PPAR Research
VolumeΒ 2008Β (2008), Article IDΒ 316306, 11 pages
doi:10.1155/2008/316306
Research Article

Statins Activate Human PPAR 𝛼 Promoter and Increase PPAR 𝛼 mRNA Expression and Activation in HepG2 Cells

Makoto Seo,1Β Ikuo Inoue,2Β Masaaki Ikeda,3,4Β Takanari Nakano,1Β Seiichiro Takahashi,2Β Shigehiro Katayama,2Β and Tsugikazu Komoda1

1Department of Biochemistry, Faculty of Medicine, Saitama Medical University, Saitama 350-0495, Japan
2Department of Endocrinology and Diabetes, Faculty of Medicine, Saitama Medical University, Saitama 350-0495, Japan
3Department of Physiology, Faculty of Medicine, Saitama Medical University, Saitama 350-0495, Japan
4Molecular Clock Project, Research Center for Genomic Medicine, Saitama Medical University, Saitama 350-0495, Japan

Received 17 June 2008; Revised 17 September 2008; Accepted 2 October 2008

Academic Editor: HowardΒ Glauert

Copyright Β© 2008 Makoto Seo 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.

Abstract

Statins increase peroxisome proliferator-activated receptor 𝛼 (PPAR 𝛼 ) mRNA expression, but the mechanism of this increased PPAR 𝛼 production remains elusive. To examine the regulation of PPAR 𝛼 production, we examined the effect of 7 statins (atorvastatin, cerivastatin, fluvastatin, pitavastatin, pravastatin, rosuvastatin, and simvastatin) on human PPAR 𝛼 promoter activity, mRNA expression, nuclear protein levels, and transcriptional activity. The main results are as follows. (1) Majority of statins enhanced PPAR 𝛼 promoter activity in a dose-dependent manner in HepG2 cells transfected with the human PPAR 𝛼 promoter. This enhancement may be mediated by statin-induced HNF-4 𝛼 . (2) PPAR 𝛼 mRNA expression was increased by statin treatment. (3) The PPAR 𝛼 levels in nuclear fractions were increased by statin treatment. (4) Simvastatin, pravastatin, and cerivastatin markedly enhanced transcriptional activity in 293T cells cotransfected with acyl-coenzyme A oxidase promoter and PPAR 𝛼 /RXR 𝛼 expression vectors. In summary, these data demonstrate that PPAR 𝛼 production and activation are upregulated through the PPAR 𝛼 promoter activity by statin treatment.

1. Introduction

Statins, 3-hydroxy-3-methylglutaryl coenzyme A (HMG-CoA) reductase inhibitors, are the most widely used drugs to lower low-density lipoprotein (LDL) cholesterol. These mechanisms have been reported that treatment with statins results in lowering intracellular cholesterol concentration, and then increasing a proteolytic activation of sterol responsive element-binding proteins (SREBPs) [1]. These transcription factors increase the cholesterol homeostasis controlling genes, such as LDL receptor, lipoprotein lipase, and cholesterol 7 𝛼 -hydroxylase [2, 3].

Currently, statins are the first choice of therapeutic agent for the treatment of hyperlipidemia. Several mega trials and large cohort studies using statins have shown that statins prevent coronary heart disease and decrease the incidence of cardiovascular events [4–6]. The reasons why cardiovascular events were decreased with statins are reported to be due to many pleiotropic effects, for example, inhibition of the proliferation and migration of endothelial cells, smooth muscle cells, and macrophages [7, 8]. Moreover, statins up-regulate the expression of endothelial nitric oxide synthesis [9] and suppress oxidative stress, as seen in the reduced formation of reactive oxygen species and p 2 2 p h o x expression [10, 11].

