MicroRNAs-Dependent Regulation of PPARs in Metabolic Diseases and Cancers

Portius, Dorothea; Sobolewski, Cyril; Foti, Michelangelo

doi:https://doi.org/10.1155/2017/7058424

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The Interplay between Metabolism, PPAR Signaling Pathway, and Cancer

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Review Article | Open Access

Volume 2017 | Article ID 7058424 | https://doi.org/10.1155/2017/7058424

MicroRNAs-Dependent Regulation of PPARs in Metabolic Diseases and Cancers

Dorothea Portius,¹Cyril Sobolewski,¹and Michelangelo Foti¹

Academic Editor: Valeria Amodeo

Received24 Aug 2016

Accepted05 Dec 2016

Published12 Jan 2017

Abstract

Peroxisome proliferator-activated receptors (PPARs) are a family of ligand-dependent nuclear receptors, which control the transcription of genes involved in energy homeostasis and inflammation and cell proliferation/differentiation. Alterations of PPARs’ expression and/or activity are commonly associated with metabolic disorders occurring with obesity, type 2 diabetes, and fatty liver disease, as well as with inflammation and cancer. Emerging evidence now indicates that microRNAs (miRNAs), a family of small noncoding RNAs, which fine-tune gene expression, play a significant role in the pathophysiological mechanisms regulating the expression and activity of PPARs. Herein, the regulation of PPARs by miRNAs is reviewed in the context of metabolic disorders, inflammation, and cancer. The reciprocal control of miRNAs expression by PPARs, as well as the therapeutic potential of modulating PPAR expression/activity by pharmacological compounds targeting miRNA, is also discussed.

1. Introduction

Peroxisome proliferator-activated receptors (PPARs) are a family of nuclear receptors involved in various biological functions but with a prominent role in metabolic homeostasis of carbohydrates and lipids [1]. The three PPAR isoforms, PPARα (NR1C1), PPARβ/δ (NR1C2), and PPARγ (NR1C3), share 60% to 80% of structural homology [2, 3] and exhibit a distinct tissue expression pattern but can exert similar or different physiological functions [3]. In the canonical model, PPARs are activated in the cytoplasm by specific ligands [1–6] and then translocate into the nucleus, where they form a complex predominantly with the nuclear receptor Retinoid-X-Receptor (RXR), to transactivate gene expression by binding to PPAR response elements (PPREs) on gene promoters [6, 7]. In contrast, noncanonical PPAR activity suppresses gene transcription through direct protein-protein interactions with other transcription factors, for example, the nuclear factor-kB (NFkB) or activated protein-1 (AP-1) [1, 3]. PPARs activity is also tightly dependent on the binding of other cofactors such as PGC1α (peroxisome proliferator-activated receptor coactivator-1α) and p300 or CREB binding protein—or on the contrary on the binding of corepressor proteins, for example, NCOR (nuclear receptor corepressor) or SMRT (silencing mediator for retinoid and thyroid hormone receptor), which hamper PPARs interactions with PPRE [3].

Through complex regulatory mechanisms, PPARs exert a tight control on energy homeostasis by modulating the expression of key genes involved in lipid metabolism [5, 6], adipocytes differentiation [5], and carbohydrate metabolism [5, 6]. The implication of PPARs in inflammatory processes and specific cancers is further suggested by recent studies (reviewed in [3, 8, 9]). These key and pleiotropic roles of PPARs in cellular processes have led to the development of pharmacologic agonists, for example, thiazolidinediones and fibrates [10, 11], to treat metabolic disorders or other diseases such as atherosclerosis [2, 5, 12]. However, long-term treatment with PPARs agonists triggers uncontrolled side effects in patients (e.g., oedema, weight gain, heart failure, and bone fractures) and in some cases they may even promote tumorigenesis [6, 8, 13]. Alternative therapeutic options to control distinct PPARs activities in specific tissues are therefore desirable but require that we deepen our understanding of the molecular mechanisms controlling PPARs expression/activity in diseases.

Recently, a wealth of studies has suggested that epigenetic mechanisms, for example, DNA methylation, histone modifications, or small noncoding RNA (i.e., microRNAs), importantly affect physiological or pathological mechanisms involved in a wide variety of diseases and cancers. In the case of PPARs, methylation of their promoters [14, 15], or histone acetylation [16], has been reported to affect PPARs expression and physiological processes under their control. More recently, other epigenetic alterations, in particular those leading to abnormal microRNAs (miRNAs) expression, have also been implicated in the regulation of PPARs expression or activity [17]. Indeed several miRNAs were reported to either directly target PPARs mRNA or to indirectly affect their expression/activities by targeting PPARs-associated cofactors and repressors, thus providing a further level of complexity in these regulatory mechanisms [18–20].

In this review, we discuss the current knowledge about miRNAs-dependent regulation of PPARs and their cofactors in physiological and pathological processes. Most of available studies dealing with this topic are restrained to metabolic diseases (e.g., diabetes, fatty liver diseases, and cardiovascular diseases) and associated cancers (e.g., liver cancers) in tissues where the role of PPARs is well characterized (e.g., liver, adipose tissue, muscles, and heart). Other rare studies investigating PPARs regulation by miRNAs in different tissues (e.g., bone marrow, neurons, and cartilage) or type of cancers (e.g., neuroblastoma, prostate cancer), unrelated to metabolic disorders, are also considered. Finally, the reciprocal regulation of specific miRNAs by PPARs, as well as potential miRNA-based pharmacological approaches to therapeutically modulate PPARs expression and/or activity, was also examined.

2. miRNAs

MicroRNAs (miRNAs) are endogenous small noncoding RNAs of approximately 16–22 nucleotides, which bind to complementary sequences (seed sequences) in the 3′UTR of target mRNAs and mediate either their decay or translation inhibition [21, 22]. miRNAs are encoded within intronic, intergenic regions or in polycistronic clusters [19, 23], and their biogenesis starts with a RNA polymerase II-dependent transcription of a primary transcript (pri-miRNA), which is then maturated by a nuclear microprocessor complex (RNase III Drosha and its mammalian double-stranded RNA-binding partner DGCR8). This leads to the release of a pre-miRNA, which is then exported into the cytoplasm by Exportin-5, where the RNase III Dicer1, together with its binding partner TARP2 (T-cell receptor gamma-chain constant region), removes the pre-miRNA hairpin loop and generates a miRNA duplex of mature miRNA (guide strand) and of a complementary strand (passenger strand or ). The guide strand and the are then associated with Argonaute proteins and incorporated into the RNA-induced silencing complex (RISC). A second maturation step is initiated within the RISC to separate both strands and the mature miRNA binds to the 3′UTR of target mRNAs. Recent evidence also indicates a pathophysiological role of the passenger strand of miRNA () in specific conditions, although it frequently appears to be degraded and devoid of any functions [19, 21, 23, 24].

More than 2000 miRNAs have been identified and it is considered that 60% of human genes are regulated by miRNAs with around 45 000 miRNA targets within the transcriptome [21–23, 25]. miRNAs act within an intricate regulatory network, where one specific miRNA can control the expression of several hundred mRNAs and conversely one mRNA can be targeted by several miRNAs [19, 23]. Through their wide action, miRNAs are involved in the control of almost all cellular functions and alterations of their expression/activity are observed in various pathological conditions including metabolic diseases and associated cancers [2, 21, 22, 25–29]. The bulk of the studies investigating PPARs and associated cofactors/repressors (e.g., RXR, NCOR) regulation by miRNAs has been performed in the frame of metabolic diseases, where the role of PPARs is the best characterized. Indeed, bioinformatics analyses using the miRWalk 2.0 platform (http://zmf.umm.uni-heidelberg.de/apps/zmf/mirwalk2/index.html), which integrates different prediction software programs for miRNA-mRNA interactions, point to multiple candidate miRNAs potentially targeting directly PPAR isoforms. However, only a restricted number of these candidates have been validated by experimental approaches (see Table 1). Combining MetaCore™ and miRWalk 2.0 based analyses in human studies exclusively revealed that 606 miRNAs were implicated in human cancers, and among those 34 are in metabolic disorders (e.g., obesity, diabetes, hepatomegaly, fatty liver diseases, hypertension, dyslipidemia, and other diabetic complications). Among the 606 cancer-related miRNAs, eight were targeting PPARα, four were targeting PPARβ/δ, and eight were targeting PPARγ. Interestingly, two miRNAs targeting PPARα (miR-21 and miR-519d) and two miRNAs targeting PPARγ (miR-27 and miR-20) were also previously associated with metabolic diseases (Figure 1). Although such predictive analyses using available software programs are subject to multiple biases and should be considered with extreme caution, they suggest that fine-tuning of PPARs signaling by miRNAs may sit at the crossroad between metabolic diseases and cancers in human.

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Figure 1

Human miRNAs targeting PPAR isoforms and involved in metabolic diseases and cancer. MetaCore pathway analysis software from Thomson Reuters was used to identify experimentally the number of validated human miRNAs involved in cancer (grey circle). Among those, the numbers of miRNAs involved in metabolic diseases, also identified by MetaCore pathway analysis, are indicated in blue circles. In red circles are the number of miRNAs identified using miRWalk 2.0 atlas and targeting PPARα (Panel (a)), PPARβ/δ (Panel (b)), and PPARγ (Panel (c)). The identities of miRNAs targeting specific PPAR isoforms and involved in both cancer and metabolic diseases are indicated in violet. miRWalk 2.0 atlas is a software integrating 12 different prediction algorithms (miRWalk 2.0, MicroT4, miRanda, miRBridge, miRDB, miRMap, miRNAMap, PICTAR2, PITA, RNA22, RNAhybrid, and TargetScan) for identification of miRNAs target mRNAs.

3. miRNAs-Dependent Regulation of PPARs in Metabolic Diseases and Cancer

3.1. miRNAs-Dependent Regulation of PPARα

PPARα is a nutritional sensor adapting metabolic homeostasis to energy deprivation [3]. It is mostly expressed in the liver, where it regulates lipid catabolism (i.e., β-oxidation) and critical genes (e.g., fatty acid transport protein 1, CD36, Acyl-CoA oxidase 1, and Carnitine palmitoyltransferase 1) involved in fatty acid transport [68] and in ketogenesis (e.g., Hmgcs2, Hmgcl) [68]. PPARα exerts also an anti-inflammatory function, as evidenced in mouse models of acute inflammation [68]. This effect results from an attenuation of proinflammatory cytokines (e.g., Il-6, Il-1β) expression as well as an upregulation of anti-inflammatory factors such as Il-1ra (Il-1 receptor antagonist) or IκBα [68]. PPARα is also expressed in other organs such as adipose tissues, heart, skeletal muscles, and kidneys, where it controls also some aspects of the glucose and lipid homeostasis (i.e., β-oxidation) [6, 68, 69]. PPARα is usually activated through the binding of specific ligands, in particular unsaturated fatty acids (-3 fatty acids), eicosanoid derivatives (e.g., 8-hydroxy-eicosatetraenoic acid, prostacyclin), or metabolized fatty acids (e.g., oxidized fatty acids) [6]. Alterations of PPARα expression or activity were associated with a variety of human pathologies such as obesity, liver diseases, inflammation, and cancers [3, 68, 69]. It is now clear that deregulations of specific miRNA can significantly contribute to PPARα abnormal signaling in these pathophysiological conditions (see experimentally validated miRNAs targeting PPARα in Table 1 and Figure 2). Such alterations have been investigated only in specific tissues, such as the liver or adipose tissue, as well as in inflammatory cells and cartilage and specific tumors (e.g., in the colon). Whether PPARα expression/activity is affected by miRNAs in other metabolically active tissues, for example, skeletal muscles or pancreas, remains to be established.

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3.1.1. miRNAs-Dependent Regulation of PPARα in the Liver

In the liver, PPARα is implicated in the lipid catabolism and inflammatory processes [68]. miRNAs-dependent alterations of PPARα signaling are reported by numerous studies to contribute to the onset of liver diseases such as nonalcoholic fatty liver disease (NAFLD) [19, 21, 29], chronic diseases associated with viral infections (HBV, HCV) [70], or hepatic cancers [30, 71].

