maintenance of ATP levels and in regulating mitochondrial electron transport was shown with SIRT3 knock-out mice (45). Constitutive expression of SIRT3 promotes the expression of mitochondrial genes, leading to enhanced mitochondrial electron transport activity (46). Viniferin increased levels of SIRT3, thereby promoting mitochondrial biogenesis and maintaining mitochondrial function.

The role of SIRT3 in regulating ROS production has been demonstrated in that overexpression of SIRT3 reduces ROS in adipocytes (4648), whereas embryonic fibroblasts from SIRT3 knock-out mice exhibited increased levels of superoxide (49). ROS accumulation is associated with the pathogenesis of HD. The increased Mn-SOD activity by viniferin enhanced the antioxidant state in mitochondria accompanied by a significant decrease in ROS levels. ROS can react with DNA, proteins, and lipids and play important roles in many physiological and pathophysiological conditions, including neurodegenerative diseases and aging (50). Although ROS are produced in multiple cell compartments, the majority of cellular ROS (about 90%) contribute to mitochondrial energy metabolism. The mitochondrial electron transport chain complex I and complex III are presumed to be major sites of ROS generation (50), where electrons escape the electron transport chain and react with molecular oxygen, leading to the generation of superoxide. There are two main ways in which ROS production is limited in vivo. The first is through the action of detoxifying enzymes, including glutathione peroxidase-1 (GPx1) and superoxide dismutases (SODs); the second is through the uncoupling proteins (51). Our data suggest that viniferin promotes deacetylation of Mn-SOD and enhances its antioxidant activity, thereby reducing ROS levels.

The mechanism(s) by which different stimuli modulate SIRT3 and activate AMPK in neurons remains to be fully elucidated. For example, activation of acetyl-CoA synthetase 2 (AceCS2) by SIRT3 may elevate the AMP/ATP ratio and consequently activate AMPK. Interestingly, it has also been shown that activation of AMPK causes an increase in the cellular NAD+/NADH ratio, consistent with a positive feedback loop needed for prolonged activation of SIRT3. It is known that activated AMPK directly phosphorylates PGC-1α (52). SIRT3 promotes mitochondrial biogenesis via PGC-1α (53). We have found that viniferin also attenuates mutant Htt-mediated decline of PGC-1α. Although PGC-1α stimulates mitochondrial biogenesis and electron transport activity, it suppresses ROS production and protects neural cells from oxidative stressor-induced death through the induction of several key ROS-detoxifying enzymes (54, 55).

Continuous supply of energy is crucial for neurons because their survival requires large amounts of energy coupled with their inability to store energy. Therefore, neurons are extremely susceptible to insults that lead to energy depletion. NAD is an essential molecule that has a pivotal role in energy metabolism, cellular redox reactions, and mitochondrial function. Recent studies have revealed that maintaining intracellular NAD is important in promoting cell survival in various types of disease. Loss of NAD decreases the ability of NAD-dependent cell survival factors to carry out energy-dependent processes, leading to cell death. Recent evidence has shown that SIRT3 is involved in mitochondrial energy metabolism and biogenesis (56) and preservation of ATP biosynthetic capacity in the heart (45). SIRT3 knock-out resulted in a marked decrease in basal ATP in vivo (57) and eliminated the role of SIRT3 in protection of cells from oxidative stress (58). Our study suggests that viniferin increases SIRT3, stimulates AMPK activities, and preserves NAD levels, and therefore, could have a pivotal role in protecting neurons from mutant Htt, which promotes bioenergetic failure.

Substantial levels of SIRT3 are expressed in the brain (46). Nonetheless, its pathophysiological role remains unclear. In this study, we show, to our knowledge for the first time, that mutant Htt down-regulates SIRT3 protein levels and provide evidence that the neuroprotective role of viniferin is mediated by SIRT3 and that viniferin further enhances the activity of the antioxidant enzyme Mn-SOD and activates AMPK. Taken together, our results indicate that viniferin enhances mitochondrial function and antioxidant activity via an increase of SIRT3 and activation of AMPK and downstream signaling pathways. This mechanism may provide a promising target for development of HD therapeutics.

Acknowledgments

We thank J. Skaggs for providing the Vitis vines and Dr. Pamela Talalay for editorial advice.

*This work was supported, in whole or in part, by National Institutes of Health Grants NINDS NS064313 (to R. H. C.) and NINDS NS16375 (to C. A. R.). This work was also supported by Grant CHDI A2120 from the CHDI Foundation, Inc. (to W. D.).

