ORIGINAL RESEARCH article
Volume 11 - 2020 | https://doi.org/10.3389/fendo.2020.00341
P2Y2 Receptor Promotes High-Fat Diet-Induced Obesity
- 1Department of Veterans Affairs Salt Lake City Health Care System, Nephrology Research, Salt Lake City, UT, United States
- 2Departments of Internal Medicine, University of Utah Health, Salt Lake City, UT, United States
- 3Jiangsu Key Laboratory of Pediatrics, Nanjing Medical University, Nanjing, China
- 4Division of Endocrinology and Metabolism, Department of Medicine, Center for the Study of Sex Differences in Health, Aging, and Disease, Georgetown University, Washington, DC, United States
- 5Department of Veterans Affairs Salt Lake City Health Care System, Geriatric Research, Education and Clinical Center, Salt Lake City, UT, United States
- 6Department of Nutrition and Integrative Physiology, University of Utah Health, Salt Lake City, UT, United States
- 7Center on Aging, University of Utah Health, Salt Lake City, UT, United States
- 8PharmaCenter Bonn, Pharmaceutical Institute, Pharmaceutical and Medicinal Chemistry, University of Bonn, Bonn, Germany
P2Y2, a G protein-coupled receptor (R), is expressed in all organs involved in the development of obesity and insulin resistance. To explore the role of it in diet-induced obesity, we fed male P2Y2-R whole body knockout (KO) and wild type (WT) mice (B6D2 genetic background) with regular diet (CNT; 10% calories as fat) or high-fat diet (HFD; 60% calories as fat) with free access to food and water for 16 weeks, and euthanized them. Adjusted for body weights (BW), KO mice consumed modestly, but significantly more HFD vs. WT mice, and excreted well-formed feces with no taint of fat or oil. Starting from the 2nd week, HFD-WT mice displayed significantly higher BW with terminal mean difference of 22% vs. HFD-KO mice. Terminal weights of white adipose tissue (WAT) were significantly lower in the HFD-KO vs. HFD-WT mice. The expression of P2Y2-R mRNA in WAT was increased by 2-fold in HFD-fed WT mice. Serum insulin, leptin and adiponectin levels were significantly elevated in the HFD-WT mice, but not in the HFD-KO mice. When induced in vitro, preadipocytes derived from KO mice fed regular diet did not differentiate and mature as robustly as those from the WT mice, as assessed by cellular expansion and accumulation of lipid droplets. Blockade of P2Y2-R by AR-C118925 in preadipocytes derived from WT mice prevented differentiation and maturation. Under basal conditions, KO mice had significantly higher serum triglycerides and showed slightly impaired lipid tolerance as compared to the WT mice. HFD-fed KO mice had significantly better glucose tolerance (GTT) as compared to HFD-fed WT mice. Whole body insulin sensitivity and mRNA expression of insulin receptor, IRS-1 and GLUT4 in WAT was significantly higher in HFD-fed KO mice vs. HFD-fed WT mice. On the contrary, the expression of pro-inflammatory molecules MCP-1, CCR2, CD68, and F4/80 were significantly higher in the WAT of HFD-fed WT vs. HFD-fed KO mice. These data suggest that P2Y2-R plays a significant role in the development of diet-induced obesity by promoting adipogenesis and inflammation, and altering the production of adipokines and lipids and their metabolism in adipose tissue, and thereby facilitates HFD-induced insulin resistance.
Overweight and obesity affect about 30% of the world population on an average, and is much higher in the United States (1). The reported prevalence of overweight and obesity among US Veterans is from 40 to 73% (2, 3). Surprisingly, the combined overweight and obesity in active duty US military personnel rose to more than 60% between 1995 and 2008 (4). Experimental, clinical and epidemiological data link obesity to the development of type 2 diabetes mellitus (T2DM), metabolic syndrome, chronic kidney disease, cardiovascular and cerebrovascular complications, and hypertension (5, 6). In addition, obesity is known to be associated with higher incidences of cancer (7). Because of these serious consequences, 1 in 5 deaths in the United States is associated with obesity. Furthermore, cost and socioeconomic burden of overweight and obesity to individuals and to the nations are huge (8–10). In view of these, in June 2013, the American Medical Association recognized obesity as a disease (11).
Diet-induced obesity or consumption of more calories than what one can utilize or burn (energy surplus) is the most common form of obesity. Although a preventable condition, in reality it is difficult to prevent or treat diet-induced obesity. The anti-obesity drugs fall into three main categories: (i) those that suppress appetite by acting on the brain; (ii) those that interfere with body's ability to absorb specific nutrients in the food, such as fat; and (iii) those that boost the body's metabolic rate. The first two categories of drugs have serious side effects, thus limiting their widespread use. In addition, the US Food and Drug Administration (FDA) withdrew some of them (e.g., sibutramine). Although drugs that boost the body's metabolic rate offer a better alternative, potentially efficacious and safer drugs are not currently available for the treatment of overweight and obesity. Although some of the newly introduced anti-obesity drugs are relatively safer, their long-term efficacy is not well-established, especially in terms of long-term usage (12, 13). Hence, there is an unmet need for determining novel drug targets for the development of efficacious therapies with non-lethal correctable side effects, for use in the clinics or in general population on a wider scale.
The study of purinergic signaling, which is mediated by extracellular nucleotides (ATP/ADP/UTP) through P2 receptors (P2Y and P2X series) is an emerging field with a vast potential for the development of novel therapies for a wide spectrum of disease conditions, in addition to unraveling physiological and pathophysiological mechanisms (14–16). For many years, our interest has been on the role of purinergic signaling in the kidney in health and disease. Specifically, we have been investigating the roles of ATP/UTP-activated P2Y2 and ADP-activated P2Y12 receptors in renal physiology and pathophysiology, with respect to water balance disorders, such as acquired nephrogenic diabetes insipidus or NDI [reviewed in Kishore et al. (17, 18)].
P2Y2 is a G protein-coupled receptor that selectively responds to ATP or UTP, but not to ADP. Activation of P2Y2 receptor results in phosphoinositide hydrolysis and release of intracellular free calcium, and diacylglycerol (DAG), and the ensuing activation of protein kinase C (PKC) among others molecular events (19, 20). Currently, there are no FDA-approved drugs for selectively blocking P2Y2 receptor. Hence, we have been using P2Y2 receptor knockout (KO) mice in our studies. In addition to its effect on renal water handling, we and other investigators have shown that P2Y2 receptor plays a role in renal sodium handling [reviewed in (21)]. During our efforts to understand how obesity affects renal handling of sodium in the P2Y2 KO mice, as early as in 2012, we serendipitously discovered that genetic deletion of P2Y2 receptor confers significant resistance for the high-fat diet (HFD)-induced obesity. Our studies revealed that this resistance is not due to less intake of food or lack of intestinal absorption of fat in the KO mice. On the other hand, cellular and molecular analyses revealed that the KO mice are able to handle energy metabolism in a different way that does not result in obesity. Specifically, we observed that P2Y2 receptor promotes obesity and insulin resistance by effects on adipogenesis and adipocyte metabolism. Here, we present experimental evidence for the role of P2Y2 receptor in adipogenesis and adipocyte metabolism and inflammation in white adipose tissue.
