The Berlin Fat Mouse Inbred (BFMI) line harbors a major recessive gene defect on chromosome 3 (jobes1) leading to juvenile obesity and metabolic syndrome. The present study aimed at the identification of metabolites that might be linked to recessively acting genes in the obesity locus. Firstly, serum metabolites were analyzed between obese BFMI and lean B6 and BFMI × B6 F1 mice to identify metabolites that are different. In a second step, a metabolite–protein network analysis was performed linking metabolites typical for BFMI mice with genes of the jobes1 region. The levels of 22 diacyl-phosphatidylcholines (PC aa), two lyso-PC and three carnitines were found to be significantly lower in obese mice compared with lean mice, while serine, glycine, arginine and hydroxysphingomyelin were higher for the same comparison. The network analysis identified PC aa C42:1 as functionally linked with the genes Ccna2 and Trpc3 via the enzymes choline kinase alpha and phospholipase A2 group 1B (PLA2G1B), respectively. Gene expression analysis revealed elevated Ccna2 expression in adipose tissue of BFMI mice. Furthermore, unique mutations were found in the Ccna2 promoter of BFMI mice which are located in binding sites for transcription factors or micro RNAs and could cause differential Ccna2 mRNA levels between BFMI and B6 mice. Increased expression of Ccna2 was consistent with higher mitotic activity of adipose tissue in BFMI mice. Therefore, we suggest a higher demand for PC necessary for adipose tissue growth and remodeling. This study highlights the relationship between metabolite profiles and the underlying genetics of obesity in the BFMI line.
Obesity results from a sedentary lifestyle with malnutrition and low physical activity and is a risk factor for the development of the metabolic syndrome. The increasing number of obese humans correlates with the incidence of diabetes mellitus and coronary heart diseases (Kopelman 2000). Therefore, biomarkers for the diagnosis of metabolic dysfunctions would be desirable to initiate prevention or therapeutic programs early in life. A new approach for biomarker identification is the metabolomics (Shaham et al. 2008; Shah et al. 2010; Wang-Sattler et al. 2012).
As an emerging technology, metabolic profiling comprises the identification and quantification of molecules with a small molecular weight in biological fluids (Nicholson et al. 1999). Metabolites are influenced by factors such as age, sex and diet but also diseases such as diabetes (Williams et al. 2005; Lutz et al. 2006; Kim et al. 2011; Mittelstrass et al. 2011; Yu et al. 2012; Wang-Sattler et al. 2012). In mice, studies suggested metabolic profiling to be a surrogate for detecting dietary-induced insulin resistance or diabetes (Shearer et al. 2008). For example, previously, N-acetyl-l-leucine was identified as a potential biomarker for diabetes (Tsutsui et al. 2011). In humans, metabolic profiling was used to find alteration of plasma lipids to differentiate between healthy and diabetic subjects (Wang et al. 2005). In addition, three lyso-phosphatidylcholines (lysoPC) were reported as potential biomarkers for overweight in humans (Kim et al. 2010). Some studies associated metabolomics and transcriptomics to uncover the relationship between metabolites and gene expressions in different species (Askenazi et al. 2003; Bono et al. 2003; Urbanczyk-Wochniak et al. 2003; Hirai et al. 2004). Albeit several epidemiological studies and genome-wide association studies have repeatedly demonstrated that the development of obesity also depends on the genetic predispositions (Stunkard et al. 1986; Allison et al. 1996; Barsh et al. 2000; Speliotes et al. 2010), most metabolomic studies have not considered the underlying genetics.
Genetically well-defined mouse inbred models for obesity can contribute to identify metabolic markers for obesity and to link them to genetic determinants. We examined the Berlin Fat Mouse Inbred (BFMI) line which develops juvenile obesity (Wagener et al. 2006). Young BFMI mice are hyperphagic and develop the metabolic syndrome with impaired insulin sensitivity which was more pronounced on a high fat diet (HFD), and high serum triglyceride levels (Meyer et al. 2009; Hantschel et al. 2011). A region on chromosome 3, named jObes1, showed strong recessive gene effects on the obesity phenotype in a linkage study in the cross BFMI × C57BL/6NCrl (B6) (Neuschl et al. 2010).
