Next Article in Journal
Combining Targeted Metabolites Analysis and Transcriptomics to Reveal Chemical Composition Difference and Underlying Transcriptional Regulation in Maca (Lepidium Meyenii Walp.) Ecotypes
Previous Article in Journal
MicroRNA-106a-5p Inhibited C2C12 Myogenesis via Targeting PIK3R1 and Modulating the PI3K/AKT Signaling
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Genes
Volume 9
Issue 7
10.3390/genes9070334
genes-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

Functional Analysis of Promoters of Genes in Lipid Metabolism and Their Transcriptional Response to STAT3 under Leptin Signals

by
Kun Wu
1,
Xiao-Ying Tan
1,2,*,
Yi-Huan Xu
1,
Guang-Hui Chen
1 and
Mei-Qin Zhuo
1
1
Laboratory of Molecular Nutrition, Fishery College, Huazhong Agricultural University, Wuhan 430070, China
2
Collaborative Innovation Center for Efficient and Health Production of Fisheries in Hunan Province, Changde 415000, China
*
Author to whom correspondence should be addressed.
Genes 2018, 9(7), 334; https://doi.org/10.3390/genes9070334
Submission received: 9 May 2018 / Revised: 23 June 2018 / Accepted: 28 June 2018 / Published: 3 July 2018
(This article belongs to the Section Animal Genetics and Genomics)
Browse Figures
Versions Notes

Abstract

:
We characterized the promoters of target genes of the signal transducer and activator of transcription 3, STAT3 (carnitine palmitoyltransferase I, CPT Iα1b, acetyl-CoA carboxylase alpha, ACCα; fatty acid synthase, FAS; and peroxisome proliferator-activated receptor gamma, PPARγ) in a teleost Pelteobagrus fulvidraco. Binding sites of STAT3 were predicted on these promoters, indicating that STAT3 probably mediated their transcriptional activities. Leptin had no effect on the activity of ACCα and PPARγ promoters, but increased CPT Iα1b promoter activity and decreased FAS promoter activity. The −979/−997 STAT3 binding site of CPT Iα1b and the −794/−812 STAT3 binding site of FAS were functional binding loci responsible for leptin-induced transcriptional activation. The study provided direct evidence that STAT3 regulated the expression of CPT Iα1b and FAS at the transcription level, and determined the STAT3 response element on promoters of CPT Iα1b and FAS under leptin signal.

1. Introduction

Lipids are essential nutrients, and provide energy sources and essential fatty acids, which play important roles in numerous physiological and metabolic processes [1]. Excessive fat accumulation and disordered lipid metabolism have become serious problems in the sustainable and healthy development of aquaculture. In general, lipid homeostasis is characterized by the balance between lipogenesis and lipolysis. During lipogenesis and lipolysis, some crucial genes, transcriptional factors and enzymes are involved in these processes. Carnitine palmitoyltransferase I (CPT I) catalyzes the conversion of fatty acid-coenzyme A (fatty acid-CoA) into fatty acid-carnitines and is one of the limiting enzymes in fatty acid β-oxidation [2]. Both acetyl-CoA carboxylase alpha (ACCα) and fatty acid synthase (FAS) catalyze the committed steps in fatty acids’ biosynthesis [3,4]. Peroxisome proliferator-activated receptor gamma (PPARγ) is an important nuclear transcription factor that modulates the expression of many target genes relevant to lipid metabolism [5]. Many studies have been conducted to explore lipid metabolism [6]. However, information relevant to the modulatory mechanism of lipid metabolism at a transcriptional level is very scarce in fish. Thus, lipid metabolism-related factors and regulatory mechanisms in fish have attracted increasing attention.
Leptin is a member of the cytokines with the class-I alpha helix [7]. To date, many studies have been undertaken to explore the physiological roles of leptin, mainly focusing on the effects of leptin on food intake and energy homeostasis [7,8], but information about its molecular mechanism is still limited in teleosts [9,10]. Our previous studies have shown that leptin downregulated lipogenesis and upregulated lipolysis in yellow catfish by regulating the mRNA expression of the key lipid metabolism-related target genes, such as CPT I, ACCα, FAS, and PPARγ [11,12]. During these processes, signal transducers and activators of transcription protein 3 (STAT3) is one member of the Janus kinases (JAK)/STAT pathway and is considered the most important factor that transmits the leptin signal [12,13]. The activated STAT3 is capable of translocating to the nucleus to alter gene transcription [14]. Recently, using the specific JAK2/STAT3 inhibitor AG490, the effects of leptin on lipid metabolism were studied in grass carp [15], yellow catfish [11,12], and Synechogobius hasta [16]. These studies offered indirect evidence about the relationship between STAT3 and the regulatory role of leptin in genes involved in lipid metabolism. In fact, transcription initiation controls the expression of genes in eukaryotic organisms. Promoters contain cis-acting sequences and are bound by many transcriptional factors. Promoters control gene expression at the transcriptional level. Thus, as the first step in deciphering the mechanism of leptin-regulating target genes relevant to lipid metabolism, it is crucial to analyze the promoters’ structure and the function of downstream target genes. At present, studies on the promoters of lipid metabolism-related genes are scarce in fish. Recently, in our laboratory, Xu et al. [17] analyzed the structure and function of CPT I promoter in grass carp, but no studies have been reported for the promoter structure and function of ACCα, FAS, and PPARγ in teleosts.
Yellow catfish (Pelteobagrus fulvidraco) are omnivorous freshwater fish commonly farmed in some Asian countries for the delicious meat and high market value. The yellow catfish is considered a potential model fish for exploring the regulatory mechanism of lipid metabolism because it possesses high lipid contents in several tissues, such as the visceral tissues, liver, and muscles [18]. The present study was conducted to identify the promoter regions of CPT Iα1b, ACCα, FAS, and PPARγ in yellow catfish, and investigated the STAT3 binding sites of their promoter regions. Our study offers innovative insights into the mechanism of leptin regulating lipid metabolism and provides direct evidence on the interaction between STAT3 and downstream genes in fish.

