- Open Access
GR-mediated transcriptional regulation of m6A metabolic genes contributes to diet-induced fatty liver in hens
Journal of Animal Science and Biotechnology volume 12, Article number: 117 (2021)
Glucocorticoid receptor (GR) mediated corticosterone-induced fatty liver syndrome (FLS) in the chicken by transactivation of Fat mass and obesity associated gene (FTO), leading to demethylation of N6-methyladenosine (m6A) and post-transcriptional activation of lipogenic genes. Nutrition is considered the main cause of FLS in the modern poultry industry. Therefore, this study was aimed to investigate whether GR and m6A modification are involved in high-energy and low protein (HELP) diet-induced FLS in laying hens, and if true, what specific m6A sites of lipogenic genes are modified and how GR mediates m6A-dependent lipogenic gene activation in HELP diet-induced FLS in the chicken.
Laying hens fed HELP diet exhibit excess (P < 0.05) lipid accumulation and lipogenic genes activation in the liver, which is associated with significantly increased (P < 0.05) GR expression that coincided with global m6A demethylation. Concurrently, the m6A demethylase FTO is upregulated (P < 0.05), whereas the m6A reader YTHDF2 is downregulated (P < 0.05) in the liver of FLS chickens. Further analysis identifies site-specific demethylation (P < 0.05) of m6A in the mRNA of lipogenic genes, including FASN, SREBP1 and SCD. Moreover, GR binding to the promoter of FTO gene is highly enriched (P < 0.05), while GR binding to the promoter of YTHDF2 gene is diminished (P < 0.05).
These results implicate a possible role of GR-mediated transcriptional regulation of m6A metabolic genes on m6A-depenent post-transcriptional activation of lipogenic genes and shed new light in the molecular mechanism of FLS etiology in the chicken.
Fatty liver syndrome (FLS) is a metabolic disease mostly observed in laying hens, which is characterized by increased lipid accumulation in the liver . FLS occurs at the rate between 4% and 20% in chickens kept in intensive systems, which may cause dramatic drop in egg production and increased mortality, leading to considerable economic losses [2, 3]. Several factors have been reported to contribute to the development of FLS, including genetics, environment, nutrition, toxic substances, and hormones [4, 5]. Among these, nutrition is considered the main cause of FLS in the modern poultry industry. Nutritionally over-fed laying hens are at risk for developing FLS , and a high-energy maize diet produces a higher incidence of FLS than a low-energy barley diet . Also, high-energy low-protein (HELP) diet is used to establish a model of FLS in some previous publications [7,8,9].
FLS is caused primarily by an imbalance of hepatic energy influx and efflux. Glucocorticoids (GC) play an important role in hepatic metabolic homeostasis. Chronically elevated GC level is a common feature of fatty liver in humans and animal models [10, 11]. The actions of GC are primarily mediated by glucocorticoid receptor (GR) . Over-activation of GR pathway leads to transcriptional up-regulation of lipogenic genes, causing hepatic steatosis . In chickens, corticosterone (CORT) is the main active form of GC . We have shown previously that excessive CORT administration causes FLS in chickens, which is characterized by excessive lipid accumulation in the liver [15,16,17]. GR is up-regulated in the liver of FLS chickens [15,16,17], yet it remains unknown how GR contributes to diet-induced FLS in the chicken.
Three families of protein components are involved in the dynamic m6A methylation. The methyltransferases complex formed by methyltransferase-like 3 (METTL3), methyltransferase-like 14 (METTL14), and Wilms’ tumor 1-associating protein (WTAP) [18,19,20] are “writers” to transfer methyl group to the adenosine of the consensus m6A motif in the target RNA. The two demethylases, termed as “erasers”, fat mass and obesity-associated protein (FTO) and α-ketoglutarate-dependent dioxygenase AlkB homolog 5 (ALKBH5) [21, 22], are responsible to remove the methyl group from the m6A. The “readers”, such as YTH-domain family 1–3 (YTHDF1–3), can recognize this methylation and regulate the RNA metabolism including stability or translation efficiency of the mRNA [23,24,25,26]. m6A modification plays a key role in lipid accumulation and energy metabolism [27, 28]. Recently, GR is reported to mediate corticosterone-induced fatty liver in the chicken by transactivation of FTO, leading to demethylation of m6A and post-transcriptional activation of lipogenic genes such as sterol regulatory element-binding protein-1 (SREBP1), fatty acid synthase (FASN) and stearoyl-CoA desaturase (SCD) . However, it remains unclear what specific sites of lipogenic genes are demethylated and which m6A binding protein is involved in mediating m6A-dependent post-transcriptional activation of lipogenic genes.
Therefore, this study was aimed to investigate whether GR and m6A modification are involved in HELP diet-induced FLS in laying hens, and if yes, what specific m6A sites of lipogenic genes are modified and how GR mediates m6A-dependent lipogenic gene activation in HELP diet-induced FLS in the chicken.
