- Open Access
Gdf11 gene transfer prevents high fat diet-induced obesity and improves metabolic homeostasis in obese and STZ-induced diabetic mice
Journal of Translational Medicine volume 17, Article number: 422 (2019)
The growth differentiation factor 11 (GDF11) was shown to reverse age-related hypertrophy on cardiomyocytes and considered as anti-aging rejuvenation factor. The role of GDF11 in regulating metabolic homeostasis is unclear. In this study, we investigated the functions of GDF11 in regulating metabolic homeostasis and energy balance.
Using a hydrodynamic injection approach, plasmids carrying a mouse Gdf11 gene were delivered into mice and generated the sustained Gdf11 expression in the liver and its protein level in the blood. High fat diet (HFD)-induced obesity was employed to examine the impacts of Gdf11 gene transfer on HFD-induced adiposity, hyperglycemia, insulin resistance, and hepatic lipid accumulation. The impacts of GDF11 on metabolic homeostasis of obese and diabetic mice were examined using HFD-induced obese and STZ-induced diabetic models.
Gdf11 gene transfer alleviates HFD-induced obesity, hyperglycemia, insulin resistance, and fatty liver development. In obese and STZ-induced diabetic mice, Gdf11 gene transfer restores glucose metabolism and improves insulin resistance. Mechanism study reveals that Gdf11 gene transfer increases the energy expenditure of mice, upregulates the expression of genes responsible for thermoregulation in brown adipose tissue, downregulates the expression of inflammatory genes in white adipose tissue and those involved in hepatic lipid and glucose metabolism. Overexpression of GDF11 also activates TGF-β/Smad2, PI3K/AKT/FoxO1, and AMPK signaling pathways in white adipose tissue.
These results demonstrate that GDF11 plays an important role in regulating metabolic homeostasis and energy balance and could be a target for pharmacological intervention to treat metabolic disease.
Growth differentiation factor 11 (GDF11), also known as bone morphogenetic protein 11, is a member of the TGF-β family playing pleiotropic roles in mammalian development . GDF11 is expressed in multiple tissues, including heart, kidney, skeletal muscle, nervous system, olfactory system, retina, pancreas, intestine. GDF11 has been considered as a rejuvenation factor capable of reversing aging-related dysfunctions in multiple organs including cardiac hypertrophy, skeletal muscle dysfunction, and cerebral vasculature dysfunction [1,2,3,4,5] although conflict results have been reported [6,7,8,9]. The correlation of blood circulation level of GDF11 with aging was conflicting in humans showing increase, decrease, or no change with aging [6, 10,11,12,13,14]. Some reports showed that the circulation level of GDF11 increased in type 2 diabetes (T2D) or obesity in humans and mice [15, 16]. However, some reports are contrary, showing no change with type 2 diabetes and obesity in humans [13, 14].
More recent studies have suggested the potential of GDF11 for the treatment of metabolic diseases such as atherosclerosis, type 2 diabetes, and diabetes-related vascular dysfunctions [15, 17, 18]. Administration of recombinant GDF11 protein (rGDF11) improved β cell function and attenuated the symptom of T2D in diabetic mice . Mei and colleagues demonstrated a reduction of atherosclerotic plaques and improvement of endothelial injury using AAV-mediated Gdf11 gene transfer in ApoE−/− mice . Employing the psoriasis-like skin inflammation model and high-fat diet (HFD) induced obese mice, Wang and colleagues demonstrated the anti-inflammatory activity of GDF11 [15, 19]. Also, GDF11 activated multiple signal pathways, such as Smad, Akt, and p38 MAPK, which were involved in the development of obesity, fatty liver, and insulin resistant [1, 20,21,22], implying that GDF11 may play an important role in obesity and obesity-related metabolic disorders. However, little is known about the function of GDF11 in the development of obesity and obesity-related metabolic disorders.
The focus of the current study is to investigate the functions of GDF11 in regulating metabolic homeostasis and energy balance in high fat diet-induced obesity mice and animals with STZ-induced diabetes. We demonstrate that GDF11 overexpression via gene transfer leads to significant improvement of metabolic homeostasis in obese mice and mice with STZ-induced diabetes, and blockade of high fat diet-induced weight gain, hyperglycemia, insulin resistance, and fatty liver development. These results support the notion that GDF11 plays a critical role in regulating metabolic homeostasis and could be considered as a therapeutic agent for the treatment of metabolic disorders.
Materials and methods
The pLIVE empty vector and pLIVE-SEAP plasmid (carrying secreted alkaline phosphatase gene) were purchased from Mirus Bio (Madison, WI, USA). The cDNA of the mouse Gdf11 gene was amplified by PCR and inserted into pLIVE vector at BamH1 and Sac1 sites to make pLIVE-GDF11 plasmid. The new plasmid construct was amplified in E. coli and extracted using endotoxin-free maxi plasmid kits from Tiangen Biotech (Beijing, China). The inserted Gdf11 gene sequence in the plasmid was verified by DNA sequencing. PrimeScript™ RT reagent kit was from Takara Bio. (Dalian, China). SYBR Green kit for real time-PCR was from Qiagen (Duesseldorf, Germany). BCA Quantitation kit for proteins was purchased from Applygen Technologies Inc. (Beijing, China). ELISA kit for GDF11 protein was from MEIMIAN (Cat. MM-44346M1, Wuhan, China). Primary antibodies against AKT (#4691), p-AKT (Thr 308, #13038), SMAD2 (#5339), p-SMAD2 (Ser 465/467, #3108), FOXO1 (#2880), AMPK (#5831), and p-AMPK (Thr172, #2535) were from Cell Signaling Technology (Danvers, CO, USA). Anti-p-FOXO1 antibody (Ser 256, ab131339) was from Abcam (Cambridge, UK). Primary antibodies against UCP1 (#23673-1-AP), UCP2 (#11081-1-AP), and β-actin (#66009-1-lg) antibodies were from Proteintech (Chicago, USA). The HRP-linked anti-mouse (Cat. ZB-2305) and anti-rabbit (Cat. ZB-2301) second antibodies were from ZSGB BIO Inc. (Beijing, China). Human insulin (Humulin) was from Eli Lilly (Indianapolis, IN, USA). Mouse Insulin ELISA kit was from Shanghai Enzyme-linked Biotechnology Co., Ltd. (Cat. ml001983, Shanghai, China). H&E staining kit was from Yulu (Cat. L11020102, Nanchang, China). The streptozotocin (STZ) was purchased from Sigma Aldrich (St. Louis, MO, USA). The high-fat diet (60% kJ/fat, 20% kJ/carbohydrate, 20% kJ/protein) and regular Chow were from Research Diets, Inc. (Cat. D12492,NJ,USA) and Keao Xieli Feed Cooperation (SPF-level mice maintaining Chow, Beijing, China), respectively.