Hepatic Steatosis. Two miRNAs were shown to alter PPARα expression in hepatocytes and to lead to steatosis development (Table 1) [19, 69]. Upregulation of miR-199a-5p was observed in various in vivo mouse models of obesity (ob/ob and db/db mice, mice fed a high-fat diet), as well as in liver samples from patients with NAFLD. In vitro analyses of hepatoma cell lines (HepG2 and murine AML12 cells) exposed to fatty acids as a surrogate model of steatosis further confirm an upregulation of miR-199a-5p, which in turn downregulates PPARα and caveolin-1 thereby promoting abnormal cellular redox equilibrium and fatty acids intracellular accumulation [37]. In human hepatic LO2 cells, Zheng et al. uncover another miRNA, miR-10b, upregulated following exposure to fatty acids and having a unique binding site in the PPARα 3′UTR sequence [32]. However, the relevance of miR-10b alterations in human liver metabolic disorders was not evaluated.

Hepatic Inflammation and Fibrosis. PPARα downregulation by miRNAs was recently suggested to trigger hepatic inflammation and fibrosis. Indeed, Loyer et al. [34] reported an upregulation of miR-21 in biliary and inflammatory cells of mice and patients with nonalcoholic steatohepatitis (NASH). They further discover that miR-21 was promoting hepatic inflammation and fibrosis by suppressing PPARα expression in these cells. Interestingly, in mice knockout, specifically for miR-21 in hepatocytes, PPARα expression was not altered, even when mice were challenged with an obesogenic diet, therefore suggesting that, in different cell types, miR-21 may have different activities and/or cellular targets [34, 72]. In hepatic stellate cells (HSCs), which are the main nonparenchymal liver cells contributing to the abnormal extracellular matrix deposition in liver fibrosis, miR-33 and miR-27a/-27b were also found upregulated and to target PPARα and the PPARα cofactor RXR, respectively. Inhibition of these miRNAs with synthetic nucleotides in rat primary and immortalized human HSCs (LX-2 cells) increased PPARα expression concomitantly with a decreased activation of the cells, thus suggesting a tight link between HSC activation and PPARα expression [35, 73].

Hepatic Carcinogenesis. The role of PPARα in cancer is still debated but few studies suggested that miRNAs-dependent alterations of PPARα expression/activity are relevant for the development of hepatocellular carcinoma (HCC). In particular, high-throughput screening of human HCC samples revealed 28 miRNAs differentially expressed with top hits for miR-9, miR-21, and miR-224 [30]. In addition to miR-21, which is discussed in the previous section, prediction software programs identified conserved miR-9 binding sites within the 3′UTR of PPARα. miR-9 upregulation correlated with tumor invasiveness, cell growth, and tumor stage, but whether this was related to a decreased PPARα expression remains unclear. Indeed, whereas the direct regulation of PPARα by miR-9 in human HCC cells was confirmed by luciferase reporter assay [31], molecular analysis of human Snu-449 and HepG2 cancer cell lines indicated an indirect role for miR-9 overexpression in PPARα downregulation [30].

3.1.2. miRNAs-Dependent Regulation of PPARα in the Adipose Tissue

PPARα assumes important functions in brown adipose tissue and adaptive thermogenesis and browning of white adipose tissue [41]. Although experimental evidence in human showing miRNAs-dependent PPARα regulation in brown/white adipose tissue is scarce, several animal models have suggested such regulatory mechanisms. For example, miR-27a and miR-27b, which are downregulated in mouse brown/white adipose tissue after cold exposure, directly modulate components of the adipocyte transcriptional network including PPARα [41]. MiR-519d, which is increased in subcutaneous white adipose tissue of obese subjects as compared to nonobese individuals, decreases fatty acid catabolism, and increases intracellular lipid accumulation by directly repressing PPARα [39]. Finally, other miRNAs upregulated in brown adipose tissue and/or white adipose tissue of diet-induced obese mice, or during human white and beige adipose differentiation, for example, miR-106b/miR-93 [74, 75] and miR-26a and miR-26b [50], have been correlated with alterations of PPARα expression. However, whether PPARα is a direct target of these miRNAs was not investigated.

3.1.3. miRNAs-Dependent Regulation of PPARα in Other Cell Types/Organs

Inflammatory Cells and Cartilage. Functional miRNAs-dependent PPARα alteration in inflammatory processes was suggested by two studies. First, miR-21, which is upregulated in cultured human endothelial cells from umbilical vein exposed to oscillatory shear stress, was shown to directly inhibit PPARα translation [33]. The decreased expression of PPARα in turn promotes AP1-dependent upregulation of VCAM-1 (vascular cell adhesion molecule-1) and MCP-1 (monocyte chemotactic protein-1), which favor the adhesion of inflammatory cells [33]. In a second study, bioinformatics and molecular analyses combined with clinical data identified an increased expression of miR-22 in osteoarthritic cartilage, which was correlated with PPARα downregulation and an increased body-mass-index (BMI) of patients [76]. However, this study did not provide any direct molecular link between miR-22 upregulation and PPARα downregulation.

Nonhepatic Cancers. The only evidence that PPARα may potentially behave as a tumor suppressor downregulated by aberrantly expressed miRNAs in transformed cells comes from a study performed in a drug-resistant colon cancer cell line (SW1116) showing that miR-506 overexpression in this cancer cell model directly affects PPARα expression [38]. In another study, the growth inhibitory properties of 1.25-dihydroxyvitamin D3 in human prostate adenocarcinoma cells (LNCaP) were associated with an increased expression of the miR-17/92 cluster, which correlated with PPARα downregulation, but whether miR-17/92 directly target PPARα was not investigated [77].

3.2. miRNAs-Dependent Regulation of PPARβ/δ

PPARβ/δ is ubiquitously expressed with the highest levels in liver, intestine, kidneys, and skeletal muscles [6, 78]. Major PPARβ/δ activators are natural ligands such as polyunsaturated fatty acids, prostaglandin derivatives (e.g., prostacyclin), or components of VLDL (Very Low Density Lipoproteins) particles [6]. This PPAR isoform regulates multiple cellular processes including developmental aspects, the lipid metabolism, insulin sensitivity, vascular function, and anti-inflammatory responses [4, 6, 44, 79]. The best-characterized role of PPARβ/δ has been described in metabolically active tissues. In the liver, PPARβ/δ appears to increase glucose utilization through the pentose-phosphate pathway and to promote lipogenesis [80]. However, in mice fed an obesogenic diet, activation of PPARβ/δ surprisingly prevents the development of steatosis [81]. In muscles and white adipose tissue, PPARβ/δ exerts an adaptive response to fasting and exercise by favoring fatty acids oxidation [82], through the direct induction of key genes involved in this process (e.g., mitochondrial CPT-1 (Carnitine palmitoyltransferase-1) and FoxO1 (Forkhead box protein O1)) [82, 83]. In brown adipose tissue, PPARβ/δ contributes to adaptive thermogenesis by inducing the expression of UCP-1 and UCP-3 [81, 82] and to β-oxidation, by upregulating several genes involved in this process (e.g., long chain acyl-CoA synthetase, Acyl-CoA oxidase). In addition to these well established roles of PPARβ/δ, this isoform was further implicated in the regulation of multiple other cellular processes including developmental aspects, vascular function, and anti-inflammatory responses [4, 6, 44, 79]. Finally, in cancer, the role of PPARβ/δ is controversial with evidence pointing at PPARβ/δ as an oncogene (e.g., in breast and prostate tumors) [84] or as a tumor suppressor (e.g., in colon cancer) [4, 6, 85]. Despite the key functions of PPARβ/δ, solid experimental evidence indicating miRNAs-dependent regulation of this isoform is very limited and restricted to studies described below (see Table 1 and Figure 2).

3.2.1. miRNAs-Dependent Regulation of PPARβ/δ in the Liver

Based on Affymetrix microarrays, in vivo inhibition of miR-122 by antisense oligonucleotides (ASO) in mice affected hundreds of hepatic mRNAs including PPARβ/δ [86]. Whether miR-122 directly targets PPARβ/δ is still undetermined; however its downregulation following injection of miR-122 inhibitors in mice was suggested to affect circadian clock-dependent energy homeostasis and in particular regulation of lipid transport and catabolism [86].

3.2.2. miRNAs-Dependent Regulation of PPARβ/δ in the Heart

By stimulating fatty acid utilization in the myocardium, PPARβ/δ exerts a protective vascular function. In a mouse model of heart failure, an impaired fatty acid oxidation and a metabolic switch towards glycolysis were attributed to the direct repression of PPARβ/δ by two miRNAs, miR-199a and miR-214, which are upregulated following aortic pressure overload and subsequent heart failure [43].

3.2.3. miRNAs-Dependent Regulation of PPARβ/δ in Monocytes/Macrophages

PPARβ/δ exerts an anti-inflammatory function, by promoting the switch from proinflammatory M1 macrophages to the anti-inflammatory M2 macrophages in the liver and in adipose tissue [44]. Bioinformatics and luciferase reporter assays revealed the presence of a functional miR-9 binding site within PPARβ/δ 3′UTR in human monocytes. Downregulation of PPARβ/δ and its targets genes was further observed in proinflammatory M1 macrophages treated with lipopolysaccharide (LPS) and correlated with an upregulation of miR-9 in these cells, thus suggesting a potential functional regulation of PPARβ/δ by miR-9 in monocytes and macrophages [44].

3.2.4. miRNAs-Dependent Regulation of PPARβ/δ in Other Cell Types/Organs

MiRNAs-dependent PPARβ/δ regulation was finally reported in hypertrophic scar formation, where PPARβ/δ promotes proliferation of fibroblasts. A decrease in miR-138 expression was noted in scar tissue as compared to paired normal skin tissues and inversely correlated with the level of PPARβ/δ. Further analyses using luciferase reporter assays and synthetic miR-138 mimics and inhibitor nucleotides in human hypertrophic scar fibroblasts (hHSFs) confirmed that PPARβ/δ is a direct target of miR-138 and the functional relevance of this regulatory mechanism in hHSFs proliferation [45].

3.3. miRNAs-Dependent Regulation of PPARγ

There are two PPARγ isoforms (PPARγ1 and PPARγ2). PPARγ1 is broadly expressed in adipose tissue, liver, intestine, kidneys, small intestine, immune cells, and endothelium, while PPARγ2 is predominantly expressed in the adipose tissue [2, 3, 6]. Activation of PPARγ is induced mostly by unsaturated fatty acids and endogenous arachidonic acid-derived metabolites (e.g., leukotriene B4 and eicosatetraenoic acid). The best-described functions of PPARγ are to transcriptionally promote adipocyte differentiation and lipogenesis as well as de novo lipogenesis in the liver [5, 87]. In addition, PPARγ controls also the expression of various adipocyte genes involved in glucose homeostasis (e.g., Glut4 expression) and endocrine signaling (e.g., adiponectin, resistin, and TNFα) affecting insulin sensitivity in other peripheral organs such as liver and muscles [2, 3, 5, 12]. Finally, several other cellular processes including cholesterol transport, kidney function, food intake, and inflammation have been suggested to be modulated by PPARγ isoforms [2, 3, 5, 12]. Consistent with the role of PPARγ in glucose and lipid homeostasis, an abnormal activity of PPARγ is often associated with the development of metabolic disorders (e.g., obesity, type 2 diabetes, and fatty liver disease) [5]. In contrast, in cancer, increasing evidence indicates a beneficial tumor suppressive role for PPARγ (e.g., gastric, pancreatic, and hepatic cancers) [2, 6, 88]. As illustrated in Table 1 and Figure 2, posttranscriptional regulation of PPARγ by miRNAs has been reported in many pathophysiological situations.

3.3.1. miRNAs-Dependent Regulation of PPARγ in the Liver

Hepatic Fibrosis. PPARγ is a negative regulator of hepatic stellate cells (HSCs) activation [89]. The induction of various miRNAs expressed in nonalcoholic steatohepatitis (NASH) and fibrosis correlated with PPARγ downregulation and overexpression of profibrogenic markers like α-SMA. Among those miRNAs, upregulation of miR-34a/-34c [52], miR-128-3p [53], and miR-130a/miR-130b [63] in activated human or rat HSCs was reported to directly bind the 3′UTR of PPARγ and to repress its expression. miRNAs-dependent PPARγ downregulation in hepatic fibrosis can also occur through indirect mechanisms. For example, in HSCs from mice treated with CCL4 to induce fibrosis, miR-132 is downregulated thereby leading to an increase of one of its targets, MeCP2 (Methyl CpG binding protein 2), and repression of PPARγ transcription via different epigenetic mechanisms [90].