3The abbreviations used are:

HD
Huntington disease
Htt
huntingtin
SOD
superoxide dismutase
ROS
reactive oxygen species
AMPK
AMP-activated protein kinase
TMRE
Tetramethylrhodamine ethyl ester
CM-H2DCFDA
5-(and-6)-chloromethyl-2′,7′-dichlorodihydrofluorescein diacetate, and acetyl ester
DMSO
dimethyl sulfoxide.

REFERENCES

1. Harper P. S. (1996) New genes for old diseases: the molecular basis of myotonic dystrophy and Huntington disease. The Lumleian Lecture 1995. J. R. Coll. Physicians Lond. 30, 221–231 [PubMed]
2. The Huntington Disease Collaborative Research Group (1993) A novel gene containing a trinucleotide repeat that is expanded and unstable on Huntington disease chromosomes. Cell 72, 971–983 [PubMed]
3. Mochel F., Haller R. G. (2011) Energy deficit in Huntington disease: why it matters. J. Clin. Invest. 121, 493–499 [PMC free article] [PubMed]
4. Stack E. C., Matson W. R., Ferrante R. J. (2008) Evidence of oxidant damage in Huntington disease: translational strategies using antioxidants. Ann. N.Y. Acad. Sci. 1147, 79–92 [PubMed]
5. Beal M. F., Kowall N. W., Ellison D. W., Mazurek M. F., Swartz K. J., Martin J. B. (1986) Replication of the neurochemical characteristics of Huntington disease by quinolinic acid. Nature 321, 168–171 [PubMed]
6. Jin Y. N., Johnson G. V. (2010) The interrelationship between mitochondrial dysfunction and transcriptional dysregulation in Huntington disease. J. Bioenerg. Biomembr. 42, 199–205 [PMC free article] [PubMed]
7. Gibson G. E., Starkov A., Blass J. P., Ratan R. R., Beal M. F. (2010) Cause and consequence: mitochondrial dysfunction initiates and propagates neuronal dysfunction, neuronal death, and behavioral abnormalities in age-associated neurodegenerative diseases. Biochim. Biophys. Acta 1802, 122–134 [PMC free article] [PubMed]
8. Stahl W. L., Swanson P. D. (1974) Biochemical abnormalities in Huntington chorea brains. Neurology 24, 813–819 [PubMed]
9. Mann V. M., Cooper J. M., Javoy-Agid F., Agid Y., Jenner P., Schapira A. H. (1990) Mitochondrial function and parental sex effect in Huntington disease. Lancet 336, 749. [PubMed]
10. Browne S. E., Bowling A. C., MacGarvey U., Baik M. J., Berger S. C., Muqit M. M., Bird E. D., Beal M. F. (1997) Oxidative damage and metabolic dysfunction in Huntington disease: selective vulnerability of the basal ganglia. Ann. Neurol. 41, 646–653 [PubMed]
11. Panov A. V., Gutekunst C. A., Leavitt B. R., Hayden M. R., Burke J. R., Strittmatter W. J., Greenamyre J. T. (2002) Early mitochondrial calcium defects in Huntington disease are a direct effect of polyglutamines. Nat. Neurosci. 5, 731–736 [PubMed]
12. Sawa A., Wiegand G. W., Cooper J., Margolis R. L., Sharp A. H., Lawler J. F., Jr., Greenamyre J. T., Snyder S. H., Ross C. A. (1999) Increased apoptosis of Huntington disease lymphoblasts associated with repeat length-dependent mitochondrial depolarization. Nat. Med. 5, 1194–1198 [PubMed]
13. Milakovic T., Johnson G. V. (2005) Mitochondrial respiration and ATP production are significantly impaired in striatal cells expressing mutant huntingtin. J. Biol. Chem. 280, 30773–30782 [PubMed]
14. Song W., Chen J., Petrilli A., Liot G., Klinglmayr E., Zhou Y., Poquiz P., Tjong J., Pouladi M. A., Hayden M. R., Masliah E., Ellisman M., Rouiller I., Schwarzenbacher R., Bossy B., Perkins G., Bossy-Wetzel E. (2011) Mutant huntingtin binds the mitochondrial fission GTPase dynamin-related protein-1 and increases its enzymatic activity. Nat. Med. 17, 377–382 [PMC free article] [PubMed]
15. Schwer B., North B. J., Frye R. A., Ott M., Verdin E. (2002) The human silent information regulator (Sir)2 homologue hSIRT3 is a mitochondrial nicotinamide adenine dinucleotide-dependent deacetylase. J. Cell Biol. 158, 647–657 [PMC free article] [PubMed]