Animals and treatment
Forty-eight Hy-Line Variety Brown laying hens (260 days of age, 1.69 ± 0.09 kg in body weight) were raised in the animal house of Nanjing Agricultural university, with the room temperature at approximately 24 °C, and the light regime of 16 L: 8D. Three hens were housed in each cage (60 cm × 46 cm × 44 cm) equipped with a nipple drinker. Hens were randomly divided into control (CON, twenty-four chickens in eight cages) and high-energy low protein diet (HELP, twenty-four chickens in eight cages) groups, fed control diet (2,610 kcal/kg metabolizable energy, 16.9% crude protein) and HELP diet (3,100 kcal/kg metabolizable energy, 12.1% crude protein), respectively, for 12 weeks. The ingredient and calculated composition of the diets used in the current study are presented in Table 1. Hens were subjected to feed restriction (110 g per hen per day) with free access to water throughout the experiment. After 12 weeks of dietary treatment, 1 hen from each cage was randomly selected and killed by rapid decapitation that is considered acceptable for euthanasia of birds according to American Veterinary Medical Association (AVMA) Guidelines for the Euthanasia of Animals: 2013 Edition. Liver samples were rapidly frozen in liquid nitrogen and kept at − 80 °C for further analysis. Among eight hens from HELP group, six hens were diagnosed as FLS according to the hepatic triglyceride (TG) content. So, the sample size was adjusted of both CON and HELP group to six. We conducted a statistical assessment with the replicate number by using G*Power 18.104.22.168 with power (1-β) set at 0.95 and α = 0.05. According to the TG content in the liver (CON = 21.62 ± 2.85 mg/g; HELP = 42.45 ± 7.62 mg/g), we have calculated the effective size d = 3.62. A sample size of 8 participants (4 per group) was needed. Therefore, 12 participants (6 per group) provide sufficient power to study the molecular mechanism underlying the diet-induced FLS in the present study.
To visualize the hepatic fat droplets, fresh frozen liver samples were embedded in optimal cutting temperature (OCT) compound and sliced into 8 μm sections. The frozen sections were stained with oil red O (Sigma Aldrich, Saint Louis, MO, USA) for 30 min, counter-stained with H&E for 30 s, then mounted in neutral resin. The slides were observed by using an optical light microscope (Olympus-BX53, Tokyo, Japan).
Determination of triglyceride content in liver
TG content in liver was measured by using TG assay kits (E1013, Applygen Technologies Inc., Beijing, China) following the manufacturer’s instructions. Briefly, 50 mg of frozen liver sample was homogenized in 1 mL of isopropanol manually in a glass homogenizer with 10 passes on ice, incubated at 4 °C for 10 min. The supernatants were collected and used to measure the hepatic TG contents following the instruction of the TG assay kit.
Determination of corticosterone content in plasma
CORT content in plasma was measured by using chicken CORT ELISA Kit (E-EL-0160c, Elabscience, TX, USA) following the manufacturer’s instructions.
Total RNA isolation and real-time PCR
Total RNA was isolated from liver sample (30 mg) using TRIzol Reagent (Invitrogen, Carlsbad, CA, USA) and reverse transcribed into cDNA by using HiScript II Q RT SuperMix for qPCR (+gDNA wiper) (R223–01, Vazyme, Nanjing, China). The coding sequences were used to design specific oligonucleotide primers (GenScript Biotech Co., Nanjing, China) for PCR (Table 2) with AceQ qPCR SYBR Green Master Mix (Q111–02, Vazyme, Nanjing, China) on the Applied Biosystems QuantStudio 6 Flex Real-Time PCR System (Applied Biosystems, Foster City, CA, USA). The relative mRNA abundance was calculated with the 2−ΔΔCt method using GAPDH as an internal reference.
Protein extraction and Western blotting analysis
Protein was extracted from 40 mg frozen liver sample as previously described . The protein concentration was determined with a Pierce BCA Protein Assay Kit (Thermo Fisher, Waltham, MA, USA). Forty micrograms of protein were used for electrophoresis on the 10% SDS-PAGE gel. Western blot analysis for SREBP1 (AB12162, Abcam, Cambridge, MA, USA, diluted 1:500), SCD (sc-30081, Santa Cruz, CA, USA, diluted 1:200), GR (Custom made for chickens by Genecreate Biotech Co., Wuhan, China, diluted 1:1,000), METTL3 (AB98009, Abcam, diluted 1:1,000), METTL14 (AB98116, Abcam, diluted 1:1,000), FTO (AB77547, Abcam, diluted 1:1,000), YTHDF1 (17479–1-AP, Proteintech, Chicago, IL, USA, diluted 1:2,000), YTHDF2 (24744–1-AP, Proteintech, diluted 1:2,000) and YTHDF3 (25537–1-AP, Proteintech, diluted 1:1,000) were carried out according to the recommended protocols provided by the manufacturers, The density of each protein band was normalized by that of Tubulin α, the internal control. All antibodies were verified to work with chicken samples in previous publications [16, 17]. Images were captured by VersaDoc 4000MP system (Bio-Rad, Hercules, CA, USA) and the band density was analyzed with Quantity One software (Bio-Rad, USA).