C57BL/6 mice (male, ~ 25 g) were purchased from Charles River Laboratories China (Beijing, China). All animals were group-housed under standard conditions at 25 ± 2 °C with a 12 h light–dark cycle with free access to food and water. The animal protocol used was approved by the Animal Ethics Committee of the Nanchang University. In studies designed to examine the effect of Gdf11 gene transfer on preventing HFD-induced obesity, mice were divided into 3 groups (5 mice each). Two groups were fed an HFD and the other with regular Chow. Each mouse was hydrodynamically injected with 25 µg (dose: 1 mg/kg) of pLIVE-GDF11 or pLIVE-SEAP control plasmid DNA, respectively, according to the previously published procedure . Body weight and food intake were measured weekly. The rectal temperature of the animals was measured by an electric rectal thermometer weekly. Blood was collected at predetermined time points, and serum was prepared and stored at − 20 °C until use.
To examine the effects of Gdf11 gene transfer on obese mice, mice were fed an HFD to establish obesity, and then divided into two groups (5 mice each). pLIVE-GDF11 or pLIVE-SEAP plasmids were hydrodynamically injected via tail vein, respectively. The volume of injected saline solution with 25 µg plasmid DNA was adjusted to 6% body weight for obese mice.
For the STZ-induced type 2 diabetic model, 15 mice were fed an HFD for 4 weeks, and injected intraperitoneally with a single dose of STZ (100 mg/kg). Blood glucose levels were measured 2 weeks later using Ultra One Touch glucosemeter (Johnson & Johnson, USA). The mice were considered diabetic when non-fasting blood glucose level was higher than 13.9 mmol/l for at least 2 consecutive days. The diabetic mice were divided into 2 groups (5 mice each) and 25 µg of plasmid DNA were hydrodynamically injected with an injection volume equal to 8% body weight. Animals were continued on an HFD for additional 4 weeks, and non-fasting blood glucose levels were determined and serum biochemistry assays were performed.
Glucose tolerance test (GTT) and insulin tolerance test (ITT)
GTT and ITT were performed during the last week of the study on the same animals with a 2-day interval for recovery. For GTT, mice were fasted for 8 h and intraperitoneally injected with glucose in saline (0.2 g/ml, 2 g/Kg). Blood glucose was determined using glucose strips at 0, 30, 60, and 120 min after injection. For ITT, animals were fasted for 6 h and then intraperitoneally injected with insulin (100 IU/ml, 0.75 U/Kg). Blood glucose level was measured at the same time points as in GTT. Total blood was collected 2 days later for serum biochemistry. Insulin levels in the blood were determined using the Mouse Insulin ELISA Kit. Insulin resistance (HOMA-IR) was calculated using the formula as previous described : HOMA-IR = (fasting insulin (ng/ml) × fasting blood glucose (mg/dl)/405).
Collected tissue samples were fixed in 10% neutrally buffered formalin for at least 24 h and embedded in paraffin following the instruction of H&E staining kit. Tissue sections were made at a thickness of 5 μm followed by H&E staining. For Oil-Red O staining, freshly collected liver samples were embedded in OCT medium and frozen in liquid nitrogen. The frozen tissues were equilibrated in a cryostat and sectioned at 8 μm in thickness. The slide sections were fixed in 10% neutrally buffered formalin for 30 min, stained with 0.5% Oil Red O in 60% isopropanol for 15 min, counterstained with hematoxylin, washed three times, and then sealed in neutral gum. Histological photographs were taken under an optical microscope equipped with a Nikon camera.
White adipose tissue was embedded in paraffin and cut at 5 μm thickness. The tissue sections were placed in citrate antigen repair buffer (pH 6.0) in the thermostatic water bath for antigen retrieval. Slices were then put into 3% BSA buffer and blocked at room temperature for 30 min. After blocking, the slices were incubated with primary antibody against F4/80 (dilution 1:500, Cat. GB11027, Wuhan Servicebio Technology Co., Ltd., Wuhan, China) at 4 °C overnight and HRP-linked secondary antibody (dilution 1:200, Cat. G1213, Wuhan Servicebio Technology Co., Ltd., Wuhan, China) for 50 min at room temperature. Then color development was performed with freshly prepared DAB coloring solution (Cat. G1212-200, Wuhan Servicebio Technology Co., Ltd., Wuhan, China). After counterstained nuclei with hematoxylin for 3 min, the slices were dehydrated and sealed.
Serum concentrations of aspartate aminotransferase (Cat. AST03, NingBo PureBio Biotechnology, Ningbo, China), alanine aminotransferase (Cat. ALT03, NingBo PureBio Biotechnology, Ningbo, China), triglycerides (E1013, Applygen Technologies Inc.), total cholesterol (E1015, Applygen Technologies Inc.), and free fatty acids (#15781, Diasy Diagnostic Systems, Frankfurt, Germany) were determined using ELISA kits. To assess the lipid contents in the liver, liver samples (100 mg) were homogenized in a mixture of chloroform and methanol (2:1, volume ratio) and incubated at 70 °C for 10 min. The homogenates were centrifuged at 2000 rpm for 5 min, and the supernatants were dried and re-dissolved in 5% Triton X-100. The amounts of cholesterol, triglyceride and free fatty acids were determined following the manufacturers’ instructions.