In view of the potential intellectual property issues related to our novel discovery made in 2012, and as mandated by the US Department of Veterans Affairs, in October 2012 we filed a provisional coversheet intellectual property protection to the United States Patent and Trademark Office (USPTO), which was followed by a regular patent application in 2013. After securing the priority date and protection for our discovery, we presented the key elements of our findings at the Kidney Week 2013 meeting (22), followed by two more meeting abstracts (23, 24). On May 1, 2014 our patent application was published online by the World Intellectual Property Organization, which is an open access information database. After establishing the originality by “prior art search” and significance of our discovery, in 2018, the USPTO granted us two patents comprehensively protecting our intellectual property (25, 26). Thus, our discovery on the potential role of P2Y2 receptor in promoting diet-induced obesity and insulin resistance pre-date the recent publications by other investigators related to this topic, which we discussed in the Discussion section.
Materials and Methods
Experimental Animals and Protocols
The animal procedures described here were approved by the Institutional Animal Care and Use Committee (IACUC) and Research Safety Committee of the Department of Veterans Affairs Salt Lake City Health Care System, and were conducted as per the guidelines of the US Public Health Service. Breeders of P2Y2 receptor knockout (KO) mice in the B6D2 genetic background and congenic wild type (WT) mice were originally obtained from Dr. Beverly Koller of the University of North Carolina at Chapel Hill, Chapel Hill, NC, United States (27, 28). These are whole body knockout mice generated by targeted mutagenesis of P2Y2 receptor in embryonic stem cells. Breeding colonies were established at the VA Salt Lake City Health Care System. KO and WT mice were bred and genotyped as described previously (29). Mice were subcutaneously implanted with microchip transponders for efficient identification and tracking (Locus Technologies, Mountain View, CA, United States). In the experiments described below, age-matched male WT and KO mice were used. Multiple animal studies were performed in generating the data presented here. Except during 24-h collections of urine and monitoring of food and water consumption, the mice were housed in groups in conventional cages with bedding. During metabolic studies, mice were housed in metabolic cages (1 mouse/cage) for a maximum of 48 h on each occasion. Irrespective of the housing conditions, unless prohibited by specific experimental manipulations, all mice had free access to food and drinking water. Mice were fed either regular rodent chow containing 10% calories as fat (control diet) or a high-fat diet (HFD) containing 60% calories as fat (HFD). The HFD was purchased from Research Diets, Inc., New Brunswick, NJ, United States (Catalog # D12492). It contains added lard and soybean oil as fat. At the end of the experimental period, mice were humanely euthanized and blood and tissues were collected for analysis as described below.
Effect of Feeding High-Fat Diet in WT and P2Y2 KO Mice
Groups of age-matched male WT and P2Y2 KO mice were fed regular rodent chow (control diet; CNT group) or high-fat diet (HFD group) for up to 16 weeks. Body weights, 24-h water and food intake and urine output were determined once in every 2 weeks by placing the mice in metabolic cages. Feces samples were also collected periodically. Glucose tolerance and insulin tolerance tests were performed during the last 2 weeks of the experimental period on different groups of mice. Mice were euthanized humanely. Blood samples were collected from the inferior vena cava during necropsy. Serum was separated after blood clotting, centrifuged and clear supernatant was used for assays. Total body white fat and organs, such as liver and kidney were collected, weighed and either processed or frozen.
Morphological Examination of Tissues
Freshly harvested tissues were fixed in 10% buffered formalin solution for a few days, then dehydrated and embedded in paraffin. Paraffin-embedded tissues were cut at a thickness of 5 μm, deparaffinized, rehydrated and stained with hematoxylin and eosin. Stained sections were examined under a Reichert light microscope, and digital pictures were taken with a Nikon 995 Coolpix camera.
Assays on Serum or Plasma
Clear supernatants of serum were used for the determination of the following, using commercial assay kits and as per the manufacturers' instructions. Serum insulin and leptin were assayed using ELISA kits from Crystal Chem, Inc., Downers Grove, IL, United States. Serum adiponectin was assayed using EIA kit from the Cayman Chemical Company, Ann Arbor, MI, United States. Serum or plasma triglycerides and glycerol were assayed colorimetrically using kits from the Cayman Chemical Company. Serum free fatty acids were assayed using a kit from BioAssay Systems, Hayward, CA, United States.
Glucose Tolerance Test
We followed a published and standard protocol to conduct glucose tolerance test [GTT; (30)]. Briefly, after fasting for 12 h with free access to drinking water, mice received an intraperitoneal injection of sterile glucose solution (1.5 g/kg body wt.) in 0.5 ml of USP grade water. During the GTT procedure, the mice were kept in warm environment to ensure adequate peripheral blood flow. Droplets of blood were obtained in conscious mice by gently pricking the dorsal pedal vein with a sterile needle. Using these droplets of blood, glucose levels were measured on a Contour Glucometer (Bayer HealthCare, LLC, Mishawaka, IN, United States). Blood samples were collected from each mouse prior to (0 min), and 30, 60, 90, and 120 min after intraperitoneal injection of glucose solution.
Insulin Tolerance Test
We followed a published and standard protocol to conduct an insulin tolerance test [ITT; (31, 32)]. Briefly, immediately before conducting the ITT, the mice were fasted for 4 h with free access to drinking water. During the test period, mice were kept in a warm environment to ensure adequate peripheral blood flow. Baseline (0 min) blood samples were collected from the dorsal pedal vein by gently pricking the conscious mice with a sterile needle. Using the droplets of blood, glucose levels were measured on a Contour Glucometer. After that mice were given intraperitoneal injections of human insulin (Humalin® R-100, Eli Lilly, Indianapolis, IN, United States) at a dose of 1 U/kg body weight using an insulin syringe. Blood samples were collected at 20, 40, 60, 80, 100, and 120 min after insulin injection for glucose determination, using the same procedure described for the 0 min sampling.
Determination of Relative mRNA Expression
Real-time RT-PCR approach was used to determine the relative mRNA expression of molecules of interest as described previously (33–35). These molecules are: P2Y2 receptor, insulin receptor, insulin receptor substrates (IRS-1 and IRS-2), GLUT-4 (glucose transporter type-4), TNFα (tumor necrosis factor-alpha), MCP-1 (monocyte chemoattractant protein-1), CCR2 (C-C chemokine receptor type-2), CD68 (cluster of differentiation 68), F4/80 (EGF-like module-containing mucin-like hormone receptor-like 1), LPL (lipoprotein lipase), HSL (hormone-sensitive lipase), ATGL (adipose triglyceride lipase), and CD36 (fatty acid translocase). Total RNA was extracted from the white adipose tissue by Triazol method, and traces of genomic DNA were removed and processed for RT-PCR by the methods established in our laboratory. After RNA was precipated, RNeasy Mini Kit and RNase-free DNase Set (Qiagen, Germantown, MD, USA) were used to remove traces of genomic DNA. cDNA was synthesized by SuperScript reverse transcription (Invitrogen, Carlsbad, CA, United States). Using gene specific primers (Table 1), real-time PCR amplifications were carried out on cDNA samples in Applied Biosystems 7,500 Real-Time PCR System (Foster City, CA, United States), with AmpliTaq Gold and SYBR Green for detection. Target gene expression was normalized to that of expression of the housekeeping gene β-actin. Data were expressed as target gene expression relative to the expression of β-actin. The relative gene expression level was normalized to the expression of β-actin and calculated using the comparative cycle threshold (ΔΔCt) method, as described by Yuan et al. (41).