RNA m6A dot blot assays
For m6A dot blot, 500 ng RNA sample was denatured at 95 °C for 5 min and transferred onto a Hybond-N+ membrane (GE Healthcare, Piscataway, NJ, USA). After UV crosslinking, the membrane was washed with TBST buffer, blocked with 5% non-fat milk, and incubated with anti-m6A antibody (AB151230, Abcam, diluted 1:1,000) overnight at 4 °C. Then, the membrane was incubated with secondary antibody at room temperature for 2 h. The signals were visualized by the chemiluminescence system (Bio-Rad, USA) and the dot density was analyzed with Quantity One software (Bio-Rad, USA), with staining of 0.02% methylene blue (in 0.3 mol/L sodium acetate, pH = 5.2) as loading control.
SELECT for detection of m6A
From the m6A-seq database obtained in a previous study on CORT-induced FLS chickens , sequences with m6A peaks were retrieved for lipogenic mRNAs including SREBP1, SCD and FASN, and subjected to specific m6A site analysis with SRAMP (http://www.cuilab.cn/sramp). One very high/high confidence m6A site was selected for each gene and verified by using a single-base elongation- and ligation-based qPCR amplification method (termed as “SELECT”). Briefly, 5 μg total RNA was incubated with 40 nmol/L Up Primer, 40 nmol/L Down Primer and 5 nmol/L dNTP in 17 μL 1× CutSmart buffer (50 mmol/L KAc, 20 mmol/L Tris-HAc, 10 mmol/L MgAc2, 100 μg/mL BSA) and annealed under the program as follows: 90 °C (1 min), 80 °C (1 min), 70 °C (1 min), 60 °C (1 min), 50 °C (1 min) and 40 °C (6 min). Next, 17 μL annealing products were incubated with a 3 μL of enzyme mixture containing 0.01 U Bst 2.0 DNA polymerase, 0.5 U SplintR ligase and 10 nmol ATP. The final 20 μL reaction mixture was incubated at 40 °C for 20 min, denatured at 80 °C for 20 min and kept at 4 °C. Quantitative PCR analysis was run under the following conditions: 95 °C, 5 min; (95 °C, 10 s; 60 °C, 45 s) for 40 cycles. The SELECT products of tested site were normalized to the RNA abundance of the mRNA transcript bearing this site. Primers used in SELECT assay are listed in the Table 3.
Chromatin immunoprecipitation (ChIP) assay
ChIP was carried out as previously described . Briefly, 200 mg frozen liver samples were ground in liquid nitrogen and washed with PBS containing protease inhibitor cocktail (Roche, Basel, Switzerland). After cross-linking in 1% formaldehyde, the reaction was stopped with 2.5 mol/L glycine. The pellets were lysed and chromatin was sonicated to an average length of ∼ 300 bp and the protein-DNA complex was diluted in ChIP dilution buffer, incubated with 2 μg of GR antibody (sc-1004, Santa Cruz, California, USA) overnight at 4 °C. A negative control was included with normal IgG or no antibody. Protein G agarose beads (sc-2003, Santa Cruz, California, USA) were added to capture the immunoprecipitated chromatin complexes. Reverse cross-linking was performed at 65 °C for 5 h to release DNA fragments from the immunoprecipitated complex and DNA was purified. The putative GREs in FTO, YTHDF1 and YTHDF2 promoters were predicted using JASPAR 2020 (http://jaspar.genereg.net) . Immunoprecipitated DNA was used as a template for real-time PCR. The primers used to amplify the sequences covering these putative GREs are listed in Table 2.
Differences between two groups were analyzed by t-test using SPSS 20.0 software (SPSS Inc., Chicago, IL, USA). Data are expressed as means ± SEM. Pearson correlation analysis was performed for correlation analysis. The differences were considered statistically significant when P < 0.05.
Lipogenic genes are activated in the liver of chickens fed HELP diet
Chickens fed HELP diet had significantly higher hepatic lipid accumulation compared with their control counterparts, as seen in Oil Red O staining (Fig. 1A) and hepatic TG (Fig. 1B) content (P < 0.05). Meanwhile, plasma CORT concentration was significantly elevated (P < 0.05) in HELP group (Fig. 1C). Moreover, hepatic expression of lipogenesis genes, such as SREBP1, FASN and SCD were significantly up-regulated (P < 0.05) at both mRNA (Fig. 1D) and protein (Fig. 1E) levels.