The aim of the present study was the identification of candidate genes which are responsible for metabolite profiles associated with obesity in the obese BFMI mouse model. We have analyzed metabolites in BFMI mice in comparison with lean B6 mice and the F1 offspring of the cross BFMI × B6 which are lean as well due to the recessive jobes1 effect. A metabolite–protein network analysis was performed connecting significantly differentially regulated metabolites with candidate genes for obesity of the jObes1 region on mouse chromosome 3.
Materials and methods
Animals and diets
In this study we used the lines BFMI860/Hber (BFMI) and C57BL/6NCrl (B6) and F1 individuals generated by crossing BFMI and B6 mice. A detailed description of the breeding history of the BFMI line is outlined in Wagener et al. (2006). In brief, the BFMI line was generated from the outbred population Berlin Fat Mouse (BFM). Founders of BFM mice were originally purchased from pet shops and subsequently selected first for low protein content, second for low body mass and high fat content and then for high fatness for 58 generations before inbreeding. As no control line of the selection experiment exists, we used B6 mice of the substrain C57BL6/NCrl as lean controls (Charles River Laboratories, Sulzfeld, Germany) which were also used to map genetic loci affecting obesity in the cross BFMI × B6 (Neuschl et al. 2010). Mice were reproduced in our animal facility at the Humboldt-Universität zu Berlin. Mice were kept at room temperature (22–24 °C) with a light dark cycle of 12 h. After weaning at the age of 3 weeks, 4–5 mice of each line (BFMI, B6 and F1) and of each sex were randomly chosen and placed on either a standard maintenance diet (SMD) containing 12.8 MJ/kg metabolizable energy with 9 % of its energy from fat, 33 % from protein content and 58 % from carbohydrates (V1534-000 ssniff R/M-H, ssniff Spezialdiäten GmbH, Soest, Germany) or a HFD containing 19.1 MJ/kg metabolizable energy with 45 % of its energy from fat, 24 % from protein content and 31 % from carbohydrates (S8074-E010 ssniff EF R/M, ssniff Spezialdiäten GmbH, Soest, Germany). The standard diet derived its fat from soy oil, whereas the high-fat diet derived its fat from coconut oil and suet. The animals had ad libitum access to diets and water. All animal treatments were in accordance to the German Animal Welfare Legislation (approval no. G0152/04, T0149/04).
Body weight, body composition, blood collection and the measurement of serum parameters
At the age of 10 weeks body weight and body fat mass were determined by a quantitative magnetic resonance analysis using the EchoMRI whole body composition analyzer (Echo Medical Systems, Houston, Texas, USA) (Taicher et al. 2003; Tinsley et al. 2004). The recorded fat mass represented the total fat mass in the body.
After a fasting period of 2 h and anesthesia with isofluran, 10 weeks old mice were sacrificed and reproductive adipose tissue, liver, brain, pancreas and blood was collected. Serum was recovered by centrifugation for 15 min at 600×g. Serum and tissues were stored at −80 °C until analysis.
Serum triglycerides were determined using the Fluitest TG (Analyticon Biotechnologies AG, Lichtenfels, Germany). Serum non-esterifies free fatty acids (NEFAs) were measured using the NEFA-HR(2) kit (Wako Chemicals GmbH, Neuss, Germany).
Measurement of metabolites
For the measurement of metabolites a 10 μl volume of serum samples was used. The Hamilton Star robotics (Bonaduz, Switzerland) was used for liquid handling of samples. A total of 163 metabolite molecules including 41 acylcarnitines, 14 amino acids, one sugar, 92 glycerophospholipids and 15 sphingolipids were measured (Table S1) using the AbsoluteIDQ TM p150 Kit following the manufacturer’s instructions (BIOCRATES Life Sciences AG, Innsbruck, Austria) on the ion trap mass spectrometry API 4000 Q TRAP LC/MS/MS System (Applied Biosystems Deutschland GmbH, Darmstadt, Germany). The AbsoluteIDQ TM p150 kit has been described in detail previously (Illig et al. 2010; Römisch-Margl et al. 2011). Analytics were calculated in μmol concentrations using the MetIQ software which was integrated in the AbsoluteIDQ TM kit. To control the quality of metabolites, the coefficients of variation (CV) were calculated using the reference samples for each metabolite and 43 metabolites with CV higher than 0.2 were excluded and 120 metabolites were remained for further analysis (Mittelstrass et al. 2011; Wang-Sattler et al. 2012).