Hepatitis C Virus (HCV) Infection. Infection of Huh-7.5 hepatoma cells with a HCV-derived JFH1 strain induces expression of miR-27a. This miRNA directly targets PPARγ thereby reducing lipid synthesis and increasing lipid secretion [91], two processes likely promoting HCV replication and virions egress.

Hepatic Carcinogenesis. PPARγ has a tumor suppressive function in hepatocarcinogenesis [7, 51, 92–95]. PPARγ downregulation in HCC correlated with upregulation of specific miRNAs [3, 93, 96], among which the best characterized ones are miR-130b and miR-27a. These two miRNAs directly target PPARγ and decrease its expression thus promoting cancer cells growth and aggressiveness [47, 55].

3.3.2. miRNAs-Dependent Regulation of PPARγ in Adipose Tissue

Adipocyte Differentiation. Regulation of PPARγ activity/expression by miRNAs represents an important posttranscriptional mechanism controlling adipocyte differentiation. Several miRNAs in murine and human preadipocytes, including miR-540, miR-302a, miR-138, miR-548d-5p, miR-130, and miR-27, were described to bind the 3′UTR of PPARγ and to decrease its expression thus preventing differentiation towards mature adipocytes [54, 57–59, 67, 97, 98]. In particular, miR-130 was reported to be downregulated in mice fed an obesogenic diet and in adipocytes of obese and type 2 diabetic patients, who also have high levels of PPARγ in adipose tissues and a low abundance of preadipocytes [54, 56, 62]. Further in vitro analyses using embryonic fibroblasts-derived preadipocytes (3T3-L1) indicated that synthetic nucleotides mimicking or inhibiting miR-130a were able to modulate PPARγ expression and its downstream target genes involved in glucose and lipid metabolism [56]. miR-27a and miR-27b are other key miRNAs regulating adipocyte differentiation, and both are downregulated during adipocyte differentiation, thus leading to an induction of PPARγ [59]. Consistent with this role, expression of miR-27a/-27b is lower in obese ob/ob mice as compared to lean animals and decreases during adipogenic differentiation of 3T3-L1 cells and mouse bone marrow derived mesenchymal stem cells (OP9 cell line). In the same study, miR-27a/miR-27b mimic nucleotides decreased PPARγ expression and prevented adipocyte differentiation. However, experimental evidence indicated that the mechanisms by which miR-27 affect PPARγ expression are indirect [98].

Inflammation. The role of PPARγ in adipose tissue inflammation is still poorly characterized, but downregulation of miR-301a, which directly targets PPARγ, was correlated with the production of proinflammatory cytokines in obese mice and in 3T3L1 preadipocytes [65].

3.3.3. miRNAs-Dependent Regulation of PPARγ in Bone Marrow

The commitment of mesenchymal stem cells (MSCs) in the bone marrow towards osteogenic or adipogenic differentiation might be also tightly dependent on PPARγ regulation by miRNAs. Indeed, miR-548d-5p, which is downregulated during adipogenic differentiation of human bone marrow derived MSCs, targets the 3′UTR of PPARγ. Overexpression of this miRNA abrogates adipogenic differentiation and increases the osteogenic potential of MSCs by downregulating PPARγ and C/EBPα [58]. Induction of other miRNAs such as miR-20 during osteogenic differentiation leads also to a direct downregulation of PPARγ [46]. In addition, miR-17-5p and miR-106a also promote adipogenesis and inhibit osteogenic differentiation in human adipose derived MSCs by indirect mechanisms, which increase C/EBPα and PPARγ expressions [99]. Finally, alterations of the osteogenic/adipogenic differentiation balance is an important component of specific osteogenic-related disorders such as osteoporosis and deregulation of the expression of miRNAs targeting PPARγ, for example, miR-210, have been involved in these diseases [64, 100].

3.3.4. miRNAs-Dependent Regulation of PPARγ in the Heart

Upregulation of miR-27b expression was shown in heart-specific smad4 knockout mice, which develop cardiac hypertrophy [61]. Overexpression of this miRNA specifically in cardiomyocytes using transgenic mice was sufficient to induce cardiac hypertrophy through PPARγ downregulation [61]. Conversely, treatment of a mouse model of heart failure with miR-27b inhibitors (antagomirs) improved cardiovascular functions by increasing PPARγ expression [61]. Similarly, in vivo inhibition of miR-128 by antagomirs protected cardiomyocytes from apoptosis in a model of myocardial ischemia/reperfusion injury and increased PPARγ expression in neonatal rat ventricular myocytes (NRVM) [101]. However, whether miR-128 modulates PPARγ through direct or indirect mechanisms was not assessed in this study.

3.3.5. miRNAs-Dependent Regulation of PPARγ in Other Cell Types/Organs

In addition to its role in hepatocytes, adipocytes, and cardiomyocytes, the relevance of miR-27b targeting of PPARγ was also highlighted in several other tissues (inflammatory cells, renal tubular cells, and pulmonary endothelial cells as well as neuroblastoma).

Inflammatory Cells. PPARγ is a potent inhibitor of M1 macrophage activation (Th1 proinflammatory macrophages) and promoter of M2 macrophage activation (Th2 anti-inflammatory macrophages) [102]. Upregulation of miR-27b in human macrophages upon LPS exposure was demonstrated to directly target PPARγ and to elicit a Th1 differentiation [49]. Although these findings suggest that miR-27b-dependent downregulation of PPARγ may represent a key process in macrophage polarization, whether miR-27b controls M2 macrophage activation via PPARγ was however not investigated.

Kidneys. Upregulation of miR-27a occurs in glucose-stimulated rat renal proximal tubular cell line (NRK-52E cells) and renal tubular epithelial cells of streptozotocin-induced diabetic rats. In these cellular contexts, the increased miR-27a expression was shown to trigger PPARγ downregulation, which in turn promoted renal fibrosis [60].

Lung. In mice and human pulmonary artery endothelial cells (HPAECs), hypoxia upregulates miR-27a expression and decreases PPARγ expression [103]. Given the important antiproliferative, and antithrombotic and vasodilatory effects of PPARγ on the lung vasculature [104], upregulation of miR-27a may thus represent an important contributor to the development of pulmonary hypertension.

Neuroblastoma Cells. Although miR-27b-dependent downregulation of PPARγ promotes cell proliferation in HCC, it may lead to opposite effects in other cancers [7, 51, 92–95]. This is the case in the SK-N-AS neuroblastoma cells and derived mouse xenografts, where miR-27b was shown to repress PPARγ expression resulting in a decreased inflammatory response and tumor growth [51, 105, 106].

4. Indirect Regulation of PPARs by miRNAs

The activity of PPARs is tightly linked to the binding of transcriptional partners (i.e., RXR, Prdm16), cofactors/repressors (e.g., PGC1α, NCOR), or other regulators (e.g., Sirt1) [3]. Most of the PPARs binding partners and cofactors are also finely tuned by specific miRNAs, which thereby indirectly regulate the expression/activity of PPARs isoforms [18, 107–112]. A brief overview of miRNAs targeting PPARs binding partners and cofactors is provided in the next section (see Figure 3).

Figure 3

miRNAs targeting PPAR transcriptional partners, cofactors/repressors, and other regulators. miRNAs that have been experimentally demonstrated to specifically target PPAR transcriptional partners (RXR and Prdm16), PPAR cofactors (Pgc1α), PPAR repressors (NCOR2), and other PPAR regulators (Sirt1) are illustrated. miRNAs identified in human studies are in blue, those identified in mouse/rat studies are in green, and those identified in both human and rodents studies are in red. PPAR: peroxisome proliferator-activated receptor α, β/δ, or γ; RXR: Retinoid-X-Receptor; Prdm16: PR domain-containing 16; Sirt1: Sirtuin-1; NCOR2: nuclear receptor corepressor 2 (SMRT); Pgc1α: peroxisome proliferator-activated receptor gamma coactivator 1; PPRE: peroxisome proliferator response element.

4.1. miRNAs-Dependent Regulation of PPARs Binding/Heterodimerization Partners

4.1.1. miRNAs-Dependent Regulation of RXRs

RXR isoforms (RXRα/β/γ) are the obligate binding partners for PPARs. Together they form heterodimeric complexes and induce gene transactivation by binding to PPAR response elements (PPREs) [3]. As illustrated in Figure 3, several miRNAs have been reported to directly target RXR isoforms thus affecting indirectly PPARs activities [108, 109, 113, 114]. For example, miR-128-2 was shown to suppress cholesterol efflux in HepG2 cells and in the liver of diet-induced obese mice by binding to the 3′UTR of RXRα and of ATP-binding cassette transporters (ABCA1 and ABCG1) and repressing their expressions [114]. Chondrogenesis, which is inhibited by RXRα, was also promoted in mesenchymal stem cells by miR-574-3p, which downregulates specifically RXRα expression [113]. Interestingly, specific miRNAs targeting PPARγ, that is, miR-34a and miR-27a/b, also control RXRα expression in liver cells [73, 98, 109]. Indeed upregulation of miR-34a, which was correlated with fibrosis development, downregulates RXRα by binding within the coding region and not the 3′UTR of this isoform in hepatocytes [109]. In the case of miR-27a and miR-27b, these two miRNAs were upregulated in rat activated HSCs and decrease RXRα expression through 3′UTR-dependent mechanisms [73, 98]. It thus appears that abnormal miRNAs-dependent inhibition of RXRα in distinct liver cells contributes to the development of hepatic fibrogenesis. Finally, inhibition of RXRα by upregulation of miR-27a was also reported in aggressive rhabdomyosarcoma (RMS) [108]. Altogether, these studies suggest that particular miRNAs, such as miR-34a and the miR-27 family, may affect PPARs signaling by simultaneously targeting different key players in this pathway.

4.1.2. miRNAs-Dependent Regulation of Prdm16

During brown adipogenesis, Prdm16 (PR domain-containing 16) instead of RXRα heterodimerizes with PPARγ2 and mediates brown adipocyte differentiation [115]. MiR-133a was demonstrated to regulate directly Prdm16 expression in immortalized brown preadipocytes [18] and inhibition of miR-133a and miR-133b led to an increased expression of adipogenic markers including PPARγ as well as differentiation towards mature brown adipocytes [18, 116, 117].

4.1.3. miRNAs-Dependent Regulation of PGC1α

PGC1α is a critical transcriptional coactivator of PPARγ in brown preadipocytes and of PPARα in white preadipocytes (3T3-L1 cells) [118]. To date only two miRNAs have been described in hepatocytes to directly target PGC1α mRNA: (i) miR-696, which is upregulated with obesity, decreases PGC1α expression in the liver of ob/ob mice [119] and (ii) miR-130a, which is downregulated in HBV-infected human hepatocytes, increases PGC1α and PPARγ expression thus favoring HBV replication [120].

4.1.4. miRNAs-Dependent Regulation of NCOR

In the absence of PPARs ligands, the transcriptional activity of PPARs is inhibited by the binding of corepressors such NCOR proteins [12]. miRNAs-dependent regulation of NCOR proteins is supported by two studies showing that (i) miR-16 in LPS-activated human monocytes (U937) and biliary epithelial cells (H69) targets SMRT (NCOR2), which leads to NF-κB-mediated transactivation of the IL-8 gene [107], and (ii) miR-100 targets SMRT (NCOR2) in glioblastoma cells thereby inhibiting their proliferation [112].