HELP diet increases hepatic GR expression and decreases global RNA m6A methylation
GR was significantly increased (P < 0.05), at both mRNA (Fig. 2A) and protein (Fig. 2B) levels, in the liver of chickens fed HELP diet. Meanwhile, HELP diet significantly decreased (P < 0.05) mRNA m6A levels (Fig. 2C) in the liver. Hepatic TG contents were negatively correlated to global m6A levels (r2 = − 0.7404, P < 0.01, Fig. 2D). No significant alterations were detected for the expression of RNA methyltransferases (METTL3 and METTL14) or the reader proteins (YTHDF1 and YTHDF3) (Figs. 2E, 3A-B, F-G), and no correlation found between hepatic TG contents and METTL3, METTL14, YTHDF1 and YTHDF3 protein content in liver (Fig. 3C-D, H, J). However, RNA demethylase FTO (Figs. 2E, 3A-B) was significantly increased (P < 0.05), and the reader protein YTHDF2 (Figs. 2E, 3F-G) was significantly decreased (P < 0.05) in the liver of chickens fed HELP diet. Moreover, hepatic TG contents are positively correlated to FTO protein content (r2 = 0.5916, P < 0.05, Fig. 3E) and negatively correlated to hepatic YTHDF2 protein content (r2 = − 0.856, P < 0.01, Fig. 3I) in FLS hens.
Levels of m6A on specific sites of lipogenic mRNAs are decreased in the liver of HELP diet-fed chickens
Specific m6A sites on 3’UTR of SREBP1, SCD and FASN mRNAs were selected for site-specific m6A quantification by SELECT method. Cycle threshold numbers were significantly increased (P < 0.05) at potential m6A site (X site, Fig. 4A, C and E), but not at the negative control site (N site, Fig. 3B, D and F), indicating decreased m6A modification on specific site of lipogenic mRNA 3’UTRs in the liver of HELP diet-fed chickens.
GR binding to the promoter of FTO and YTHDF2 genes is modulated in the liver of HELP diet-fed chickens
ChIP-PCR analysis revealed changes of GR binding on the promoter of FTO and YTHDF2 genes. Fragments containing putative GREs on the promoter of FTO (Fig. 5A), YTHDF2 (Fig. 5B) and YTHDF1 (Fig. 5C) were amplified after chromatin immunoprecipitation with GR antibody. GR binding to the fragment of FTO gene promoter (Fig. 5A) was significantly increased (P < 0.05), while that to the fragment 1 of YTHDF2 gene promoter (Fig. 5B) was significantly decreased (P < 0.05), in the liver of HELP diet-fed chickens. In contrast, GR binding to the fragment 2 of YTHDF2 or YTHDF1 gene promoter was not affected.
Accumulating evidences indicate that FTO-dependent RNA demethylation and nonalcoholic fatty liver disease are closely intertwined [32, 33]. FTO-dependent demethylation of m6A leads to an increase in lipogenic expression in hepatocytes through m6A modification [34, 35]. Previously, we used chronic administration of corticosterone (CORT) to establish an in vivo FLS model in the juvenile chickens, and to induce excessive lipid accumulation in primary chicken hepatocytes in vitro with combined treatment of oleic acid and dexamethasone (OA/DEX) . In both in vivo and in vitro models, we found that GR-mediated transactivation of FTO and m6A demethylation contribute to lipogenic gene activation. Interestingly, HELP diet-induced FLS is also associated with global m6A demethylation and the activation of lipogenic genes in the liver of laying hens. It may not be totally unexpected, because all these fatty liver models, no matter how they are induced, share the same hormonal and biochemical status of elevated CORT and lipid concentration in the blood.
The major mechanism by which m6A exerts its effects is recruiting m6A-binding proteins . m6A can be recognized by proteins that contain a YTH (YT521B homology) domain  or alternatively by eukaryotic initiation factor 3 (eIF3) [38, 39]. The functions of m6A-binding proteins are context-dependent, which means that different m6A-binding proteins bind m6A on different regions of mRNA to exert different functions in gene regulation . Among three m6A-binding proteins determined in the present study, YTHDF2 was down-regulated at both mRNA and protein levels, indicating YTHDF2-mediated gene regulation. YTHDF2 binds transcripts carrying m6A in 3’UTR to induce mRNA degradation partially through recruiting the CCR4-NOT deadenylase complex . YTHDF2 was reported to selectively recognize m6A sites in FASN mRNA, leading to increased FASN mRNA decay and decreased FASN protein content in HepG2 cell lines . Previously, we conducted a m6A-seq analysis to elaborate the epitranscriptomic modification of m6A in the liver of CORT-induced FLS chickens . From this published database, we selected some CORT-responsive m6A peaks in 3’UTR of the lipogenic transcripts, and identified specific HELP-responsive m6A sites on 3’UTR of lipogenic mRNAs, including SREBP1, SCD and FASN, with SELECT analysis. It is possible that the down-regulation of YTHDF2 impairs m6A-dependent lipogenic mRNA degradation, which leads to augmented lipogenesis and excessive lipid accumulation in the liver of FLS hens.