Studies on Cultured Predipocytes Derived From the Mice
The process of adipogenesis involves a determination step, in which vascular stromal or stem cells differentiate into preadipocytes, followed by terminal differentiation and maturation into adipocytes (42–44). Since the steps from the preadipocytes can be replicated in vitro, we conducted studies on cultured preadipocytes derived from the mice. Preadipocytes were harvested, cultured and induced to differentiate and mature to adipocytes as per the standard procedures (45). Briefly, the epididymal fat pads were removed, minced, and digested using collagenase at 37°C for 40 min. The digest was centrifuged at low speed, and the infranatant just below the floating layer of cells and oil was removed and transferred to a sterile tube. The infranatant was centrifuged at 500 xg for 10 min and the pellet of cells was collected. Red blood cells in the pellet were removed by the use of lysis buffer and the pellet was washed in plating medium and suspended in fresh plating medium (DMEM/F12 containing 10% FBS). Suspended cells were seeded into 24-well sterile culture plates and incubated at 37°C. When cells reached 90% confluence, they were induced to differentiate using differentiation medium (DMEM, FBS 5%, IBMX 0.25 mM, dexamethasone 0.5 mM, insulin 850 nM, indomethacin 100 μM, penicillin and streptomycin). Forty-eight hours later cells were changed to maintenance medium (DMEM, FBS 10%, insulin 17 nM, penicillin and streptomycin) fresh maintenance medium was replaced every 2 days. Altogether, in about a week after treating with induction medium, adipocytes were fully differentiated and matured with accumulation of fat. Cells were fixed in 10% buffered formalin for 1 h, washed with water and stained for 2 h with a working solution of Oil Red O. Cells were then rinsed repeatedly with water and photographed under an inverted microscope. AR-C118925, a potent, selective and competitive antagonist of P2Y2 receptor was synthesized in the laboratory of Dr. Christa E. Müller, co-author and supplied to us (46). Stock solutions of AR-C118925 (40 mM in DMSO) were diluted freshly in culture medium before using.
Studies on 3T3-L1 Cells
The 3T3-L1, a preadipocyte cell line, has become the gold standard for investigating preadipocyte differentiation and maturation into adipocytes. This cell line faithfully recapitulates the steps in differentiation and maturation of preadipocytes into adipocytes. Differentiation is triggered with a standard cocktail of agents to initiate the cascade of synchronous steps in the differentiation process. The 3T3-L1 cell line was purchased from the ATCC (American Type Culture Collection), Manassas, VA, United States. We have established 3T3-L1 cell line cultures in our laboratory, and using a standard protocol successfully induced them to differentiate and maturate into adipocytes, with accumulation of lipids which stained red with Oil Red O. Briefly, 3T3-L1 cells were cultured in DMEM containing 10%FBS. Two days post confluence, cells were cultured in differentiation medium (DMEM containing 10% FBS, 1 μM dexamethasone, 0.5 mM IBMX and 1 μg/ml insulin) for 2 days. After that, cells were cultured in maintenance medium (DMEM containing 10% FBS and 1 μg/ml insulin) until they accumulated fat droplets. Cells were stained with Oil Red O as described for adipocyte cultures above.
Lipid Tolerance Test
Lipid tolerance test (LTT) was performed using a standard protocol (47). Groups of WT and KO mice (N = 6 per group) fed HFD for 14 weeks were fasted overnight (12–14 h), with free access to drinking water. Baseline blood samples (~30 μl) were collected from the saphenous vein from conscious mice into heparinized microtubes (Microvettes®, Sarstedt, Nümbrecht, Germany). Following that, each mouse was injected intraperitoneally with 200 μl of Intralipid 20% (vol/vol) fat emulsion (Sigma Chemical, Co., St. Louis, MO). After that, blood samples (~30 μl each) were collected at 1, 2, and 4-h time points. During this collection period, mice had free access to drinking water, but not food. Collected blood samples were centrifuged and clear plasma was used to assay triglyceride levels.
All quantitative data were expressed as mean ± SEM. Comparisons among of the group means were made by analysis of variance (ANOVA), followed by the assessment of statistical significance by the Tukey-Kramer Multiple Comparison test. When the means of only two groups were compared, either unpaired t-test or Mann-Whitney non-parametric test were used. P-values < 0.05 were considered significant. GraphPad Instat (GraphPad Software, La Jolla, CA, United States) was used for statistical analysis.
Effect of Feeding High-Fat Diet in WT and P2Y2 KO Mice
The effect of feeding HFD in WT and KO mice was monitored as a function time for up to 16 weeks and compared with the effect of feeding regular or CNT diet. As shown in Figure 1A, feeding HFD to WT mice resulted in steady and significant increases in the mean body weights as a function of time as compared to CNT-fed WT mice. In fact, significant increases in mean weights in HFD-fed WT mice could be seen as early as 2 weeks. On the contrary, there were no such increases in the mean weights of HFD-fed KO mice as compared to the CNT-fed KO mice. This resulted in a difference of about 22% in the mean weights of HFD-fed WT vs. HFD-fed KO mice at the end of the experimental period. It is interesting to note that even at day 0 the CNT-fed KO mice had significantly lower mean body weight as compared to the age-matched CNT-fed WT mice. This finding suggests a tendency for leanness in P2Y2 KO mice. However, based on this finding, one may also argue that since the baseline mean weights in the P2Y2 KO mice were significantly lower than the baseline mean weights in the WT mice, the observed increase in the body weights is only relative. However, the mean weight gains in the WT and KO mice fed HFD were 30 and 15%, respectively. The scatter graph (Figure 1B) reveals that despite the expected spread, all the HFD-fed WT mice had terminal body weights higher than the mean body weight in the HFD-fed KO mice. Finally, Figure 1C shows picture of one of the obese WT mice fed HFD next to an average weighing KO mouse fed HFD after 16 weeks of feeding.
Figure 1. Body weights of WT and P2Y2 KO mice fed regular or high-fat diets. (A) Shows changes in the mean body weights over the time in WT and P2Y2 KO mice fed regular (CNT) or high-fat (HFD) diets. (N = 6 mice/genotype in CNT groups and N = 14 mice/genotype in HFD groups). *P < 0.05 or better as compared to the corresponding mean weights in the HFD-fed KO mice by direct comparison by unpaired t-test. (B) Shows scatter graph of terminal body weights in HFD-fed WT and P2Y2 KO mice. (C) Shows picture of one of the obese WT mice fed HFD vs. an average weighing KO mouse fed HFD after 16 weeks of feeding.