ANOVA of phenotypes and metabolites
Phenotypic data were analyzed by performing the analysis of variance (ANOVA) to assess the effect of lines using the SAS version 9.1.3 (SAS Institute Inc., Cary, NC, USA). Multiple pairwise comparisons were Bonferroni-corrected. Gene expression data analysis was performed using a two tailed student’s t-test (GraphPad Prism 5 Software, San Diego, CA/USA). Differences were considered statistically significant at p < 0.05.
The remaining 120 out of 163 metabolites were log-transformed to remove skewness. In a first analysis the effects of sex, diet, and line on metabolite levels of BFMI, B6, and F1 mice were assessed by ANOVA. To further test the recessive allele effect associated with obesity in BFMI mice, B6 and F1 mice were combined to one group which was compared with BFMI mice in a second analysis. B6 and F1 mice were both lean and did not differ in fat deposition.
Metabolites differing significantly between BFMI mice and the group of B6 and F1 mice, that showed the expected recessive allele effect, were selected for further analyses.
Random forest, stepwise selection methods and candidate metabolite selection
To select candidate metabolites that are linked to genetic differences between obese and lean mice, we applied two more methods, the non-parametric random forest (Breiman 2001) and the parametric stepwise selection, which assessed the metabolites as a group. The supervised classification method random forest was used to select metabolites of importance among the 31 highest ranking variables between the two groups of obese and lean mice. Those 31 metabolites showed most impact on obesity in the internal permutation test of random forest. Furthermore, selected metabolites were used for a stepwise selection method on the logistic regression model. Here, metabolites were used which showed both significantly different concentrations between the two compared groups in the logistic regression and which were also selected using random forest. Those metabolites were added and dropped from the model one by one. Akaike’s Information Criterion (AIC) was used to evaluate the performance of the subsets of metabolites used in the models. The model with minimal AIC was finally chosen and metabolites left in this model were potential independent metabolites that best distinguish lean from obese mice. Correlated metabolites with less separation power were dropped. The area under the receiver-operating-characteristic curves (ROC) was used to evaluate the models and a likelihood ratio test was used to compare the models. Calculations were performed under the R statistical environment (R Core Team 2013).
Metabolite–protein interactions from the Human Metabolome Database (HMDB) (Wishart et al. 2009) and protein–protein interactions in the Search Tool for the Retrieval of Interacting Genes/Proteins (STRING) (Jensen et al. 2009) were used to construct a network containing relationships between metabolites, enzymes and obesity-related genes (He et al. 2012; Xu et al. 2013). The candidate metabolites were assigned to the HMDB IDs using the metaP-Server (Kastenmuller et al. 2011). Their associated enzymes were derived according to the annotations provided by HMDB. We chose six obesity candidate genes of the jObes1 region on chromosome 3 to connect metabolites through the associated enzymes. In the search for links, we allowed an intermediate protein through STRING and optimization by eliminating edges with a STRING score below 0.7 and undirected paths. The sub-networks were connected by the shortest path from metabolites to obesity candidate genes.