2. Materials and Methods

2.1. Animals and Reagents

Juvenile yellow catfish were purchased from a commercial farm (Wuhan, China) and used for promoter cloning. HepG2 cell lines were from the Cell Resource Center of our college. Dulbecco’s Modified Eagle’s medium (DMEM), 0.25% trypsin-EDTA, and fetal bovine serum (FBS) were purchased from Gibco (ThermoFisher Scientific, Waltham, MA, USA). Recombinant human leptin (HPLC class) and other reagents were from Sigma–Aldrich (St. Louis, MA, USA). The Ethics Committee of Huazhong Agricultural University (HZAU) checked and approved our present experimental protocols on animals and cells (identification code: Fish-2016-0420, Date: 19 April 2016).

2.2. Promoter Cloning and Plasmid Construction

Based on our previous studies [5,19,20], we identified the 5′ cDNA sequences and the transcription start sites (TSS) of ACCα (GenBank number MH253822), CPT1α1b (GenBank number JQ074176), FAS (GenBank number MH253823) and PPARγ (GenBank number KF614118) of yellow catfish. The protocols of promoter cloning followed the method described in Xu et al. [17]. Briefly, genomic DNA was extracted from yellow catfish tail fins using a commercial kit (Omega, Norcross, GA, USA). In order to determine the position of the first intron of ACCα, CPT1α1b, FAS, and PPARγ, we designed various primers (shown in Table S1). The hiTAIL-PCR (high-efficiency thermal asymmetric interlaced-PCR) method [21] was used to clone the promoter sequences, and the specific primers with overlapping sequence are listed in Table S1. In order to produce the luciferase reporter constructs, we purified the PCR product and pGl3-Basic vectors (Promega, Fitchburg, WI, USA), and then digested them using endonucleases. Then we used ClonExpress II One Step Cloning Kit (Vazyme, Piscataway, NJ, USA) to ligate the products. Based on the distance from its TSS, we named the plasmids pGl3-2234/+51 of ACCα vector, pGl3-2155/+24 of CPT1α1b vector, pGl3-1960/+39 of FAS vector, and pGl3-2033/+63 of PPARγ vector, respectively. With the Erase-a-Base system (Promega) using templates of pGl3-2234/+51 of ACCα vector, we generated plasmids pGl3-402/+51, pGl3-793/+51, pGl3-1154/+51, pGl3-1518/+51, and pGl3-1914/+51 of ACCα vector. Similarly, using pGl3-2155/+24 of CPT1α1b vector as a template, we generated pGl3-387/+24, pGl3-726/+24, pGl3-1120/+24, pGl3-1480/+24, and pGl3-1709/+24; using pGl3-1960/+39 of FAS vector as a template, we generated the plasmids pGl3-326/+39, pGl3-746/+39, pGl3-1152/+39, pGl3-1380/+39, and pGl3-1525/+39; using template pGl3-2033/+63, we generated the plasmids pGl3-439/+63, pGl3-671/+63, pGl3-784/+63, pGl3-1241/+63, and pGl3-1575/+63, respectively. The primer sequences for plasmid construction are shown in Table S2.

2.3. Sequence Analysis

In order to analyze the promoter regions of ACCα, CPT1α1b, FAS, and PPARγ genes, we predicted the putative transcription factor binding sites (TFBS) using MatInspector online (http://www.genomatix.de/) and the JASPAR database (http://jaspar.genereg.net/). The reference binding site sequences are listed in Table S3. The Clustal-W multiple alignment algorithm was used to assess the sequence alignments.

2.4. Plasmid Transfections and Activities Assays of Luciferase

Plasmid transfections into HepG2 cells and activities assays of luciferase followed the methods described in our recent publication [17]. Briefly, HepG2 cells were cultured in DMEM medium + 10% FBS in an incubator with 5% CO2 at 37 °C. Plasmids were transiently transfected into HepG2 using Lipofectamine 2000 (Invitrogen, Carlsbad, CA, USA). The reporter plasmids were co-transfected with 35 ng pRL-TK as a control. After 4 h, DMEM (10% FBS) or DMEM (10% FBS) + 200 ng/mL leptin was used to replace the transfection medium. We chose the leptin concentration based on our publications [11,12,16]. Then, at the end of the 24-h incubation, we used the Dual-Luciferase Reporter Assay System to measure the relative luciferase activity, and the analytical protocols followed the manufacture’s manuals.

2.5. Site-Mutation Assays of STAT3 Binding Sites on the Promoter Regions of ACCα, CPT1α1b, FAS, and PPARγ

To identify the STAT3 binding sites on the promoter regions of ACCα, CPT1α1b, FAS, and PPARγ in yellow catfish, we used QuickChange II Site-Directed Mutagenesis Kit (Vazyme) to conduct site-directed mutagenesis. pGl3-ACCα-2234, pGl3-CPT1α1b-2151, pGl3-FAS-1960, and pGl3-PPARγ-2033 were used as the templates. The primers for mutagenesis are shown in Table S4. The constructs were named CMut-STAT3-1, CMut-STAT3-2, FMut-STAT3-1, FMut-STAT3-2, and FMut-STAT3-3, respectively. Then, we used Lipofectamine 2000 (Invitrogen) to co-transfect the pRL-TK and constructs into HepG2 cells. After 4-h transfection, we used DMEM (10% FBS) or DMEM (10% FBS) + 200 ng/mL leptin to replace the transfection medium. After a 24-h incubation, we harvested cells and the luciferase activity was determined based on the procedure mentioned above.

2.6. Electrophoretic Mobility-Shift Assay (EMSA) for Determining the Functional Binding Sites of STATs on the Promoter Regions

Proteins for electrophoretic mobility-shift sssay (EMSA) were extracted from HepG2 cells. EMSA assays were conducted to determine the functional binding sites of STAT3 on the promoter regions of ACCα, CPT1α1b, FAS, and PPARγ, based on the methods described by Xu et al. [17]. Cytoplasmic and nuclear extracts were obtained following the protocols of Read et al. [22]. Protein contents were determined following the bicinchoninic acid assay (BCA) method [23]. Each oligonucleotide duplex of STAT3 binding sites was incubated with 10 μg nuclear extracts according to LightShift Chemiluminescent EMSA Kit (Invitrogen), and each unlabeled probe was pre-incubated for 10 min prior to the addition of biotin-labeled probe. The reaction was allowed to proceed for 30 min after the addition of biotin-labeled probe at room temperature, and then they were detected by electrophoresis on 6% native polyacrylamide gels. Competition analyses were performed by using 100-fold excess of unlabeled oligonucleotide duplex with or without the mutation. These oligonucleotide sequences for EMSA were shown in Table S5.