Food Intake and Appearance of Fecal Matter in WT and P2Y2 KO Mice Fed HFD
Lower body weight could be due to reduced intake of food or loss of undigested fat in the fecal matter, for the observed resistance of the KO mice to HFD-diet feeding. In order to test these possibilities, we determined the 24-h food intake and examined the fecal matter in WT and KO mice (Figure 2A). We found that net food intake was modestly, but significantly higher in the KO vs. WT mice. This difference was pronounced when the data were adjusted to the body weight (Figure 2B). Furthermore, we visually evaluated for signs of loss of undigested or partially digested fat in the feces. For this, fecal matter was collected by placing the mice in metabolic cages. The collected fecal matter was gently placed on an absorbent paper and left for a several minutes at room temperature, and then visually assessed and photographed. This procedure was repeated three times over the course of feeding high-fat diet, in addition to routine observation of fecal matter every 2 weeks in metabolic cages. The criteria of visual evaluation are based on the facts that loss of undigested or partially digested fat results in (i) not well-formed feces, and (ii) stains the absorbent paper with oil. As shown in Figure 2C, none of these two was observed, suggesting that there was no loss of fat in the feces. These data suggest that the observed resistance of the P2Y2 KO mice to diet-induced obesity was not due to less consumption of food or loss of undigested food in the feces.
Figure 2. Food intake and appearance of fecal matter in WT and P2Y2 KO mice fed HFD. (A,B) Show food intake in HFD-fed WT and KO mice at 12 week point expressed as g/day or g/g body weight per day, respectively (N = 12 mice per genotype). (C) Shows representative samples of well-formed feces in HFD-fed WT and KO mice without any signs of fat or oil. The green color of the feces is due to the dye added to high-fat diet for identification.
Morphological Appearance and Terminal Weights of White Adipose Tissue in WT and P2Y2 KO Mice fed HFD
Figure 3 upper panels show representative morphology of white adipose tissue in WT and P2Y2 KO mice fed regular (CNT) or high-fat (HFD) diets, as determined by hematoxyln-eosin stained sections under light microscope. All panels are displayed at the same final magnification. Feeding HFD to WT mice resulted in large increases in the size of the fat cells. The corresponding increases in KO mice were far less. In fact, the size of the fat cells in the HFD-fed KO mice was similar to the size of the fat cells in the control diet-fed WT mice. Furthermore, in control diet-fed KO mice the fat cells appear to be not fully loaded with fat. Figure 3A,B show terminal mean weights of abdominal white adipose tissue in WT and P2Y2 KO mice fed CNT or HFD diets, expressed as total amount per animal or adjusted to body weight, respectively. As shown, feeding HFD to WT mice resulted in significant 2.97- and 2.52-fold increases in the fat content, when expressed as amount per mouse or adjusted to body weight, respectively. On the other hand, the corresponding increases in the KO mice were 1.47- and 1.23-fold, only. Figure 3C shows mRNA expression of P2Y2 receptor in white fat increased by ~2-fold in WT mice after feeding HFD. These observations suggest that P2Y2 receptor may be playing a role in the adipogenesis and adipose tissue expansion.
Figure 3. Morphological appearance and mean terminal weights of white adipose tissue in WT and P2Y2 KO mice fed regular of high-fat diets. Upper panels show representative profiles of hematoxylin-eosin stained paraffin sections of white adipose tissue from WT and KO mice fed regular (CNT) or high-fat (HFD) diets for 16 weeks. All profiles are shown at the same final magnification (200x). (A,B) Show the mean terminal weights of white adipose tissue in WT and KO mice fed regular (CNT) or high-fat (HFD) diets, as mg total weight per mouse or as mg/20 g body weight, respectively (N = 6 mice/genotype for CNT; N = 12–14 mice/genotype for HFD). Statistics by ANOVA followed by Tukey-Kramer Multiple Comparison Test. (C) Shows mRNA expression of P2Y2 receptor relative to the mRNA expression of β-actin in the white fat of WT mice fed regular or high-fat diets (N = 6 mice/group); statistics by unpaired t-test.
Terminal Serum Insulin, Leptin, and Adiponectin Levels in WT and P2Y2 KO Mice fed HFD
Figure 4A shows that feeding HFD resulted in 2.3-fold higher terminal serum insulin levels in WT, but not in KO mice. Leptin and adiponectin are hormones elaborated by white adipose tissue (adipocytokines). They have several functions in energy homeostasis and regulation. Hence, we determined the terminal serum levels of leptin and adiponectin in the WT and P2Y2 KO mice fed CNT or HFD diets. As shown in the Figure 4B, feeding HFD to WT mice resulted in ~4-fold increase in serum leptin levels. The corresponding increase in KO mice was only 1.46-fold. Figure 4C shows that feeding HFD to WT mice resulted in significant 1.25-fold increase in serum adiponectin, whereas there was no change in the serum adiponectin levels in KO mice following HFD feeding.
Figure 4. Terminal serum insulin, leptin and adiponectin levels in WT and P2Y2 KO mice fed regular or high-fat diets. Serum samples were assayed for insulin, leptin and adiponectin using commercial ELISA or EIA kits. (A) Shows serum insulin levels; (B) shows serum leptin levels; (C) shoes serum adiponectin levels; in WT and P2Y2 KO mice fed regular or high-fat diet (N = 6 mice/genotype on CNT diet and N = 10–13 mice/genotype on HFD diet). Statistics by ANOVA followed by Tukey-Kramer Multiple Comparison Test.
Glucose Tolerance Test in WT and P2Y2 KO Mice fed Regular or High-Fat Diets
Since the P2Y2 KO mice were resistant to HFD-induced weight gain, we conducted glucose tolerance test (GTT) in WT and P2Y2 KO mice fed CNT or HFD diets. Figure 5A shows the GTT curves for all the four groups tested. Figure 5B shows all time points of GTT in HFD-fed WT and KO mice with statistical differences indicated on the bars. As shown in Figure 5B, at all the time points examined, HFD-fed WT mice had significantly higher blood glucose levels as compared to the HFD-fed KO mice. Figure 5C gives the area under curve (AUC) for all the four groups, derived from the data presented in Figure 5A. As shown the HFD-fed WT mice group has the highest value for AUC as compared to all other groups.
Figure 5. Glucose tolerance test in WT and P2Y2 KO mice fed regular or high-fat diet for 14 weeks. Glucose tolerance test was conducted toward the end of the experimental period of feeding high-fat diet. (A) Mean blood glucose values in all groups at different time points after administration of glucose. N = 5 mice/genotype in CNT diet, N = 12 mice/genotype on high-fat diet. (B) Blood glucose values in high-fat diet fed WT and KO mice at different time points. N = 12 mice/genotype; statistics shown are by direct comparison by unpaired t-test. (C) Area under curve (AUC) for the data shown in (A).