4.1.5. miRNAs-Dependent Regulation of Sirtuin-1

The NAD-dependent deacetylase Sirtuin-1 (Sirt1) is a critical regulator of PPAR signaling and of energy homeostasis [121]. Posttranscriptional control of SIRT1 and other sirtuins by miRNAs represents important regulatory mechanism for this protein family and has been extensively reviewed elsewhere [111]. Among the various miRNAs directly targeting SIRT1, miR-217 [122], miR-181a [123], miR-29 [124], and miR-34a [125] in particular were shown to affect hepatic lipid metabolism, insulin sensitivity, or carcinogenesis by modulating SIRT1 expression. Of note, miR-34a is also a direct regulator of PPARγ and RXRα expression [111, 125–128] therefore supporting again the biological relevance of fine-tuning PPARs signaling by modulating several factors involved in this transcriptional pathway.

5. miRNAs Regulated by PPARs

Recent evidence indicates that the expression of particular miRNAs can also be under the transcriptional control of PPARs [129] (see Figure 4). Most of the studies reviewed here rely on the identification of PPAR response elements (PPREs) within the promoter of genes encoding pri-miRNAs or on the effects of PPARs agonists [17, 96, 130, 131]. miRNAs described to date to be regulated by PPARs are short-listed in Table 2.

(a)

(b)

5.1. PPARα- and PPARβ/δ-Dependent Regulation of miRNAs Expression

Limited information is available on PPARα- and PPARβ/δ-dependent regulation of miRNAs expression. PPARα was suggested to promote the expression of let-7 and miR-200c in hepatic cancer cells. Indeed, expression of let-7, which targets c-myc in hepatocytes, was decreased in mice treated with the PPARα agonist Wy-14,643, which in turn fostered myc-dependent liver oncogenesis [71]. In Huh-7 hepatoma cells, PPARα in synergy with another nuclear receptor, that is, LRH-1 (liver receptor homolog-1), was proposed also to drive miR-200c transcription through a direct binding to its promoter [132]. Although the role of miR-200c in HCC was not investigated in this study, miR-200 was previously shown to have tumor suppressive activities by inhibiting cell migration [135]. Regarding PPARβ/δ, treatment of HUVEC endothelial cells with a PPARβ/δ agonist (GW501516) led to an increase of miR-100 expression, which improved lipidemia and vascular function [136]. However, as for the study using PPARα agonists, a direct binding of PPARβ/δ to the miR-100 promoter was not investigated and additional experiments are required to confirm these data and exclude off-target effects of pharmacological agonists of PPARβ/δ.

5.2. PPARγ-Dependent Regulation of miRNAs Expression

In contrast to the other PPAR isoforms, PPARγ was reported to regulate several miRNAs in distinct pathophysiological processes (see Table 2).

Endothelial Functions. miR-98, which is reduced in endothelial cells of patients suffering from idiopathic pulmonary hypertension (IPAH) and of mouse models of this disease, directly targets endothelin-1 (ET1). PPARγ was shown to exert a beneficial role in pulmonary hypertension (PH) by attenuating, likely through activation of miR-98, ET1 expression. In support of this hypothesis, activation of PPARγ with specific agonists (e.g., rosiglitazone) restores miR-98 expression in hypoxic mouse and in primary human pulmonary artery endothelial cells (PAECs); however whether PPARγ is a direct regulator of miR-98 was not assessed [103].

Adipocytes Differentiation and Function. PPARγ agonists (rosiglitazone and pioglitazone) modulated the expression of 27 different miRNAs in human subcutaneous and visceral adipocytes. Among those, miR-329, miR-145, and miR-339-5p are involved, based on predictive bioinformatics analyses, in metabolic (e.g., insulin signaling) and proliferative (e.g., Wnt/β-catenin signaling) pathways [17, 134]. Interestingly, miR-329 and miR-145 contain a PPRE in their promoters and both miRNAs also bind to PPARγ 3′UTR, thus suggesting the existence of positive feedback loop mechanisms regulating expressions of these miRNAs and PPARγ [17]. In human subcutaneous adipocytes and bovine preadipocytes, PPARγ also induces the expression of miR-378, which is located in the first intron of PPARγ coactivator-1β (PGC1β) [98, 134, 137]. Finally, a list of potential miRNAs, directly regulated by PPARγ and involved in 3T3-L1 adipose differentiation, was identified by crossing datasets of miRNAs containing putative PPARγ binding site with datasets of miRNAs altered during 3T3-L1 differentiation. Authors of this study identified miR-103-1, miR-182/miR-96/miR-183, miR-205, and miR-378 as potential PPARγ-regulated miRNAs, whose expression was further induced in 3T3-L1 cells treated by rosiglitazone. Chip analyses also revealed that these miRNAs are directly regulated by PPARγ through PPRE present in their host genes (PanK3 and PGC1β) [138].

Inflammation. Exposure of bone marrow derived macrophages (BMDMs) to Th2 stimuli (i.e., IL-4) triggers the expression of miR-223 through a direct binding of PPARγ in PPREs within the promoter of pre-miR-223. This effect was further enhanced by a PPARγ agonist (i.e., pioglitazone) and inhibited by a PPARγ antagonist (i.e., GW9662). Since PPARγ-dependent M2 activation is inhibited in BMDMs from miR-223 knockout mice, these data suggest that miR-223 and its target genes (e.g., Rasa1 and genuine) are key effectors of macrophages polarization [133].

Fibrosis. Whether PPARγ may control fibrotic processes through miRNAs-dependent mechanisms is not well established, but one study supports this concept. Indeed, Dharap et al., reported that miR-145, which contains a PPAR response element in its promoter [17, 96], was increased in rosiglitazone-treated hypertrophic scar fibroblasts (HSFDs), thus leading to a direct decrease of SMAD3 expression and collagen synthesis [131].

Carcinogenesis. A direct effect of PPARγ on the expression of specific miRNAs through binding of PPRE in their promoters was demonstrated for three different types of cancer cell lines. In hepatoma HepG2 cells, miR-122 was strongly induced in cells treated with DNA methylation or histone deacetylase inhibitors via a direct binding of PPARγ/RXRα in the pre-miR-122 promoter [139]. In ovarian cancer cells (i.e., Ovcar3, CaOv3, and Skov3 cells), PPARγ also directly regulates the transcription of miR-125b and silencing of miR-125 impaired the growth inhibitory capacity of PPARγ agonists [130]. Finally, miR-145, which is downregulated in colorectal cancer cells (Caco2, Sw480, HCT116, and HT29) and colorectal tumor tissues, is induced by the PPARγ agonist (i.e., rosiglitazone) via direct binding of PPARγ to PPRE in the promoter encoding pre-miR-145 [96, 131].

6. miRNAs-Based Therapies to Target PPARs Expression/Activity

Targeting tissue-specific miRNAs with pharmacological compounds may represent novel and valuable alternative therapeutic approaches to PPAR agonists or antagonists [10–13]. Different methods have been developed to modulate miRNA expressions in vivo. Of particular interest are chemically modified synthetic oligonucleotides inhibiting or mimicking endogenous miRNAs that display increased affinity for their targets and great stability in the serum. Currently, these oligonucleotides bear modifications on the 2′- or 3′-position of the nucleic acid ribose backbone. For example, antagomiRs (3′-cholesterol-conjugated, 2′-O-Me oligonucleotides with terminal phosphorothioate modifications), antisense modified oligonucleotides (AMO) (2′-O-methoxyethyl phosphorothioate modified antisense oligonucleotide or 2′-fluoro-modified antisense oligonucleotides), or locked nucleic acids (LNA) represent potent inhibitors of miRNAs expression/activity. These synthetic nucleotides are usually administered by intravenous injection and hopefully soon orally with a good efficiency [140, 141]. When administered by intravenous injection they can broadly reach every tissue but tends to accumulate in particular organs, such as the liver or the kidneys [26]. Special formulations such as liposomes or polyethylenimine-formulated nanoparticles as miRNA nanocarriers have been developed to improve tissue-specific distribution, circulation time, and clearance of the miRNAs-like compounds [26, 142, 143]. Of particular interest, microvesicles (MVs) were shown to represent efficient and functional miRNA delivery tools as it was demonstrated in animals and in the case of miR-130b [144, 145]. Other alternative methods to target specific tissues have been also developed such as inclusion of oligonucleotides into liposomal or oleic-based nanoparticles, which target preferentially the liver [142]. Finally, viruses with specific tropisms, for example, adenoassociated viruses (AAV), have been used in animal models to robustly express or inhibit specific miRNAs in particular tissues and may represent an interesting alternative to chemically modified nucleotides [26]. Importantly, abnormal levels of circulating miRNAs stimulate toll-like receptors therefore promoting inflammation and favoring the development of chronic diseases such as metabolic and cardiovascular disorders as well as cancers. Interestingly, chemically modified synthetic oligonucleotides, in particular those modified in the 2′ position of the ribose, have the ability to reduce, but not completely prevent, such unintended immune responses [26, 146].

Several miRNA inhibitors have been tested in preclinical studies with rodents or primates in the context of various pathologies (e.g., miR-155 in inflammatory diseases, miR-208 in cardiac remodeling) including metabolic diseases (e.g., miR-103/107 for type 2 diabetes and obesity) [26]. However, only few of them, for example, miR-122 inhibitors (Miravirsen) to treat HCV infection, are currently being tested in human clinical trials [26, 147–149]. Unfortunately, none of the miRNAs known to potentially target PPAR isoforms are under clinical trials in human. Only preclinical studies were performed for miR-33 and miR-21 [26], which targets directly PPARα (Figures 2-3). In African green monkeys, inhibition of mir-33a/b with specific antagomiRs increased the hepatic expression of ABCA1, thus leading to an increase of HDL (high density lipoprotein) and a decrease in VLDL (very low density lipoproteins) and triglycerides plasma levels [150]. Inhibition of miR-21 in mice with an antisense oligonucleotide prevented hepatic lipid accumulation in animals fed an obesogenic diet [151].

The (pre)clinical use of synthetic nucleotides mimicking endogenous miRNAs is less developed compared to miRNAs inhibitors and currently only miR-34 mimics nucleotides are tested to treat some cancers [26, 152]. MRX34, a liposome-formulated miR-34 mimic-based drug is currently in phase I study for melanoma patients. This miR-34 mimic achieved positive outcomes as a monotherapeutic agent in patients with renal cell carcinoma, acral melanoma, and HCC (http://www.mirnatherapeutics.com/pipeline/mirna-pipeline.html) [26]. However, other in vivo studies indicated that miR-34a/c could also activate hepatic stellate cells and promote fibrogenesis by targeting PPARy and repressing RXRα and Sirt1 [52, 109]. Other miRNAs, such as miR-27 or miR-9, are also able to regulate the expression/activities of different PPARs isoforms in distinct tissues. Therefore, although miRNAs-based therapies are promising, the potential pleiotropic effects of systemic administration of pharmacological miRNAs inhibitors or mimics call also for cautiousness in their therapeutic use since they can likely lead, as in the case of PPARs agonists/antagonists, to conflicting and unwanted side effects.

7. Conclusion

The pivotal role of abnormal PPARs signaling in the development and the progression of various pathologies including metabolic diseases, inflammation, and cancer is now well established. However, the mechanisms and extent to which miRNAs contribute to alterations of PPARs expressions and/or activities in physiopathological conditions are currently still poorly understood and represent an important developing field of research. Conversely, the fact that PPARs can drive the expression of specific miRNAs, which may target in turn hundreds of different mRNAs, opens also a new dimension in our understanding of the physiological and pathological roles of PPARs isoforms. Given the tissue-specific and pleiotropic action of PPARs in various cellular processes described herein, it is likely that posttranscriptional regulation of PPARs and related cofactors by miRNAs is tissue- and process-specific. In addition, the simplistic view that only changes in the intracellular levels of miRNAs impact the expression of target genes is likely incorrect. Indeed increasing evidence indicates that the activity and bioavailability of miRNAs are also key factors to consider in these regulatory mechanisms. This concept is further supported by the emerging role of long noncoding RNAs [31] and RNA-binding proteins, which could interfere with the activity/expression of specific miRNAs [153, 154] and regulation of their target genes. Further studies are thus required to deepen our knowledge of miRNAs-based posttranscriptional regulatory mechanisms controlling PPARs expressions and activities.