The peroxisome proliferator-activated receptors (PPARs) belong to the nuclear receptor superfamily and play an important role in the regulation of lipid and glucose metabolism and adipocyte differentiation [12, 13]. PPAR 𝛼 is expressed in the liver, kidney, heart, and muscle where it regulates energy homeostasis. PPAR 𝛼 forms a heterodimer with retinoid X receptor 𝛼 (RXR 𝛼 ), which enhances its binding to peroxisome proliferator response elements (PPREs) and activates target genes. PPAR 𝛼 activates the uptake and catabolism of fatty acids that result in a decrease of triglyceride (TG), stimulate gluconeogenesis, and enhance high-density lipoprotein synthesis [14, 15]. Fibrates, which are a ligand for PPAR 𝛼 , have been reported to lower the serum TG levels [16]. Some statins were also reported to decrease the serum TG levels to same extent [17–19]. Although it is reported that several statins increase PPAR 𝛼 [20, 21], it is not clear how statins regulate nuclear transcription, and PPAR 𝛼 mRNA expression and activity. Previously, simvastatin activated mouse PPAR 𝛼 promoter and induced the transcription of PPAR 𝛼 gene [22], but there is no report that statins activate the human PPAR 𝛼 promoter and transcription of this gene.

In the present study, we investigated the effect of 7 statins (atorvastatin, cerivastatin, fluvastatin, pitavastatin, pravastatin, rosuvastatin, simvastatin) on the regulation of PPAR 𝛼 mRNA expression and PPAR 𝛼 protein levels in nuclear fraction of the human hepatoblastoma cell line (HepG2 cells). We also investigated the effect of statin treatment on the promoter activity of the human PPAR 𝛼 gene. In addition, we investigated whether statin treatment could induce transcriptional activity of PPAR 𝛼 .

2. Materials and Methods

2.1. Reagents and Cell Culture

Seven statins were kindly provided as follows; atorvastain (Warner-Lambert Co., Ltd.), cerivastatin (Bayel Co., Ltd.), fluvastatin (Novartis Co., Ltd.), pitavastatin (Kowa Co., Ltd.), pravastatin (Sankyo Co., Ltd.), and rosuvastatin (AstraZeneca Ltd.). Simvastatin was purchased from Wako Pure Chemical Industries, Ltd. (Tokyo, Japan). Fenofibric acid (FA) was kindly provided by Kaken Pharmaceutical Co., Ltd. Atorvastatin, cerivastatin, fluvastatin, pitavastatin, rosuvastatin, and FA were dissolved in dimethyl sulfoxide (DMSO); simvastatin was dissolved in ethanol, and pravastatin was dissolved in distilled water. In all assays, the final concentrations of DMSO and ethanol were less than 0.5%. HepG2 cells was purchased from JCRB (cell number: JCRB1054) and human kidney 293T cells (293T cells) from Dainippon Pharmaceutical Co., Ltd. They were cultured in Dulbecco's modified Eagle's medium (DMEM) (Invitrogen) containing 10% heat-inactivated fetal bovine serum (FBS) (JRH Biosciences) and PNS antibiotic mixture (Invitrogen) at 3 7 ∘ C in 5 % C O 2 .

2.2. Cloning of the PPAR 𝛼 Promoter and Plasmid Constructions

To generate human PPAR 𝛼 promoter-reporter plasmid, we referred to the genomic sequence that has been reported previously [23]. Human PPAR 𝛼 promoter containing βˆ’ 1 5 5 3 bp to + 8 8 b p was obtained by polymerase chain reaction (PCR) with human genomic DNA (Clontech) using a forward primer 5 ξ…ž -CATAAGCTTACCCCACGAGATATGCAGGAT- 3 ξ…ž (including a Hind III site, underlined) and a reverse primer 5 ξ…ž -CGTAAGCTTCGCAAGAGTCCTCGGTGTGT- 3 ξ…ž (including a Hind III site, underlined). This promoter was cloned into the Hind III site of a pGL3-Basic vector (Promega). Plasmid DNA used for transfection was prepared using the Wizard Plus Minipreps DNA Purification System (Promega). Nucleotide sequences of this plasmid were confirmed by sequencing using ABI PRISM 310 Genetic Analyzer (Applied Biosystems).

2.3. Luciferase Assay of PPAR 𝛼 Promoter Activity

HepG2 cells were transfected using Lipofectamine 2000 (Invitrogen) according to the manufacturer’s protocols. The cells ( 1 Γ— 1 0 5 cells/well) were seeded in 24-well plates (Falcon) and incubated for 18 hours before transfection. The cells were transfected with the use of Lipofectamine 2000 with 1 πœ‡ g of human PPAR 𝛼 promoter-reporter plasmid and 0 . 1 πœ‡ g of pRL-TK (Promega), a renilla luciferase reporter vector as internal control for transfection efficiency. After 3 hours, the transfection medium was replaced by 10% FBS-DMEM plus the various amounts of statin (0, 1, 10, 25, and 5 0 πœ‡ M ) or vehicle (DMSO, ethanol, or distilled water) and the cells were incubated for 24 hours. Luciferase activities were quantified using a Dual-Luciferase Reporter Assay System (Promega) according to the manufacturer’s protocols.