Insulin Tolerance Test and Insulin Receptor Status in WT and P2Y2 KO Mice
To gain further insights into the glucose homeostasis in P2Y2 KO mice, we conducted insulin tolerance test (ITT) in WT and P2Y2 KO mice fed HFD. As shown in Figure 6A, the KO mice displayed better insulin sensitivity, with significantly lower blood glucose values at two time points following insulin administration. We further probed relative mRNA expression of insulin receptor and insulin receptor substrate (IRS)-1 and−2 in the white adipose tissue of WT and P2Y2 KO mice fed regular or HFD. As shown in Figure 6B, although there were no significant differences in the expression of insulin receptor between the WT and KO mice fed regular diet, feeding HFD resulted in a significant difference between these two groups, with KO mice having higher values. In parallel, we observed that the IRS-1 expression levels were significantly higher in the KO mice fed HFD vs. HFD-fed WT mice (Figure 6C). On the other hand, feeding HFD resulted in lower levels of expression of GLUT4 (glucose transporter type-4) in the adipose tissue of both WT and KO mice. However, the decrease was more pronounced in the WT mice, resulting in significantly higher expression levels of GLUT4 in the KO mice vs. WT mice (Figure 6D).
Figure 6. Insulin tolerance test and insulin receptor status in WT and P2Y2 KO mice fed regular or high-fat diet for 13 weeks. Insulin tolerance test was conducted toward the end of experimental period of feeding high-fat diet. (A) Insulin tolerance test in high-fat diet fed WT and P2Y2 KO mice (N = 4 mice/genotype). *P < 0.05 compared to the same time point in KO-HFD group. Real-time RT-PCR approach was used to determine the mRNA expression of insulin receptor (B), insulin receptor substrates (C), and GLUT4 (D) relative to the expression of β-acting in the white adipose tissues of WT or P2Y2 KO mice fed regular (CNT) or high-fat (HFD) diets (N = 6 or 7 per group). Statistics by ANOVA followed by Tukey-Kramer Multiple Comparison Test.
Expression of Inflammatory Cytokines and Related Molecules in the White Adipose Tissue of HFD-Fed WT and P2Y2 KO Mice
Inflammation in the adipose tissue is one of the contributory factors for insulin resistance. Hence, we determined the mRNA expression of inflammatory cytokines and related molecules in the white adipose tissue of HFD-fed WT and P2Y2 KO mice. As shown in Figure 7, the expression levels of MCP-1 (monocyte chemoattractant protein-1), CCR2 (C-C chemokine receptor type-2), CD68 (cluster of differentiation 68), and F4/80 (EGF-like module-containing mucin-like hormone receptor-like 1) are significantly higher in the WT mice vs. KO mice after feeding HFD.
Figure 7. Inflammatory cytokines and related molecules in the white adipose tissue of WT and P2Y2 KO mice fed high-fat diet. Real-time RT-PCR approach was used to determine the expression of inflammatory cytokines and related molecules relative to the mRNA expression of β-actin in the white adipose tissue of HFD fed WT and P2Y2 KO mice. N = 7 mouse samples per group for each parameter. Statistics shown are by direct comparison of the two groups by unpaired t-test. TNF-α (tumor necrosis factor-alpha), MCP-1 (monocyte chemoattractant protein-1), CCR2 (C-C chemokine receptor type-2), CD68 (cluster of differentiation 68), and F4/80 (EGF-like module-containing mucin-like hormone receptor-like 1)
In vitro Differentiation and Maturation of Preadipocytes Derived From WT and P2Y2 KO Mice
Figure 8 shows that when preadipocytes from the WT mice were induced to differentiate and mature, there was robust response with accumulation of copious amounts of triglycerides in the mature adipocytes. On the contrary, the differentiation and maturation of preadipocytes derived from the P2Y2 KO mice under identical conditions was very weak with scant accumulation of triglycerides in the cells. These observations suggest that P2Y2 receptor is needed for the differentiation and maturation of preadipocytes into adipocytes, also known as adipogenesis.
Figure 8. In vitro induced differentiation and maturation of pre-adipocytes derived from WT or P2Y2 KO mice. Preadipocytes harvested from WT and P2Y2 receptor KO mice fed regular diet were induced to differentiate and mature in vitro. Matured cells were stained with Oil Red to visualize cellular content of triglycerides. The similar looking dark or gray spots in un-induced panels were apparently due to artifacts in the optical pathway, and were not related to the cultures per se, which have distinct appearances.
Suppression of in vitro Differentiation and Maturation of Preadipocytes by AR-C118925
There is a possibility that genetic deletion of P2Y2 receptor might have resulted in alterations in the expression of other related genes that could impact adipogenesis. In order to test this possibility, we performed an experiment using pharmacological approach to block P2Y2 receptor in preadipocytes derived from WT mice. For this, we used AR-C118925, a potent, and selective competitive antagonist of P2Y2 receptor. As shown the Figure 9, when preadipocytes derived from WT mice were induced in the presence of 5 or 10 μM of AR-C118925 in the medium, adipogenesis was suppressed to a large extent, with the higher concentration of the drug having a larger effect. At these concentrations, as well as even higher concentrations we tested, AR-C118925 did not cause cell death, and the cells were viable. These observations support a direct role for P2Y2 receptor in adipogenesis.
Figure 9. Effect of blockade of P2Y2 receptor on in vitro differentiation and maturation of pre-adipocytes from WT mice. Preadipocytes harvested from WT mice fed regular diet were induced to differentiate and mature in the absence of presence of AR-C118925, a selective and potent antagonist of P2Y2 receptor, at 5 or 10 μM concentration in the culture medium. Cells were stained with Oil Red to visualize cellular content of triglycerides.
Suppression of in vitro Maturation of 3T3-L1 Cells Into Adipocytes by AR-C118925
The 3T3-L1 cell line have fibroblast-like morphology, but they differentiate into adipocytes when induced by a cocktail of reagents. We used this cell line to obtain further evidence that the observed effect of genetic deletion or pharmacological blockade of P2Y2 receptor on adipogenesis is not cell type-dependent. As shown in Figure 10, the maturation of 3T3-L1 cells into adipocytes with accumulation of triglycerides was markedly suppressed in the presence of 10 μM AR-C118925. Furthermore, as observed in WT mice fed high-fat diet (Figure 3), maturation of 3T3-L1 cells into adipocytes was associated with a 2-fold increase in the mRNA expression of P2Y2 receptor (bar graph in Figure 10). These observations lend further supportive evidence that P2Y2 receptor has a role in adipogenesis.
Figure 10. Effect of blockade of P2Y2 receptor on differentiation and maturation of cultured 3T3-L1 cells into adipocytes. 3T3-L1 cells were induced to differentiate and mature into adipocytes in the absence or presence of AR-C118925, a selective and potent antagonist of P2Y2 receptor at a concentration of 10 μM in the culture medium. Cells were stained with Oil Red to visualize cellular content of triglycerides. Bar graph shows upregulation of P2Y2 receptor mRNA during maturation and differentiation of the 3T3-L1 cells into adipocytes (N = 4 cultures per condition). *P < 0.02 vs. un-induced group by unpaired t-test.