The molecular mechanism by which HELP-diet induces hepatic up-regulation of YTHDF2 in the chicken is unknown. YTHDF2 is negatively regulated by miR-145/miR-495/miR-493-3p at post-transcriptional level in hepatocellular carcinoma cells and prostate cancer cells [43,44,45]. Moreover, YTHDF2 can be SUMOylated in vivo and in vitro at the site of K571, which significantly increases its binding affinity with m6A-modified mRNAs . HIF-2α is reported to transrepress YTHDF2 in hepatocellular carcinoma cells . Based on the observation that YTHDF2 is down-regulated at both mRNA and protein level, we come up with a hypothesis that GR may directly transactivate YTHDF2. Silicon analysis using JASPAR online database identifies 2 putative GR binding sites for YTHDF2. These binding sites were then functionally validated using ChIP-PCR. Indeed, GR binding to YTHDF2 gene promoter is decreased in the liver of hens fed HELP diet. It remains a mystery how GR binding to the promoter of FTO and YTHDF2 genes is distinctively regulated, leading to FTO up-regulation and YTHDF2 down-regulation in HELP diet-induced FLS. Some unidentified co-factors must come into play to coordinate the down-stream effectors of GR action.
In this study, GR was upregulated at both mRNA and protein levels in the liver of hens fed HELP diet. The altered GR binding to the promoter of FTO and YTHDF2 genes indicate HELP diet-induced modulation in GR activation. GR can be activated via both ligand-dependent  and ligand-independent manners . Previously, we reported CORT-dependent GR activation in the liver of CORT-treated chickens [16, 50]. In this study, chickens are not treated with CORT and the plasma CORT level was not determined. Therefore, we cannot draw a conclusion whether the altered GR expression and binding is dependent on CORT. Nevertheless, GR can be activated by cellular stressors through p38 MAPK-mediated phosphorylation of Ser134, which is a hormone-independent phosphorylation site on the human GR . GR can also be activated by various stimuli in the absence of glucocorticoid ligands, such as elevated temperature, excessive inflammation, and cancer [52,53,54]. Therefore, both ligand-dependent and ligand-independent pathways are possible in HELP diet-induced alteration in hepatic GR activation.
The present results have shown that GR-mediated transcriptional regulation of FTO and YTHDF2 contributes to lipogenic gene activation by site-specific demethylation in HELP diet-induced chicken FLS. These findings add YTHDF2-mediated m6A modification as a new component of GR signaling in the regulation of fat metabolism in the liver and shed new light on developing effective therapeutic strategies in the prevention and treatment of HELP diet-induced chicken FLS.
Availability of data and materials
The datasets used and analyzed during the current study available from the corresponding author upon request.
α-ketoglutarate-dependent dioxygenase AlkB homolog 5
Eukaryotic initiation factor 3
Fatty acid synthase
Fatty liver syndrome
Fat mass and obesity associated gene
Single-base elongation- and ligation-based qPCR amplification method
Sterol regulatory element-binding protein-1
Wilms’ tumor 1-associating protein
YTH-domain family 1–3
Wolford JH, Polin D. Lipid accumulation and hemorrhage in livers of laying chickens. A study on fatty liver-hemorrhagic syndrome (FLHS). Poult Sci. 1972;51(5):1707–13. https://doi.org/10.3382/ps.0511707.
Grimes TM. Causes of disease in two commercial flocks of laying hens. Aust Vet J. 1975;51(7):337–43. https://doi.org/10.1111/j.1751-0813.1975.tb15942.x.
Zhang Y, Liu Z, Liu R, Wang J, Zheng M, Li Q, et al. Alteration of hepatic gene expression along with the inherited phenotype of acquired fatty liver in chicken. Genes. 2018;9(4):199. https://doi.org/10.3390/genes9040199.
Trott KA, Giannitti F, Rimoldi G, Hill A, Woods L, Barr B, et al. Fatty liver hemorrhagic syndrome in the backyard chicken: a retrospective histopathologic case series. Vet Pathol. 2014;51(4):787–95. https://doi.org/10.1177/0300985813503569.
Choi YI, Ahn HJ, Lee BK, Oh ST, An BK, Kang CW. Nutritional and hormonal induction of fatty liver syndrome and effects of dietary lipotropic factors in egg-type male chicks. Asian-Australas J Anim Sci. 2012;25(8):1145–52. https://doi.org/10.5713/ajas.2011.11418.
Pearson AW, Curtis MJ, Butler EJ. Bacterial endotoxins and the pathogenesis of fatty liver--haemorrhagic syndrome in the laying hen. Res Vet Sci. 1981;31(2):259–61. https://doi.org/10.1016/S0034-5288(18)32507-4.
Jiang S, Cheng HW, Cui LY, Zhou ZL, Hou JF. Changes of blood parameters associated with bone remodeling following experimentally induced fatty liver disorder in laying hens. Poult Sci. 2013;92(6):1443–53. https://doi.org/10.3382/ps.2012-02800.