Analysis of mouse energy metabolism
The individual mouse was placed in a gas-tight metabolic cage and acclimated for 1 day before the parameters of energy metabolism were determined using a TSE-PhenoMaster system (TSE Systems, Germany) as previously described . The parameters monitored include water and food consumption, total animal activity, the volume of O2 (VO2) and CO2 (VCO2), and respiratory exchange ratio (RER). VO2 was calculated by the equation: “VO2” [ml/h/kg] = FlowML [ml/h] * (V1 [%^2] + V2 [%^2])/(N2Ref[%] * BodyWeight[kg] * 100.0 [%]). VCO2 was calculated by the equation: “VCO2” [ml/h/kg] = FlowML [ml/h]*dCO2 [%]/(BodyWeight [kg] * 100.0 [%]). RER was calculated by the equation: RER = VCO2 [ml/h/kg]/VO2 [ml/h/kg]. Energy expenditure (EE) was calculated by the equation: EE = 3.941 × VO2 + 1.106 × VCO2.
Analysis of gene expression
Real-time PCR was performed to determine the expression level of selected genes. Total RNA was isolated from the mouse liver, white and brown adipose tissues using TRIzol reagents from Invitrogen. One μg of total RNA was reverse-transcribed to generate the first-strand cDNA using PrimeScript™ RT reagent kit. RT-PCR was performed using SYBR Green kit. GAPDH RNA served as an internal control and data were normalized using GAPDH RNA level as 1. All primer sequences employed are summarized in Additional file 1: Table S1.
Proteins in brown and white adipose tissue were extracted by adipose tissue protein extraction kit (BB-312262, BestBio, Shanghai, China). Briefly, 100 mg adipose tissue was homogenized in 500 μl protein extraction buffer with protease inhibitors. The homogenate was incubated for 30 min at 4 °C and centrifuged for 15 min at 12,000g at 4 °C. The supernatant was collected and centrifuged one more time using the same condition. The concentration of total proteins was detected by BCA Quantitation Kits. The same amount of sample (100 µg total protein) was loaded in each well and resolved by SDS-PAGE. The protein bands after electrophoretic separation were transferred to Immobilon-P PVDF Membrane by Mini-PROTEAN® Tetra system at 200 mA for 90 min with transfer buffer (25 mM Tris, 189 mM Glycine, 200 ml MeOH, 800 ml ddH2O). Primary antibodies (dilution 1:2000) were added and incubated overnight at 4 °C. After washing, the HRP-linked anti-mouse second antibody (dilution 1:2500) or anti-rabbit second antibody (dilution 1:2500) were added and incubated for 120 min. The specific protein bands were visualized using a Chemiluminescence imager. The relative levels of protein were scaled to the level of β-actin. The relative levels of the phosphorylated protein were normalized to the signal of their total abundance of that protein.
Statistical analysis was performed by using the Student’s t-test, one-way ANOVA, or nonparametric test. Normality and homogeneity of variances were analyzed using Shapiro–Wilk test and Levene’s test respectively. Post-hoc comparisons were performed using LSD and SNK test in oneway ANOVA. If the data was still not a normal distribution after log transformation, Kruskal–Wallis H test and Mann–Whitney U test were performed. Results were expressed as the mean ± SEM. P < 0.05 was considered significantly different.
Establishment of Gdf11 overexpression in mice
Hydrodynamic tail vein injection was used to establish overexpression of Gdf11 gene in the liver. Animals fed regular Chow food were set as the Chow control without any treatment. Mice fed HFD and hydrodynamically injected with pLIVE-SEAP plasmids (carrying secreted alkaline phosphatase gene) were set as the HFD control. The serum level of GDF11 protein was measured after hydrodynamic injection of pLIVE-GDF11 plasmids (HFD/GDF11 group). The serum concentration of GDF11 reached a peak level at about 14500 pg/ml within 48 h, and a slight decline was observed 3 days after the injection (Fig. 1a). At the end of the test, the serum concentration of GDF11 stayed at approximately 4800 pg/ml, eightfold higher than the background level at 600 pg/ml. Persistent Gdf11 expression was confirmed by qPCR of mRNA isolated from the liver. A high level of Gdf11 mRNA was readily detected at the end of experiments (Fig. 1b). Compared to control animals, overexpression of Gdf11 did not cause liver damage as demonstrated by serum levels of AST and ALT (Fig. 1c).
Impacts of pLIVE-GDF11 delivery on high-fat diet-induced weight gain and food intake
Results in Fig. 1d shows that overexpression of Gdf11 gene prevented HFD-induced weight gain. Eight weeks after plasmid injection, control mice fed an HFD and injected with pLIVE-SEAP control plasmid showed an average body weight of 41.7 ± 1.4 g comparing to 32.1 ± 1.3 g for mice injected with pLIVE-GDF11 which is slightly higher than 28.6 ± 0.4 g of animals fed regular Chow. The size difference between treated and control animals are apparent judging by their appearance (Fig. 1e). Both accumulative and average food intake in Gdf11-treated animals fed an HFD are slightly lower than HFD-fed control mice. However, there is no statistical significance between control and pLIVE-GDF11 injected animals fed an HFD (Fig. 1f, g). One group of Chow food fed mice were also treated with GDF11 (Chow/GDF11), and no significant difference was observed in body weight change and blood glucose between Chow and Chow/GDF11 groups (Additional file 2: Figure S1).
Gdf11 gene transfer suppressed HFD-induced hypertrophy
To explore the impact of GDF11 on adipocytes, different adipose tissues were collected at the end of the experiment. Comparing to regular mice fed a regular Chow (Fig. 2a), HFD-fed control animals had significantly larger size of epididymal (EWAT), perirenal (PWAT), and part of subcutaneous (SWAT, including inguinal (IWAT), dorsolumbar subcutaneous (dlWAT), and anterior subcutaneous (asWAT)) white adipose tissues. WAT in Gdf11-treated animals are significantly smaller than HFD-fed control mice as confirmed by WAT weights (Fig. 2b). BATs in HFD-fed control animals weigh slightly more than those of animals either fed a regular Chow or HFD with the injection of pLIVE-GDF11 plasmids. H&E staining was performed on WAT and BAT on all animals (Fig. 2c). Average size of white adipocytes in HFD-fed control animals are significantly bigger than that of animals with Gdf11 overexpression and animals fed a regular Chow (EWAT 146.6 ± 4.8 μm vs. 81.1 ± 2.8 μm; SWAT 126.6 ± 3.6 μm vs. 91.6 ± 2.7 μm; IWAT 90.8 ± 2.4 μm vs. 48.6 ± 1.1 μm, Fig. 2d). Crown-like structures, an indication of macrophage infiltration into WAT, were seen in EWAT of HFD-fed control animals (Fig. 2c). In BAT, HFD-fed control animals show more lipid accumulation than those of Chow-fed control and the animals injected with pLIVE-GDF11 plasmids (Fig. 2c). These results demonstrate that Gdf11 gene transfer suppressed the HFD-induced hypertrophy.