16. Lombard D. B., Alt F. W., Cheng H. L., Bunkenborg J., Streeper R. S., Mostoslavsky R., Kim J., Yancopoulos G., Valenzuela D., Murphy A., Yang Y., Chen Y., Hirschey M. D., Bronson R. T., Haigis M., Guarente L. P., Farese R. V., Jr., Weissman S., Verdin E., Schwer B. (2007) Mammalian Sir2 homolog SIRT3 regulates global mitochondrial lysine acetylation. Mol. Cell. Biol. 27, 8807–8814 [PMC free article] [PubMed]
17. Koehn F. E., Carter G. T. (2005) The evolving role of natural products in drug discovery. Nat. Rev. Drug Disc. 4, 206–220 [PubMed]
18. Feher M., Schmidt J. M. (2003) Property distributions: differences between drugs, natural products, and molecules from combinatorial chemistry. J. Chem. Inf. Comput. Sci. 43, 218–227 [PubMed]
19. Joyner P. M., Cichewicz R. H. (2011) Bringing natural products into the fold: exploring the therapeutic lead potential of secondary metabolites for the treatment of protein-misfolding-related neurodegenerative diseases. Nat. Prod. Rep. 28, 26–47 [PubMed]
20. Richard T., Pawlus A. D., Iglésias M. L., Pedrot E., Waffo-Teguo P., Mérillon J. M., Monti J. P. (2011) Neuroprotective properties of resveratrol and derivatives. Ann. N.Y. Acad. Sci. 1215, 103–108 [PubMed]
21. Vang O., Ahmad N., Baile C. A., Baur J. A., Brown K., Csiszar A., Das D. K., Delmas D., Gottfried C., Lin H. Y., Ma Q. Y., Mukhopadhyay P., Nalini N., Pezzuto J. M., Richard T., Shukla Y., Surh Y. J., Szekeres T., Szkudelski T., Walle T., Wu J. M. (2011) What is new for an old molecule? Systematic review and recommendations on the use of resveratrol. PLoS One 6, e19881. [PMC free article] [PubMed]
22. Maher P., Dargusch R., Bodai L., Gerard P. E., Purcell J. M., Marsh J. L. (2011) ERK activation by the polyphenols fisetin and resveratrol provides neuroprotection in multiple models of Huntington disease. Hum. Mol. Genet. 20, 261–270 [PMC free article] [PubMed]
23. Pallos J., Bodai L., Lukacsovich T., Purcell J. M., Steffan J. S., Thompson L. M., Marsh J. L. (2008) Inhibition of specific HDACs and sirtuins suppresses pathogenesis in a Drosophila model of Huntington disease. Hum. Mol. Genet. 17, 3767–3775 [PubMed]
24. Parker J. A., Arango M., Abderrahmane S., Lambert E., Tourette C., Catoire H., Néri C. (2005) Resveratrol rescues mutant polyglutamine cytotoxicity in nematode and mammalian neurons. Nat. Genet. 37, 349–350 [PubMed]
25. Ho D. J., Calingasan N. Y., Wille E., Dumont M., Beal M. F. (2010) Resveratrol protects against peripheral deficits in a mouse model of Huntington disease. Exp. Neurol. 225, 74–84 [PubMed]
26. Wang Q., Xu J., Rottinghaus G. E., Simonyi A., Lubahn D., Sun G. Y., Sun A. Y. (2002) Resveratrol protects against global cerebral ischemic injury in gerbils. Brain Res. 958, 439–447 [PubMed]
27. Trettel F., Rigamonti D., Hilditch-Maguire P., Wheeler V. C., Sharp A. H., Persichetti F., Cattaneo E., MacDonald M. E. (2000) Dominant phenotypes produced by the HD mutation in STHdhQ111 striatal cells. Hum. Mol. Genet. 9, 2799–2809 [PubMed]
28. Wang W., Duan W., Igarashi S., Morita H., Nakamura M., Ross C. A. (2005) Compounds blocking mutant huntingtin toxicity identified using a Huntington disease neuronal cell model. Neurobiol. Dis. 20, 500–508 [PubMed]
29. Brand M. D., Buckingham J. A., Esteves T. C., Green K., Lambert A. J., Miwa S., Murphy M. P., Pakay J. L., Talbot D. A., Echtay K. S. (2004) Mitochondrial superoxide and aging: uncoupling-protein activity and superoxide production. Biochem. Soc. Symp. 203–213 [PubMed]