Terminal Serum Triglycerides, Free Fatty Acids, and Glycerol and Lipid Tolerance Test in the WT and P2Y2 KO Mice
Since P2Y2 KO mice were resistant to HFD-induced weight gain, and preadipocytes derived from them show impaired adipogenesis in vitro, we determined triglyceride, free fatty acid and glycerol levels in the serum of WT and P2Y2 KO mice fed CNT or HFD. As shown in Figure 11A, the serum triglyceride levels were significantly higher in the KO mice fed CNT or HFD as compared to the WT mice fed corresponding diets. No significant differences were seen in the serum free fatty acid levels in different groups of mice, although there is a tendency for increased levels in HFD-fed WT or KO mice (Figure 11B). On the other hand, feeding HFD resulted in significantly higher serum glycerol in both WT and KO mice (Figure 11C). To gain further insights into the lipid metabolism in the WT and KO mice fed with HFD, we conducted intraperitoneal lipid tolerance test (LTT) in these mice. As shown in Figure 11D, we observed slightly better lipid tolerance in WT mice as compared to the KO mice, although the differences between the mean values during the peak were not statistically significant.
Figure 11. Terminal serum triglycerides, free fatty acids and glycerol and lipid tolerance test in the WT and P2Y2 KO mice. Serum samples collected at euthanasia (16-weeks of treatment) were assayed for triglycerides (A), free fatty acids (B) and glycerol (C) by using commercial assay kits. N = 6 samples/genotype for CNT diet, and N = 11 or 13/genotype for HFD groups. Statistics by ANOVA followed by Tukey-Kramer Multiple Comparison Test. (D) Lipid tolerance test (conducted after 14 weeks of HFD treatment): groups of mice (N = 6 mice/genotype) were injected intraperitoneally with 200 μl of Intralipid 20% (vol/vol) fat emulsion, and blood samples were collected at different time points as shown. Plasma samples were analyzed for triglyceride concentration using a commercial colorimetric assay kit. *significantly different from the mean value sin WT mice at the corresponding time point by direct comparison by unpaired t-test.
Relative Expression of Lipases and Fatty Acid Translocase in WT and P2Y2 KO Mice Fed Regular or HFD
To understand the lipolytic activity that may explain the observed significant changes in serum triglyceride and glycerol, we determined the mRNA expression of lipoprotein lipase (LPL), hormone-sensitive lipase (HSL), adipose triglyceride lipase (ATGL) and fatty acid translocase (CD36) in white fat of WT and P2Y2 KO mice fed CNT or HFD. As shown in Figure 12A, regular diet-fed KO mice had significantly higher levels of LPL as compared to the regular diet-fed WT mice. Such a difference in the expression of LPL in the HFD-fed WT vs. KO mice could not be seen. Feeding HFD to WT mice resulted in significant increases in the CD36 as compared to HFD-fed KO mice (Figure 12B). On the other hand, feeding HFD resulted in significant differences between the WT and KO mice with respect to HSL and ATGL (Figures 12C,D).
Figure 12. Relative mRNA expression of lipases in the white adipose tissue of WT and P2Y2 KO mice fed regular or high-fat diets for 16 weeks. Real-time RT-PCR approach was used to determine the mRNA expression of lipases relative to the mRNA expression of β-actin. (A), lipoprotein lipase (LPL); (B), fatty acid translocase (CD36); (C), hormone-sensitive lipase (HSL); and (D), adipose triglyceride lipase (ATGL). N = 6 samples per group. Statistics by ANOVA followed by Tukey-Kramer Multiple Comparison Test.
In this communication, using a mouse model of genetic deletion of P2Y2 receptor, we present compelling experimental evidence that the P2Y2 receptor promotes diet-induced obesity. Specifically, we have shown that: (i) P2Y2 receptor knockout mice are significantly resistant to HFD-induced obesity or weight gain; (ii) P2Y2 receptor promotes HFD-induced inflammation in adipose tissue; (iii) when fed HFD, P2Y2 receptor negatively impacts glucose homeostasis; (iv) P2Y2 receptor is needed for adipogenesis and expansion of adipose tissue; (v) P2Y2 receptor is involved in adipose tissue lipid metabolism; and (vi) the above observed phenomena are not due to reduced consumption of food or loss of undigested fat in the feces (steatorrhea). Hence, we believe that P2Y2 receptor is a potential target for the prevention or treatment of diet-induced obesity, the most common form of obesity seen all over the world.
P2Y2 receptor is a widely expressed purinergic receptor, and it has been the most studied P2 receptor. RT-PCR performed in our laboratory indicated that P2Y2 receptor is expressed in organs or tissues involved in the development of obesity and insulin resistance, such as skeletal muscle, intestines, liver, pancreas, and white and brown adipose tissues (data not shown). The whole-body knockout mice used in this study were generated by targeted mutagenesis of the P2ry2 gene in mouse embryonic stem cells. No differences were detected between the P2Y2 KO and WT mice on histological examination of organs analyzed, including the kidney, heart, testis, pancreas, liver, trachea, lungs, salivary glands and gastrointestinal tract (27, 28). In our experience with these mutant mice for more than a decade, we found that they live a normal and apparently healthy life, and have longevity comparable to the WT mice. We and other investigators have shown that these mice do exhibit renal differences from WT when under various stressors, as previously published (29, 48).
In the current study, we show that KO mice are significantly resistant to high-fat diet (HFD) induced weight gain or obesity. These findings are in agreement with those of Merz et al. (49) who studied the effects of a high-fat/high sugar diet fed for 20 weeks to male P2Y2 whole-body KO mice on a different background strain (C57Bl6). Thus, the finding of relatively “lean phenotype” appears robust and independent of background strain, and dietary sugar. Furthermore, we excluded the possibility of reduced food intake or energy loss in the feces. Food consumption was modestly, but significantly higher in the KO mice vs. WT mice, when normalized to body weight, and feces were free from oil. In fact, we noted that for the same age and sex, the KO mice consistently weighed less than the WT mice, which can be observed in this study on day 0 (Figure 1A), i.e., before starting the HFD. In line with the above in vivo observations with respect to body weight, the WT mice on HFD showed large and significant increases in the amount of white fat, whereas the corresponding increases in the KO mice was not significant. Morphological examination of white adipose tissue from the WT and KO mice fed regular or high-fat diet also revealed alterations that are consistent with the increased amount of white fat in the WT, but not in the KO mice. The absence of P2Y2 receptor in CNT diet-fed KO mice resulted in smaller and poorly filled adipocytes as compared to the CNT diet-fed WT mice. These differences were more pronounced between the HFD-fed WT vs. KO mice. Thus, the morphological examination suggests that P2Y2 receptor is needed for the accumulation of lipids and expansion of adipocyte size. Interestingly, the increased amount of white adipose tissue in WT mice was associated with a 2-fold increase in the mRNA expression of P2Y2 receptor. This suggest that P2Y2 receptor is potentially involved in the expansion of white adipose tissue in response to high-fat diet.