GDF11 improves HFD-induced glucose intolerance and insulin resistance
Obesity usually accompanies hyperglycemia, glucose intolerance and hyperinsulinemia . To investigate the impact of Gdf11 gene transfer on glucose metabolism and metabolic homeostasis, we performed GTT and ITT. Results in Fig. 3a show that mice injected with Gdf11 gene showed a lower non-fasting and fasting glucose level comparing to that of HFD-fed control mice. GTT assay showed that GDF11-treated animals had a higher glucose clearance rate (Fig. 3b). The area under the curve (AUC) of GTT confirmed that Gdf11 overexpression improved glucose tolerance (Fig. 3c). ITT assay showed that blood glucose levels in animals with Gdf11 gene transfer responds to insulin injection more readily than the HFD-fed control and similar to animals fed regular Chow (Fig. 3d). Blood insulin level in pLIVE-GDF11 plasmid injected mice (0.75 ± 0.10 ng/ml) was significantly lower than that of HFD-fed control mice (0.99 ± 0.08 ng/ml) (Fig. 3e), indicating that mice treated with Gdf11 gene were more sensitive to insulin administration. HOMA-IR confirmed that Gdf11 gene transfer suppressed the development of insulin resistance (Fig. 3f). These results demonstrate the activity of GDF11 in suppressing HFD-induced glucose intolerance and insulin resistance.
GDF11 blocks the development of HFD-induced fatty liver and hepatic steatosis
Obesity is usually associated with excessive fat accumulation in the liver . Results in Fig. 4a, b showed that Gdf11 gene transfer blocked HFD-induced fat accumulation in the liver. Gdf11 gene transfer resulted in a smaller liver comparing to that of HFD-fed control (Fig. 4a, b). H&E and Oil Red O staining showed that pLIVE-GDF11 treated mice had less and smaller lipid droplets and vacuoles in the liver comparing to HFD-fed control mice (Fig. 4a). The serum concentration of triacylglycerol and total cholesterol in GDF11-treated mice were significantly lower than HFD-fed control (Fig. 4c, d). Serum free fatty acid levels are similar among 3 animal groups (Fig. 4e). These results demonstrate that Gdf11 gene transfer prevented HFD-induced fatty liver development.
GDF11 improves metabolic homeostasis in obese mice
Beneficial effects of Gdf11 gene transfer in preventing HFD-induced obesity and metabolic disorders such as glycemia, insulin resistance, and fatty liver have prompted us to explore its effects on animals with obesity. Toward this end, mice fed an HFD for 12 weeks (similar body weight around 44–48 g) were hydrodynamically injected with 25 µg of pLIVE-GDF11 or control plasmids (Fig. 5a). Gdf11 gene transfer did not induce significant loss of body weight of the obese mice (Fig. 5b). H&E staining was performed on WAT on all animals (Fig. 5c). The average size of white adipocytes in animals with Gdf11 overexpression was similar to that of obese control animals (Fig. 5d). There was no significant difference in food intake between pLIVE-GDF11 and pLIVE-SEAP treated groups (Fig. 5e, f). GTT and ITT were performed on these animals 4 weeks after gene transfer. GTT assay showed that animals with Gdf11 gene transfer exhibited a higher glucose clearance rate (Fig. 5g). The AUC of GTT confirmed the improvement of glucose tolerance in GDF11 treated mice (Fig. 5h). ITT assay also showed an improvement of insulin sensitivity in mice treated with GDF11 (Fig. 5i). Gdf11 gene transfer reduced HFD-induced fat accumulation in the liver (Fig. 5j–l). Gdf11 gene transfer resulted in a lower liver weight comparing to that of obese control mice (Fig. 5j). H&E and Oil Red O staining showed that GDF11-treated mice had less and smaller lipid droplets and vacuoles in liver sections comparing to obese control mice (Fig. 5k, l). These results demonstrate that GDF11 ameliorates glucose intolerance and insulin resistance, improves glucose homeostasis, and reduces hepatic steatosis of obese mice.
Impact of Gdf11 gene transfer on STZ-induced type 2 diabetic mice
Similar study was conducted on mice with STZ-induced type 2 diabetes following the protocol shown in Fig. 6a. The body weight of these two group mice was similar 4 weeks after treatment (Fig. 6b). No significant difference in food intake was observed in these two group mice. Results in Fig. 6c showed that Gdf11 gene transfer decreased the non-fasting blood glucose level and kept at a low level for more than 1 month. GTT assay demonstrated that Gdf11 gene transfer improved glucose tolerance (Fig. 6d, e). No significant difference was seen in blood insulin levels between GDF11 treated and control mice (Fig. 6f). ITT assay showed a higher response to injected insulin, and HOMA-IR showed a decrease in insulin resistance in GDF11 treated mice (Fig. 6g, h). These results demonstrate that hydrodynamic injection of pLIVE-GDF11 plasmids had an anti-diabetic effect and improved glucose metabolism in STZ-induced type 2 diabetic mice.
GDF11 increased oxygen consumption and energy expenditure
In order to investigate how GDF11 affected the body weight gain in HFD feeding mice, we conducted a series of measurements on animals housed in a metabolic cage. The oxygen consumption (VO2 and VCO2) was increased in GDF11 treated mice compared with HFD-fed control animals (Fig. 7a–d). The energy expenditure was upregulated after GDF11 treatment (Fig. 7e, f). The respiratory exchange ratio and activity were similar between GDF11 treated mice and HFD-fed control animals (Fig. 7g, h). The rectal temperature was tested weekly after gene transfer. The average rectal temperature also a little bit higher (~ 0.4 °C) in GDF11-treated mice than HFD-fed control and Chow-fed animals (Fig. 7i). These results demonstrate that Gdf11 gene transfer elevates oxidation and energy expenditure in HFD-fed mice.
