MicroRNA-34a (miR-34a) is thought to be involved in nonalcoholic fatty liver disease (NAFLD). However, the association between altered expression of miR-34a and the pathophysiological features of NAFLD remains unclear. Here, we investigated the mechanisms by which miR-34a influences NAFLD through the PPARα-related pathway. Real-time quantitative PCR, western blotting and other assays kit were used to investigate the expression and function of miR-34a in an NAFLD model. Cultured cells transfected with miR-34a inhibitor and C57BL/6 mice injected with the miR-34a inhibitor through vein tail were conducted for the effects of miR-34a on its target. MiR-34a levels were significantly upregulated in steatosis-induced hepatocytes and in liver tissues of high-fat diet-fed mice. The upregulation of miR-34a resulted in the downregulation of hepatic PPARα and SIRT1 that are the direct targets of miR-34a. Silencing miR-34a led to an initially increased expression of PPARα, SIRT1 and PPARα’s downstream genes. Activation of the central metabolic sensor AMPK was also increased. The miR-34a inhibitor suppressed lipid accumulation and improved the degree of steatosis. Taken together, our data indicated that decreased expression of miR-34a potentially contributes to altered lipid metabolism in NAFLD. Downregulation of miR-34a may be a therapeutic strategy against NAFLD by regulating its target PPARα and SIRT1.
Nonalcoholic fatty liver disease (NAFLD), one of the leading causes of chronic liver disease worldwide, comprises a spectrum of diseases, ranging from simple steatosis to steatohepatitis (NASH). Patients with NASH may develop cirrhosis and hepatocellular carcinoma (HCC). However, the pathogenesis of NAFLD remains largely unknown1. Recently, a new class of RNA regulatory genes, known as microRNAs (miRNAs), has introduced a new layer of gene regulation in eukaryotes. Mature miRNAs are a class of naturally occurring, small non-coding RNA molecules, about 21–25 nucleotides in length. They function to downregulate gene expression by translational repression, mRNA cleavage and deadenylation2,3. They are receiving growing attention because of numerous reports of their dysregulation in human diseases and their potential as diagnostic and therapeutic targets. Several miRNAs have been described as the important regulators of liver pathophysiology, including NAFLD, cirrhosis and HCC4,5,6.
MiRNAs also have crucial functions in metabolic regulation and are aberrantly expressed in metabolic disease7,8. Recently, miR-34a has been reported to emerge as a specific miRNA modulated in liver disease. Hepatic miR-34a levels are highly elevated in both dietary and leptin-deficient ob/ob obese mice9. Consistent with these initial findings, miR-34a is increased in patients of NAFLD10,11 as well as in a mouse model of steatohepatitis11,12,13. Furthermore, miR-34a suppresses SIRT1, which regulates the activity of AMP kinase (AMPK), a known regulator of energy metabolism14.
The peroxisome proliferator-activated receptor-α (PPARα) is a member of the nuclear receptor superfamily. Upon ligand binding, PPAR forms a heterodimer with the retinoid X receptor, interacts with PPAR response elements in the target genes and regulate their expressions15,16,17. Of three PPAR isoforms, PPARα is essential to modulate lipid transport and metabolism, mainly through activating mitochondrial and peroxisomal fatty acid β–oxidation pathways. PPARα regulates the constitutive transcription of genes encoding fatty acid (FA)-metabolizing enzymes and mitochondrial FA oxidation (FAO) activity, primarily in the liver18. PPARα activators, such as the widely prescribed fibrate drugs, ameliorate hepatic steatosis through enhancing mitochondrial FAO in mice19. Furthermore, PPARα exhibits an anti-inflammatory effect after feeding with a high-fat diet (HFD)20.
Here, we report that elevated miR-34a in NAFLD directly targets the transcription factor PPARα. Furthermore, in vitro and in vivo silencing of miR-34a in free fatty acid (FFA) or HFD-induced NAFLD models demonstrated the therapeutic feasibility of targeting miR-34a to treat NAFLD.