Gene expression analysis and sequencing
Gene expression analyses were performed with SMD-fed male mice of BFMI, B6 and F1 (n = 5–9 per group). Total RNA was isolated from liver, brain and pancreas using the nucleic acid and protein purification kit (Machery-Nagel, Düren, Germany) following the suppliers protocol, and from reproductive adipose tissue by acid guanidinium thiocyanate–phenol–chloroform extraction. Genomic DNA was removed using the Turbo DNA-free TM Kit (Applied Biosystems, Foster City CA/USA; Ambion, Austin TX/USA). 1 μg RNA was reverse-transcribed into cDNA using AccuScript® High Fidelity Transcriptase and oligo-dT primers according to the manufacturer’s instructions (Stratagene Europe, Agilent Technologies, Waldbronn, Germany). Primers for quantitative real-time PCR were designed using Primer3 software (http://frodo.wi.mit.edu/) and are given in Table S4. Primers were checked with a 20 μl control PCR contained 50 ng cDNA, 10 μM of each primer pair and 1 Unit FIRE-Pol® DNA Polymerase (Solis BioDyne, Tartu, Estonia) with a three step PCR standard program. Fragment length of PCR products were checked on an agarose gel. Quantitative real-time PCR was performed in a total reaction volume of 10 μl containing MasterMix Plus for SYBR® Assay (Eurogentec, Cologne, Germany), 10 ng cDNA and 10 μM of the gene specific primers. Triplicates were measured on ViiaTM 7 Real-Time PCR System (Applied Biosystems, Darmstadt, Germany). Gene expression was calculated as relative quantity (RQ) using the ΔΔCt method (Livak and Schmittgen 2001). As endogenous controls, Rps25 and b-Actin were chosen and gene expression was calculated relative to the group of B6 and F1 mice, normalized to a value of 1.
The coding region and 420 bp upstream of the first exon of Ccna2 were sequenced using cDNA and genomic DNA of BFMI and B6 mice, respectively. Genomic DNA was extracted from spleen using phenol and chloroform in a standard procedure. Sequencing primers were designed with DNASTAR software (DNASTAR Inc., Madison, USA) and are given in Table S4. PCR products, amplified using standard methods, were cut from a 2.0 % agarose gel and purified using GeneJETTM Gel Extraction Kit (Fermentas, St. Leon-Rot, Germany). The sequence reactions in both directions were performed with BigDye® Terminator v1.1 Ready Reaction Cycle Sequencing Kit and an ABI PRISM® 310 Genetic Analyser (Applied Biosystems, Darmstadt, Germany) following manufacturers instruction. Sequences were assembled and analyzed using the DNASTAR software (DNASTAR Inc., Madison, USA). The chromosome position of found variations and reference alleles are based on Ensembl release 67—May 2012, Mouse (NCBIM37). Transcription factor binding sites were determined with the web tool CONSITE (Sandelin et al. 2004) using human and mouse transcription factor model matrices and a scoring threshold of 80 %. The 3′ UTR of the Ccna2 reference transcript (NM_009828) was scanned for binding sites of known mouse miRNAs using the web program PITA (Kertesz et al. 2007) with standard parameters. Resulting energetic scores estimate the free binding energy in the seed region of the miRNA–mRNA duplex and thus the binding strength of the miRNA to the given 3′UTR site. Only scores equal or below −10 were considered as these are likely to be functional in endogenous miRNA expression levels (Kertesz et al. 2007). Expression data of transcription factors were taken from the arrays GeneAtlas MOE430 and GNF1M via the web tool BioGPS (http://biogps.org). MicroRNA expression data were obtained from the Gene Expression Atlas (http://www.ebi.ac.uk/gxa/).
Results and discussion
Phenotypic and metabolic characteristics of BFMI, B6 and F1 mice
Ten weeks old BFMI males on standard maintenance diet (SMD) had a 4.1 and 4.6 and females a 3.0 and 2.2 times higher body fat content compared to male and female B6 and F1 mice (p < 0.001) respectively (Table 1). Feeding a high-fat diet (HFD), all mice gained additional fat mass. Due to the recessive jObes1 effect in BFMI mice leading to obesity (Neuschl et al. 2010) BFMI males showed 3.1- and 2.2-fold and females 3.0- and 2.8-fold higher body fat content at 10 weeks compared with its B6 and F1 counterparts (p < 0.001), respectively (Table 1). In addition, serum concentrations of NEFAs were about 1.4 times elevated (p < 0.01) in both sexes of BFMI mice fed an SMD compared with lean F1 and B6 mice. The differences were lower in HFD-fed mice with only 1.05 and 1.25 times increased NEFAs in BFMI males and females, respectively. In accordance to the recessive jObes1 effect, F1 and B6 males showed no statistical difference in their body fat content and NEFA serum levels, neither on SMD nor on HFD (Table 1). In contrast, serum triglyceride levels of BFMI mice were about two times as high as in B6 mice on both diets and both sexes (p < 0.001), but they showed no difference to lean F1 animals which had also high triglyceride serum levels.