2.7. Statistical Analysis

Results were presented as mean ± SEM (standard error of mean). Before analysis, we used the Kolmogornov–Smirnov test to determine the normality of distribution of all data. The Student’s t-test was used to compare the differences between the wild type (WT) and drug-treated group. Significance levels were set to p < 0.05. We used SPSS 19.0 software (SPSS, Chicago, IL, USA) to conduct the statistical analyses.

3. Results

3.1. Cloning and Sequence Analysis of the Promoter Regions of ACCα, CPT Iα1b, FAS, and PPARγ

In the present study, 2249 bp of ACCα promoter (GenBank accession No. MH253818), 2231 bp of CPT1α1b promoter (GenBank accession No. MH253819), 2022 bp of FAS promoter (GenBank accession No. MH253820), and 2171 bp of PPARγ promoter (GenBank accession No. MH253821) were cloned (Figure S1). The first nucleotide of 5′ cDNA of ACCα, CPT Iα1b, FAS and PPARγ was designated as +1. On the ACCα promoter region, we predicted several core promoter elements, such as a TATA-box (TBP) located from −24 bp to −40 bp and two CCAAT-boxes (nuclear transcription factor Y, NF-Y) located at −50 bp to −64 bp and −91 bp to −105 bp (Figure S2). We also predicted a cluster of binding sites of several transcription factors on the promoter region of ACCα gene, including HNF4α, STAT3, SREBP1, and PPARγ (Figure S2). On the core promoter of CPT1α1b, two GC-boxes (Sp1) were identified and there were two STAT3 binding sites located from −802 bp to −812 bp and from −979 bp to −997 bp (Figure S3). On the region of FAS promoter, we also discovered three STAT3 binding sites, which were located at the positions from –794 bp to −812 bp, −1571 bp to −1584 bp, and −1831 bp to −1845 bp, respectively. In addition, the binding sites of SREBP1 and PPARγ were also predicted (Figure S4). The binding sites of transcription factors such as STAT3, STAT5, CREB, and HNF4α were predicted on the region of PPARγ promoter (Figure S5).

3.2. 5′-Deletion Assay of the Promoter Regions of ACCα, CPT Iα1b, FAS, and PPARγ

According to the Erase-a-Base kit (Promega), we randomly generated plasmids of different size and selected six appropriate plasmids for each promoter to perform the deletion assay. The relative luciferase activity of the promoter of ACCα significantly increased when the sequence from −1518 bp to −1914 bp of ACCα promoter was absent. Subsequent absence to −1154 bp significantly reduced the relative luciferase activity (Figure 1A).
For the CPT Iα1b promoter, the sequence deletion from −2155 bp to −1480 bp showed no significant effects on luciferase activity, but the deletion from −1480 bp to −1120 bp reduced the luciferase activity (Figure 1B).
For the FAS promoter, the position deletion from −1960 bp to −1525 bp and −1152 bp to −746 bp upregulated the relative luciferase activity significantly (Figure 1C). In contrast, the position deletion from −1525 bp to −1380 bp and −746 bp to −326 bp downregulated the relative luciferase activity significantly.
For PPARγ promoter, the sequence deletion between −2033 bp and −1575 bp increased the relative luciferase activity significantly. In contrast, the deletion between −1241 and −784 bp reduced the relative luciferase activity significantly (Figure 1D).
To investigate the response of promoters induced by leptin, we further used 200 ng/mL leptin to incubate HepG2 for 24 h and performed the 5′ deletion assay; the results are presented in Figure 2A. Compared with the control, leptin incubation did not significantly influence the relative luciferase activity of ACCα. No significant differences in relative luciferase activity were found between different deletion plasmid groups. In the leptin-treated group, the sequence deletion between −2155 bp and −1120 bp of CPT Iα1b promoter showed no significant influences on luciferase activity; however, further deletion to −726 bp downregulated the relative luciferase activity significantly. Meanwhile, the relative luciferase activity of the promoter region between −2155 bp and −1120 bp was significantly higher than that in the control (Figure 2B). Under leptin incubation, the region deletions between −1960 bp and −1525 bp, and −1380 to −1152 bp of FAS promoter significantly increased the relative luciferase activity. Leptin significantly decreased the luciferase activities of pGl3-1960/+39 and pGl3-1380/+39 (Figure 2C). Neither differences between different deletion plasmids nor differences between the control and the leptin-treated group were found in a deletion assay of PPARγ promoters (Figure 2D).

3.3. Site-Mutation Analysis of STAT3 Binding Sites on the Promoter Regions of CPT1α1b and FAS

Based on the results of 5′-deletion assay, we performed the site mutation in the regions of CPT Iα1b and FAS promoters that may possess STAT3 binding sites. The mutation of the −802/−812 STAT3 binding site (CMut-STAT3-2) did not change the leptin-induced elevation of luciferase activity, suggesting that this site played no role in the CPT Iα1b transcriptional response to leptin. The mutation of the −984/−994 STAT3 binding site (CMut-STAT3-1) downregulated the leptin-induced relative luciferase activity significantly. Similarly, the co-mutation of −984/−994 plus −802/−812 STAT3 binding sites (CMut-STAT3-12) also decreased the leptin-induced increase of luciferase activity, indicating that the −984/−994 STAT3 binding site positively mediated CPT Iα1b transcription (Figure 3A). For the FAS promoter, compared with the pGl3-1960/+39 vector (WT), the mutation of the −798/−808 STAT3 binding site (FMut-STAT3-3) significantly increased the relative luciferase activity, but the mutation of −1832/−1842 STAT3 binding site (FMut-STAT3-1) or −1572/−1582 STAT3 binding site (FMut-STAT3-2) did not significantly affect the relative luciferase activity in the leptin group. In contrast with the WT pGl3-1960/+39 FAS vector, the co-mutation of −798/−808 plus −1832/−1842 (FMut-STAT3-13), −798/−808 plus −1572/−1582 (FMut-STAT3-23) and −798/−808 plus −1832/−1842 plus −1572/−1582 (FMut-STAT3-123) STAT3 binding sites suppressed the leptin-induced decrease of luciferase activity (Figure 3B). The result reflected that the −1832/−1842 and −1572/−1582 binding sites could not regulate the transcription of FAS after leptin stimulation, and the −798/−808 STAT3 binding site negatively mediated the regulation of FAS transcription.