Materials and Methods
Cell lines, cell culture, in vitro model of cellular steatosis and miRNA transfection
The human normal hepatocyte cell line L02 cells was obtained from the Shanghai Institute of Cell Biology, Shanghai, China and were cultured in Dulbecco’s modified eagle medium (DMEM) cell culture media supplemented with 10% (v/v) Fetal Bovine Serum(FBS) (Gibco, California, USA) under an atmosphere of 5% CO2 at 37 °C. Fat overloading induction of cells was done mainly according to the method in which L02 cells was exposed to a mixture of FFA (oleate and palmitate) at a final ratio of 2:1 and final concentration of 1 mM.
miRNA and small interfering RNA transfection
To assess the influence of miR-34a inhibitor on cellular steatosis, cells were treated with FFA after 24 hours of miR-34a inhibitor transfection and harvested after 24 hours incubation with FFA. The day before transfection, the cells were plated in growth medium without antibiotics at a density of 30–40%. The transfection of hsa-miR-34a inhibitor (5′- ACA ACC AGC UAA GAC ACU GCC A-3′), chemically synthesized by Invitrogen (Carlsbad, USA) was performed using Lipofectamine 2000 (Invitrogen, Carlsbad, USA) according to the manufacturer’s protocol. The nonsense single-strand RNA (5′-CAG UAC UUU UGU GUA GUA CAA-3′), chemically synthesized by Invitrogen (Carlsbad, USA) were transfected into the negative control (NC) group. The 5′ end of the fluorescence-labeled miR-34a inhibitor was used to determine the transfection efficacy. The cell images were obtained using a phase-contrast microscope at an appropriate magnification (Olympus, Japan).
Animals models of NAFLD
Male C57BL/6 mice, 4 weeks of age, each weighing 18–20 g, were purchased from Vital River and acclimated for 1 week after arrival before they were used for experiments. All mice were bred in-house in a pathogen-free facility and maintained in a 12-hour day/night cycle at controlled room temperature and provided free access to food and water. After one week of acclimatization to laboratory conditions, the mice were then randomly divided into two groups: (1) control group (n = 18): animals treated with the standard chow diet (SCD, 8% rice bran, 51% maize, 30% soybean powder, 3% bone powder, 1.3% multivitamin and 6.7% mineral); (2) HFD group (n = 18): animals given a HFD (75% SCD, 2% cholesterol, 15% lard and 8% yolk powder). Six mice of each group were sacrificed at weeks 4, 8 and 12 after being placed on the respective diet. Livers were quickly excised, cleaned completely with ice-cold phosphate-buffered saline (PBS) and preserved in liquid nitrogen until use. Pieces of the remaining liver tissues were processed for histology. All animal studies were approved by the Animal Care and Use Committee of Zhejiang University in accordance with the Chinese guidelines for the care and use of laboratory animals.
Tail vein injection of lentiviral vector
Male C57BL/6 mice, 4 weeks of age, each weighing 18–20 g, were purchased from Vital River and acclimated for 1 week after arrival before they were used for experiments. The sequence of miR-34a inhibitor was built to pLenti6.3/TO/V5 vector (Invitrogen, Carlsbad, USA), the virus titer was 2 × 108 TU/ml. The mice had the standard chow (control group, SCD) or a HFD for 4 weeks. After 4 weeks, the HFD group was divided into three groups: one was kept in the same conditions, a third group was maintained on HFD injected with 100 μl of pLenti6.3/TO/V5 vector via the tail vein and a forth group was maintained on HFD injected with an equal volume of negative control siRNA (NC) for 4 more weeks. The animals were then sacrificed. Blood was collected just before sacrifice for serum biochemical analysis. Livers were quickly excised, cleaned completely with ice-cold PBS and preserved in liquid nitrogen until use. Pieces of the remaining liver tissues were processed for histology and Oil red O staining.
Oil red O staining, triglyceride level assay and H&E staining
Intracellular neutral lipids were stained with Oil red O and mice liver pathological damage was measured by hematoxylin and eosin (H&E) staining, as described in the Supplementary materials and methods. Intracellular and liver triglycerides were determined using a triglyceride assay kit (GPO-POD; Applygen Technologies Inc., Beijing, China), according to the manufacturer’s instructions.
Real-time quantitative PCR (qPCR) and western blotting analyses
Procedures of RNA extraction, qPCR and western blotting were described in the Supplementary data.
MiR-34a target prediction and validation
MiR-34a target prediction was carried out using the algorithms Target Scan Human V6.2 and PicTar. To validate the candidate miR-34a predicted targets, luciferase reporter assays were carried out. More detailed protocols are described in the Supplementary data.