Assay of terminal serum samples showed significantly increased levels of insulin, leptin and adiponectin in HFD-fed WT mice. In contrast, in the HFD-fed KO mice there were no such significant increases. Adiponectin levels may be elevated in the WT-HFD mice due to the development of peripheral adiponectin resistance (50). In general, higher adiponectin levels are associated with improved prognosis in regards to the development of type 2 diabetes mellitus, inflammation, and obesity. Nonetheless, studies conducted in mice specifically, have shown that plasma adiponectin levels can rise over the course of HFD feeding (51), which is consistent with our observations. Thus, WT mice developed many of the standard features of metabolic syndrome after chronic consumption of the high-fat diet, while KO mice were relatively protected. It is unclear from our current study, which, if any of these effects, were direct results of reduced P2Y2 signaling in metabolic tissues, e.g., adipose or liver, or rather than general effects of reduced obesity and inflammatory sequelae. Additional studies with cell-specific P2Y2 deletion are needed to clarify these mechanisms.
Another interesting aspect of our study is how P2Y2 receptor affects glucose homeostasis and insulin sensitivity. HFD-fed WT mice had significantly higher blood glucose levels as compared to HFD-fed KO mice at all the time points of the glucose tolerance test. One can argue that this is because the KO mice were not as obese as the WT mice after feeding HFD. However, the significantly lower mean fasting blood glucose levels in KO mice vs. WT mice suggest that the KO mice are inherently having better glucose homeostasis. The significant differences observed between the WT and KO mice with respect to the insulin tolerance test also suggest that P2Y2 receptor may likely to play a significant role in promoting insulin resistance. This is further supported by the higher level of expression of insulin receptor, insulin receptor substrate-1 (IRS-1) and glucose transporter type-4 (GLUT4) in the white adipose tissue of HFD-fed KO mice vs. HFD-fed WT mice.
Both lipid metabolism and inflammation in white adipose tissue are known to be altered in obesity, and contribute for the development of insulin resistance in obese subjects. Hence, we examined the mRNA expression of inflammatory cytokines and associated molecules in the white adipose tissue of WT and KO mice fed HFD. We observed significantly higher expression of MCP-1, CCR2, CD68, and F4/80 in the white fat of WT mice, as compared to the white fat of KO mice. This finding may also contribute to better glucose homeostasis in the KO vs. WT mice fed HFD. In this context, it has been reported that P2Y2 receptors induce increased MCP-1 synthesis and release from rat alveolar and peritoneal macrophages (52).
Parallel in vitro experiments with preadipocytes derived from the WT or KO mice confirmed that P2Y2 receptor is involved in the differentiation and maturation of preadipocytes into adipocytes with accumulation of lipids in the cells. The suppression of in vitro differentiation and maturation of preadipocytes derived from WT mice by the competitive P2Y2 receptor antagonist, AR-C118925 further validated the involvement of P2Y2 receptor in adipogenesis. Finally, the replication of the effect of AR-C118925 in the 3T3-L1 cell line induced to differentiate into adipocytes provides clinching evidence that the effect seen is independent of cell type, but is related to the activity of P2Y2 receptor. It is interesting to note that just like adipose tissue in vivo, differentiation and maturation of the 3T3-L1 cell line into adipocytes was associated with a 2-fold increase in the P2Y2 receptor mRNA expression.
Adipocytes are derived from pluripotent MSC (mesenchymal stromal cells) that have the capacity to develop into several cell types, such as adipocytes, myocytes, chondrocytes, and osteocytes [reviewed in (53)]. These stem cells reside in the vascular stroma of adipose tissue. When appropriately stimulated (e.g., ATP excess states), these stem cells undergo a process of commitment in which the progenitor cells become restricted to adipocyte lineage. Recruitment to this lineage gives rise to preadipocytes, which when induced, undergo mitotic clonal expansion and differentiate into adipocytes. It has been reported that human adipose tissue derived MSC express several purinergic receptors (P2X and P2Y series), but with a predominant role for P2Y2 and P2Y6 receptors in eliciting intracellular calcium response (54). There is also evidence that purinergic receptors play a role in stem cell differentiation (55). Li et al. (56) concluded that UTP suppresses osteogenic differentiation of bone marrow-derived stromal cells, while enhancing adipogenic differentiation by activating P2Y2 receptor. The effect was apparently mediated through the ERK1/2 signaling pathway. Hence, one may conclude that resistance of the P2Y2 KO mice to HFD-induced obesity may be due to non-committal of the vascular stromal cells into preadipocytes. Our in vitro data where preadipocytes isolated from the P2Y2 KO mice showed impaired differentiation and maturation into adipocytes suggests a role for P2Y2 receptor in this process. However, one can still argue that there may be fewer preadipocytes in the preparation from the P2Y2 KO mice due to non-committal of vascular stromal cells into the preadipocyte lineage. Our in vitro data on preadipocytes derived from the WT mice, where AR-C118925 suppressed adipogenesis counters that argument. This is further strengthened by the suppression of differentiation and maturation of 3T3-L1 cells into adipocytes by AR-C118925. Despite the above, it is possible that P2Y2 receptor may be playing a role in the committal of vascular stromal cells into adipocyte lineage, in addition to its role in the differentiation and maturation of preadipocytes. This aspect needs further investigation using appropriate methods, which are beyond the scope of this communication. The commitment of MSC toward adipogenic or osteogenic lineage involves various signaling pathways. These pathways include: the β-catenin-dependent Wnt, Hedgehog (Hh) and Bone Morphogenetic Protein (BMP) signaling pathways [reviewed in (57)].
The major energy reserve, the triglycerides (TAG) stored in the white adipose tissue, constantly go through cycles of lipolysis and re-esterification in an orderly manner. This is a complex process involving several hormones, receptors, enzymes and other molecules. Since we observed distinct differences in the morphology of white adipocytes in WT and KO mice, suggesting decreased accumulation of TAG in the adipocytes of KO mice, we assayed terminal serum samples for TAG and its metabolites, namely free fatty acids and glycerol, and conducted an intraperitoneal lipid tolerance test. Analysis of serum samples revealed elevated levels of triglycerides in P2Y2 KO mice, irrespective of the dietary regimen, which may reflect altered lipid metabolism in the adipose tissue. However, serum glycerol levels were elevated in both WT and KO mice on HFD relative to control diet, with no genotype difference. Despite these alterations in the serum, the observed differences between HFD-fed WT and KO mice with respect to the lipid tolerance test are minor, and not statistically significant. In fact, if taken as percent changes from baseline or 0 h, these numerical differences were obliterated. It is also possible that the KO mice are able to metabolize lipids more efficiently as compared to the WT mice, as suggested by the metabolic phenotypic data (24). Determination of mRNA expression of key lipases in the white adipose tissue provided some insights into the observed differences in blood lipids. The relatively higher activities of lipoprotein lipase (LPL), hormone-sensitive lipase and adipose triglyceride lipase (ATGL) in KO mice may result in increased blood levels of free fatty acids. However, due to differences in the rates of utilization of free fatty acids between the WT and KO mice, the observed differences in the activities of LPL and ATGL in KO mice might not be reflected in corresponding differences in blood levels of free fatty acids. Based on the current observations, it appears that P2Y2 receptor promotes accumulation of TAG in adipocytes, and suppression of this receptor activity enhances lipolysis resulting in release of free fatty acids and glycerol into the blood. Thus, it appears that the observed changes in the lipid metabolism in the KO mice are due to decreased adipogenesis in the absence of P2Y2 receptor. Obviously, the altered lipid metabolism in the adipocyte of WT and KO mice fed HFD needs further investigation including its effect on hepatic lipid metabolism.