For the determination of metabolite profiles, metabolites were first compared between the high-fatness selected obese BFMI line with lean B6 and BFMI × B6 F1 mice in both sexes and on two diets. Out of 163 targeted metabolites 120 were above the detection limit and passed the quality control and, therefore, were used in this study; 14 metabolites differed between BFMI and B6 or between BFMI and F1 mice (Table S2). B6 and F1 mice did not differ in their metabolite concentrations indicating that the recessive genetic defect of BFMI mice is mainly responsible for metabolic differences when comparing lean and BFMI mice. Although sex differences in the metabolic profile had been reported in humans (Lutz et al. 2006; Mittelstrass et al. 2011), ANOVA provided evidence that the sex had no effect in this study. Furthermore, also the diet had almost no effect, except for diacyl-phosphatidylcholine (PC aa) C42:2 which was affected by diet, but not by line (Table S2). Therefore, the metabolite PC aa C42:2 as well as the factors sex and diet were not considered in subsequent analyses. As the focus of this study was on differences in metabolite concentrations due to genetic variations between obese BFMI and lean B6 and F1 mice, all BFMI mice of the SMD and HFD groups were combined to one group of obese mice whereas all B6 and F1 mice were combined to a group of lean mice. This is consistent with our expectation of the recessive mode of action of the obesity effect of the BFMI line leading to juvenile obesity. Due to the increase of group sizes further 18 metabolites were identified to be different between obese BFMI and the lean mice in addition to the 13 metabolites that differed between BFMI and either B6 or F1 mice (Table 2). Overall, BFMI mice had a reduction in 12 serum PC aa, 10 PC ae, 2 lysoPC, 3 acylcarnitines and increased levels of 3 amino acids and 1 sphingomyeline when comparing to lean mice. Because these 31 metabolites differed between obese BFMI and lean B6 and F1 mice, we suggest that at least one gene of the genomic chromosome 3 region, responsible for obesity in BFMI mice, accounts for the amount of at least one metabolite in serum of the mice.
Most metabolites that differed between obese and lean mice belonged to the group of glycerophospholipids that were all significantly lower in BFMI mice (p < 0.05). The glycerophospholipid PC aa C42:1 showed highest significance (p = 0.005). The amino acids serine, glycine and arginine and one hydroxyshingomyelin C22:1 (SM (OH) C22:1) were higher in BFMI mice.
Selection of candidate metabolites
Using the 31 metabolites that were found to be significantly different between lean and obese mice, the random forest analysis identified the acylcarnitine C14, the amino acid serine and PC aa C42:1 with high confidential ROC curve AUC-scores of 0.752, 0.711 and 0.725, respectively, as those metabolites that were mainly affected by the genetic background and explained best the genetic differences between lean and obese mice. Serum serine level was increased in the obese line compared with lean mice, while the amount of acylcarnitine C14 and PC aa C42:1 was reduced in BFMI mice. To find the obesity candidate genes which might be involved in the regulation of metabolites, the selected candidate metabolites were connected to obesity candidate genes of the chromosome 3 jObes1 region by a network analyses. Out of the three significant metabolites, only PC aa C42:1 showed a functional link to the obesity candidate genes of the jObes1 locus. In detail, PC aa C42:1 showed a connection to the genes encoding for cyclin A2 (Ccna2) and the transient receptor potential cation channel subfamily C, member 3 (Trpc3) (Fig. 1) of the jObes1 locus. The interaction is given via the enzymes choline kinase alpha (CHKA) and PLA2G1B, respectively.