Results are expressed as means ± standard deviation. The significance of the difference in means was determined by a two-tailed Student t test and ANOVA test. Values of P < 0.05 were considered significant and are indicated by asterisks in the figures.
Increased levels of miR-34a in L02 cells with FFA and C57BL/6 mice with HFD
Q-PCR demonstrated significantly higher expression of miR-34a in FFA-induced L02 cells compared with the controls (Figure S1A). Intriguingly, there was a correlated increase of miR-34a expression in mice when the HFD feed time was extended from 4 weeks to 12 weeks (Fig. 1A).
Inhibition of miR-34a expression alleviates hepatocellular steatosis in vitro
L02 cells transfected with 50 nM miR-34a inhibitor or NC were cultured in full media with or without FFA mixtures. There was an approximately 67% reduction of the miR-34a level in L02 cells treated with the inhibitor (Fig. 1B). As depicted in Fig. 1C, Oil red O staining demonstrated that increased lipid stores were present in hepatocytes treated with FFA for 24 hours. The increases were markedly attenuated in cells transfected with the miR-34a inhibitor. As expected, L02 cells transfected with miR-34a inhibitor resulted in a significant (23%) reduction in cellular triglyceride compared with NC after FFA exposure (P < 0.05) (Fig. 1D). Collectively, these results demonstrated that miR-34a could regulate the steatosis level in FFA-cultured L02 cells.
Inhibition of miR-34a expression alleviates hepatic steatosis in vivo
To further evaluate the effect of miR-34a on HFD-induced hepatic steatosis in vivo, we adopted the ‘lentiviral tail vein injection’ method to deliver the miR-34a inhibitor into mouse hepatocytes. C57BL/6 mice that had been fed with a high-fat diet for 4 weeks were treated with 100 μl saline, miR-34a inhibitor at 2*107 TU of pLenti6.3/TO/V5 vector or NC. There was an approximately 63% reduction in the miR-34a level in mouse liver tissues (Fig. 2A). As shown in Fig. 2B H&E staining and Fig. 2C Oil Red O staining demonstrated that the miR-34a inhibitor attenuated the steatosis degree in the liver tissues. In accordance with morphological findings, hepatic TG was reduced by 35% in mice injected with the miR-34a inhibitor, compared with the NC after 4 weeks of an HFD diet (P < 0.05) (Fig. 2D). Furthermore, liver weight/body weight ratio (liver index) reduced significantly in the miR-34a inhibitor groups (Fig. 2E). Liver inflammation or fibrosis was not significant observed in these experimental groups.
Serum levels of aspartate aminotransferase (AST) and alanine aminotransferase (ALT) have been regarded as markers of liver injury. The HFD resulted in a significant (P < 0.01) increase in the circulating levels of AST and total cholesterol (TC). However, HFD had no significant effects on ALT and TG. The levels of AST were significantly reduced in HFD-induced hepatic steatosis mice treated with miR-34a inhibitor compared to HFD-induced hepatic steatosis mice treated with NC duplex, indicating that the miR-34a inhibitor could attenuate liver injury (Figure S1B and Figure S1C).
The lipid pathway transcriptional regulator PPARα is a direct target of miR-34a in the liver
Two computational methods (TargetScan and PicTar) were used to identify miR-34a targets. Among the hundreds of predicted targets, PPARα is closely associated with lipid metabolism in NAFLD15,17,21 and was chosen for further validation in 293T cells using luciferase reporter assays. Figure 3A shows the predicted miR-34a-binding sites in 3′ UTR of PPARα.
Furthermore, the wild-type PPARα, or a mutant PPARα, with the miRNA seed sequence deleted, was co-transfected with miR-34a mimics into 293T cells. The miR-34a mimics suppressed the luciferase activity of the wide-type PPARα 3′ UTR 5080 site by 44%. However, full mutation of the PPARα 3′ UTR 5080 site seed sequence abrogated the repressive ability of miR-34a, demonstrating the specificity of the miR-34a target sequence in PPARα (Fig. 3B).