2.4. Real-Time Reverse Transcription (RT)-PCR Analysis

HepG2 cells ( 2 Γ— 1 0 5 cells/dish) were incubated with various amounts of statin (0, 5, 10, and 2 0 πœ‡ M , pravastatin was 50, 100, and 2 5 0 πœ‡ M ) at 3 7 ∘ C for 24 hours. After treatment with statins, cells were homogenized in 1 mL of ISOGEN (Nippongene), and then total RNA was extracted with chloroform and precipitated with ethanol. First-strand cDNA was generated from total RNA with random hexamers and MuLV transcriptase (Applied Biosystems) according to the manufacturer’s protocols. PCR reactions were performed with TaqMan Universal PCR Master Mix and TaqMan Gene Expression Assays (Applied Biosystems). Identification numbers of the assay mixture of target gene-specific primers and probes were as follows: human PPAR 𝛼 , Hs00231882_m1; 18S ribosomal RNA (house-keeping gene), Hs99999901_s1. Real-time PCR reactions were performed with thermal cycling conditions of 2 minutes at 5 0 ∘ C , 10 minutes at 9 5 ∘ C , and 40 cycles of 15 seconds at 9 5 ∘ C and 1 minute at 6 0 ∘ C using ABI PRISM 7900HT Sequence Detection System (Applied Biosystems). PPAR 𝛼 mRNA levels were normalized to 18S ribosomal RNA levels, and are presented as fold difference of statin-treated cells compared with untreated cells.

2.5. Western Blot Analysis

HepG2 cells ( 2 Γ— 1 0 5 cells/dish) were seeded in 60 mm dishes (Falcon) and incubated for 18 hours. Then, the cells were incubated with 10 and 2 5 πœ‡ M statin at 3 7 ∘ C for 24 hours. After treatment with statins, cells were washed with ice-cold phosphate buffered saline and collected. After centrifugation (15,000×g), the cytoplasmic and nuclear proteins of the cells were extracted with NE-PER Nuclear and Cytoplasmic Extraction Reagents (PIERCE) according to the manufacturer’s protocols and the proteins concentration was determined with a BCA Protein Assay kit (PIERCE). Aliquots ( 1 5 πœ‡ g ) of cytoplasmic or nuclear proteins were electrophoresed on 9% sodium dodecyl sulfate-polyacrylamide gels and transferred to polyvinylidene difluoride membranes (Millipore). The membranes were blocked with BlockingOne (Nacalai Tesque, Inc.), and incubated overnight with goat anti-PPAR 𝛼 IgG antibody (sc-1985, Santa Cruz) (diluted 1:1000 with BlockingOne) or mouse anti-hepatocyte nuclear factor-4 𝛼 (HNF-4 𝛼 ) IgG antibody (Clone no.: H1415, Perseus Proteomics Co., Ltd.). After washing four times with Tris-buffered saline-containing 0.5% Tween 20, signals from Western blots were obtained using horseradish peroxidase-conjugated secondary anti-goat antibody (diluted 1:2000 with BlockingOne) and visualized with the ECL detection system (Amersham Biosciences). The PPAR 𝛼 protein levels were quantified with an imaging analyzer (Densitograph, ATTO). The data are expressed as % of control.

2.6. Luciferase Assay of PPRE Activity

Constructions of pCI-PPAR 𝛼 and pCI-RXR 𝛼 expression plasmids were described previously [24]. Briefly, the full-length human PPAR 𝛼 (GenBank accession no. L_02932) and human RXR 𝛼 (GenBank accession no. X_52773) were prepared by PCR. The specific DNA fragmant of human PPAR 𝛼 was cloned into the SalI-NotI sites of the pCI-neo mammalian expression vector (Promega). The human RXR 𝛼 was also cloned into the XhoI-NotI sites of the pCI-neo. The human acyl-coenzyme A oxidase (AOX) promoter (GenBank accession no. NT_010641) construct containing the PPREs was previously cloned into the KpnI-NcoI sites of pGL3-Basic vector [25].