30. Sapkota G. P., Kieloch A., Lizcano J. M., Lain S., Arthur J. S., Williams M. R., Morrice N., Deak M., Alessi D. R. (2001) Phosphorylation of the protein kinase mutated in Peutz-Jeghers cancer syndrome, LKB1/STK11, at Ser-431 by p90RSK and cAMP-dependent protein kinase, but not its farnesylation at Cys-433, is essential for LKB1 to suppress cell growth. J. Biol. Chem. 276, 19469–19482 [PubMed]
31. Lin J., Wu P. H., Tarr P. T., Lindenberg K. S., St-Pierre J., Zhang C. Y., Mootha V. K., Jäger S., Vianna C. R., Reznick R. M., Cui L., Manieri M., Donovan M. X., Wu Z., Cooper M. P., Fan M. C., Rohas L. M., Zavacki A. M., Cinti S., Shulman G. I., Lowell B. B., Krainc D., Spiegelman B. M. (2004) Defects in adaptive energy metabolism with CNS-linked hyperactivity in PGC-1α null mice. Cell 119, 121–135 [PubMed]
32. Cui L., Jeong H., Borovecki F., Parkhurst C. N., Tanese N., Krainc D. (2006) Transcriptional repression of PGC-1α by mutant huntingtin leads to mitochondrial dysfunction and neurodegeneration. Cell 127, 59–69 [PubMed]
33. Weydt P., Pineda V. V., Torrence A. E., Libby R. T., Satterfield T. F., Lazarowski E. R., Gilbert M. L., Morton G. J., Bammler T. K., Strand A. D., Cui L., Beyer R. P., Easley C. N., Smith A. C., Krainc D., Luquet S., Sweet I. R., Schwartz M. W., La Spada A. R. (2006) Thermoregulatory and metabolic defects in Huntington disease transgenic mice implicate PGC-1α in Huntington disease neurodegeneration. Cell Metab. 4, 349–362 [PubMed]
34. Cimen H., Han M. J., Yang Y., Tong Q., Koc H., Koc E. C. (2010) Regulation of succinate dehydrogenase activity by SIRT3 in mammalian mitochondria. Biochemistry 49, 304–311 [PMC free article] [PubMed]
35. Yang Y., Cimen H., Han M. J., Shi T., Deng J. H., Koc H., Palacios O. M., Montier L., Bai Y., Tong Q., Koc E. C. (2010) NAD+-dependent deacetylase SIRT3 regulates mitochondrial protein synthesis by deacetylation of the ribosomal protein MRPL10. J. Biol. Chem. 285, 7417–7429 [PMC free article] [PubMed]
36. Yang Y., Hubbard B. P., Sinclair D. A., Tong Q. (2010) Characterization of murine SIRT3 transcript variants and corresponding protein products. J. Cell. Biochem. 111, 1051–1058 [PMC free article] [PubMed]
37. Kahn B. B., Alquier T., Carling D., Hardie D. G. (2005) AMP-activated protein kinase: ancient energy gauge provides clues to modern understanding of metabolism. Cell Metab. 1, 15–25 [PubMed]
38. Kemp B. E., Stapleton D., Campbell D. J., Chen Z. P., Murthy S., Walter M., Gupta A., Adams J. J., Katsis F., van Denderen B., Jennings I. G., Iseli T., Michell B. J., Witters L. A. (2003) AMP-activated protein kinase, super metabolic regulator. Biochem. Soc. Trans. 31, 162–168 [PubMed]
39. Hawley S. A., Boudeau J., Reid J. L., Mustard K. J., Udd L., Mäkelä T. P., Alessi D. R., Hardie D. G. (2003) Complexes between the LKB1 tumor suppressor, STRAD α/β and MO25 α/β are upstream kinases in the AMP-activated protein kinase cascade. J. Biol. 2, 28. [PMC free article] [PubMed]
40. Woods A., Johnstone S. R., Dickerson K., Leiper F. C., Fryer L. G., Neumann D., Schlattner U., Wallimann T., Carlson M., Carling D. (2003) LKB1 is the upstream kinase in the AMP-activated protein kinase cascade. Curr. Biol. 13, 2004–2008 [PubMed]
41. Shaw R. J., Kosmatka M., Bardeesy N., Hurley R. L., Witters L. A., DePinho R. A., Cantley L. C. (2004) The tumor suppressor LKB1 kinase directly activates AMP-activated kinase and regulates apoptosis in response to energy stress. Proc. Natl. Acad. Sci. U.S.A. 101, 3329–3335 [PubMed]
42. Verdin E., Hirschey M. D., Finley L. W., Haigis M. C. (2010) Sirtuin regulation of mitochondria: energy production, apoptosis, and signaling. Trends Biochem. Sci. 35, 669–675 [PMC free article] [PubMed]