GDF11 suppressed the inflammatory genes in WAT and elevated expression of thermogenesis genes in BAT
To investigate the underlying mechanisms of GDF11 in preventing HFD-induced obesity and obesity-associated complications, the mRNA levels of inflammatory genes were examined in WAT. HFD feeding markedly increased the expression of Ccl2, Tnfα, F4/80, Cd68, Cd11b, and Cd11c genes (Fig. 8a). Gdf11 gene transfer significantly suppressed the expression of these genes in HFD-fed mice. The crown-like structures, an indication of macrophage infiltration into WAT, were labeled by F4/80 antibody in EWAT of mice. Significant less of F4/80 labeled crown-like structures were observed in GDF11-treated mice compared with HFD-fed control animals (Fig. 8b). These data indicate that GDF11 prevented HFD-induced inflammation and macrophage infiltration.
GDF11 treatment also significantly upregulated the mRNA expression of Elovl3, Ucp1, Ucp2, and Cidea in BAT comparing to that of HFD-fed control animals (Fig. 8c). The protein level of Ucp1 and Ucp2 in BAT was also higher in GDF11 treated mice compared with HFD-fed control group (Fig. 8d). These results suggest that GDF11 increased thermogenesis.
GDF11 altered the expression of genes involved in glucose and lipid metabolism in the liver
To investigate the underlying mechanisms of GDF11 activity in preventing obesity and obesity-related complications, we also assessed the mRNA level of selected genes involved in glucose and lipid metabolism in the liver. Gdf11 gene transfer significantly suppressed the expression of fatty acid translocase gene (Cd36) compared to that in HFD-fed control animals (Fig. 8e). No significant differences were seen in mRNA levels of Pparγ1, Pparγ2, Acc1, Fas, Scd1, and Srebp1c between animals with or without Gdf11 gene transfer (Fig. 8e). GDF11 treatment also significantly reduced the expression of gluconeogenesis gene G6p comparing to that of the HFD-fed group but did not alter the expression of gluconeogenesis gene Pepck (Fig. 8g). Additionally, GDF11 treatment did not change the expression of genes involved in fatty acid β oxidation including Cpt1α, Cpt1 β, Acadl, and Acadm in GDF11 treated mice (Fig. 8f).
GDF11 activated TGF-β/Smad2, AMPK, and PI3K/AKT/FoxO1 signaling pathways
To further investigate the possible signaling pathways by which GDF11 prevents obesity and obesity-related complications, western blotting was performed to examine the canonical and noncanonical signal cascades of GDF11 in WAT. GDF11 is a member of the TGF-β family, having the canonical TGF-β/Smad signaling cascade . The phosphorylation level of Smad2 in white adipose tissue was significantly increased in GDF11 treated mice compared to that in HFD-fed control mice (Fig. 9a). No significant differences were observed in the phosphorylation level of Smad2 between HFD control and Chow groups. No significant differences were seen in total protein level of Smad2 between animals with or without GDF11 treatment. We further detected the noncanonical pathways possibly involved in GDF11 cascades. Gdf11 gene transfer significantly increased AMPK phosphorylation in WAT compared to that in HFD-fed control mice (Fig. 9b), indicating that GDF11 activated the AMPK signaling pathways. In addition, Gdf11 gene transfer significantly increased the phosphorylation level of AKT compared to that in HDF-fed control animals (Fig. 9c). The FoxO1 phosphorylation, a downstream event of AKT activation, was also significantly increased in the WAT of GDF11 treated mice compared to HFD-fed control (Fig. 9c), indicating that GDF11 activated the PI3K/AKT/FoxO1 pathway.
In this study, we demonstrate that hydrodynamic transfer of Gdf11 gene prevented HFD induced obesity, hyperglycemia, insulin resistance and fatty liver in mice. Gdf11 gene transfer also improved metabolic homeostasis in obese mice and mice with STZ-induced diabetes.
The finding that GDF11 is capable of improving glucose metabolism and metabolic homeostasis is consistent with the results of previous studies using db/db and STZ-induced diabetic mice as an animal model [15, 17]. Two mechanisms might be involved. First of all, it is possible that overexpression of GDF11 promoted β-cell differentiation and development of pancreas through Smad2 and PI3K/AKT/FoxO1 signal pathways [17, 26, 27] as previously shown that administration of rGDF11 protein or AAV-GDF11 vectors increased the survival of β-cells in diabetic mice . Results in Fig. 9 confirmed that GDF11 activated TGF-β/Smad2 and PI3K/AKT/FoxO1 pathways in WAT. The second possibility is that GDF11 blocks pathways that lead to metabolic disorders that involve inflammatory cytokines and activation of macrophages [21, 22, 28]. It was previously shown that GDF11 has anti-inflammatory effects [15, 19, 29]. Treatment with rGDF11 attenuated inflammation in psoriasis-like skin inflammation mice and obese mice [15, 19]. rGDF11 or AAV-mediated Gdf11 gene transfer reduced inflammatory cytokines and suppressed the expression of inflammatory genes in aortas, and increased anti-inflammation cytokine IL10 in apoE−/− mice . The conclusions of these earlier studies are supported by our results demonstrating that GDF11 suppressed the expression of inflammatory genes in WAT including Tnfα and Ccl2 and macrophage marker genes such as F4/80, Cd68, Cd11b, and Cd11c in adipose tissue (Fig. 8a). GDF11 also reduced the development of crown-like structures in adipose tissue, a sign of macrophage infiltration and migration into WAT (Figs. 2c, 8b). As inflammation is known for its role in inducing obesity and metabolic complications, the anti-inflammation function of GDF11 is likely one of the reasons for the beneficial effects seen in animals employed in our study (Fig. 9d). In addition, GDF11-induced decrease in expression of gluconeogenesis gene G6P (Fig. 8g), the downstream of PI3K/AKT/FoxO1 signal pathway, in the liver, may also play critical role in reducing blood glucose level and reestablishing glucose homeostasis (Fig. 9d). Moreover, AMPK activity was induced by GDF11 (Fig. 9b), which may also play an important role in glucose uptake, and glucose homeostasis [30, 31].