The ability of miR-34a in regulating the endogenous PPARα gene and protein expression was tested. The mRNA and protein levels of PPARα were both increased in L02 cells transfected with the miR-34a inhibitor and cultured for 24 h complete medium and 24h FFA medium, compared with the cells transfected with the NC duplex (Fig. 3C and Figure S1D). In addition, the expression of PPARα was increased in HFD-induced hepatic steatosis mice treated with the miR-34a inhibitor compared to the HFD-induced hepatic steatosis mice treated with the NC duplex (Fig. 3D and Figure S1E). These data suggested that miR-34a downregulated the expression of PPARα by targeting the PPARα-3′ UTR 5080 site to facilitate translational repression or mRNA degradation.
Altered SIRT1 protein expression in L02 cells and liver tissues of mice
The protein level of SIRT1 was increased in L02 cells transfected with the miR-34a inhibitor compared with the cells transfected with the NC duplex (Fig. 3C) and the expression of SIRT1 was increased in HFD-induced hepatic steatosis mice treated with the miR-34a inhibitor compared to the HFD-induced hepatic steatosis mice treated with the NC duplex (Fig. 3D).
Altered PPARα target metabolic genes expression in L02 cells and liver tissues of mice
When the miR-34a inhibitor was transfected or injected, the expression of fatty acid β-oxidation-related genes including CPT1 and CPT2 were significantly increased compared to NC in cells or in liver tissues (Fig. 4A-D). Interestingly, the expression of liver fatty acid transport-related genes, including SLC27A4, ACBD3 and SLC27A1, were significantly reduced in FFA induced steatosis cells or HFD induced steatotic liver compared with control groups (Fig. 4A-D). When transfected or injected with the miR-34a inhibitor, the expression of ACBD3, SLC27A4 and SLC27A1 were significantly increased compared with the NC, but the expression of ACBD3 in C57BL/6 liver tissue did not increased after injecting with the miR-34a inhibitor (Fig. 4A-D), indicating that they could be responsible, or contribute to, the observed phenotype. In summary, the miR-34a inhibitor significantly altered the expressions of genes related to metabolic pathways in vitro and in vivo.
Inhibition of miR-34a expression increased the AMPK phosphorylation pathway
To elucidate the mechanism by which the miR-34a inhibitor reduced TG accumulation in L02 cells, we assessed the effect of miR-34a on lipid metabolism pathways. Increased AMPK phosphorylation is associated with enhanced lipid metabolism, especially increased fatty acid β-oxidation22,23. We found that AMPK phosphorylation was significantly reduced, with the pAMPK/AMPKα1 ratio reduced by about 27% in FFA induced cells compared with control cells (Fig. 5A). The miR-34a inhibitor increased the pAMPK/AMPKα1 ratio compared with the NC. These data suggested a role for AMPK in miR-34a’s effects on fat accumulation in vitro.
Activated (phosphorylated) AMPK levels were also observed in whole liver extracts of mice treated with the miR-34a inhibitor (2 × 107 TU) compared with the NC. The total AMPKα1 protein level was unchanged in the miR-34a inhibitor-treated mice, but the levels of phosphorylated AMPKα1 were increased nearly 2-fold compared with the NC (Fig. 5B). Figure 6 showed the summarizing of miR-34a-PPARα-AMPK regulation in steatosis.
NAFLD is a multistep process and its pathogenesis has not been clearly delineated. In the present study, we identified a role of miR-34a in regulating the degree of steatosis by directly targeting PPARα. To the best of our knowledge, this has not been done before. We aimed to examine the importance of miR-34a for liver function by inhibiting miR-34a with an antisense oligonucleotide. Additionally, we have uncovered an unexpected role for miR-34a in regulation of hepatic lipid metabolism. This newly identified miR-34a-PPARα pathway provides a novel clue to the pathogenesis of steatosis formation in NAFLD. MiR-34a might become a target for the treatment of NAFLD.
The expression of miR-34a is increased in hepatic fibrosis24, HCV infection10, alcoholic liver disease25, HCC26,27,28 and NAFLD29,30. However, it was unclear how miR-34a contributes functionally to the development of NAFLD. Our data demonstrated that miR-34a was upregulated in livers of NAFLD mice and this increased expression was primarily detected in FFA-induced steatosis hepatocytes, suggesting that increased expression of miR-34a in hepatic steatosis is an important part of a protective negative regulatory feedback mechanism aimed at limiting disease progression by preventing excessive lipid accumulation in the liver.