Abbreviations

AP-1:	Activator protein-1
ApoA:	Apolipoprotein-A
BAT:	Brown adipose tissue
CD36:	Cluster of differentiation 36
FAT:	Fatty acid translocase
C/EBPα:	CCAAT/enhancer-binding protein α
C. elegans:	Caenorhabditis elegans
COX-2:	Cyclooxygenase-2
CRC:	Colorectal carcinoma
CREB:	cAMP response element-binding protein
CVD:	Cardiovascular disease
DEN:	Diethylnitrosamine
DGCR8:	DiGeorge syndrome chromosomal region 8
ECM:	Extracellular matrix
FABP:	Fatty acid binding protein
Glut4:	Glucose-transporter 4
HCC:	Hepatocellular carcinoma
HCV/HBV:	Hepatitis C/B virus
HFD:	High fat diet
HSC:	Hepatic stellate cells
IRS-1/2:	Insulin receptor substrates-1/2
lncRNA:	Long noncoding RNA
LPL:	Lipoprotein lipase
LPS:	Lipopolysaccharide
LRH-1:	Liver receptor homolog-1
MCP-1:	Monocyte chemoattractant protein-1
miRNA:	MicroRNA
MSC:	Mesenchymal stem cell
NAFLD:	Nonalcoholic fatty liver disease
NASH:	Nonalcoholic steatohepatitis
NCOR:	Nuclear receptor corepressor
ncRNA:	Noncoding RNA
NFB:	Nuclear factor-B
PGE2:	Prostaglandin E2
PGC1:	Peroxisome proliferator-activated receptor gamma coactivator-1
PPAR:	Peroxisome proliferator-activated receptor
PPRE:	Peroxisome proliferator response element
Prdm16:	PR domain-containing 16
RISC:	RNA-induced silencing complex
ROS:	Reactive oxygen species
RXR:	Retinoid-X-Receptor
siRNA:	Small interfering RNA
Sirt1:	Sirtuin 1
SMRT:	Silencing mediator for retinoid and thyroid hormone receptor
sncRNA:	Small noncoding RNA
STAT1:	Signal transducer and activator of transcription 1
T2DM:	Type 2 diabetes mellitus
TARP2:	T-cell receptor gamma-chain constant region
TNF-α:	Tumor necrosis factor-α
TZD:	Thiazolidinedione
UCP-1:	Uncoupling protein-1
UTR:	Untranslated region
VCAM:	Vascular cell adhesion protein
WAT:	White adipose tissue.

Competing Interests

The authors declare that they have no competing interests.

Authors’ Contributions

Dorothea Portius and Cyril Sobolewski have equal contributions.

Acknowledgments

Work in the Foti laboratory is supported by the Swiss National Science Foundation (Grant nos. 310030-152618 and CRSII3-160717), the Swiss Cancer Research Foundation (Grant no. KFS-3246-08-2013), the Bo & Kerstin Hjelt Diabetes Foundation, the FLAGS Foundation, the Fondation Romande pour la Recherche sur le Diabetes, and the EFSD/Lilly European Diabetes Research Programme.