The fact that no significant weight gain was seen in GDF11-treated animals while there was no difference in their food intake (Fig. 1f, g) and activity compared to the HFD-fed control animals suggests that GDF11-treated animals consume more energy than HFD-fed control animals, which was confirmed by metabolic cage assay that the oxygen consumption and energy expenditure were significantly increased after GDF11 treatment (Fig. 7). The higher level of energy consumption is likely achieved by converting food energy to heat which is released. The rectal temperature was a little bit higher in GDF11-treated mice comparing with HFD-fed control and Chow animals (Fig. 7i). GDF11-induced increase in Ucp1 and Ucp2 expression seen in BAT (Fig. 8c, d) supports the notion that heat release is the mechanism that prevents the animals with Gdf11 gene transfer from gaining weight. Increased thermogenesis is also supported by elevated expression of Elovl3 which is an important component for lipid recruitment in BAT . Elovl3 gene expression is significantly increased during cold stimulation linking Elovl3 to the thermogenic process . These suggest that GDF11-mediated thermogenesis and energy consumption play important roles in prevention of HFD-induced obesity and metabolic disorders.
Previous studies have demonstrated that GDF11 binds to activin type I/II receptors and activates the canonical TGF-β/Smad signaling pathway. TGF-β/Smad pathway was involved in improving islet β-cell function, glucose homeostasis, and lipid metabolism [17, 34,35,36]. In the current study, we also revealed that GDF11 significantly increased the phosphorylation of SMAD2 in WAT (Fig. 9a). In addition, GDF11 also increased the phosphorylation of AKT and FoxO1 (Fig. 9c) which play an important role in the PI3K/AKT/FoxO1 signal cascade critical for regulating lipid metabolism and glucose homeostasis in adipose tissue, liver, pancreas, and skeletal muscle [37, 38]. Moreover, the phosphorylation of AMPK was also upregulated by GDF11 (Fig. 9b). It is known that PI3K/AKT/FoxO1 and AMPK pathways, the noncanonical GDF11 signal cascades, have cross-talk with canonical TGF-β/Smad cascade of GDF11 influencing metabolic homeostasis [31, 39, 40]. These results suggest that GDF11 function in preventing metabolic disorders is achieved through TGF-β/Smad2, PI3K/AKT/FoxO1, and AMPK pathways.
Hydrodynamic injection of Gdf11 gene generated the sustained blood circulating level of GDF11 and long-term anti-diabetic effects, indicating that GDF11 has therapeutic potential in treating diabetes and obesity-related metabolic diseases. However, the detailed mechanisms of GDF11 in preventing obesity and fatty liver remain elusive, as well as the mechanisms of GDF11 in regulating oxygen consumption, thermogenesis, and inflammation. Further studies are needed to investigate the mechanisms of GDF11 in regulating adipocyte development and metabolic homeostasis. Moreover, the hydrodynamic tail vein injection is a physical method of gene delivery to hepatocytes in the liver . The overexpressed GDF11 was secreted into the blood circulation and reached multiple tissues. Additional work is needed to investigate the long term effect of GDF11 in bone, skeletal muscle, and other tissues where GDF11 activities have been demonstrated [16, 42, 43]. Differences reported in different animal models about GDF11 functions need additional investigation. For example, the role of GDF11 on the development of skeletal muscle was different in young and aged mice . AAV-mediated Gdf11 gene transfer blocks the growth and development of skeletal muscle in neonatal mice , but supplementary of GDF11 in old mice restored skeletal muscle dysfunctions, enhanced muscle fibers, and increased the number of multinucleated myotubes . Controversial results have also been reported about the function of GDF11 in aging-related cardiac hypertrophy, cerebral vasculature dysfunctions, and cachexia [1, 15, 45, 46]. The effects of GDF11 on aging have been the focus of GDF11-related research in recent years, and future studies will surely shine light on these seeming controversy results.
In summary, we demonstrate that Gdf11 gene transfer alleviated HFD-induced obesity, hyperglycemia, insulin resistance and fatty liver development in mice. GDF11 also improves glucose homeostasis in obese mice and mice with STZ-induced diabetes. The mechanism study revealed that GDF11 upregulated energy expenditure, upregulated thermogenic genes in BAT, suppressed the expression of inflammatory genes in WAT, and decreased expression of genes responsible for lipid and glucose metabolism in the liver. The signal mechanism underlying the beneficial effects of GDF11 includes TGF-β/Smad2, PI3K/AKT/FoxO1, and AMPK pathways. GDF11 function demonstrated here would suggest a potential use of GDF11 by gene transfer for the treatment of metabolic diseases.
Availability of data and materials
The datasets used and/or analysed during the current study are available from the corresponding author on reasonable request.
growth differentiation factor 11
glucose tolerance test
insulin tolerance test
homeostatic model assessment for insulin resistance
white adipose tissue
epididymal white adipose tissue
subcutaneous white adipose tissue
inguinal white adipose tissue
dorsolumbar subcutaneous white adipose tissue
anterior subcutaneous white adipose tissue
brown adipose tissue
area under the curve
Walker RG, Poggioli T, Katsimpardi L, Buchanan SM, Oh J, Wattrus S, et al. Biochemistry and biology of GDF11 and myostatin: similarities, differences, and questions for future investigation. Circ Res. 2016;118(7):1125–42. https://doi.org/10.1161/CIRCRESAHA.116.308391(discussion 2).
Loffredo FS, Steinhauser ML, Jay SM, Gannon J, Pancoast JR, Yalamanchi P, et al. Growth differentiation factor 11 is a circulating factor that reverses age-related cardiac hypertrophy. Cell. 2013;153(4):828–39. https://doi.org/10.1016/j.cell.2013.04.015.
Wang A, Yan X, Zhang C, Du C, Long W, Zhan D, et al. Characterization of fibroblast growth factor 1 in obese children and adolescents. Endocr Connect. 2018. https://doi.org/10.1530/EC-18-0141.
Sinha M, Jang YC, Oh J, Khong D, Wu EY, Manohar R, et al. Restoring systemic GDF11 levels reverses age-related dysfunction in mouse skeletal muscle. Science. 2014;344(6184):649–52. https://doi.org/10.1126/science.1251152.
Katsimpardi L, Litterman NK, Schein PA, Miller CM, Loffredo FS, Wojtkiewicz GR, et al. Vascular and neurogenic rejuvenation of the aging mouse brain by young systemic factors. Science. 2014;344(6184):630–4. https://doi.org/10.1126/science.1251141.