Several studies indicated that serum level of miR-34a was higher in participants with NAFLD30. MiR-34a, apoptosis and acetylated p53 increased with disease severity. UDCA inhibited the miR-34a/SIRT1/p53 pathway31. Upregulation of miR-34a was found in livers of streptozotocin-induced diabetic mice, demonstrating that miR-34a is strongly dysregulated in NAFLD. The development of NASH was accompanied by prominent changes in the expression of miRNAs, including miR-29c, miR-34a, miR-155 and miR-200b. Interestingly, changes in the expression of these miRNAs and the protein levels of their targets, including Cebp-β, Socs 1, Zeb-1 and E-cadherin, in the livers of DBA/2J mice fed MCD were more pronounced compared with control mice. These results showed that alterations in the expression of miRNAs are prominent events during development of NASH and strongly suggest that the severity of and susceptibility to NASH may be determined by variations in miRNA expression response12.
MiRNAs negatively regulate their target mRNAs posttranscriptionally by binding to the 3′ UTR. In the present study, TargetScan and PicTar were used to identify potential targets of miR-34a. We then focused on PPARα because it plays a pivotal role in hepatic steatosis and metabolic pathways17,21. We confirmed the regulation of the predicted miR-34a targeted mRNAs by measuring both mRNA and protein levels in cells and mice after miR-34a inhibitor treatment, indicating that miRNA regulation could result in mRNA degradation and translational regulation of the predicted targets. Furthermore, the specific binding effect between miR-34a and the wild-type luciferase construct verified the potential post-transcriptional regulation of miR-34a on PPARα.
SIRT1, a mammalian ortholog of Sir2 (silent information regulator 2), is an NAD-dependent deacetylase that acts as a master metabolic sensor of NAD and modulates cellular metabolism32,33. In our research, we also found that protein levels of SIRT1 were significantly increased in cells and mice liver tissues after miR-34a inhibitor treatment. These results were consistent with the previous research. Choi et al.34, recently showed that hepatic miR-34a, which is elevated in obesity, directly targets and decreases SIRT1 expression.
Given the abundance of miR-34a in the liver, it was expected to play an important role in maintenance of liver lipid metabolism. In the present study, H&E staining and Oil red O staining both demonstrated that the miR-34a inhibitor attenuated the steatosis in the liver tissues and in L02 cells. In accordance with morphological findings, TG levels in L02 cells and liver tissues were reduced in the miR-34a inhibitor group. Furthermore, liver weight/body weight ratio (liver index) was also reduced significantly in the miR-34a inhibitor group. In HFD group, the liver index was reduced significantly compared to SCD group, which may be due to the body weight gain was much greater than the liver weight gain.
Surprisingly, the most apparent consequence of miR-34a inhibition in HFD mice over 4 weeks was a decrease in plasma AST, by about 15% in mice compared to NC after 4 weeks of HFD treatment. These results will be helpful for studies in evaluating the prospects for therapeutically inhibiting miR-34a to lower AST levels in humans.
The mitochondrial carnitine system plays a crucial role in β-oxidation. CPT1 catalyzes the esterification of long-chain acyl-CoAs to L-carnitine for transport into mitochondria for FAO. The acyl-carnitine conjugate is converted back to the acyl-CoA ester inside mitochondria by CPT235. In the present study, we found that the miR-34a inhibitor activates AMPK, an enzyme that functions as a fuel gauge to monitor the status of cellular energy and activates the expression of genes of FAO. The activated AMPK increased CPT1 and CPT2 levels, leading to an increase in the transport of FA into mitochondria and stimulating the oxidation of mitochondrial palmitoyl-CoA. These observations begin to explain the mechanisms for increased FAO after inhibition of miR-34a, identifying AMPK as a mediator of increased FAO in liver of miR-34a inhibitor treatment.
In cells, there are several families of lipid-binding proteins, such as Acyl-coenzyme A binding domains (ACBDs), fatty acid transport proteins (FATPs or SLC27As) and fatty acid binding proteins (FABPs), which function coordinately to regulate homeostasis and the function of fatty acids. In our study, the expression of energy metabolism-related genes including SLC27A1, SLC27A4 and ACBD3, which act downstream of PPARα, were increased in the L02 cells and the liver of miR-34a inhibitor treated mice, which suggested some of the differences in fat accumulation may have been caused by increased FA uptake into the cells36.