To measure the transcriptional activation of PPRE, 293T cells ( 0 . 5 Γ— 1 0 5 cells/well) were seeded in collagen type I-coated 24-well plate (Iwaki) and incubated for 18 hours before transfection. The cells were transfected using Lipofectamine 2000 with 0 . 5 πœ‡ g of human AOX promoter-reporter plasmid, 0 . 1 πœ‡ g of pRL-TK as internal control for transfection efficiency and either 0 . 2 5 πœ‡ g of pCI-PPAR 𝛼 and pCI-RXR 𝛼 expression vectors or 0 . 5 πœ‡ g of pCI-neo vector. After 3 hours, the transfection medium was replaced by 10% FBS-DMEM plus the various amounts of statin (0, 1, 10, 25, and 5 0 πœ‡ M ), fenofibric acid (0, 1, 10, 50, 1 0 0 πœ‡ M ), or vehicle (DMSO, ethanol, or distilled water) and the cells were incubated for 24 hours. Luciferase activities were quantified using a Dual-Luciferase Reporter Assay System (Promega) according to the manufacturer’s protocols.

2.7. Statistical Analysis

All data are presented as the means Β± SEM. Statistical analysis was performed using ANOVA followed by the Dunnett test or Scheffe test (StatView software). Statistical significance was considered as 𝑃 < . 0 5 .

3. Results

3.1. Statins Increased PPAR 𝛼 mRNA Expression in HepG2 Cells

We first examined the effect of simvastatin on the PPAR 𝛼 mRNA expression in HepG2 cells. The time-course study for the PPAR 𝛼 mRNA expression in HepG2 cells treated with 1 0 πœ‡ M simvastatin is shown in Figure 1. Simvastatin significantly increased PPAR 𝛼 mRNA expression by 2.0-fold (versus the control) at 12 and 24 hours.

316306.fig.001
Figure 1: Time-course of PPAR 𝛼 mRNA expression in HepG2 cells after treatment with 1 0 πœ‡ M simvastatin. The data are expressed as % of controls at 0 hour. Values are presented as the mean Β± SEM of three separate experiments, significantly different from control at βˆ— 𝑃 < . 0 5 , βˆ— βˆ— 𝑃 < . 0 1 .

We next examined the effect of atorvastatin, cerivastatin, fluvastatin, pitavastatin, pravastatin, rosuvastatin, and simvastatin for 24 hours on PPAR 𝛼 mRNA expression in HepG2 cells. PPAR 𝛼 mRNA expression following treatment of HepG2 cells with various amounts of statin is shown in Figure 2. In Figure 2(a), atorvastatin ( 2 0 πœ‡ M ), cerivastatin (5, 10, and 2 0 πœ‡ M ), fluvastatin (5, 10, and 2 0 πœ‡ M ), pitavastatin ( 2 0 πœ‡ M ), rosuvastatin ( 1 0 πœ‡ M ), and simvastatin ( 1 0 πœ‡ M ) significantly increased PPAR 𝛼 mRNA expression by more than 1.5-fold (versus the control). Pravastatin did not increase PPAR 𝛼 mRNA expression at these concentrations, but the higher concentrations of pravastatin-treatment (100 and 2 5 0 πœ‡ M ) significantly increased PPAR 𝛼 mRNA expression (Figure 2(b)).

fig2
Figure 2: PPAR 𝛼 mRNA expression in HepG2 cells after treatment with atorvastatin (Ator), cerivastatin (Ceri), fluvastatin (Flu), pitavastatin (Pita), pravastatin (Pra), rosuvastatin (Rosu), and simvastatin (Sim) for 24 hours. (a) Each statin was used at concentrations of 5, 10, and 2 0 πœ‡ M . Nontreated cells (statin concentration 0 πœ‡ M ) were the control. (b) Pravastatin was used at higher concentrations of 20, 50, 100, and 2 5 0 πœ‡ M . Nontreated cells (pravastatin concentration 0 πœ‡ M ) were the control. The data are expressed as % of controls. Values are presented as the mean Β± SEM of three separate experiments, significantly different from control at βˆ— 𝑃 < . 0 5 , βˆ— βˆ— 𝑃 < . 0 1 .
3.2. Statins Increased Human PPAR 𝛼 Promoter Activity