Egerman MA, Cadena SM, Gilbert JA, Meyer A, Nelson HN, Swalley SE, et al. GDF11 increases with age and inhibits skeletal muscle regeneration. Cell Metab. 2015;22(1):164–74. https://doi.org/10.1016/j.cmet.2015.05.010.
Harper SC, Brack A, MacDonnell S, Franti M, Olwin BB, Bailey BA, et al. Is growth differentiation factor 11 a realistic therapeutic for aging-dependent muscle defects? Circ Res. 2016;118(7):1143–50. https://doi.org/10.1161/CIRCRESAHA.116.307962(discussion 50).
Smith SC, Zhang X, Zhang X, Gross P, Starosta T, Mohsin S, et al. GDF11 does not rescue aging-related pathological hypertrophy. Circ Res. 2015;117(11):926–32. https://doi.org/10.1161/CIRCRESAHA.115.307527.
Hammers DW, Merscham-Banda M, Hsiao JY, Engst S, Hartman JJ, Sweeney HL. Supraphysiological levels of GDF11 induce striated muscle atrophy. EMBO Mol Med. 2017;9(4):531–44. https://doi.org/10.15252/emmm.201607231.
Semba RD, Zhang P, Zhu M, Fabbri E, Gonzalez-Freire M, Carlson OD, et al. Relationship of circulating growth and differentiation factors 8 and 11 and their antagonists as measured using liquid chromatography-tandem mass spectrometry with age and skeletal muscle strength in healthy adults. J Gerontol A Biol Sci Med Sci. 2019;74(1):129–36. https://doi.org/10.1093/gerona/gly255.
Jin M, Song S, Guo L, Jiang T, Lin ZY. Increased serum GDF11 concentration is associated with a high prevalence of osteoporosis in elderly native Chinese women. Clin Exp Pharmacol Physiol. 2016;43(11):1145–7. https://doi.org/10.1111/1440-1681.12651.
Fadini GP, Menegazzo L, Bonora BM, Mazzucato M, Persano S, de Kreutzenberg SV, Avogaro A. Effects of age, diabetes, and vascular disease on growth differentiation factor 11: first-in-human study. Diab Care. 2015;38(8):e118–9.
Schafer MJ, Atkinson EJ, Vanderboom PM, Kotajarvi B, White TA, Moore MM, et al. Quantification of GDF11 and myostatin in human aging and cardiovascular disease. Cell Metab. 2016;23(6):1207–15. https://doi.org/10.1016/j.cmet.2016.05.023.
Anon-Hidalgo J, Catalan V, Rodriguez A, Ramirez B, Silva C, Galofre JC, et al. Circulating GDF11 levels are decreased with age but are unchanged with obesity and type 2 diabetes. Aging (Albany NY). 2019;11(6):1733–44. https://doi.org/10.18632/aging.101865.
Mei W, Xiang G, Li Y, Li H, Xiang L, Lu J, et al. GDF11 protects against endothelial injury and reduces atherosclerotic lesion formation in apolipoprotein E-null mice. Mol Ther. 2016;24(11):1926–38. https://doi.org/10.1038/mt.2016.160.
Poggioli T, Vujic A, Yang P, Macias-Trevino C, Uygur A, Loffredo FS, et al. Circulating growth differentiation factor 11/8 levels decline with age. Circ Res. 2016;118(1):29–37. https://doi.org/10.1161/CIRCRESAHA.115.307521.
Li H, Li Y, Xiang L, Zhang J, Zhu B, Xiang L, et al. GDF11 attenuates development of type 2 diabetes via improvement of islet beta-cell function and survival. Diabetes. 2017;66(7):1914–27. https://doi.org/10.2337/db17-0086.
Zhang J, Li Y, Li H, Zhu B, Wang L, Guo B, et al. GDF11 improves angiogenic function of EPCs in diabetic limb ischemia. Diabetes. 2018;67(10):2084–95. https://doi.org/10.2337/db17-1583.
Wang W, Qu R, Wang X, Zhang M, Zhang Y, Chen C, et al. GDF11 antagonizes psoriasis-like skin inflammation via suppression of NF-kappaB signaling pathway. Inflammation. 2019;42(1):319–30. https://doi.org/10.1007/s10753-018-0895-3.
Gordon KJ, Blobe GC. Role of transforming growth factor-beta superfamily signaling pathways in human disease. Biochim Biophys Acta. 2008;1782(4):197–228. https://doi.org/10.1016/j.bbadis.2008.01.006.
Gao M, Zhang C, Ma Y, Bu L, Yan L, Liu D. Hydrodynamic delivery of mIL10 gene protects mice from high-fat diet-induced obesity and glucose intolerance. Mol Ther. 2013;21(10):1852–61. https://doi.org/10.1038/mt.2013.125.
Xu H, Barnes GT, Yang Q, Tan G, Yang D, Chou CJ, et al. Chronic inflammation in fat plays a crucial role in the development of obesity-related insulin resistance. J Clin Investig. 2003;112(12):1821–30. https://doi.org/10.1172/JCI19451.
Antunes LC, Elkfury JL, Jornada MN, Foletto KC, Bertoluci MC. Validation of HOMA-IR in a model of insulin-resistance induced by a high-fat diet in Wistar rats. Arch Endocrinol Metab. 2016;60(2):138–42. https://doi.org/10.1590/2359-3997000000169.
Chen Z, Wang GX, Ma SL, Jung DY, Ha H, Altamimi T, et al. Nrg4 promotes fuel oxidation and a healthy adipokine profile to ameliorate diet-induced metabolic disorders. Mol Metab. 2017;6(8):863–72. https://doi.org/10.1016/j.molmet.2017.03.016.
Yanovski SZ, Yanovski JA. Obesity prevalence in the United States—up, down, or sideways? N Engl J Med. 2011;364(11):987–9. https://doi.org/10.1056/NEJMp1009229.
Harmon EB, Apelqvist AA, Smart NG, Gu X, Osborne DH, Kim SK. GDF11 modulates NGN3+ islet progenitor cell number and promotes beta-cell differentiation in pancreas development. Development. 2004;131(24):6163–74. https://doi.org/10.1242/dev.01535.
Dichmann DS, Yassin H, Serup P. Analysis of pancreatic endocrine development in GDF11-deficient mice. Dev Dyn. 2006;235(11):3016–25. https://doi.org/10.1002/dvdy.20953.