3.4. EMSA of Each STAT3 Binding Sequence

Based on the results of the mutation assays above, we speculated that STAT3 could bind with the sequence from −979 bp to −997 bp of CPT Iα1b promoter and from −794 bp to −812 bp of FAS promoter. Therefore, we next used EMSA assay to measure their ability to physically interact with STAT3. When STAT3 binding sequence was used as the probe, the 100-fold unlabeled STAT3 binding sites (between −979 bp and −997 bp of CPT Iα1b promoter) competed for binding; in contrast, the 100-fold unlabeled Mut-STAT3 binding sites declined this competition significantly, indicating that this region could be bound by STAT3. Meanwhile, the increased brightness of bands under leptin treatment reflected that leptin promoted the binding process between STAT3 and this binding position on CPT Iα1b promoter (Figure 4A). Similarly, when the STAT3 binding sequence was used as the probe, the 100-fold unlabeled STAT3 binding site (between −794 bp and −812 bp of FAS promoter) competed for binding; in contrast, the 100-fold unlabeled Mut-STAT3 binding region downregulated this competition significantly, suggesting that this region could be bound by STAT3. In addition, compared with the corresponding bands in the non-leptin group, leptin reduced the brightness of bands, indicating that leptin mediated the transcriptional regulation of FAS by STAT3 (Figure 4B).

4. Discussion

Previous studies indicated that STAT3 played important roles in leptin-induced change of mRNA levels of lipid metabolism-related genes [11,12,16], but direct evidence of a link between STAT3 and lipid metabolism was not sought. The present study focused on several key genes (ACCα, CPT Iα1b, FAS, and PPARγ) that were regulated by leptin.
In our current study, one TATA-box and two CAAT-boxes were found in the core ACCα promoter region in yellow catfish. The TATA-box was commonly sited 25 bp upstream from the TSS and helps to identify the transcriptional initiation. In contrast, in humans, Mao et al. [24] reported that the ACCα core promoter regions possessed multiple Sp1 binding sites instead of the TATA-box or CAAT-box. The differences in core promoters between fish and humans reflect the complexity and diversity of transcriptional modulation among different species. In yellow catfish, the upstream of CPT Iα1b TSS contains neither a TATA box nor a CAAT box. Instead, we found Sp1 binding sites in the core promoter region. Studies suggested that TATA-less promoters usually possessed various Sp1 binding sites in their promoter regions [25]. Steffen et al. [26] also suggested that Sp1 could drive the basal expression of CPT Iα in the rat. Interestingly, CPT Iα1b core promoter of grass carp possesses a classical TATA-box, whereas in the promoter of CPT Iα2a, another isoform of CPT Iα, Sp1, and NF-Y replaces the TATA-box [17]. Thus, it is plausible that transcription initiation of various isoforms of CPT Iα gene presents diverse mechanisms. The core promoter region of yellow catfish FAS contains a classic TATA-box and CAAT-boxes. In contrast, in mammals, Amy et al. [27] reported that the transcription initiation of mammal FAS started with multiple Sp1. The present study indicated that yellow catfish had only one PPARγ promoter with the transcription initiation of classic TATA-box and CAAT-box. In the mouse, different splicing yielded two PPARγ promoters and both of the two isoforms contained a putative TATA-box [28]. In general, although the function of the same gene is similar between fish and mammals, the basic elements and pathways of transcription initiation of core promoters are not always conserved.
Our current study showed that the ACCα promoter of yellow catfish contained a SREBP1 binding site at −344/−353 bp and a PPARγ binding site at −366/−388 bp. Similarly, Mao et al. [24] reported that two SREBP binding sites were located about 230 bp upstream from the TSS in the human ACCα promoter regions. Moreover, the promoter regions at −402/+51 bp of ACCα positively modulated their promoter activities, suggesting that SREBP1 and PPARγ were potential positive regulators for the activity of ACCα promoter. SREBP1 and PPARγ are critical transcriptional factors for modulating lipogenesis [29], and they positively regulated ACCα mRNA expression [30,31]. On the yellow catfish CPT Iα1b promoter, we found a cluster of TFBS, such as HNF4α (−395/−419 bp) and PPARα (−348/−370 bp), in agreement with the structure of grass carp CPT Iα promoter [17]. Our study found that the sequence deletion from −387 bp to +24 bp significantly reduced the CPT Iα1b promoter activity. Considering that PPARα and HNF4α play important roles in regulating CPT I expression [32], PPARα and HNF4α may positively regulate CPT Iα1b promoter activity by combining the binding sites from −387 bp to +24 bp. The SREBP1 and PPAR family are now well established as key transcription factors for the positive regulation of FAS expression [33,34,35]. In the present study, we found several binding sites of SREBP1 and PPARγ on the FAS promoter. Furthermore, deletion of the regions for these binding sites significantly decreased the promoter activity. In addition, we found multiple STAT3 binding sites on the FAS promoter and the deletion analysis suggested that STAT3 was a potential negative regulator of FAS promoter activity; the PPARγ promoter of yellow catfish contained a CREB binding site at −1943/−1963 bp. Herzig et al. [36] pointed out that CREB was able to inhibit hepatic PPARγ expression. Our result showed that deletion of the region where CREB binding sites were located (−1575/−2033 bp) increased the PPARγ promoter activity, which further supports the regulatory role of CREB on PPARγ expression at the transcriptional level.
Recently, studies in our laboratory demonstrated the importance of STAT3 in regulating genes expression under leptin action [11,12,16]. However, information is scarce on the promoters of downstream target genes in fish, which precludes further speculation. Here, we analyzed the change of promoter activity using leptin incubation. Compared with the control, after deleting partial sequences of the ACCα and PPARγ promoters, the activity of promoters of ACCα and PPARγ remained relatively constant after leptin incubation. However, our previous studies indicated that leptin downregulated the expression of ACCα and PPARγ [11,12,16]. The apparent differences might be attributable to binding sites being located outside of the region we cloned. Compared with the control, leptin significantly increased the activity of CPT Iα1b promoter from −726 bp to −2155 bp, indicating that leptin promoted CPT Iα1b transcription, in agreement with previous studies in grass carp [15] and yellow catfish [11,12,16]. Studies suggested that leptin stimulated fatty acid oxidation [37,38]. CPT I is a rate-limiting enzyme for fatty acid β-oxidation. Taken together, initiating the CPT I transcription is the first and most important step by which leptin activates fatty acid oxidation. In addition, in the leptin-treated group, deletion of the sequence from −1120 bp to −726 bp of CPT Iα1b promoter significantly reduced the relative luciferase activity, indicating that the binding site that regulates CPT Iα1b transcription may fall in this region. For FAS, we found that leptin inhibited its promoter activity. FAS mediates the regulation of fatty acid biosynthesis [4]. Song et al. [11] indicated that leptin reduced its enzyme activity in vivo. Our study offered evidence that leptin downregulated FAS expression at the transcriptional level, which may be responsible for the reduction in its activity. Moreover, we identified two regions (−1960/−1525 bp and −1380/−1152 bp) related to regulation of the FAS promoter.
Having determined the key promoter regions that mediated the transcriptional regulation of CPT Iα1b and FAS, we next explored whether STAT3 exerts regulatory action directly through these response elements. According to the putative results, two STAT3 binding sites were located in the region from −1120 bp to −726 bp. However, in the CPT Iα1b promoter, site mutation on the −979/−997 STAT3 binding site, but not on the −802/−812 binding site, reduced the leptin-induced increase of promoter activities. Furthermore, an EMSA assay showed that the positions from −979 bp to −997 bp were a functional binding locus, and leptin promoted the binding of STAT3 to this site because of the stronger bands in the leptin-treated group. In the FAS promoter, we screened three possible STAT3 binding sites and found that leptin inhibited FAS gene expression via the STAT3 response element located from −794 bp to −812 bp on the FAS promoter. STAT3 is one member of the STAT family, which is implicated in programming gene expression [39]. Several studies pointed out that leptin administration caused the activation of STAT3 [11,12,15,16,40], and the activated STAT3 dimer subsequently entered the nucleus and regulated the transcription of target genes [41]. However, to the best of our knowledge, information is extremely scarce about the direct relationship between STAT3 and leptin-induced changes in lipid metabolism. For the first time, our study has indicated that STAT3 could directly bind with the promoter regions of CPT Iα1b and FAS, which potentially mediate the regulation of lipid metabolism by leptin.