To investigate the mechanism by which statins increase PPAR 𝛼 mRNA expression, we cloned the human PPAR 𝛼 promoter region ( βˆ’ 1 5 5 3 to + 8 8  bp) and examined promoter activity in HepG2 cells transfected with the human PPAR 𝛼 promoter-reporter plasmid. Figure 3 shows the PPAR 𝛼 promoter activity following treatment of HepG2 cells with various amounts of statin for 24 hours. Except for pravastatin, 6 statins significantly increased PPAR 𝛼 promoter activity in a dose-dependent manner. Atorvastatin, cerivastatin, fluvastatin, rosuvastatin, and simvastatin increased PPAR 𝛼 promoter activity by more than 1.5-fold (versus the control). However, pravastatin only slightly increased PPAR 𝛼 promoter activity that was significant only at 1 0 πœ‡ M .

316306.fig.003
Figure 3: PPAR 𝛼 promoter activity in HepG2 cells transfected with human PPAR 𝛼 promoter-reporter plasmid after treatment with atorvastatin (Ator), cerivastatin (Ceri), fluvastatin (Flu), pitavastatin (Pita), pravastatin (Pra), rosuvastatin (Rosu), and simvastatin (Sim) for 24 hours. Each statin was used at doses of 1, 10, 25, and 5 0 πœ‡ M . Nontreated cells (statin concentration 0 πœ‡ M ) were the control. The data are expressed as % of controls. Values are presented as the mean Β± SEM of three separate experiments, significantly different from control at βˆ— 𝑃 < . 0 5 , βˆ— βˆ— 𝑃 < . 0 1 .
3.3. Statins Increased PPAR 𝛼 Levels in Nuclear Fraction

We next examined the increasing effect of statins on PPAR 𝛼 protein levels in nuclear fraction of HepG2 cells. Results are shown in Figure 4. In a nuclear fraction of HepG2 cells treated with 1 0 πœ‡ M statin, PPAR 𝛼 protein levels were significantly increased by treatment with rosuvastatin (Figure 4(a)). Moreover, PPAR 𝛼 protein levels were significantly increased by treatment with 2 5 πœ‡ M of pitavastatin, simvastatin, and atorvastatin, and the other statins slightly increased PPAR 𝛼 protein levels (Figure 4(b)). However, in a cytoplasmic fraction, PPAR 𝛼 protein levels were not changed by the treatment with 10 and 2 5 πœ‡ M statins.

fig4
Figure 4: The Western blots represent PPAR 𝛼 protein levels in nuclear fractions of HepG2 cells after treatment with 1 0 πœ‡ M (a) and 2 5 πœ‡ M (b) of statin for 24 hours (Cont., control; Ator, atorvastatin; Ceri, cerivastatin; Flu, fluvastatin; Pita, pitavastatin; Pra, pravastatin; Rosu, rosuvastatin; Sim, simvastatin). The PPAR 𝛼 protein levels were quantified with an imaging analyzer. The data are expressed as % of control. Values are presented as the mean Β± SEM of three separate experiments, significantly different from control at βˆ— 𝑃 < . 0 5 , βˆ— βˆ— 𝑃 < . 0 1 .
3.4. Statins Increased PPAR 𝛼 Activity

We next examined the effect of statins on the transcriptional activity of PPAR 𝛼 in 293T cells transfected with human AOX promoter-reporter plasmid containing PPREs region, human PPAR 𝛼 , and RXR 𝛼 expression plasmids. In Figure 5(a), fenofibric acid that was used as a positive control increased PPAR 𝛼 activity in a dose-dependent manner. In Figure 5(b), the treatment with cerivastatin ( 1 0 πœ‡ M ) and simvastatin ( 5 0 πœ‡ M ) significantly increased transcriptional activity of PPAR 𝛼 by more than 1.5-fold (versus the control). Fluvastatin, pitavastatin, pravastatin, and rosuvastatin tended to increase transcriptional activity of PPAR 𝛼 by 1.2- to 1.4-fold (versus the control). However, atorvastatin did not increase the transcriptional activity of PPAR 𝛼 .