Rozenboim I, Mahato J, Cohen NA, Tirosh O. Low protein and high-energy diet: a possible natural cause of fatty liver hemorrhagic syndrome in caged white Leghorn laying hens. Poult Sci. 2016;95(3):612–21. https://doi.org/10.3382/ps/pev367.
Song Y, Ruan J, Luo J, Wang T, Yang F, Cao H, et al. Abnormal histopathology, fat percent and hepatic apolipoprotein a I and apolipoprotein B100 mRNA expression in fatty liver hemorrhagic syndrome and their improvement by soybean lecithin. Poult Sci. 2017;96(10):3559–63. https://doi.org/10.3382/ps/pex163.
Targher G, Bertolini L, Rodella S, Zoppini G, Zenari L, Falezza G. Associations between liver histology and cortisol secretion in subjects with nonalcoholic fatty liver disease. Clin Endocrinol. 2006;64(3):337–41. https://doi.org/10.1111/j.1365-2265.2006.02466.x.
Vegiopoulos A, Herzig S. Glucocorticoids, metabolism and metabolic diseases. Mol Cell Endocrinol. 2007;275(1–2):43–61. https://doi.org/10.1016/j.mce.2007.05.015.
Hollenberg SM, Weinberger C, Ong ES, Cerelli G, Oro A, Lebo R, et al. Primary structure and expression of a functional human glucocorticoid receptor cDNA. Nature. 1985;318(6047):635–41. https://doi.org/10.1038/318635a0.
Beaupere C, Liboz A, Fève B, Blondeau B, Guillemain G. Molecular mechanisms of glucocorticoid-induced insulin resistance. Int J Mol Sci. 2021;22(2):623. https://doi.org/10.3390/ijms22020623.
Costantini D, Fanfani A, Dell'omo G. Effects of corticosteroids on oxidative damage and circulating carotenoids in captive adult kestrels (Falco tinnunculus). J Comp Physiol B. 2008;178(7):829–35. https://doi.org/10.1007/s00360-008-0270-z.
Hu Y, Sun Q, Liu J, Jia Y, Cai D, Idriss AA, et al. In ovo injection of betaine alleviates corticosterone-induced fatty liver in chickens through epigenetic modifications. Sci Rep. 2017;7(1):40251. https://doi.org/10.1038/srep40251.
Hu Y, Sun Q, Hu Y, Hou Z, Zong Y, Omer NA, et al. Corticosterone-induced lipogenesis activation and lipophagy inhibition in chicken liver are alleviated by maternal betaine supplementation. J Nutr. 2018;148(3):316–25. https://doi.org/10.1093/jn/nxx073.
Hu Y, Feng Y, Zhang L, Jia Y, Cai D, Qian SB, et al. GR-mediated FTO transactivation induces lipid accumulation in hepatocytes via demethylation of m(6) a on lipogenic mRNAs. RNA Biol. 2020;17(7):930–42. https://doi.org/10.1080/15476286.2020.1736868.
Liu J, Yue Y, Han D, Wang X, Fu Y, Zhang L, et al. A METTL3-METTL14 complex mediates mammalian nuclear RNA N6-adenosine methylation. Nat Chem Biol. 2014;10(2):93–5. https://doi.org/10.1038/nchembio.1432.
Ping XL, Sun BF, Wang L, Xiao W, Yang X, Wang WJ, et al. Mammalian WTAP is a regulatory subunit of the RNA N6-methyladenosine methyltransferase. Cell Res. 2014;24(2):177–89. https://doi.org/10.1038/cr.2014.3.
Wang X, Feng J, Xue Y, Guan Z, Zhang D, Liu Z, et al. Structural basis of N(6)-adenosine methylation by the METTL3-METTL14 complex. Nature. 2016;534(7608):575–8. https://doi.org/10.1038/nature18298.
Jia G, Fu Y, Zhao X, Dai Q, Zheng G, Yang Y, et al. N6-methyladenosine in nuclear RNA is a major substrate of the obesity-associated FTO. Nat Chem Biol. 2011;7(12):885–7. https://doi.org/10.1038/nchembio.687.
Zheng G, Dahl JA, Niu Y, Fedorcsak P, Huang CM, Li CJ, et al. ALKBH5 is a mammalian RNA demethylase that impacts RNA metabolism and mouse fertility. Mol Cell. 2013;49(1):18–29. https://doi.org/10.1016/j.molcel.2012.10.015.
Wang X, Lu Z, Gomez A, Hon GC, Yue Y, Han D, et al. N6-methyladenosine-dependent regulation of messenger RNA stability. Nature. 2014;505(7481):117–20. https://doi.org/10.1038/nature12730.
Wang X, Zhao BS, Roundtree IA, Lu Z, Han D, Ma H, et al. N(6)-methyladenosine modulates messenger RNA translation efficiency. Cell. 2015;161(6):1388–99. https://doi.org/10.1016/j.cell.2015.05.014.