Recently it has been reported that constitutive P2Y2 receptor activity suppresses basal lipolysis in human adipocytes. Ali et al. (58) showed that pharmacological antagonism or knockdown of P2Y2 receptor increases intracellular cAMP levels and enhances basal lipolysis. They also observed that acute enhancement of basal lipolysis following P2Y2 receptor antagonism alters the profile of secreted adipokines leading to long-term adaptive decrease in lipolysis. Based on their findings, Ali et al. (58) concluded that basal lipolysis and adipokine secretion are controlled by autocrine purinergic signaling in human adipocytes. Our above observations on the alterations in plasma lipids and adipokines in P2Y2 receptor KO mice fed high-fat diet are consistent with this report.
Adamson et al. (59) investigated whether mice lacking P2Y2 receptor on myeloid cells, achieved by transplanting bone marrow from P2Y2 receptor knockout mice into normal mice, are protected against acute and chronic inflammation. Based on their data, they concluded that P2Y2 receptor on myeloid cells is important in mediating acute inflammation but is dispensable for the development of whole body insulin resistance in diet-induced obese mice. Thus, it appears that deletion of P2Y2 receptor in adipocytes and other organs, is needed to prevent insulin resistance in obese mice. This aspect needs to be further evaluated using cell-specific knockout models of P2Y2 receptor.
Finally, a recent review of the involvement of purinergic signaling in obesity by Burnstock and Gentile (60) states that currently, no wholly successful pharmacological treatments are available for obesity and related adverse consequences. It also adds that in recent years, hints obtained from several experimental animal models support the notion that purinergic signaling, acting through ATP-gated ion channels (P2X), G protein-coupled receptors (P2Y), and adenosine receptors (P1), is involved in obesity, both at peripheral and central levels. Thus, while this review provides “proof of concept” for the involvement of purinergic signaling in obesity, our data provide much needed evidence by focusing on the role of P2Y2 receptor in diet-induced obesity. Furthermore, a recent report by Negri et al. (61) also confirmed that P2Y2 receptor is a regulator of the formation of cardiac adipose tissue and its fat-associated lymphoid clusters. Using the same model of P2Y2 receptor knockout mouse, but in C57/Bl6 genetic background, specifically the report presented similar findings as shown in this paper with respect to the role of P2Y2 receptor in differentiation and maturation of preadipocytes derived from pericardial fat, and promoting inflammation in pericardial adipose tissue. Thus, it is clear that P2Y2 receptor plays a role in adipogenesis and thus diet-induced obesity.
We demonstrated that genetic deletion of P2Y2 receptor significantly protects mice against high-fat diet-induced obesity. Based on the experimental evidence presented, this protection is not due to reduced consumption of food or loss of undigested fat through feces. On the other hand, in vivo and in vitro data suggest that P2Y2 receptor plays a role in adipogenesis and expansion of adipose tissue, adipocyte lipid metabolism, and inflammation in white adipose tissue, and thus promotes glucose intolerance and/or insulin resistance. We consider that this communication represents a significant forward step in our understanding of the pathophysiology of obesity as it relates to purinergic signaling.
Data Availability Statement
The datasets generated for this study are available on request to the corresponding author.
The animal study was reviewed and approved by Institutional Animal Care and Use Committee of the VA Salt Lake City Health Care System.
Parts of this work has been presented at the Kidney Week 2013 of the American Society of Nephrology, November 2013, Atlanta, GA, Experimental Biology 2015 meeting, April 2015, Boston, MA, and Kidney Week 2016 of the American Society of Nephrology, November 2016, Chicago, IL, and appeared as printed abstracts in the proceedings of those meetings (23, 24).
YZ, CE, and BK were involved in conception and design of research and drafted the manuscript. YZ and BK performed the experiments and prepared the figures. CM synthesized and analyzed AR-C118925 and provided expert advice on its use. LL provide expert advice on induction of adipogenesis in vitro. YZ, CE, LL, and BK interpreted results of the experiments. YZ, CE, LL, CM, and BK edited and revised the manuscript and approved the final version of the manuscript.
This work was mainly supported by the Merit Review Program of the US Department of Veterans Affairs, and the resources and facilities at the VA SLC Health Care System, Salt Lake City, Utah (YZ, BK, and LL). Additional funding sources include Eye Foundation of America, Morgan Town, WV, and National Kidney Foundation of Utah & Idaho, Provo, Utah. CE was supported by Georgetown University Biograduate Research Organization and a Marriott Cardiovascular Fellowship. LL was supported by VA Merit Review I01BX004492 and NIH R01 AG048366. CM was supported by Deutsche Forschungsgemeinschaft (FOR2372, GRK1873, SFB1328).
The use of P2Y2 receptor antagonists for the prevention and/or treatment of diet-induced obesity is proprietary to the US Department of Veterans Affairs and the University of Utah Research Foundation in partnership with Georgetown University, and is protected by US Patents No. 10,107,795 and 10,024.846 (25, 26) and International Patent Filing WO 2014066830.
Conflict of Interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
The authors thank Dr. Beverly Koller for generously supplying breeders of P2Y2 receptor null and congenic wild type mice, and Kristina M. Heiney, David L. Strasburg, Anna Brandes, and Tao Liu for technical assistance.
WT, Wild Type; KO, Knockout; CNT, Control diet; HFD, High-fat diet; R, Receptor; BW, Body Weight.
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Keywords: purinergic signaling, obesity, adipose tissue, AR-C 118925, insulin resistance, inflammation, glucose homeostasis, lipid tolerance
Citation: Zhang Y, Ecelbarger CM, Lesniewski LA, Müller CE and Kishore BK (2020) P2Y2 Receptor Promotes High-Fat Diet-Induced Obesity. Front. Endocrinol. 11:341. doi: 10.3389/fendo.2020.00341
Received: 22 January 2020; Accepted: 30 April 2020;
Published: 03 June 2020.
Edited by:Claire Joanne Stocker, University of Buckingham, United Kingdom
Reviewed by:Lila Oyama, Federal University of São Paulo, Brazil
Diana Patricia Portales-Perez, Universidad Autónoma de San Luis Potosí, Mexico
Copyright © 2020 Zhang, Ecelbarger, Lesniewski, Müller and Kishore. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Bellamkonda K. Kishore, firstname.lastname@example.org