fig5
Figure 5: The transcriptional activity of PPAR 𝛼 in HepG2 cells transfected with human acyl-CoA oxidase (AOX) promoter-reporter plasmid after treatment with fenofibric acid (FA) and statins for 24 hours. (a) FA was used at doses of 1, 10, 50, and 1 0 0 πœ‡ M . Nontreated cells (FA concentration 0 πœ‡ M ) were the control. (b) Atorvastatin (Ator), cerivastatin (Ceri), fluvastatin (Flu), pitavastatin (Pita), pravastatin (Pra), rosuvastatin (Rosu), and simvastatin (Sim) for 24 hours. Each statin was used at doses of 1, 10, 25, and 5 0 πœ‡ M . Nontreated cells (statin concentration 0 πœ‡ M ) were the control. The data are expressed as % of control. Values are presented as the mean Β± SEM of three separate experiments, significantly different from control at βˆ— 𝑃 < . 0 5 , βˆ— βˆ— 𝑃 < . 0 1 .
3.5. Statins Increased HNF-4 𝛼 Levels in Nuclear Fraction

Next, to elucidate the downstream effects of statins on transcriptional activation by PPAR 𝛼 , we detected HNF-4 𝛼 levels in nuclear fraction of HepG2 cells treated with statins by the use of Western blot analysis. Results are shown in Figure 6. At 1 0 πœ‡ M statin treatment, fluvastatin, pravastatin, and rosuvastatin significantly increased HNF-4 𝛼 levels in nuclear fraction (Figure 6(a)). Moreover, at 2 5 πœ‡ M statin treatment, except for cerivastatin, 6 statins significantly increased HNF-4 𝛼 levels in nuclear fraction (Figure 6(b)).

fig6
Figure 6: The Western blots represent HNF-4 𝛼 levels in nuclear fractions of HepG2 cells after treatment with atorvastatin (Ator), cerivastatin (Ceri), fluvastatin (Flu), pitavastatin (Pita), pravastatin (Pra), rosuvastatin (Rosu), and simvastatin (Sim) for 24 hours. Each statin was used at doses of 10 (a) or 25 (b) πœ‡ M . Nontreated cells (statin concentration 0 πœ‡ M ) were the control. HNF-4 𝛼 protein levels were quantified with an imaging analyzer. The data are expressed as % of control. Values are presented as the mean Β± SEM of three separate experiments, significantly different from control at βˆ— 𝑃 < . 0 5 , βˆ— βˆ— 𝑃 < . 0 1 .

4. Discussion

The main findings of the present study were (1) most statins increased PPAR 𝛼 mRNA expression, which might be caused via PPAR 𝛼 promoter activation, (2) atorvastatin, pitavastatin, and simvastatin significantly increased PPAR 𝛼 protein levels in nuclear fraction, (3) some, not but all, statins interacted with AOX promoter containing PPRE and increased PPAR 𝛼 activity, and (4) the PPAR 𝛼 promoter activity could be regulated by the increase of statin-induced HNF-4 𝛼 .

Statin therapy has been reported to reduce the incidence of cardiovascular disease risk in patients with the metabolic syndrome and hyperlipidemia [26], and these benefits have been regarded to mainly derive from their lipid-lowering effect. However, recent studies have suggested that there are additional, beneficial anti-inflammatory effects of stains, which are independent of their cholesterol-lowering effect [27, 28]. There are many reports that the anti-inflammatory effects of statins are induced via PPARs signaling-pathway [11, 29].

Our present results show that most statins increased PPAR 𝛼 mRNA expression in HepG2 cells after 24 hours treatment, especially atorvastatin, cerivastatin, fluvastatin, pitavastatin, rosuvastatin, and simvastatin (more than 1.5-fold versus control). Statins are classified into hydrophilic compounds and lipophilic compounds. In this study, the majority of the statins are lipophilic compounds, but pravastatin and rosuvastatin are hydrophilic compounds. Our results of PPAR 𝛼 mRNA expression in HepG2 cells treated with statins show that higher concentrations of pravastatin (100 and 2 5 0 πœ‡ M ) significantly increased PPAR 𝛼 mRNA expression. Therefore, in hydrophilic statin (pravastatin), the higher concentrations compared with other statins would be required for increase PPAR 𝛼 mRNA expression.