5. Conclusion

In conclusion, we identified and characterized the promoter regions of ACCα, CPT1α1b, FAS, and PPARγ genes from yellow catfish. The promoters of ACCα, CPT1α1b, FAS, and PPARγ genes presented different structures on their core regions. 5′ deletion mutant analysis indicated the modulatory features of these promoters at the transcriptional level. Leptin treatment increased the activity of the CPT1α1b promoter and decreased the activity of the FAS promoter. Furthermore, leptin regulated the transcriptional activities of CPT1α1b and FAS through STAT3, and the functional binding locus of STAT3 on the promoter regions of CPT Iα1b and FAS genes was identified.

Supplementary Materials

The following are available at https://www.mdpi.com/2073-4425/9/7/334/s1. Table S1: Primers used for ACCα, CPT1α1b, FAS, and PPARγ promoter cloning. Table S2: Primers used for 5′-deletion plasmids construction. Table S3: The reference binding site sequences. Table S4: Primers used for site mutation analysis. Table S5: Primers used for electrophoretic mobility-shift assay.

Author Contributions

X.-Y.T. and K.W. designed the experiment; K.W. undertook the experiments and sample analysis with skilled help from Y.-H.X., G.-H.C. and M.-Q.Z.; X.-Y.T. and K.W. analyzed all the experimental data; Y.-H.X., G.-H.C. and M.-Q.Z. offered some crucial suggestions for data analysis; K.W. drafted the present paper, and X.-Y.T. revised the paper. All the authors read the paper and approved the present submission.

Funding

This study was financially supported by funds from the National Natural Science Foundation of China (grant nos. 31572605, 31001101).