Monteiro R, Azevedo I. Chronic inflammation in obesity and the metabolic syndrome. Mediators Inflamm. 2010. https://doi.org/10.1155/2010/289645.
Li W, Wang W, Liu L, Qu R, Chen X, Qiu C, et al. GDF11 antagonizes TNF-alpha-induced inflammation and protects against the development of inflammatory arthritis in mice. FASEB J. 2019;33(3):3317–29. https://doi.org/10.1096/fj.201801375RR.
Lin SC, Hardie DG. AMPK: sensing glucose as well as cellular energy status. Cell Metab. 2018;27(2):299–313. https://doi.org/10.1016/j.cmet.2017.10.009.
Day EA, Ford RJ, Steinberg GR. AMPK as a therapeutic target for treating metabolic diseases. Trends Endocrinol Metab. 2017;28(8):545–60. https://doi.org/10.1016/j.tem.2017.05.004.
Jorgensen JA, Zadravec D, Jacobsson A. Norepinephrine and rosiglitazone synergistically induce Elovl3 expression in brown adipocytes. Am J Physiol Endocrinol Metab. 2007;293(5):E1159–68. https://doi.org/10.1152/ajpendo.00213.2007.
Westerberg R, Mansson JE, Golozoubova V, Shabalina IG, Backlund EC, Tvrdik P, et al. ELOVL3 is an important component for early onset of lipid recruitment in brown adipose tissue. J Biol Chem. 2006;281(8):4958–68. https://doi.org/10.1074/jbc.M511588200.
Nomura M, Zhu HL, Wang L, Morinaga H, Takayanagi R, Teramoto N. SMAD2 disruption in mouse pancreatic beta cells leads to islet hyperplasia and impaired insulin secretion due to the attenuation of ATP-sensitive K+ channel activity. Diabetologia. 2014;57(1):157–66. https://doi.org/10.1007/s00125-013-3062-2.
Seong HA, Manoharan R, Ha H. Smad proteins differentially regulate obesity-induced glucose and lipid abnormalities and inflammation via class-specific control of AMPK-related kinase MPK38/MELK activity. Cell Death Dis. 2018;9(5):471. https://doi.org/10.1038/s41419-018-0489-x.
Zhu Q, Chang A, Xu A, Luo K. The regulatory protein SnoN antagonizes activin/Smad2 protein signaling and thereby promotes adipocyte differentiation and obesity in mice. J Biol Chem. 2018;293(36):14100–11. https://doi.org/10.1074/jbc.RA118.003678.
Huang X, Liu G, Guo J, Su Z. The PI3K/AKT pathway in obesity and type 2 diabetes. Int J Biol Sci. 2018;14(11):1483–96. https://doi.org/10.7150/ijbs.27173.
Xing YQ, Li A, Yang Y, Li XX, Zhang LN, Guo HC. The regulation of FOXO1 and its role in disease progression. Life Sci. 2018;193:124–31. https://doi.org/10.1016/j.lfs.2017.11.030.
Hardie DG, Schaffer BE, Brunet A. AMPK: an energy-sensing pathway with multiple inputs and outputs. Trends Cell Biol. 2016;26(3):190–201. https://doi.org/10.1016/j.tcb.2015.10.013.
Guo X, Wang XF. Signaling cross-talk between TGF-beta/BMP and other pathways. Cell Res. 2009;19(1):71–88. https://doi.org/10.1038/cr.2008.302.
Suda T, Liu D. Hydrodynamic gene delivery: its principles and applications. Mol Ther. 2007;15(12):2063–9. https://doi.org/10.1038/sj.mt.6300314.
Jin Q, Qiao C, Li J, Li J, Xiao X. Neonatal systemic AAV-mediated gene delivery of GDF11 inhibits skeletal muscle growth. Mol Ther. 2018;26(4):1109–17. https://doi.org/10.1016/j.ymthe.2018.01.016.
Liu W, Zhou L, Zhou C, Zhang S, Jing J, Xie L, et al. GDF11 decreases bone mass by stimulating osteoclastogenesis and inhibiting osteoblast differentiation. Nat Commun. 2016;7:12794. https://doi.org/10.1038/ncomms12794.
Gamer LW, Cox KA, Small C, Rosen V. Gdf11 is a negative regulator of chondrogenesis and myogenesis in the developing chick limb. Dev Biol. 2001;229(2):407–20. https://doi.org/10.1006/dbio.2000.9981.
Zhang Y, Wei Y, Liu D, Liu F, Li X, Pan L, et al. Role of growth differentiation factor 11 in development, physiology and disease. Oncotarget. 2017;8(46):81604–16. https://doi.org/10.18632/oncotarget.20258.
Jones JE, Cadena SM, Gong C, Wang X, Chen Z, Wang SX, et al. Supraphysiologic administration of GDF11 induces cachexia in part by upregulating GDF15. Cell Rep. 2018;22(6):1522–30. https://doi.org/10.1016/j.celrep.2018.01.044.
Financial support was provided by National Natural Science Foundation of China (NSFC-31771400, NSFC-81728006, NSFC-81501129, NSFC-81860662, NSFC-81760160), Natural Science Foundation of Jiangxi Province (20161BAB215200, 20171ACB21001, 20171BCB23029), Science and Technology Project of Jiangxi Provincial Education Department No. 150111, Science and Technology Project of Health and Family Planning Commission of Jiangxi Provence No. 20175534.
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Additional file 2: Figure S1. Impacts ofGdf11gene transfer on Chow-fed mice. Chow-fed mice were injected with pLIVE-GDF11 or control plasmids and continued on HFD for 6 weeks. (A) Change of body weight after gene transfer; (B) Daily food intake; (C) Fasting blood glucose level after gene transfer; (D) Serum glucose level in GTT 6 weeks after gene transfer.
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Lu, B., Zhong, J., Pan, J. et al. Gdf11 gene transfer prevents high fat diet-induced obesity and improves metabolic homeostasis in obese and STZ-induced diabetic mice. J Transl Med 17, 422 (2019) doi:10.1186/s12967-019-02166-1
- Insulin resistance
- Glucose homeostasis
- Fatty liver
- Hydrodynamic gene transfer