There are many reports that statins increase PPAR 𝛼 mRNA expression [11, 21]; however, there are no reports about the effect of statins on human PPAR 𝛼 promoter activity. We, therefore, cloned the human PPAR 𝛼 promoter region ( βˆ’ 1 5 5 3 b p to + 8 8 b p ) and measured the promoter activity in HepG2 cells treated with statins. Our present results show that 6 statins (except for pravastatin) significantly increased PPAR 𝛼 promoter activity in a dose-dependent manner. Although the effect of statins on mouse PPAR 𝛼 promoter activity has been reported previously [22], our present study is the first to report the effect of statins on human PPAR 𝛼 promoter activity.

PPAR 𝛼 promoter region includes many transcription factor binding domains, such as HNF-4 𝛼 , PPRE, E-Box, early growth response factor (Egr-1), and transcription factor Sp1. HNF-4 𝛼 is a nuclear receptor that plays a key role in liver-specific gene expression. Previously, it was reported that human PPAR 𝛼 promoter region contains HNF-4 𝛼 response element ( βˆ’ 1 , 4 9 2 b p to βˆ’ 1 , 4 8 3 b p ), and HNF-4 𝛼 induces human PPAR 𝛼 promoter activity [23]. Therefore, we detected HNF-4 𝛼 levels in nuclear fraction of statin-treated HepG2 cells. In our present studies, all statins ( 2 5 πœ‡ M ) significantly increased HNF-4 𝛼 in nuclear fractions. This result shows that statins may regulate PPAR 𝛼 gene transcription mediated by downstream transcriptional factors (e.g., HNF-4 𝛼 ). Further studies will be necessary to elucidate molecular mechanisms of statins to regulate the other transcriptional factors related to PPAR 𝛼 gene transcription.

Previously, we reported that cerivastatin, fluvastatin, and simvastatin increased nuclear translocation of PPAR 𝛼 protein [11]. Our present results show that the 7 statins utilized in the present studies increased nuclear translocation of PPAR 𝛼 protein in HepG2 cells compared with nontreated control cells. We next examined the effect of statins on transcriptional analysis of human AOX promoter in 293T cells cotransfected with human PPAR 𝛼 and RXR 𝛼 expression vector. 293T cells were used for these studies expressed very low levels of endogenous PPAR 𝛼 production when treated with statins (data not shown). Our present results show that simvastatin increased human AOX promoter-transcriptional activity via PPAR 𝛼 /RXR 𝛼 heterodimer. In fact, we identified the upregulation of human AOX mRNA on HepG2 cells and 293T cells treated with statins (data not shown). PPAR 𝛼 is a ligand-activated transcription factor and is activated by fatty acid, arachidonic acid [30], and several fibric acids [31]. PPAR 𝛼 -dependent transcriptional activation of many genes is well documented, and direct, ligand-enhanced interactions between PPAR 𝛼 and the coactivators, p300/cAMP-response element-binding protein (CREB-) binding protein (p300/CBP), steroid receptor coactivator-1 (SRC-1), PPAR-binding protein (PBP), and PPAR 𝛾 coactivator-1 (PGC-1) are thought to play a role in PPAR 𝛼 activation [32–34]. The recruitment of specific coactivators and the release of corepressors (e.g., nuclear receptor corepressor, NCoR) that associate with the liganded PPAR 𝛼 /RXR 𝛼 heterodimer allow further fine control of gene transcription. PPAR 𝛼 /RXR 𝛼 heterodimer can also bind to PPRE in the unliganded state [35]. The molecular structures of the PPAR 𝛼 /RXR 𝛼 heterodimeric complex and coactivators remain to be elucidated. Further studies will be necessary to be undertaken of the molecular mechanisms of statin regulation of the gene transcription by binding to PPREs in the promoter region of target genes.

In conclusion, statins activate PPAR 𝛼 promoter and then up-regulate PPAR 𝛼 mRNA expression in HepG2 cells. The effect on PPAR 𝛼 transcription is likely regulated by various downstream transcriptional factors (e.g., HNF-4 𝛼 ). Statins increase PPAR 𝛼 protein levels in nuclear fraction, and moreover, some statins, such as cerivastatin, fluvastatin, and simvastatin, significantly activate the transcription of the PPAR 𝛼 target genes.

Acknowledgment

The authors would like to greatly appreciate the experimental assistance to Ms. Sawako Satoh, Ayako Go, and Noriko Fukushima.

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