Obesity candidate gene characterization
To characterize the potential impact of the obesity candidate genes on the lower PC aa C42:1 serum metabolite level in BFMI mice, gene expression analyses of the network genes Ccna2, Chka, Pla2g1b and Trpc3 were performed. Although weakly expressed, the obesity candidate gene Ccna2 was 2.3-times up-regulated in BFMI compared with B6 and F1 mice in the reproductive adipose tissue (Fig. 2). However, the adipogenic mRNA amount of Chka encoding the interacting enzyme did not differ between BFMI and B6 mice. In the liver, only Chka was found to be expressed, whereas Ccna2 mRNA was not detected. The hepatic Chka expression did not differ between groups. Pla2g1b and Trpc3 were expressed neither in the reproductive adipose tissue nor in the liver, but could be detected in the pancreatic and brain tissue, respectively. However, as only Ccna2 and Chka were expressed in adipose tissue which is one of the main sites for metabolite metabolism, only Ccna2 seems to be the obesity gene which contributes to reduced serum phosphatidylcholine concentrations in BFMI mice.
To further characterize the different expressions of Ccna2 between BFMI and B6 mice, comparative sequencing of the promoter and coding regions was performed. Overall, 29 mutations were found when comparing the sequences, thereof 24 SNPs and five InDels. One deletion in the promoter region, two SNPs in the 5′ untranslated region (UTR), one coding SNP in exon 1, one SNP and three InDels in the 3′UTR were unique to the BFMI line compared with the reference sequence of B6 and the SNP database (Welcome Trust Sanger Institute, http://www.sanger.ac.uk/cgi-bin/modelorgs/mousegenomes/snps.pl) (Table 3). The two SNPs in the protein coding region were synonymous. The in silico analysis of the detected variants revealed seven SNPs and one InDel in the sequenced 420 bp promoter region as well as two SNPs in the 5′-UTR/exon1 region that are predicted to gain or lose transcription factor binding sites or modify the binding capacity in BFMI mice compared with B6 (Table 3). Furthermore, seven SNPs and two insertions create new micro RNA recognition sites and one SNP, one deletion and the two insertions lead to the loss of micro RNA binding sites in the 3′ UTR (Table 3). Since some transcription factors and micro RNAs occur in the adipose tissue (Table S3), both variations in the promoter and the 3′ UTR could affect the amount of Ccna2 transcripts in the adipose tissue.
Metabolite pathways and the biological context
Generally, PCs account for 50 % of eukaryotic membrane phospholipids (van Meer et al. 2008) and are essential for coating lipid droplet surfaces (Krahmer et al. 2011). Further, PCs stimulate adipocyte differentiation and increase triglyceride levels of 3T3-L1 and preadipocytes (Zhang et al. 2009). Apart from structural functions of PCs in membranes, they serve as substrates for the synthesis of diacylglycerides and subsequent triglycerides and free fatty acids in the liver. In the BFMI line lowered levels of several serum PCs and higher triglyceride and free fatty acid synthesis compared with lean mice also indicate the important role of PCs in fat metabolism. Therefore, PC emerged as most interesting metabolite in connection with obesity, but a direct link between the specified PC aa C42:1 and obesity has not been found in the literature now.
Within the metabolite–protein network the interaction of PC aa 42:1 with the obesity candidate genes Ccna2 and Trpc3 was given via the enzymes CHKA and PLA2G1B, respectively. However, only Ccna2 and Chka were expressed in adipose tissue which is one of the main sites for metabolite metabolism. Thus, Ccna2 seemed to be the obesity gene which contributed to lower serum PC concentrations in BFMI mice. The functional role of the pathway including the enzyme CHKA and PC aa C42:1 became evident as CHKA catalyzes the initial phosphorylation step of choline within PC synthesis via the cytidine diphosphocholine pathway (Kent 2005). CCNA2 in turn is a cyclin family member, which is well known to regulate mitotic cell division by associating to cyclin dependent protein kinases (Johnson and Walker 1999). A gene disruption resulted in embryonic lethality (Murphy et al. 1997) demonstrating its essential regulatory role. An elevated expression of Ccna2 in the reproductive adipose tissue of BFMI mice likely leads to increased mitotic activity of adipocytes. While there was no indication for an increased adipocyte number in BFMI mice (Wagener et al. 2010), the size of adipocytes was increased to compensate the higher lipid storage and an ongoing turnover of adipocytes can be assumed. This assumption is in line with human studies reporting on more newly generated adipocytes in obese adults than in lean adults, despite constant adipocyte numbers (Spalding et al. 2008).