References

I. Issemann and S. Green, “Activation of a member of the steroid hormone receptor superfamily by peroxisome proliferators,” Nature, vol. 347, no. 6294, pp. 645–650, 1990.
View at: Publisher Site | Google Scholar
R. M. Evans, G. D. Barish, and Y.-X. Wang, “PPARs and the complex journey to obesity,” Nature Medicine, vol. 10, no. 4, pp. 355–361, 2004.
View at: Publisher Site | Google Scholar
S. Polvani, “Peroxisome proliferator activated receptors at the crossroad of obesity, diabetes, and pancreatic cancer,” World Journal of Gastroenterology, vol. 22, no. 8, pp. 2441–2459, 2016.
View at: Publisher Site | Google Scholar
G. M. G. Attianese and B. Desvergne, “Integrative and systemic approaches for evaluating PPARβ/δ (PPARD) function,” Nuclear Receptor Signaling, 2015.
View at: Publisher Site | Google Scholar
M. Ahmadian, J. M. Suh, N. Hah et al., “PPARγ signaling and metabolism: the good, the bad and the future,” Nature Medicine, vol. 19, no. 5, pp. 557–566, 2013.
View at: Publisher Site | Google Scholar
B. Grygiel-Górniak, “Peroxisome proliferator-activated receptors and their ligands: nutritional and clinical implications—a review,” Nutrition Journal, vol. 13, no. 1, article no. 17, 2014.
View at: Publisher Site | Google Scholar
J. M. Peters, Y. M. Shah, and F. J. Gonzalez, “The role of peroxisome proliferator-activated receptors in carcinogenesis and chemoprevention,” Nature Reviews Cancer, vol. 12, no. 3, pp. 181–195, 2012.
View at: Publisher Site | Google Scholar
A. S. Laganà, S. G. Vitale, A. Nigro et al., “Pleiotropic actions of Peroxisome Proliferator-Activated Receptors (PPARs) in dysregulated metabolic homeostasis, inflammation and cancer: current evidence and future perspectives,” International Journal of Molecular Sciences, vol. 17, no. 7, article 999, 2016.
View at: Publisher Site | Google Scholar
E. Fuentes, L. Guzmán-Jofre, R. Moore-Carrasco, and I. Palomo, “Role of PPARs in inflammatory processes associated with metabolic syndrome (Review),” Molecular Medicine Reports, vol. 8, no. 6, pp. 1611–1616, 2013.
View at: Publisher Site | Google Scholar
C. J. Bailey, A. A. Tahrani, and A. H. Barnett, “Future glucose-lowering drugs for type 2 diabetes,” The Lancet Diabetes and Endocrinology, vol. 4, no. 4, pp. 350–359, 2016.
View at: Publisher Site | Google Scholar
B. Gross and B. Staels, “PPAR agonists: multimodal drugs for the treatment of type-2 diabetes,” Best Practice and Research in Clinical Endocrinology and Metabolism, vol. 21, no. 4, pp. 687–710, 2007.
View at: Publisher Site | Google Scholar
S. Sugii and R. M. Evans, “Epigenetic codes of PPARγ in metabolic disease,” FEBS Letters, vol. 585, no. 13, pp. 2121–2128, 2011.
View at: Publisher Site | Google Scholar
C. V. Rizos, A. Kei, and M. S. Elisaf, “The current role of thiazolidinediones in diabetes management,” Archives of Toxicology, vol. 90, no. 8, pp. 1861–1881, 2016.
View at: Publisher Site | Google Scholar
R. Barres and J. R. Zierath, “DNA methylation in metabolic disorders,” American Journal of Clinical Nutrition, vol. 93, no. 4, pp. 897S–900S, 2011.
View at: Publisher Site | Google Scholar
K. Fujiki, F. Kano, K. Shiota, and M. Murata, “Expression of the peroxisome proliferator activated receptor γ gene is repressed by DNA methylation in visceral adipose tissue of mouse models of diabetes,” BMC Biology, vol. 7, article no. 38, 2009.
View at: Publisher Site | Google Scholar
M. K. Ramlee, Q. Zhang, M. Idris et al., “Histone H3 K27 acetylation marks a potent enhancer element on the adipogenic master regulator gene Pparg2,” Cell Cycle, vol. 13, no. 21, pp. 3414–3422, 2014.
View at: Publisher Site | Google Scholar
A. Dharap, C. Pokrzywa, S. Murali, B. Kaimal, and R. Vemuganti, “Mutual induction of transcription factor PPARγ and microRNAs miR-145 and miR-329,” Journal of Neurochemistry, vol. 135, no. 1, pp. 139–146, 2015.
View at: Publisher Site | Google Scholar
W. Liu, P. Bi, T. Shan et al., “miR-133a regulates adipocyte browning in vivo,” PLOS Genetics, vol. 9, no. 7, Article ID e1003626, 2013.
View at: Publisher Site | Google Scholar
V. Rottiers and A. M. Näär, “MicroRNAs in metabolism and metabolic disorders,” Nature Reviews Molecular Cell Biology, vol. 13, no. 4, pp. 239–251, 2012.
View at: Publisher Site | Google Scholar
Z. Yang, T. Cappello, and L. Wang, “Emerging role of microRNAs in lipid metabolism,” Acta Pharmaceutica Sinica B, vol. 5, no. 2, pp. 145–150, 2015.
View at: Publisher Site | Google Scholar
J. A. Deiuliis, “MicroRNAs as regulators of metabolic disease: pathophysiologic significance and emerging role as biomarkers and therapeutics,” International Journal of Obesity, vol. 40, no. 1, pp. 88–101, 2016.
View at: Publisher Site | Google Scholar
C. L. Holley and V. K. Topkara, “An introduction to small non-coding RNAs: miRNA and snoRNA,” Cardiovascular Drugs and Therapy, vol. 25, no. 2, pp. 151–159, 2011.
View at: Publisher Site | Google Scholar
S. L. Ameres and P. D. Zamore, “Diversifying microRNA sequence and function,” Nature Reviews Molecular Cell Biology, vol. 14, no. 8, pp. 475–488, 2013.
View at: Publisher Site | Google Scholar
M. A. Goldgraben, R. Russell, O. M. Rueda, C. Caldas, and A. Git, “Double-stranded microRNA mimics can induce length-and passenger strand-dependent effects in a cell type-specific manner,” RNA, vol. 22, no. 2, pp. 193–203, 2016.
View at: Publisher Site | Google Scholar
C. Fernandez-Hernando, C. M. Ramírez, L. Goedeke, and Y. Suárez, “MicroRNAs in metabolic disease,” Arteriosclerosis, Thrombosis, and Vascular Biology, vol. 33, no. 2, pp. 178–185, 2013.
View at: Publisher Site | Google Scholar
E. van Rooij and S. Kauppinen, “Development of microRNA therapeutics is coming of age,” EMBO Molecular Medicine, vol. 6, no. 7, pp. 851–864, 2014.
View at: Publisher Site | Google Scholar
A. Lujambio and S. W. Lowe, “The microcosmos of cancer,” Nature, vol. 482, no. 7385, pp. 347–355, 2012.
View at: Publisher Site | Google Scholar
G. A. Calin and C. M. Croce, “MicroRNA signatures in human cancers,” Nature Reviews Cancer, vol. 6, no. 11, pp. 857–866, 2006.
View at: Publisher Site | Google Scholar
C. Sobolewski, N. Calo, D. Portius, and M. Foti, “MicroRNAs in fatty liver disease,” Seminars in Liver Disease, vol. 35, no. 1, pp. 12–25, 2015.
View at: Publisher Site | Google Scholar
A. Drakaki, M. Hatziapostolou, C. Polytarchou et al., “Functional microRNA high throughput screening reveals miR-9 as a central regulator of liver oncogenesis by affecting the PPARA-CDH1 pathway,” BMC Cancer, vol. 15, no. 1, article no. 542, 2015.
View at: Publisher Site | Google Scholar
M. Cui, Z. Xiao, Y. Wang et al., “Long noncoding RNA HULC modulates abnormal lipid metabolism in hepatoma cells through an mir-9-mediated RXRA signaling pathway,” Cancer Research, vol. 75, no. 5, pp. 846–857, 2015.
View at: Publisher Site | Google Scholar
L. Zheng, G.-C. Lv, J. Sheng, and Y.-D. Yang, “Effect of miRNA-10b in regulating cellular steatosis level by targeting PPAR-α expression, a novel mechanism for the pathogenesis of NAFLD,” Journal of Gastroenterology and Hepatology, vol. 25, no. 1, pp. 156–163, 2010.
View at: Publisher Site | Google Scholar
J. Zhou, K.-C. Wang, W. Wu et al., “MicroRNA-21 targets peroxisome proliferators-activated receptor-α in an autoregulatory loop to modulate flow-induced endothelial inflammation,” Proceedings of the National Academy of Sciences of the United States of America, vol. 108, no. 25, pp. 10355–10360, 2011.
View at: Publisher Site | Google Scholar
X. Loyer, V. Paradis, C. Hénique et al., “Liver microRNA-21 is overexpressed in non-alcoholic steatohepatitis and contributes to the disease in experimental models by inhibiting PPARa expression,” Gut, vol. 65, no. 11, pp. 1882–1894, 2015.
View at: Publisher Site | Google Scholar
Z.-J. Li, P.-H. Ou-Yang, and X.-P. Han, “Profibrotic effect of miR-33a with Akt activation in hepatic stellate cells,” Cellular Signalling, vol. 26, no. 1, pp. 141–148, 2014.
View at: Publisher Site | Google Scholar
W. Hu, X. Wang, X. Ding et al., “MicroRNA-141 represses HBV replication by targeting PPARA,” PLoS ONE, vol. 7, no. 3, Article ID e34165, 2012.
View at: Publisher Site | Google Scholar
B. Li, Z. Zhang, H. Zhang et al., “Aberrant miR199a-5p/caveolin1/PPARα axis in hepatic steatosis,” Journal of Molecular Endocrinology, vol. 53, no. 3, pp. 393–403, 2014.
View at: Publisher Site | Google Scholar
J. L. Tong, C. P. Zhang, F. Nie et al., “MicroRNA 506 regulates expression of PPAR alpha in hydroxycamptothecin- resistant human colon cancer cells,” FEBS Letters, vol. 585, no. 22, pp. 3560–3568, 2011.
View at: Publisher Site | Google Scholar
R. Martinelli, C. Nardelli, V. Pilone et al., “MiR-519d overexpression is associated with human obesity,” Obesity, vol. 18, no. 11, pp. 2170–2176, 2010.
View at: Publisher Site | Google Scholar
P. Gurha, T. Wang, A. H. Larimore et al., “microRNA-22 promotes heart failure through coordinate suppression of PPAR/ERR-nuclear hormone receptor transcription,” PLoS ONE, vol. 8, no. 9, Article ID e75882, 2013.
View at: Publisher Site | Google Scholar
L. Sun and M. Trajkovski, “MiR-27 orchestrates the transcriptional regulation of brown adipogenesis,” Metabolism: Clinical and Experimental, vol. 63, no. 2, pp. 272–282, 2014.
View at: Publisher Site | Google Scholar
D. Baek, J. Villén, C. Shin, F. D. Camargo, S. P. Gygi, and D. P. Bartel, “The impact of microRNAs on protein output,” Nature, vol. 455, no. 7209, pp. 64–71, 2008.
View at: Publisher Site | Google Scholar
H. El Azzouzi, S. Leptidis, E. Dirkx et al., “The Hypoxia-Inducible MicroRNA Cluster miR-199a~214 targets myocardial PPARδ and impairs mitochondrial fatty acid oxidation,” Cell Metabolism, vol. 18, no. 3, pp. 341–354, 2013.
View at: Publisher Site | Google Scholar
P. Thulin, T. Wei, O. Werngren et al., “MicroRNA-9 regulates the expression of peroxisome proliferator-activated receptor δ in human monocytes during the inflammatory response,” International Journal of Molecular Medicine, vol. 31, no. 5, pp. 1003–1010, 2013.
View at: Publisher Site | Google Scholar
Y.-Y. Xiao, P.-J. Fan, S.-R. Lei, M. Qi, and X.-H. Yang, “MiR-138/peroxisome proliferator-activated receptor β signaling regulates human hypertrophic scar fibroblast proliferation and movement in vitro,” Journal of Dermatology, vol. 42, no. 5, pp. 485–495, 2015.
View at: Publisher Site | Google Scholar
J.-F. Zhang, W.-M. Fu, M.-L. He et al., “MiRNA-20a promotes osteogenic differentiation of human mesenchymal stem cells by co-regulating BMP signaling,” RNA Biology, vol. 8, no. 5, pp. 829–838, 2011.
View at: Publisher Site | Google Scholar
S. Li, J. Li, B.-Y. Fei et al., “MiR-27a promotes hepatocellular carcinoma cell proliferation through suppression of its target gene peroxisome proliferator-activated receptor γ,” Chinese Medical Journal, vol. 128, no. 7, pp. 941–947, 2015.
View at: Publisher Site | Google Scholar
B.-Y. Kang, K. K. Park, D. E. Green et al., “Hypoxia mediates mutual repression between microRNA-27a and PPARγ in the pulmonary vasculature,” PLoS ONE, vol. 8, no. 11, Article ID e79503, 2013.
View at: Publisher Site | Google Scholar
C. Jennewein, A. Von Knethen, T. Schmid, and B. Brüne, “MicroRNA-27b contributes to lipopolysaccharide-mediated peroxisome proliferator-activated receptor γ (PPARγ) mRNA destabilization,” Journal of Biological Chemistry, vol. 285, no. 16, pp. 11846–11853, 2010.
View at: Publisher Site | Google Scholar
M. Karbiener, C. Fischer, S. Nowitsch et al., “microRNA miR-27b impairs human adipocyte differentiation and targets PPARgamma,” Biochemical and Biophysical Research Communications, vol. 390, no. 2, pp. 247–251, 2009.
View at: Google Scholar
J.-J. Lee, A. Drakaki, D. Iliopoulos, and K. Struhl, “MiR-27b targets PPARγ to inhibit growth, tumor progression and the inflammatory response in neuroblastoma cells,” Oncogene, vol. 31, no. 33, pp. 3818–3825, 2012.
View at: Publisher Site | Google Scholar
X. Li, Y. Chen, S. Wu et al., “MicroRNA-34a and microRNA-34c promote the activation of human hepatic stellate cells by targeting peroxisome proliferator-activated receptor γ,” Molecular Medicine Reports, vol. 11, no. 2, pp. 1017–1024, 2015.
View at: Publisher Site | Google Scholar
D. Povero, N. Panera, A. Eguchi et al., “Lipid-induced hepatocyte-derived extracellular vesicles regulate hepatic stellate cells via microRNA targeting Peroxisome Proliferator-Activated Receptor-γ,” CMGH Cellular and Molecular Gastroenterology and Hepatology, vol. 1, no. 6, pp. 646.e4–663.e4, 2015.
View at: Publisher Site | Google Scholar
E. K. Lee, M. J. Lee, K. Abdelmohsen et al., “miR-130 suppresses adipogenesis by inhibiting peroxisome proliferator-activated receptor γ expression,” Molecular and Cellular Biology, vol. 31, no. 4, pp. 626–638, 2011.