The central metabolic sensor AMPK is a key regulatory enzyme that promotes ATP-generating pathways, such as FAO and inhibits energy-storage pathways, such as FA synthesis22,37. We observed that miR-34a inhibition in cells and mice were consistent with increased AMPK activity. These results support the role of AMPK as a mediator of miR-34a’s effects on PPARα and its target genes. Hou et al.38 reported that the overexpression of SIRT1 stimulated the basal AMPK signaling in HepG2 cells and in the mouse liver. In our study, miR-34a inhibition also stimulated AMPK signaling though PPARα in cells and mice liver. Therefore, we think miR-34a-mediated PPARα regulation and SIRT1-AMPK pathway may be two separate regulatory mechanisms in steatosis, but there was a certain link between them, beacause both of them stimulated AMPK signaling.
Increased FAO after miR-34a inhibition led to a significant improvement in liver steatosis. These NAFLD cells and mice represent a state of prolonged caloric excess, which results in obesity, hyperlipidemia and hepatic steatosis. Our data suggested that miR-34a played a significant role in promoting lipid synthesis and inhibiting FAO in liver and as such, may be a therapeutic target for metabolic diseases.
In summary, our study demonstrated that miR-34a was upregulated in NAFLD and has a novel regulatory role as an important regulator of lipid metabolism. PPARα, a direct target of miR-34a, was upregulated after miR-34a inhibitor treatment, which induced transcriptions of CPT1 and CPT2 (both involved in fatty acid β-oxidation), SLC27A1, SLC27A4 and ACBD3 (all involved in fatty acid transport), causing the decrease of TG, liver index, as well as the activated AMPK pathway. Furthermore, SIRT1 was also upregulated after miR-34a inhibitor treatment. The present study contributes to our understanding the pathogenesis of steatosis formation in NAFLD and may lead to novel therapies for NAFLD that target upstream molecules at the miRNA level.
How to cite this article: Ding, J. et al. Effect of miR-34a in regulating steatosis by targeting PPARα expression in nonalcoholic fatty liver disease. Sci. Rep. 5, 13729; doi: 10.1038/srep13729 (2015).
Dowman, J. K., Armstrong, M. J., Tomlinson, J. W. & Newsome, P. N. Current therapeutic strategies in non-alcoholic fatty liver disease. Diabetes, Obesity and Metabolism 13, 692–702, doi: 10.1111/j.1463-1326.2011.01403.x (2011).
Jinek, M. & Doudna, J. A. A three-dimensional view of the molecular machinery of RNA interference. Nature 457, 405–412, doi: 10.1038/nature07755 (2009).
Krol, J., Loedige, I. & Filipowicz, W. The widespread regulation of microRNA biogenesis, function and decay. Nature Reviews Genetics, doi: 10.1038/nrg2843 (2010).
Ceccarelli, S., Panera, N., Gnani, D. & Nobili, V. Dual Role of MicroRNAs in NAFLD. International Journal of Molecular Sciences 14, 8437–8455, doi: 10.3390/ijms14048437 (2013).
Kerr, T. A., Korenblat, K. M. & Davidson, N. O. MicroRNAs and liver disease. Translational research: the journal of laboratory and clinical medicine 157, 241–252, doi: 10.1016/j.trsl.2011.01.008 (2011).
Lakner, A. M., Bonkovsky, H. L. & Schrum, L. W. microRNAs: fad or future of liver disease. World journal of gastroenterology: WJG 17, 2536–2542, doi: 10.3748/wjg.v17.i20.2536 (2011).
Lee, J. & Kemper, J. K. Controlling SIRT1 expression by microRNAs in health and metabolic disease. Aging 2, 527–534 (2010).
Rottiers, V. & Näär, A. M. MicroRNAs in metabolism and metabolic disorders. Nature Reviews Molecular Cell Biology 13, 239–250, doi: 10.1038/nrm3313 (2012).
Lee, J. et al. A Pathway Involving Farnesoid X Receptor and Small Heterodimer Partner Positively Regulates Hepatic Sirtuin 1 Levels via MicroRNA-34a Inhibition. Journal of Biological Chemistry 285, 12604–12611, doi: 10.1074/jbc.M109.094524 (2010).
Cermelli, S., Ruggieri, A., Marrero, J. A., Ioannou, G. N. & Beretta, L. Circulating microRNAs in patients with chronic hepatitis C and non-alcoholic fatty liver disease. PLoS ONE 6, e23937, doi: 10.1371/journal.pone.0023937 (2011).