Shi H, Wang X, Lu Z, Zhao BS, Ma H, Hsu PJ, et al. YTHDF3 facilitates translation and decay of N(6)-methyladenosine-modified RNA. Cell Res. 2017;27(3):315–28. https://doi.org/10.1038/cr.2017.15.
Liu N, Dai Q, Zheng G, He C, Parisien M, Pan T. N(6)-methyladenosine-dependent RNA structural switches regulate RNA-protein interactions. Nature. 2015;518(7540):560–4. https://doi.org/10.1038/nature14234.
Wang X, Zhu L, Chen J, Wang Y. mRNA m6A methylation downregulates adipogenesis in porcine adipocytes. Biochem Biophys Res Commun. 2015;459(2):201–7. https://doi.org/10.1016/j.bbrc.2015.02.048.
Zhao X, Yang Y, Sun BF, Shi Y, Yang X, Xiao W, et al. FTO-dependent demethylation of N6-methyladenosine regulates mRNA splicing and is required for adipogenesis. Cell Res. 2014;24(12):1403–19. https://doi.org/10.1038/cr.2014.151.
Duan Y, Fu W, Wang S, Ni Y, Zhao R. Effects of tonic immobility (TI) and corticosterone (CORT) on energy status and protein metabolism in pectoralis major muscle of broiler chickens. Comp Biochem Physiol A Mol Integr Physiol. 2014;169:90–5. https://doi.org/10.1016/j.cbpa.2013.12.019.
Feng Y, Dong H, Sun B, Hu Y, Yang Y, Jia Y, et al. METTL3/METTL14 transactivation and m(6)A-dependent TGF-β1 translation in activated Kupffer cells. Cell Mol Gastroenterol Hepatol. 2021;12(3):839–56. https://doi.org/10.1016/j.jcmgh.2021.05.007.
Fornes O, Castro-Mondragon JA, Khan A, van der Lee R, Zhang X, Richmond PA, et al. JASPAR 2020: update of the open-access database of transcription factor binding profiles. Nucleic Acids Res. 2020;48(D1):D87–92. https://doi.org/10.1093/nar/gkz1001.
Mizuno TM. Fat mass and obesity associated (FTO) gene and hepatic glucose and lipid metabolism. Nutrients. 2018;10(11). https://doi.org/10.3390/nu10111600.
Severson TJ, Besur S, Bonkovsky HL. Genetic factors that affect nonalcoholic fatty liver disease: a systematic clinical review. World J Gastroenterol. 2016;22(29):6742–56. https://doi.org/10.3748/wjg.v22.i29.6742.
Kang H, Zhang Z, Yu L, Li Y, Liang M, Zhou L. FTO reduces mitochondria and promotes hepatic fat accumulation through RNA demethylation. J Cell Biochem. 2018;119(7):5676–85. https://doi.org/10.1002/jcb.26746.
Bartosovic M, Molares HC, Gregorova P, Hrossova D, Kudla G, Vanacova S. N6-methyladenosine demethylase FTO targets pre-mRNAs and regulates alternative splicing and 3′-end processing. Nucleic Acids Res. 2017;45(19):11356–70. https://doi.org/10.1093/nar/gkx778.
Meyer KD, Jaffrey SR. Rethinking m(6) a readers, writers, and erasers. Annu Rev Cell Dev Biol. 2017;33(1):319–42. https://doi.org/10.1146/annurev-cellbio-100616-060758.
Xu Y, Zhang W, Shen F, Yang X, Liu H, Dai S, et al. YTH domain proteins: a family of m(6) a readers in cancer progression. Front Oncol. 2021;11:629560. https://doi.org/10.3389/fonc.2021.629560.
Meyer KD, Patil DP, Zhou J, Zinoviev A, Skabkin MA, Elemento O, et al. 5′ UTR m(6) a promotes cap-independent translation. Cell. 2015;163(4):999–1010. https://doi.org/10.1016/j.cell.2015.10.012.
Zhou J, Wan J, Gao X, Zhang X, Jaffrey SR, Qian SB. Dynamic m(6) a mRNA methylation directs translational control of heat shock response. Nature. 2015;526(7574):591–4. https://doi.org/10.1038/nature15377.
Shi H, Wei J, He C. Where, when, and how: context-dependent functions of RNA methylation writers, readers, and erasers. Mol Cell. 2019;74(4):640–50. https://doi.org/10.1016/j.molcel.2019.04.025.
Du H, Zhao Y, He J, Zhang Y, Xi H, Liu M, et al. YTHDF2 destabilizes m(6)A-containing RNA through direct recruitment of the CCR4-NOT deadenylase complex. Nat Commun. 2016;7(1):12626. https://doi.org/10.1038/ncomms12626.