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Sargent, J.R.; Tocher, D.R.; Bell, J.G. The lipids. In Fish Nutrition, 3rd ed.; Halver, J.E., Ronald, W.H., Eds.; Elsevier: Amsterdam, The Netherlands, 2003; pp. 181–257. ISBN 978-0-12-319652-1. [Google Scholar]
  2. Kerner, J.; Hoppel, C. Fatty acid import into mitochondria. Biochim. Biophys. Acta 2000, 1486, 1–17. [Google Scholar] [CrossRef]
  3. Davis, M.S.; Solbiati, J.; Cronan, J.E. Overproduction of acetyl-CoA carboxylase activity increases the rate of fatty acid biosynthesis in Escherichia coli. J. Biol. Chem. 2000, 275, 28593–28598. [Google Scholar] [CrossRef] [PubMed]
  4. Richard, N.; Kaushik, S.; Larroquet, L.; Panserat, S.; Corraze, G. Replacing dietary fish oil by vegetable oils has little effect on lipogenesis, lipid transport and tissue lipid uptake in rainbow trout (Oncorhynchus mykiss). Br. J. Nutr. 2006, 96, 299–309. [Google Scholar] [CrossRef] [PubMed]
  5. Zheng, J.L.; Zhuo, M.Q.; Luo, Z.; Pan, Y.X.; Song, Y.F.; Huang, C.; Zhu, Q.L.; Hu, W.; Chen, Q.L. Peroxisome proliferator-activated receptor gamma (PPARγ) in yellow catfish Pelteobagrus fulvidraco: Molecular characterization, mRNA expression and transcriptional regulation by insulin in vivo and in vitro. Gen. Comp. Endocrinol. 2015, 212, 51–62. [Google Scholar] [CrossRef] [PubMed]
  6. Sheridan, M.A. Lipid dynamics in fish: Aspects of absorption, transportation, deposition and mobilization. Comp. Biochem. Physiol. 1988, 90, 679–690. [Google Scholar] [CrossRef]
  7. Klok, M.D.; Jakobsdottir, S.; Drent, M.L. The role of leptin and ghrelin in the regulation of food intake and body weight in humans: A review. Obes. Rev. 2007, 8, 21–34. [Google Scholar] [CrossRef] [PubMed]
  8. Friedman, J.M.; Halaas, J.L. Leptin and the regulation of body weight in mammals. Nature 1998, 395, 763–770. [Google Scholar] [CrossRef] [PubMed]
  9. Gong, Y.; Luo, Z.; Zhu, Q.L.; Zheng, J.L.; Tan, X.Y.; Chen, Q.L.; Lin, Y.C.; Lu, R.H. Characterization and tissue distribution of leptin, leptin receptor and leptin receptor overlapping transcript genes in yellow catfish Pelteobagrus fulvidraco. Gen. Comp. Endocrinol. 2013, 182, 1–6. [Google Scholar] [CrossRef] [PubMed]
  10. Volkoff, H.; Eykelbosh, A.J.; Peter, R.E. Role of leptin in the control of feeding of goldfish Carassius auratus: Interactions with cholecystokinin, neuropeptide Y and orexin A, and modulation by fasting. Brain Res. 2003, 972, 90–109. [Google Scholar] [CrossRef]
  11. Song, Y.F.; Wu, K.; Tan, X.Y.; Zhang, L.H.; Zhuo, M.Q.; Pan, Y.X.; Chen, Q.L. Effects of recombinant human leptin administration on hepatic lipid metabolism in yellow catfish Pelteobagrus fulvidraco: In vivo and in vitro studies. Gen. Comp. Endocrinol. 2015, 212, 92–99. [Google Scholar] [CrossRef] [PubMed]
  12. Wu, K.; Tan, X.Y.; Xu, Y.H.; Chen, Q.L.; Pan, Y.X. JAK and STAT members of yellow catfish Pelteobagrus fulvidraco and their roles in leptin affecting lipid metabolism. Gen. Comp. Endocrinol. 2016, 226, 14–26. [Google Scholar] [CrossRef] [PubMed]
  13. Bates, S.H.; Stearns, W.H.; Dundon, T.A.; Schubert, M.; Tso, A.W.; Wang, Y.; Banks, A.S.; Lavery, H.J.; Haq, A.K.; Maratos-Flier, E.A.; et al. STAT3 signalling is required for leptin regulation of energy balance but not reproduction. Nature 2003, 421, 856–859. [Google Scholar] [CrossRef] [PubMed]
  14. Gorissen, M.; de Vrieze, E.; Flik, G.; Huising, M.O. STAT genes display differential evolutionary rates that correlate with their roles in the endocrine and immune system. J. Endocrinol. 2011, 209, 175–184. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  15. Lu, R.H.; Liang, X.F.; Wang, M.; Zhou, Y.; Bai, X.L.; He, Y. The role of leptin in lipid metabolism in fatty degenerated hepatocytes of the grass carp Ctenopharyngodon idellus. Fish Physiol. Biochem. 2012, 38, 1759–1774. [Google Scholar] [CrossRef] [PubMed]
  16. Wu, K.; Tan, X.Y.; Wei, C.C.; You, W.J.; Zhuo, M.Q.; Song, Y.F. Isolation and expression analysis of STAT members from Synechogobius hasta and their roles in leptin affecting lipid metabolism. Int. J. Mol. Sci. 2016, 17, 406. [Google Scholar] [CrossRef] [PubMed]
  17. Xu, Y.H.; Luo, Z.; Wu, K.; Fan, Y.F.; You, W.J.; Zhang, L.H. Structure and functional analysis of promoters from two liver isoforms of CPT I in grass carp Ctenopharyngodon idella. Int. J. Mol. Sci. 2017, 18, 2405. [Google Scholar] [CrossRef] [PubMed]
  18. Luo, Z.; Tan, X.Y.; Zheng, J.L.; Chen, Q.L.; Liu, C.X. Quantitative dietary zinc requirement of juvenile yellow catfish (Pelteobagrus fulvidraco), and effects on hepatic intermediary metabolism and antioxidant responses. Aquaculture 2011, 319, 150–155. [Google Scholar] [CrossRef]
  19. Zheng, J.L.; Luo, Z.; Zhu, Q.L.; Chen, Q.L.; Gong, Y. Molecular characterization, tissue distribution and kinetic analysis of carnitine palmitoyltransferase I in juvenile yellow catfish Pelteobagrus fulvidraco. Genomics 2013, 101, 195–203. [Google Scholar] [CrossRef] [PubMed]
  20. Zheng, J.L.; Luo, Z.; Zhu, Q.L.; Tan, X.Y.; Chen, Q.L.; Sun, L.D.; Hu, W. Molecular cloning and expression pattern of 11 genes involved in lipid metabolism in yellow catfish Pelteobagrus fulvidraco. Gene 2013, 531, 53–63. [Google Scholar] [CrossRef] [PubMed]