An increased adipocyte turnover in BFMI mice required PCs as an essential membrane component. PC aa C42:1 seemed to be one of the major membrane PCs that may be regulated by Ccna2 in the obese line. The demand for high PC amounts for membrane production was jointly responsible for lower available serum PCs in BFMI mice, in particular as cytidinediphosphocholine pathway seemed to be normal which was indicated by unchanged Chka expression between obese and lean mice.
Since no hepatic Ccna2 expression could be detected in BFMI and B6 mice, we suggest a tissue-specific expression pattern which goes along with the specific increase of adipocyte production in obese subjects. The genetic modifications in the promoter region of Ccna2 cause new or lost putative transcription factor binding sites in the BFMI line and might be responsible for differential regulation of expression between lean and obese mice. Furthermore, an increase in mRNA stability due to the comprehensive variations in the 3′ untranslated region cannot be excluded and could lead to increased translation ending in a higher CCNA2 protein availability within the adipose tissue of BFMI mice. Since several binding sites of transcription factors and miRNAs that occur in adipose tissues are modified, the transcriptional or translational regulation of the alternative Ccna2 haplotype in BFMI is likely.
The second pathway branch linked Trpc3 with PC aa C42:1 via PLA2G1B. Trpc3 as a member of the transient receptor potential superfamily encodes for cation channels. Cations such as calcium are required for PLA2G1B action which is secreted by the pancreas into the intestinal lumen to digest dietary fatty acids (Carey et al. 1983). Since no gene expression of Trpc3 was observed either in the reproductive adipose tissue or in the liver between BFMI and B6 mice, we assumed that this pathway is not involved in the regulation of PC aa C42:1.
In the present study, serum metabolites of genetically obese BFMI and lean mice were compared. Secondly, significantly different metabolites were linked with underlying obesity candidate genes revealing PC aa C42:1 as being influenced by the genetic background for obesity in BFMI mice. Ccna2 and Trpc3 were selected as candidate genes affecting PC aa C42:1 serum levels via the enzymes CHKA and PLA2G1B. To uncover the biological context of the specified PC aa C42:1 and respective genes, expression analysis and comparative sequencing were performed in BFMI and lean mice. Unique mutations in the Ccna2 promoter of obese mice were identified which are located either in transcription factor or micro RNA binding sites. These genetic modifications are postulated to affect Ccna2 gene expression in adipose tissue likely leading to higher mitotic activity of adipocytes. In conclusion, adipose tissue growth and remodeling are increased in obese mice and cause a higher demand of specific PCs.
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We thank Claudia Hantschel for preparation of cDNA, Ying He for support in bioinformatics and Cornelia Prehn, Werner Roemisch-Margl, Julia Scarpa, Katharina Sckell and Arsin Sabunchi for the metabolomics measurements performed at the Helmholtz Zentrum München, Genome Analysis Centre, Metabolomics Core Facility. This research and Asja Wagener were supported by grants from the German National Genome Research Network (NGFN: 01GS0829) and in part by a grant from the German Federal Ministry of Education and Research (BMBF) to the German Center for Diabetes Research (DZD e.V.). Nadine Schäfer and Marion Millrose were supported by the German Research Foundation (GRK1208).
Conflict of interest
The authors declare that they have no conflict of interests.
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Schäfer, N., Yu, Z., Wagener, A. et al. Changes in metabolite profiles caused by genetically determined obesity in mice. Metabolomics 10, 461–472 (2014). https://doi.org/10.1007/s11306-013-0590-1