View at: Publisher Site | Google Scholar
K. Tu, X. Zheng, C. Dou et al., “MicroRNA-130b promotes cell aggressiveness by inhibiting peroxisome proliferator-activated receptor gamma in human hepatocellular carcinoma,” International Journal of Molecular Sciences, vol. 15, no. 11, pp. 20486–20499, 2014.
View at: Publisher Site | Google Scholar
Y. Jiao, M. Zhu, X. Mao et al., “MicroRNA-130a expression is decreased in Xinjiang Uygur patients with type 2 diabetes mellitus,” American Journal of Translational Research, vol. 7, no. 10, pp. 1984–1991, 2015.
View at: Google Scholar
Z. Yang, C. Bian, H. Zhou et al., “MicroRNA hsa-miR-138 inhibits adipogenic differentiation of human adipose tissue-derived mesenchymal stem cells through adenovirus EID-1,” Stem Cells and Development, vol. 20, no. 2, pp. 259–267, 2011.
View at: Publisher Site | Google Scholar
J. Sun, Y. Wang, Y. Li, and G. Zhao, “Downregulation of PPARγ by miR-548d-5p suppresses the adipogenic differentiation of human bone marrow mesenchymal stem cells and enhances their osteogenic potential,” Journal of Translational Medicine, vol. 12, no. 1, article no. 168, 2014.
View at: Publisher Site | Google Scholar
S. Y. Kim, A. Y. Kim, H. W. Lee et al., “miR-27a is a negative regulator of adipocyte differentiation via suppressing PPARγ expression,” Biochemical and Biophysical Research Communications, vol. 392, no. 3, pp. 323–328, 2010.
View at: Publisher Site | Google Scholar
X. Hou, J. Tian, J. Geng et al., “MicroRNA-27a promotes renal tubulointerstitial fibrosis via suppressing PPARγ pathway in diabetic nephropathy,” Oncotarget, vol. 7, no. 30, pp. 47760–47776, 2016.
View at: Publisher Site | Google Scholar
J. Wang, Y. Song, Y. Zhang et al., “Cardiomyocyte overexpression of miR-27b induces cardiac hypertrophy and dysfunction in mice,” Cell Research, vol. 22, no. 3, pp. 516–527, 2012.
View at: Publisher Site | Google Scholar
C. Kim, H. Lee, Y. M. Cho, O.-J. Kwon, W. Kim, and E. K. Lee, “TNFα-induced miR-130 resulted in adipocyte dysfunction during obesity-related inflammation,” FEBS Letters, vol. 587, no. 23, pp. 3853–3858, 2013.
View at: Publisher Site | Google Scholar
L. Lu, J. Wang, H. Lu et al., “MicroRNA-130a and -130b enhance activation of hepatic stellate cells by suppressing PPARγ expression: a rat fibrosis model study,” Biochemical and Biophysical Research Communications, vol. 465, no. 3, pp. 387–393, 2015.
View at: Publisher Site | Google Scholar
X.-D. Liu, F. Cai, L. Liu, Y. Zhang, and A.-L. Yang, “MicroRNA-210 is involved in the regulation of postmenopausal osteoporosis through promotion of VEGF expression and osteoblast differentiation,” Biological Chemistry, vol. 396, no. 4, pp. 339–347, 2015.
View at: Publisher Site | Google Scholar
H. Li, M. Xue, J. Xu, and X. Qin, “MiR-301a is involved in adipocyte dysfunction during obesity-related inflammation via suppression of PPARγ,” Pharmazie, vol. 71, no. 2, pp. 84–88, 2016.
View at: Google Scholar
B.-C. Jeong, I.-H. Kang, and J.-T. Koh, “MicroRNA-302a inhibits adipogenesis by suppressing peroxisome proliferator-activated receptor γ expression,” FEBS Letters, vol. 588, no. 18, pp. 3427–3434, 2014.
View at: Publisher Site | Google Scholar
L. Chen, Y. Chen, S. Zhang et al., “MiR-540 as a novel adipogenic inhibitor impairs adipogenesis via suppression of PPARγ,” Journal of Cellular Biochemistry, vol. 116, no. 6, pp. 969–976, 2015.
View at: Publisher Site | Google Scholar
M. Pawlak, P. Lefebvre, and B. Staels, “Molecular mechanism of PPARα action and its impact on lipid metabolism, inflammation and fibrosis in non-alcoholic fatty liver disease,” Journal of Hepatology, vol. 62, no. 3, pp. 720–733, 2015.
View at: Publisher Site | Google Scholar
P. Misra and J. K. Reddy, “Peroxisome proliferator-activated receptor-α activation and excess energy burning in hepatocarcinogenesis,” Biochimie, vol. 98, no. 1, pp. 63–74, 2014.
View at: Publisher Site | Google Scholar
R. K. Lyn, R. Singaravelu, S. Kargman et al., “Stearoyl-CoA desaturase inhibition blocks formation of hepatitis C virus-induced specialized membranes,” Scientific Reports, vol. 4, article 4549, 2014.
View at: Publisher Site | Google Scholar
Y. M. Shah, K. Morimura, Q. Yang, T. Tanabe, M. Takagi, and F. J. Gonzalez, “Peroxisome proliferator-activated receptor α regulates a microRNA-mediated signaling cascade responsible for hepatocellular proliferation,” Molecular and Cellular Biology, vol. 27, no. 12, pp. 4238–4247, 2007.
View at: Publisher Site | Google Scholar
N. Calo, P. Ramadori, C. Sobolewski et al., “Stress-activated miR-21/miR-21^∗ in hepatocytes promotes lipid and glucose metabolic disorders associated with high-fat diet consumption,” Gut, vol. 65, no. 11, pp. 1871–1881, 2016.
View at: Publisher Site | Google Scholar
J. Ji, J. Zhang, G. Huang, J. Qian, X. Wang, and S. Mei, “Over-expressed microRNA-27a and 27b influence fat accumulation and cell proliferation during rat hepatic stellate cell activation,” FEBS Letters, vol. 583, no. 4, pp. 759–766, 2009.
View at: Publisher Site | Google Scholar
M. Karbiener and M. Scheideler, “MicroRNA functions in brite/brown fat—novel perspectives towards anti-obesity strategies,” Computational and Structural Biotechnology Journal, vol. 11, no. 19, pp. 101–105, 2014.
View at: Publisher Site | Google Scholar
Y. Wu, J. Zuo, Y. Zhang et al., “Identification of miR-106b-93 as a negative regulator of brown adipocyte differentiation,” Biochemical and Biophysical Research Communications, vol. 438, no. 4, pp. 575–580, 2013.
View at: Publisher Site | Google Scholar
D. Iliopoulos, K. N. Malizos, P. Oikonomou, and A. Tsezou, “Integrative MicroRNA and proteomic approaches identify novel osteoarthritis genes and their collaborative metabolic and inflammatory networks,” PLoS ONE, vol. 3, no. 11, article e3740, 2008.
View at: Publisher Site | Google Scholar
W.-L. W. Wang, J. E. Welsh, and M. Tenniswood, “1,25-Dihydroxyvitamin D₃ modulates lipid metabolism in prostate cancer cells through miRNA mediated regulation of PPARA,” The Journal of Steroid Biochemistry and Molecular Biology, vol. 136, no. 1, pp. 247–251, 2013.
View at: Publisher Site | Google Scholar
L. Salvadó, L. Serrano-Marco, E. Barroso, X. Palomer, and M. Vázquez-Carrera, “Targeting PPARβ/δ for the treatment of type 2 diabetes mellitus,” Expert Opinion on Therapeutic Targets, vol. 16, no. 2, pp. 209–223, 2012.
View at: Publisher Site | Google Scholar
S. A. Ross and C. D. Davis, “MicroRNA, nutrition, and cancer prevention,” Advances in Nutrition, vol. 2, no. 6, pp. 472–485, 2011.
View at: Publisher Site | Google Scholar
C. H. Lee, P. Olson, A. Hevener et al., “PPARdelta regulates glucose metabolism and insulin sensitivity,” Proceedings of the National Academy of Sciences of the United States of America, vol. 103, no. 9, pp. 3444–3449, 2006.
View at: Google Scholar
Y.-X. Wang, C.-H. Lee, S. Tiep et al., “Peroxisome-proliferator-activated receptor δ activates fat metabolism to prevent obesity,” Cell, vol. 113, no. 2, pp. 159–170, 2003.
View at: Publisher Site | Google Scholar
E. Ehrenborg and A. Krook, “Regulation of skeletal muscle physiology and metabolism by peroxisome proliferator-activated receptor δ,” Pharmacological Reviews, vol. 61, no. 3, pp. 373–393, 2009.
View at: Publisher Site | Google Scholar
B. Gross, M. Pawlak, P. Lefebvre, and B. Staels, “PPARs in obesity-induced T2DM, dyslipidaemia and NAFLD,” Nature Reviews Endocrinology, vol. 13, no. 1, pp. 36–49, 2016.
View at: Publisher Site | Google Scholar
R. L. Stephen, M. C. U. Gustafsson, M. Jarvis et al., “Activation of peroxisome proliferator-activated receptor δ stimulates the proliferation of human breast and prostate cancer cell lines,” Cancer Research, vol. 64, no. 9, pp. 3162–3170, 2004.
View at: Publisher Site | Google Scholar
J. M. Peters, F. J. Gonzalez, and R. Müller, “Establishing the Role of PPARβ/δ in Carcinogenesis,” Trends in Endocrinology & Metabolism, vol. 26, no. 11, pp. 595–607, 2015.
View at: Publisher Site | Google Scholar
D. Gatfield, G. Le Martelot, C. E. Vejnar et al., “Integration of microRNA miR-122 in hepatic circadian gene expression,” Genes and Development, vol. 23, no. 11, pp. 1313–1326, 2009.
View at: Publisher Site | Google Scholar
M. Aprile, M. R. Ambrosio, V. D'Esposito et al., “PPARG in human adipogenesis: differential contribution of canonical transcripts and dominant negative isoforms,” PPAR Research, vol. 2014, Article ID 537865, 11 pages, 2014.
View at: Publisher Site | Google Scholar
M. Pancione, L. Sabatino, A. Fucci et al., “Epigenetic silencing of peroxisome proliferator-activated receptor γ is a biomarker for colorectal cancer progression and adverse patients' outcome,” PLoS ONE, vol. 5, no. 12, Article ID e14229, 2010.
View at: Publisher Site | Google Scholar
M. Peyrou, P. Ramadori, L. Bourgoin, and M. Foti, “PPARs in liver diseases and cancer: epigenetic regulation by microRNAs,” PPAR Research, vol. 2012, Article ID 757803, 16 pages, 2012.
View at: Publisher Site | Google Scholar
J. Mann, D. C. K. Chu, A. Maxwell et al., “MeCP2 controls an epigenetic pathway that promotes myofibroblast transdifferentiation and fibrosis,” Gastroenterology, vol. 138, no. 2, pp. 705.e4–714.e4, 2010.
View at: Publisher Site | Google Scholar
T. Shirasaki, M. Honda, T. Shimakami et al., “MicroRNA-27a regulates lipid metabolism and inhibits hepatitis C virus replication in human hepatoma cells,” Journal of Virology, vol. 87, no. 9, pp. 5270–5286, 2013.
View at: Publisher Site | Google Scholar
L. Q. Cao, X. L. Wang, Q. Wang et al., “Rosiglitazone sensitizes hepatocellular carcinoma cell lines to 5-fluorouracil antitumor activity through activation of the PPARgamma signaling pathway,” Acta Pharmacologica Sinica, vol. 30, no. 9, pp. 1316–1322, 2009.
View at: Google Scholar
J. Yu, B. Shen, E. S. H. Chu et al., “Inhibitory role of peroxisome proliferator-activated receptor gamma in hepatocarcinogenesis in mice and in vitro,” Hepatology, vol. 51, no. 6, pp. 2008–2019, 2010.
View at: Publisher Site | Google Scholar
K. L. Schaefer, K. Wada, H. Takahashi et al., “Peroxisome proliferator-activated receptor γ inhibition prevents adhesion to the extracellular matrix and induces anoikis in hepatocellular carcinoma cells,” Cancer Research, vol. 65, no. 6, pp. 2251–2259, 2005.
View at: Publisher Site | Google Scholar
K. Yoshizawa, D. P. Cioca, S. Kawa, E. Tanaka, and K. Kiyosawa, “Peroxisome proliferator-activated receptor γ ligand troglitazone induces cell cycle arrest and apoptosis of hepatocellular carcinoma cell lines,” Cancer, vol. 95, no. 10, pp. 2243–2251, 2002.
View at: Publisher Site | Google Scholar
A. Panza, C. Votino, A. Gentile et al., “Peroxisome proliferator-activated receptor γ-mediated induction of microRNA-145 opposes tumor phenotype in colorectal cancer,” Biochimica et Biophysica Acta—Molecular Cell Research, vol. 1843, no. 6, pp. 1225–1236, 2014.
View at: Publisher Site | Google Scholar
B.-C. Jeong, I.-H. Kang, and J.-T. Koh, “MicroRNA-302a inhibits adipogenesis by suppressing peroxisome proliferator-activated receptor γ expression,” FEBS Letters, vol. 588, no. 18, pp. 3427–3434, 2014.
View at: Publisher Site | Google Scholar
Q. Lin, Z. Gao, R. M. Alarcon, J. Ye, and Z. Yun, “A role of miR-27 in the regulation of adipogenesis,” FEBS Journal, vol. 276, no. 8, pp. 2348–2358, 2009.
View at: Publisher Site | Google Scholar
H. Li, T. Li, S. Wang et al., “MiR-17-5p and miR-106a are involved in the balance between osteogenic and adipogenic differentiation of adipose-derived mesenchymal stem cells,” Stem Cell Research, vol. 10, no. 3, pp. 313–324, 2013.
View at: Publisher Site | Google Scholar
M. Sun, X. Zhou, L. Chen et al., “The regulatory roles of microRNAs in bone remodeling and perspectives as biomarkers in osteoporosis,” BioMed Research International, vol. 2016, Article ID 1652417, 11 pages, 2016.
View at: Publisher Site | Google Scholar
C. S. Lutz and A. L. Cornett, “Regulation of genes in the arachidonic acid metabolic pathway by RNA processing and RNA-mediated mechanisms,” Wiley Interdisciplinary Reviews: RNA, vol. 4, no. 5, pp. 593–605, 2013.
View at: Publisher Site | Google Scholar
A. Croasdell, P. F. Duffney, N. Kim, S. H. Lacy, P. J. Sime, and R. P. Phipps, “PPARγ and the innate immune system mediate the resolution of inflammation,” PPAR Research, vol. 2015, Article ID 549691, 20 pages, 2015.
View at: Publisher Site | Google Scholar
B. Kang, K. K. Park, J. M. Kleinhenz et al., “Peroxisome proliferator–activated receptor γ and microRNA 98 in hypoxia-induced endothelin-1 signaling,” American Journal of Respiratory Cell and Molecular Biology, vol. 54, no. 1, pp. 136–146, 2016.