43. Saunders L. R., Verdin E. (2007) Sirtuins: critical regulators at the crossroads between cancer and aging. Oncogene 26, 5489–5504 [PubMed]
44. Kim S. H., Lu H. F., Alano C. C. (2011) Neuronal Sirt3 protects against excitotoxic injury in mouse cortical neuron culture. PLoS One 6, e14731. [PMC free article] [PubMed]
45. Ahn B. H., Kim H. S., Song S., Lee I. H., Liu J., Vassilopoulos A., Deng C. X., Finkel T. (2008) A role for the mitochondrial deacetylase Sirt3 in regulating energy homeostasis. Proc. Natl. Acad. Sci. U.S.A. 105, 14447–14452 [PubMed]
46. Shi T., Wang F., Stieren E., Tong Q. (2005) SIRT3, a mitochondrial sirtuin deacetylase, regulates mitochondrial function and thermogenesis in brown adipocytes. J. Biol. Chem. 280, 13560–13567 [PubMed]
47. Bell E. L., Emerling B. M., Ricoult S. J., Guarente L. (2011) SirT3 suppresses hypoxia-inducible factor 1α and tumor growth by inhibiting mitochondrial ROS production. Oncogene 30, 2986–2996 [PMC free article] [PubMed]
48. Bell E. L., Guarente L. (2011) The SirT3 divining rod points to oxidative stress. Mol. Cell 42, 561–568 [PMC free article] [PubMed]
49. Tao R., Karliner J. S., Simonis U., Zheng J., Zhang J., Honbo N., Alano C. C. (2007) Pyrroloquinoline quinone preserves mitochondrial function and prevents oxidative injury in adult rat cardiac myocytes. Biochem. Biophys. Res. Commun. 363, 257–262 [PMC free article] [PubMed]
50. Balaban R. S., Nemoto S., Finkel T. (2005) Mitochondria, oxidants, and aging. Cell 120, 483–495 [PubMed]
51. Arsenijevic D., Onuma H., Pecqueur C., Raimbault S., Manning B. S., Miroux B., Couplan E., Alves-Guerra M. C., Goubern M., Surwit R., Bouillaud F., Richard D., Collins S., Ricquier D. (2000) Disruption of the uncoupling protein-2 gene in mice reveals a role in immunity and reactive oxygen species production. Nat. Genet. 26, 435–439 [PubMed]
52. Schwer B., Bunkenborg J., Verdin R. O., Andersen J. S., Verdin E. (2006) Reversible lysine acetylation controls the activity of the mitochondrial enzyme acetyl-CoA synthetase 2. Proc. Natl. Acad. Sci. U.S.A. 103, 10224–10229 [PubMed]
53. Ying W., Garnier P., Swanson R. A. (2003) NAD+ repletion prevents PARP-1-induced glycolytic blockade and cell death in cultured mouse astrocytes. Biochem. Biophys. Res. Commun. 308, 809–813 [PubMed]
54. St-Pierre J., Drori S., Uldry M., Silvaggi J. M., Rhee J., Jäger S., Handschin C., Zheng K., Lin J., Yang W., Simon D. K., Bachoo R., Spiegelman B. M. (2006) Suppression of reactive oxygen species and neurodegeneration by the PGC-1 transcriptional coactivators. Cell 127, 397–408 [PubMed]
55. Uldry M., Yang W., St-Pierre J., Lin J., Seale P., Spiegelman B. M. (2006) Complementary action of the PGC-1 coactivators in mitochondrial biogenesis and brown fat differentiation. Cell Metab. 3, 333–341 [PubMed]
56. Jin L., Galonek H., Israelian K., Choy W., Morrison M., Xia Y., Wang X., Xu Y., Yang Y., Smith J. J., Hoffmann E., Carney D. P., Perni R. B., Jirousek M. R., Bemis J. E., Milne J. C., Sinclair D. A., Westphal C. H. (2009) Biochemical characterization, localization, and tissue distribution of the longer form of mouse SIRT3. Protein Sci. 18, 514–525 [PubMed]
57. Hallows W. C., Lee S., Denu J. M. (2006) Sirtuins deacetylate and activate mammalian acetyl-CoA synthetases. Proc. Natl. Acad. Sci. U.S.A. 103, 10230–10235 [PubMed]
58. Pillai V. B., Sundaresan N. R., Kim G., Gupta M., Rajamohan S. B., Pillai J. B., Samant S., Ravindra P. V., Isbatan A., Gupta M. P. (2010) Exogenous NAD blocks cardiac hypertrophic response via activation of the SIRT3-LKB1-AMP-activated kinase pathway. J. Biol. Chem. 285, 3133–3144 [PMC free article] [PubMed]

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