Sun D, Zhao T, Zhang Q, Wu M, Zhang Z. Fat mass and obesity-associated protein regulates lipogenesis via m(6) a modification in fatty acid synthase mRNA. Cell Biol Int. 2021;45(2):334–44. https://doi.org/10.1002/cbin.11490.
Yang Z, Li J, Feng G, Gao S, Wang Y, Zhang S, et al. MicroRNA-145 modulates N(6)-methyladenosine levels by targeting the 3′-untranslated mRNA region of the N(6)-methyladenosine binding YTH domain family 2 protein. J Biol Chem. 2017;292(9):3614–23. https://doi.org/10.1074/jbc.M116.749689.
Du C, Lv C, Feng Y, Yu S. Activation of the KDM5A/miRNA 495/YTHDF2/m6A-MOB3B axis facilitates prostate cancer progression. J Exp Clin Cancer Res. 2020;39(1):223. https://doi.org/10.1186/s13046-020-01735-3.
Li J, Meng S, Xu M, Wang S, He L, Xu X, et al. Downregulation of N(6)-methyladenosine binding YTHDF2 protein mediated by miR-493-3p suppresses prostate cancer by elevating N(6)-methyladenosine levels. Oncotarget. 2018;9(3):3752–64. https://doi.org/10.18632/oncotarget.23365.
Hou G, Zhao X, Li L, Yang Q, Liu X, Huang C, et al. SUMOylation of YTHDF2 promotes mRNA degradation and cancer progression by increasing its binding affinity with m6A-modified mRNAs. Nucleic Acids Res. 2021;49(5):2859–77. https://doi.org/10.1093/nar/gkab065.
Hou J, Zhang H, Liu J, Zhao Z, Wang J, Lu Z, et al. YTHDF2 reduction fuels inflammation and vascular abnormalization in hepatocellular carcinoma. Mol Cancer. 2019;18(1):163. https://doi.org/10.1186/s12943-019-1082-3.
Newton R, Holden NS. Separating transrepression and transactivation: a distressing divorce for the glucocorticoid receptor? Mol Pharmacol. 2007;72(4):799–809. https://doi.org/10.1124/mol.107.038794.
Scheschowitsch K, Leite JA, Assreuy J. New insights in glucocorticoid receptor signaling-more than just a ligand-binding receptor. Front Endocrinol. 2017;8:16. https://doi.org/10.3389/fendo.2017.00016.
Omer NA, Hu Y, Idriss AA, Abobaker H, Hou Z, Yang S, et al. Dietary betaine improves egg-laying rate in hens through hypomethylation and glucocorticoid receptor-mediated activation of hepatic lipogenesis-related genes. Poult Sci. 2020;99(6):3121–32. https://doi.org/10.1016/j.psj.2020.01.017.
Galliher-Beckley AJ, Williams JG, Cidlowski JA. Ligand-independent phosphorylation of the glucocorticoid receptor integrates cellular stress pathways with nuclear receptor signaling. Mol Cell Biol. 2011;31(23):4663–75. https://doi.org/10.1128/mcb.05866-11.
Sanchez ER. Heat shock induces translocation to the nucleus of the unliganded glucocorticoid receptor. J Biol Chem. 1992;267(1):17–20. https://doi.org/10.1016/S0021-9258(18)48448-7.
Verhoog NJ, Du Toit A, Avenant C, Hapgood JP. Glucocorticoid-independent repression of tumor necrosis factor (TNF) alpha-stimulated interleukin (IL)-6 expression by the glucocorticoid receptor: a potential mechanism for protection against an excessive inflammatory response. J Biol Chem. 2011;286(22):19297–310. https://doi.org/10.1074/jbc.M110.193672.
Ritter HD, Antonova L, Mueller CR. The unliganded glucocorticoid receptor positively regulates the tumor suppressor gene BRCA1 through GABP beta. Mol Cancer Res. 2012;10(4):558–69. https://doi.org/10.1158/1541-7786.mcr-11-0423-t.
This work was supported by the National Natural Science Foundation of China (31972638); the National Key Research and Development Program of China (2016YFD0500502); the Fundamental Research Funds for the Central Universities (KYZ201212), the Priority Academic Program Development of Jiangsu Higher Education Institutions (PAPD) and Jiangsu Collaborative Innovation Centre of Meat Production and Processing, Quality and Safety Control.
Ethics approval and consent to participate
The experimental protocol was approved by the Animal Ethics Committee of Nanjing Agricultural University. The sampling procedures complied with the “Guidelines on Ethical Treatment of Experimental Animals” (2006) No. 398 set by the Ministry of Science and Technology, China.
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The authors declare that they have no competing interests.
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Feng, Y., Li, Y., Jiang, W. et al. GR-mediated transcriptional regulation of m6A metabolic genes contributes to diet-induced fatty liver in hens. J Animal Sci Biotechnol 12, 117 (2021). https://doi.org/10.1186/s40104-021-00642-7
- Fatty liver syndrome