  21. Primers, P. High-efficiency thermal asymmetric interlaced PCR for amplification of unknown flanking sequences. Biotechniques 2007, 43, 649–656. [Google Scholar] [Green Version]
  22. Read, M.A.; Cordle, S.R.; Veach, R.A.; Carlisle, C.D.; Hawiger, J. Cell-free pool of CD14 mediates activation of transcription factor NF-kappa B by lipopolysaccharide in human endothelial cells. Proc. Natl. Acad. Sci. USA 1993, 90, 9887–9891. [Google Scholar] [CrossRef] [PubMed]
  23. Smith, P.K.; Krohn, R.I.; Hermanson, G.T.; Mallia, A.K.; Gartner, F.H.; Provenzano, M.D.; Fujimoto, E.K.; Goeke, N.M.; Olson, B.J.; Klenk, D.C. Measurement of protein using bicinchoninic acid. Anal. Biochem. 1985, 150, 76–85. [Google Scholar] [CrossRef]
  24. Mao, J.; Chirala, S.S.; Wakil, S.J. Human acetyl-CoA carboxylase 1 gene: Presence of three promoters and heterogeneity at the 5′-untranslated mRNA region. Proc. Natl. Acad. Sci. USA 2003, 100, 7515–7520. [Google Scholar] [CrossRef] [PubMed]
  25. Smale, S.T.; Kadonaga, J.T. The RNA polymerase II core promoter. Annu. Rev. Biochem. 2003, 72, 449–479. [Google Scholar] [CrossRef] [PubMed]
  26. Steffen, M.L.; Harrison, W.R.; Elder, F.F. Expression of the rat liver carnitine palmitoyltransferase I (CPT-Ia) gene is regulated by Sp1 and nuclear factor Y: Chromosomal localization and promoter characterization. Biochem. J. 1999, 340, 425–432. [Google Scholar] [CrossRef] [PubMed]
  27. Amy, C.M.; Williams-Ahlf, B.; Naggert, J.; Smith, S. Molecular cloning of the mammalian fatty acid synthase gene and identification of the promoter region. Biochem. J. 1990, 271, 675–679. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  28. Zhu, Y.; Qi, C.; Korenberg, J.R.; Chen, X.N.; Noya, D.; Rao, M.S.; Reddy, J.K. Structural organization of mouse peroxisome proliferator-activated receptor gamma (mPPAR gamma) gene: Alternative promoter use and different splicing yield two mPPAR gamma isoforms. Proc. Natl. Acad. Sci. USA 1995, 92, 7921–7925. [Google Scholar] [CrossRef] [PubMed]
  29. Horton, J.D.; Shimomura, I.; Ikemoto, S.; Bashmakov, Y.; Hammer, R.E. Overexpression of sterol regulatory element-binding protein-1a in mouse adipose tissue produces adipocyte hypertrophy, increased fatty acid secretion, and fatty liver. J. Biol. Chem. 2003, 278, 36652–36660. [Google Scholar] [CrossRef] [PubMed]
  30. Zhang, Y.; Yin, L.; Hillgartner, F.B. SREBP-1 integrates the actions of thyroid hormone, insulin, cAMP, and medium-chain fatty acids on ACCα transcription in hepatocytes. J. Lipid Res. 2003, 44, 356–368. [Google Scholar] [CrossRef] [PubMed]
  31. Saneyasu, T.; Shiragaki, M.; Nakanishi, K.; Kamisoyama, H.; Honda, K. Effects of short term fasting on the expression of genes involved in lipid metabolism in chicks. Comp. Biochem. Physiol. 2013, 165, 114–118. [Google Scholar] [CrossRef] [PubMed]
  32. Lee, W.J.; Kim, M.; Park, H.S.; Kim, H.S.; Jeon, M.J.; Oh, K.S.; Koh, E.H.; Won, J.C.; Kim, M.S.; Oh, G.T.; et al. AMPK activation increases fatty acid oxidation in skeletal muscle by activating PPARα and PGC-1. Biochem. Biophys. Res. Commun. 2006, 340, 291–295. [Google Scholar] [CrossRef] [PubMed]
  33. Schoonjans, K.; Staels, B.; Auwerx, J. Role of the peroxisome proliferator-activated receptor (PPAR) in mediating the effects of fibrates and fatty acids on gene expression. J. Lipid Res. 1996, 37, 907–925. [Google Scholar] [PubMed]
  34. Sekiya, M.; Yahagi, N.; Matsuzaka, T.; Takeuchi, Y.; Nakagawa, Y.; Takahashi, H.; Okazaki, H.; Iizuka, Y.; Ohashi, K.; Gotoda, T.; et al. SREBP-1-independent regulation of lipogenic gene expression in adipocytes. J. Lipid Res. 2007, 48, 1581–1591. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  35. Joseph, S.B.; Laffitte, B.A.; Patel, P.H.; Watson, M.A.; Matsukuma, K.E.; Walczak, R.; Collins, J.L.; Osborne, T.F.; Tontonoz, P. Direct and indirect mechanisms for regulation of fatty acid synthase gene expression by liver X receptors. J. Biol. Chem. 2002, 277, 11019–11025. [Google Scholar] [CrossRef] [PubMed]
  36. Herzig, S.; Hedrick, S.; Morantte, I.; Koo, S.H.; Galimi, F.; Montminy, M. CREB controls hepatic lipid metabolism through nuclear hormone receptor PPAR-γ. Nature 2003, 426, 190–193. [Google Scholar] [CrossRef] [PubMed]
  37. Minokoshi, Y.; Kim, Y.B.; Peroni, O.D.; Fryer, L.G.; Muller, C.; Carling, D.; Kahn, B.B. Leptin stimulates fatty-acid oxidation by activating AMP-activated protein kinase. Nature 2002, 415, 339–343. [Google Scholar] [CrossRef] [PubMed]
  38. Steinberg, G.R.; Bonen, A.; Dyck, D.J. Fatty acid oxidation and triacylglycerol hydrolysis are enhanced after chronic leptin treatment in rats. Am. J. Physiol. 2002, 282, E593–E600. [Google Scholar] [CrossRef] [PubMed]
  39. Horvath, C.M. STAT proteins and transcriptional responses to extracellular signals. Trends Biochem. Sci. 2000, 25, 496–502. [Google Scholar] [CrossRef]
  40. Sanchez-Margalet, V.; Martin-Romero, C. Human leptin signaling in human peripheral blood mononuclear cells: Activation of the JAK-STAT pathway. Cell Immunol. 2001, 211, 30–36. [Google Scholar] [CrossRef] [PubMed]
  41. Morton, G.J.; Cummings, D.E.; Baskin, D.G.; Barsh, G.S.; Schwartz, M.W. Central nervous system control of food intake and body weight. Nature 2006, 443, 289–295. [Google Scholar] [CrossRef] [PubMed]
Genes 09 00334 g001 550