Tryndyak, V. P. et al. Plasma microRNAs are sensitive indicators of inter-strain differences in the severity of liver injury induced in mice by a choline- and folate-deficient diet. Toxicol Appl Pharmacol 262, 52–59, doi: 10.1016/j.taap.2012.04.018 (2012).
Pogribny, I. P. et al. Difference in expression of hepatic microRNAs miR-29c, miR-34a, miR-155 and miR-200b is associated with strain-specific susceptibility to dietary nonalcoholic steatohepatitis in mice. Laboratory Investigation 90, 1437–1446, doi: 10.1038/labinvest.2010.113 (2010).
Li, S. et al. Differential expression of microRNAs in mouse liver under aberrant energy metabolic status. J Lipid Res 50, 1756–1765, doi: 10.1194/jlr.M800509-JLR200 (2009).
Smith, J. J. et al. Small molecule activators of SIRT1 replicate signaling pathways triggered by calorie restriction in vivo. BMC Systems Biology 3, 31, doi: 10.1186/1752-0509-3-31 (2009).
Wahli, W., Braissant, O. & Desvergne, B. Peroxisome proliferator activated receptors: transcriptional regulators of adipogenesis, lipid metabolism and more. Chemistry & biology 2, 261–266 (1995).
Dongiovanni, P. & Valenti, L. Peroxisome Proliferator-Activated Receptor Genetic Polymorphisms and Nonalcoholic Fatty Liver Disease: Any Role in Disease Susceptibility? PPAR Research 2013, 1–8, doi: 10.1155/2013/452061 (2013).
Latruffe, N. & Vamecq, J. Peroxisome proliferators and peroxisome proliferator activated receptors (PPARs) as regulators of lipid metabolism. Biochimie 79, 81–94 (1997).
Aoyama, T. et al. Altered constitutive expression of fatty acid-metabolizing enzymes in mice lacking the peroxisome proliferator-activated receptor alpha (PPARalpha). The Journal of biological chemistry 273, 5678–5684 (1998).
Nakajima, T. et al. Bezafibrate at Clinically Relevant Doses Decreases Serum/Liver Triglycerides via Down-Regulation of Sterol Regulatory Element-Binding Protein-1c in Mice: A Novel Peroxisome Proliferator-Activated Receptor -Independent Mechanism. Molecular Pharmacology 75, 782–792, doi: 10.1124/mol.108.052928 (2009).
Stienstra, R. et al. Peroxisome Proliferator-Activated Receptor α Protects against Obesity-Induced Hepatic Inflammation. Endocrinology 148, 2753–2763, doi: 10.1210/en.2007-0014 (2007).
Reddy, J. K. & Hashimoto, T. Peroxisomal beta-oxidation and peroxisome proliferator-activated receptor alpha: an adaptive metabolic system. Annual review of nutrition 21, 193–230, doi: 10.1146/annurev.nutr.21.1.193 (2001).
Fryer, L. G. & Carling, D. AMP-activated protein kinase and the metabolic syndrome. Biochemical Society transactions 33, 362–366, doi: 10.1042/bst0330362 (2005).
Hardie, D. G. Minireview: The AMP-Activated Protein Kinase Cascade: The Key Sensor of Cellular Energy Status. Endocrinology 144, 5179–5183, doi: 10.1210/en.2003-0982 (2003).
Li, W.-Q. et al. The rno-miR-34 family is upregulated and targets ACSL1 in dimethylnitrosamine-induced hepatic fibrosis in rats. FEBS Journal 278, 1522–1532, doi: 10.1111/j.1742-4658.2011.08075.x (2011).
Meng, F. et al. Epigenetic Regulation of miR-34a Expression in Alcoholic Liver Injury. The American Journal of Pathology 181, 804–817, doi: 10.1016/j.ajpath.2012.06.010 (2012).
Passi, A. G., Bernardi, C., Soffientini, U., Piacente, F. & Tonetti, M. G. Effects of MicroRNAs on Fucosyltransferase 8 (FUT8) Expression in Hepatocarcinoma Cells. PLoS ONE 8, e76540, doi: 10.1371/journal.pone.0076540 (2013).
Chiu, L. Y. et al. Identification of differentially expressed microRNAs in human hepatocellular adenoma associated with type I glycogen storage disease: a potential utility as biomarkers. Journal of gastroenterology 49, 1274–1284, doi: 10.1007/s00535-013-0890-2 (2014).
Dang, Y., Luo, D., Rong, M. & Chen, G. Underexpression of miR-34a in hepatocellular carcinoma and its contribution towards enhancement of proliferating inhibitory effects of agents targeting c-MET. PloS one 8, e61054, doi: 10.1371/journal.pone.0061054 (2013).
Cheung, O. et al. Nonalcoholic steatohepatitis is associated with altered hepatic MicroRNA expression. Hepatology 48, 1810–1820, doi: 10.1002/hep.22569 (2008).
Yamada, H. et al. Associations between circulating microRNAs (miR-21, miR-34a, miR-122 and miR-451) and non-alcoholic fatty liver. Clinica Chimica Acta 424, 99–103, doi: 10.1016/j.cca.2013.05.021 (2013).
Castro, R. E. et al. miR-34a/SIRT1/p53 is suppressed by ursodeoxycholic acid in the rat liver and activated by disease severity in human non-alcoholic fatty liver disease. J Hepatol 58, 119–125, doi: 10.1016/j.jhep.2012.08.008 (2013).
Guarente, L. Sirtuins as potential targets for metabolic syndrome. Nature 444, 868–874, doi: 10.1038/nature05486 (2006).
Gerhart-Hines, Z. et al. Metabolic control of muscle mitochondrial function and fatty acid oxidation through SIRT1/PGC-1alpha. EMBO J 26, 1913–1923, doi: 10.1038/sj.emboj.7601633 (2007).
Choi, S.-E. et al. Elevated microRNA-34a in obesity reduces NAD+levels and SIRT1 activity by directly targeting NAMPT. Aging Cell 12, 1062–1072, doi: 10.1111/acel.12135 (2013).
Bonnefont, J. P. et al. Carnitine palmitoyltransferases 1 and 2: biochemical, molecular and medical aspects. Molecular aspects of medicine 25, 495–520, doi: 10.1016/j.mam.2004.06.004 (2004).
Lenz, L. S. et al. Adipocyte-specific Inactivation of Acyl-CoA Synthetase Fatty Acid Transport Protein 4 (Fatp4) in Mice Causes Adipose Hypertrophy and Alterations in Metabolism of Complex Lipids under High Fat Diet. Journal of Biological Chemistry 286, 35578–35587, doi: 10.1074/jbc.M111.226530 (2011).
Kahn, B. B., Alquier, T., Carling, D. & Hardie, D. G. AMP-activated protein kinase: Ancient energy gauge provides clues to modern understanding of metabolism. Cell Metabolism 1, 15–25, doi: 10.1016/j.cmet.2004.12.003 (2005).
Hou, X. et al. SIRT1 Regulates Hepatocyte Lipid Metabolism through Activating AMP-activated Protein Kinase. Journal of Biological Chemistry 283, 20015–20026, doi: 10.1074/jbc.M802187200 (2008).
This research was supported by The National Natural Science Foundation of China No.81230012, No.81170378 and No.81370008. We thank all members of the laboratory for insightful discussions and full help.
The authors declare no competing financial interests.
Electronic supplementary material
About this article
Cite this article
Ding, J., Li, M., Wan, X. et al. Effect of miR-34a in regulating steatosis by targeting PPARα expression in nonalcoholic fatty liver disease. Sci Rep 5, 13729 (2015). https://doi.org/10.1038/srep13729
Acta Pharmacologica Sinica (2022)
Bioinformatics analysis reveals molecular connections between non-alcoholic fatty liver disease (NAFLD) and COVID-19
Journal of Cell Communication and Signaling (2022)
Astaxanthin attenuates hepatic steatosis in high-fat diet-fed rats by suppressing microRNA-21 via transactivation of nuclear factor erythroid 2-related factor 2
Journal of Physiology and Biochemistry (2022)
Advances of microRNAs in regulating mitochondrial function: new potential application in NAFLD treatment
Molecular Biology Reports (2022)
NAFLD mark: an accurate model based on microRNA-34 for diagnosis of non-alcoholic fatty liver disease patients
Journal of Genetic Engineering and Biotechnology (2021)