View at: Publisher Site | Google Scholar
D. E. Green, R. L. Sutliff, and C. M. Hart, “Is peroxisome proliferator-activated receptor gamma (PPARγ) a therapeutic target for the treatment of pulmonary hypertension?” Pulmonary Circulation, vol. 1, no. 1, pp. 33–47, 2011.
View at: Publisher Site | Google Scholar
T. Liu, H. Tang, Y. Lang, M. Liu, and X. Li, “MicroRNA-27a functions as an oncogene in gastric adenocarcinoma by targeting prohibitin,” Cancer Letters, vol. 273, no. 2, pp. 233–242, 2009.
View at: Publisher Site | Google Scholar
Y. Tsuchiya, M. Nakajima, S. Takagi, T. Taniya, and T. Yokoi, “MicroRNA regulates the expression of human cytochrome P450 1B1,” Cancer Research, vol. 66, no. 18, pp. 9090–9098, 2006.
View at: Publisher Site | Google Scholar
R. Zhou, X. Li, G. Hu, A.-Y. Gong, K. M. Drescher, and X.-M. Chen, “MiR-16 targets transcriptional corepressor SMRT and modulates NF-kappaB-regulated transactivation of interleukin-8 gene,” PLoS ONE, vol. 7, no. 1, Article ID e30772, 2012.
View at: Publisher Site | Google Scholar
L. Tombolan, M. Zampini, S. Casara et al., “MicroRNA-27a contributes to rhabdomyosarcoma cell proliferation by suppressing RARA and RXRA,” PLoS ONE, vol. 10, no. 4, Article ID e0125171, 2015.
View at: Publisher Site | Google Scholar
Y. Oda, M. Nakajima, K. Tsuneyama et al., “Retinoid X receptor α in human liver is regulated by miR-34a,” Biochemical Pharmacology, vol. 90, no. 2, pp. 179–187, 2014.
View at: Publisher Site | Google Scholar
M. J. Ochs, D. Steinhilber, and B. Suess, “MicroRNA involved in inflammation: control of eicosanoid pathway,” Frontiers in Pharmacology, vol. 2, article no. 39, 2011.
View at: Publisher Site | Google Scholar
S.-E. Choi and J. K. Kemper, “Regulation of SIRT1 by microRNAs,” Molecules and Cells, vol. 36, no. 5, pp. 385–392, 2013.
View at: Publisher Site | Google Scholar
B. M. Alrfaei, R. Vemuganti, and J. S. Kuo, “microRNA-100 targets SMRT/NCOR2, reduces proliferation, and improves survival in glioblastoma animal models,” PLoS ONE, vol. 8, no. 11, Article ID e80865, 2013.
View at: Publisher Site | Google Scholar
D. Guérit, D. Philipot, P. Chuchana et al., “Sox9-regulated miRNA-574-3p inhibits chondrogenic differentiation of mesenchymal stem cells,” PLoS ONE, vol. 8, no. 4, Article ID e62582, 2013.
View at: Publisher Site | Google Scholar
Y. K. Adlakha, S. Khanna, R. Singh, V. P. Singh, A. Agrawal, and N. Saini, “Pro-apoptotic miRNA-128-2 modulates ABCA1, ABCG1 and RXRα expression and cholesterol homeostasis,” Cell Death & Disease, vol. 4, article e780, 2013.
View at: Google Scholar
P. Seale, B. Bjork, W. Yang et al., “PRDM16 controls a brown fat/skeletal muscle switch,” Nature, vol. 454, no. 7207, pp. 961–967, 2008.
View at: Publisher Site | Google Scholar
H. Yin, A. Pasut, V. D. Soleimani et al., “MicroRNA-133 controls brown adipose determination in skeletal muscle satellite cells by targeting Prdm16,” Cell Metabolism, vol. 17, no. 2, pp. 210–224, 2013.
View at: Publisher Site | Google Scholar
M. Trajkovski, K. Ahmed, C. C. Esau, and M. Stoffel, “MyomiR-133 regulates brown fat differentiation through Prdm16,” Nature Cell Biology, vol. 14, no. 12, pp. 1330–1335, 2012.
View at: Publisher Site | Google Scholar
R. B. Vega, J. M. Huss, and D. P. Kelly, “The coactivator PGC-1 cooperates with peroxisome proliferator-activated receptor α in transcriptional control of nuclear genes encoding mitochondrial fatty acid oxidation enzymes,” Molecular and Cellular Biology, vol. 20, no. 5, pp. 1868–1876, 2000.
View at: Publisher Site | Google Scholar
Z. Fang, P. Li, W. Jia, T. Jiang, Z. Wang, and Y. Xiang, “miR-696 plays a role in hepatic gluconeogenesis in ob/ob mice by targeting PGC-1α,” International Journal of Molecular Medicine, vol. 38, no. 3, pp. 845–852, 2016.
View at: Publisher Site | Google Scholar
J.-Y. Huang, S.-F. Chou, J.-W. Lee et al., “MicroRNA-130a can inhibit hepatitis B virus replication via targeting PGC1α and PPARγ,” RNA, vol. 21, no. 3, pp. 385–400, 2015.
View at: Publisher Site | Google Scholar
C. Cantó and J. Auwerx, “Targeting sirtuin 1 to improve metabolism: all you need is NAD⁺?” Pharmacological Reviews, vol. 64, no. 1, pp. 166–187, 2012.
View at: Publisher Site | Google Scholar
H. Yin, M. Hu, R. Zhang, Z. Shen, L. Flatow, and M. You, “MicroRNA-217 promotes ethanol-induced fat accumulation in hepatocytes by down-regulating SIRT1,” Journal of Biological Chemistry, vol. 287, no. 13, pp. 9817–9826, 2012.
View at: Publisher Site | Google Scholar
B. Zhou, C. Li, W. Qi et al., “Downregulation of miR-181a upregulates sirtuin-1 (SIRT1) and improves hepatic insulin sensitivity,” Diabetologia, vol. 55, no. 7, pp. 2032–2043, 2012.
View at: Publisher Site | Google Scholar
C. L. Kurtz, E. E. Fannin, C. L. Toth, D. S. Pearson, K. C. Vickers, and P. Sethupathy, “Inhibition of miR-29 has a significant lipid-lowering benefit through suppression of lipogenic programs in liver,” Scientific Reports, vol. 5, Article ID 12911, 2015.
View at: Publisher Site | Google Scholar
X.-F. Tian, F.-J. Ji, H.-L. Zang, and H. Cao, “Activation of the miR-34a/SIRT1/p53 signaling pathway contributes to the progress of liver fibrosis via inducing apoptosis in hepatocytes but not in HSCs,” PLoS ONE, vol. 11, no. 7, Article ID e0158657, 2016.
View at: Publisher Site | Google Scholar
F. Zhang, J. Cui, X. Liu et al., “Roles of microRNA-34a targeting SIRT1 in mesenchymal stem cells,” Stem Cell Research and Therapy, vol. 6, no. 1, article 195, 2015.
View at: Publisher Site | Google Scholar
A. L. McCubbrey, J. D. Nelson, V. R. Stolberg et al., “MicroRNA-34a negatively regulates efferocytosis by tissue macrophages in part via SIRT1,” Journal of Immunology, vol. 196, no. 3, pp. 1366–1375, 2016.
View at: Publisher Site | Google Scholar
K. Duan, Y.-C. Ge, X.-P. Zhang et al., “miR-34a inhibits cell proliferation in prostate cancer by downregulation of SIRT1 expression,” Oncology Letters, vol. 10, no. 5, pp. 3223–3227, 2015.
View at: Publisher Site | Google Scholar
X. Liu, X. Chen, X. Yu et al., “Regulation of microRNAs by epigenetics and their interplay involved in cancer,” Journal of Experimental and Clinical Cancer Research, vol. 32, no. 1, article 96, 2013.
View at: Publisher Site | Google Scholar
S. Luo, J. Wang, Y. Ma, Z. Yao, and H. Pan, “PPARγ inhibits ovarian cancer cells proliferation through upregulation of miR-125b,” Biochemical and Biophysical Research Communications, vol. 462, no. 2, pp. 85–90, 2015.
View at: Publisher Site | Google Scholar
H.-Y. Zhu, C. Li, Z. Zheng et al., “Peroxisome proliferator-activated receptor-γ (PPAR-γ) agonist inhibits collagen synthesis in human hypertrophic scar fibroblasts by targeting Smad3 via miR-145,” Biochemical and Biophysical Research Communications, vol. 459, no. 1, pp. 49–53, 2015.
View at: Publisher Site | Google Scholar
Y. Zhang, Z. Yang, R. Whitby, and L. Wang, “Regulation of miR-200c by nuclear receptors PPARα, LRH-1 and SHP,” Biochemical and Biophysical Research Communications, vol. 416, no. 1-2, pp. 135–139, 2011.
View at: Publisher Site | Google Scholar
W. Ying, A. Tseng, R. C.-A. Chang et al., “MicroRNA-223 is a crucial mediator of PPARγ-regulated alternative macrophage activation,” Journal of Clinical Investigation, vol. 125, no. 11, pp. 4149–4159, 2015.
View at: Publisher Site | Google Scholar
J. Yu, X. Kong, J. Liu et al., “Expression profiling of PPARγ-regulated MicroRNAs in human subcutaneous and visceral adipogenesis in both genders,” Endocrinology, vol. 155, no. 6, pp. 2155–2165, 2014.
View at: Publisher Site | Google Scholar
C.-M. Wong, L. Wei, S. L.-K. Au et al., “MiR-200b/200c/429 subfamily negatively regulates Rho/ ROCK signaling pathway to suppress hepatocellular carcinoma metastasis,” Oncotarget, vol. 6, no. 15, pp. 13658–13670, 2015.
View at: Publisher Site | Google Scholar
X. Fang, L. Fang, A. Liu, X. Wang, B. Zhao, and N. Wang, “Activation of PPAR-δ induces microRNA-100 and decreases the uptake of very low-density lipoprotein in endothelial cells,” British Journal of Pharmacology, vol. 172, no. 15, pp. 3728–3736, 2015.
View at: Publisher Site | Google Scholar
S.-Y. Liu, Y.-Y. Zhang, Y. Gao et al., “MiR-378 plays an important role in the differentiation of bovine preadipocytes,” Cellular Physiology and Biochemistry, vol. 36, no. 4, pp. 1552–1562, 2015.
View at: Publisher Site | Google Scholar
E. John, A. Wienecke-Baldacchino, M. Liivrand, M. Heinäniemi, C. Carlberg, and L. Sinkkonen, “Dataset integration identifies transcriptional regulation of microRNA genes by PPARγ in differentiating mouse 3T3-L1 adipocytes,” Nucleic Acids Research, vol. 40, no. 10, pp. 4446–4460, 2012.
View at: Publisher Site | Google Scholar
K. Song, C. Han, J. Zhang et al., “Epigenetic regulation of microRNA-122 by peroxisome proliferator activated receptor-gamma and hepatitis b virus X protein in hepatocellular carcinoma cells,” Hepatology, vol. 58, no. 5, pp. 1681–1692, 2013.
View at: Publisher Site | Google Scholar
L. G. Tillman, R. S. Geary, and G. E. Hardee, “Oral delivery of antisense oligonucleotides in man,” Journal of Pharmaceutical Sciences, vol. 97, no. 1, pp. 225–236, 2008.
View at: Publisher Site | Google Scholar
S. Mitragotri, P. A. Burke, and R. Langer, “Overcoming the challenges in administering biopharmaceuticals: formulation and delivery strategies,” Nature Reviews Drug Discovery, vol. 13, no. 9, pp. 655–672, 2014.
View at: Publisher Site | Google Scholar
X. Wang, B. Yu, W. Ren et al., “Enhanced hepatic delivery of siRNA and microRNA using oleic acid based lipid nanoparticle formulations,” Journal of Controlled Release, vol. 172, no. 3, pp. 690–698, 2013.
View at: Publisher Site | Google Scholar
C. J. Cheng, W. M. Saltzman, and J. F. Slack, “Canonical and non-canonical barriers facing antimiR cancer therapeutics,” Current Medicinal Chemistry, vol. 20, no. 29, pp. 3582–3593, 2013.
View at: Publisher Site | Google Scholar
S. Pan, X. Yang, Y. Jia, R. Li, and R. Zhao, “Microvesicle-shuttled miR-130b reduces fat deposition in recipient primary cultured porcine adipocytes by inhibiting PPAR-γ expression,” Journal of Cellular Physiology, vol. 229, no. 5, pp. 631–639, 2014.
View at: Publisher Site | Google Scholar
S. Pan, X. Yang, Y. Jia et al., “Intravenous injection of microvesicle-delivery miR-130b alleviates high-fat diet-induced obesity in C57BL/6 mice through translational repression of PPAR-γ,” Journal of Biomedical Science, vol. 22, article 86, 2015.
View at: Publisher Site | Google Scholar
F. Olivieri, M. R. Rippo, F. Prattichizzo et al., “Toll like receptor signaling in “inflammaging”: microRNA as new players,” Immunity and Ageing, vol. 10, article no. 11, 2013.
View at: Publisher Site | Google Scholar
R. E. Lanford, E. S. Hildebrandt-Eriksen, A. Petri et al., “Therapeutic silencing of microRNA-122 in primates with chronic hepatitis C virus infection,” Science, vol. 327, no. 5962, pp. 198–201, 2010.
View at: Publisher Site | Google Scholar
S. Ottosen, T. B. Parsley, L. Yang et al., “In vitro antiviral activity and preclinical and clinical resistance profile of miravirsen, a novel anti-hepatitis C virus therapeutic targeting the human factor miR-122,” Antimicrobial Agents and Chemotherapy, vol. 59, no. 1, pp. 599–608, 2015.
View at: Publisher Site | Google Scholar
J. Stenvang, A. Petri, M. Lindow, S. Obad, and S. Kauppinen, “Inhibition of microRNA function by antimiR oligonucleotides,” Silence, vol. 3, no. 1, article 1, 2012.
View at: Publisher Site | Google Scholar
K. J. Rayner, C. C. Esau, F. N. Hussain et al., “Inhibition of miR-33a/b in non-human primates raises plasma HDL and lowers VLDL triglycerides,” Nature, vol. 478, no. 7369, pp. 404–407, 2011.
View at: Publisher Site | Google Scholar
H. Wu, R. Ng, X. Chen, C. J. Steer, and G. Song, “MicroRNA-21 is a potential link between non-alcoholic fatty liver disease and hepatocellular carcinoma via modulation of the HBP1-p53-Srebp1c pathway,” Gut, vol. 65, no. 11, pp. 1850–1860, 2015.
View at: Publisher Site | Google Scholar
M. Agostini and R. A. Knight, “miR-34: from bench to bedside,” Oncotarget, vol. 5, no. 4, pp. 872–881, 2014.
View at: Publisher Site | Google Scholar
L. E. Young, A. E. Moore, L. Sokol, N. Meisner-Kober, and D. A. Dixon, “The mRNA stability factor HuR inhibits MicroRNA-16 targeting of COX-2,” Molecular Cancer Research, vol. 10, no. 1, pp. 167–180, 2012.
View at: Publisher Site | Google Scholar
S. Geisler and J. Coller, “RNA in unexpected places: long non-coding RNA functions in diverse cellular contexts,” Nature Reviews Molecular Cell Biology, vol. 14, no. 11, pp. 699–712, 2013.
View at: Publisher Site | Google Scholar

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