Figure 1. 5′ unidirectional deletion assays of the promoter regions of ACCα (acetyl-CoA carboxylase alpha), CPT Iα1b (acetyl-CoA carboxylase alpha), FAS (fatty acid synthase,), and PPARγ (peroxisome proliferator-activated receptor gamma) of yellow catfish. (A) Assays for the ACCα promoter; (B) assays for the CPT Iα1b promoter; (C) assays for the FAS promoter; (D) assays for the PPARγ promoter. Values mean the ratio of activities of firefly to Renilla luciferase, normalized to the control plasmid. Results are shown as mean ± standard error of mean (SEM) (n = 3). Asterisk (*) means significant differences between two groups (p < 0.05).
Figure 1. 5′ unidirectional deletion assays of the promoter regions of ACCα (acetyl-CoA carboxylase alpha), CPT Iα1b (acetyl-CoA carboxylase alpha), FAS (fatty acid synthase,), and PPARγ (peroxisome proliferator-activated receptor gamma) of yellow catfish. (A) Assays for the ACCα promoter; (B) assays for the CPT Iα1b promoter; (C) assays for the FAS promoter; (D) assays for the PPARγ promoter. Values mean the ratio of activities of firefly to Renilla luciferase, normalized to the control plasmid. Results are shown as mean ± standard error of mean (SEM) (n = 3). Asterisk (*) means significant differences between two groups (p < 0.05).
Genes 09 00334 g001
Genes 09 00334 g002 550
Figure 2. 5′ unidirectional deletion assays for promoter regions of ACCα, CPT Iα1b, FAS and PPARγ after leptin treatment. (A) Assays for the ACCα promoter region; (B) assays for the CPT Iα1b promoter region; (C) assays for the FAS promoter region; (D) assays for the PPARγ promoter region. Values showed the ratio of activities of firefly to Renilla luciferase, normalized to the control. Results were presented as mean ± SEM (n = 3). Asterisk (*) indicates significant differences between different 5′ unidirectional deletion plasmids under the same treatment (p < 0.05). Different letters indicate significant differences between different treatments in the same plasmid (p < 0.05).
Figure 2. 5′ unidirectional deletion assays for promoter regions of ACCα, CPT Iα1b, FAS and PPARγ after leptin treatment. (A) Assays for the ACCα promoter region; (B) assays for the CPT Iα1b promoter region; (C) assays for the FAS promoter region; (D) assays for the PPARγ promoter region. Values showed the ratio of activities of firefly to Renilla luciferase, normalized to the control. Results were presented as mean ± SEM (n = 3). Asterisk (*) indicates significant differences between different 5′ unidirectional deletion plasmids under the same treatment (p < 0.05). Different letters indicate significant differences between different treatments in the same plasmid (p < 0.05).
Genes 09 00334 g002
Genes 09 00334 g003 550
Figure 3. Assays of predicted STAT3 binding sites after site-directed mutagenesis. (A) Site mutagenesis of STAT3 on pGl3-CPTIα1b-2155 vector; (B) site mutagenesis of STAT3 on pGl3-FAS-1960 vector. Values mean the ratio of activities of firefly to Renilla luciferase, normalized to the control. Results were presented as mean ± SEM (n = 3). Asterisk (*) indicates significant differences between different 5′ unidirectional deletion plasmids under the same treatment (p < 0.05). Different letters indicates significant differences between different treatments in the same plasmid (p < 0.05).
Figure 3. Assays of predicted STAT3 binding sites after site-directed mutagenesis. (A) Site mutagenesis of STAT3 on pGl3-CPTIα1b-2155 vector; (B) site mutagenesis of STAT3 on pGl3-FAS-1960 vector. Values mean the ratio of activities of firefly to Renilla luciferase, normalized to the control. Results were presented as mean ± SEM (n = 3). Asterisk (*) indicates significant differences between different 5′ unidirectional deletion plasmids under the same treatment (p < 0.05). Different letters indicates significant differences between different treatments in the same plasmid (p < 0.05).
Genes 09 00334 g003
Genes 09 00334 g004 550
Figure 4. EMSA of predicted STAT3 binding sequence. (A) STAT3 binding sequences sited between −979 bp and −997 bp of CPT Iα1b promoter; (B) STAT3 binding sequences sited between −794 bp and −812 bp of FAS promoter. NP, nuclear protein.
Figure 4. EMSA of predicted STAT3 binding sequence. (A) STAT3 binding sequences sited between −979 bp and −997 bp of CPT Iα1b promoter; (B) STAT3 binding sequences sited between −794 bp and −812 bp of FAS promoter. NP, nuclear protein.
Genes 09 00334 g004

Share and Cite

MDPI and ACS Style

Wu, K.; Tan, X.-Y.; Xu, Y.-H.; Chen, G.-H.; Zhuo, M.-Q. Functional Analysis of Promoters of Genes in Lipid Metabolism and Their Transcriptional Response to STAT3 under Leptin Signals. Genes 2018, 9, 334. https://doi.org/10.3390/genes9070334

AMA Style

Wu K, Tan X-Y, Xu Y-H, Chen G-H, Zhuo M-Q. Functional Analysis of Promoters of Genes in Lipid Metabolism and Their Transcriptional Response to STAT3 under Leptin Signals. Genes. 2018; 9(7):334. https://doi.org/10.3390/genes9070334

Chicago/Turabian Style

Wu, Kun, Xiao-Ying Tan, Yi-Huan Xu, Guang-Hui Chen, and Mei-Qin Zhuo. 2018. "Functional Analysis of Promoters of Genes in Lipid Metabolism and Their Transcriptional Response to STAT3 under Leptin Signals" Genes 9, no. 7: 334. https://doi.org/10.3390/genes9070334

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop