- Open Access
Sex-specific lipid molecular signatures in obesity-associated metabolic dysfunctions revealed by lipidomic characterization in ob/ob mouse
Biology of Sex Differences volume 10, Article number: 11 (2019)
The response to overfeeding is sex dependent, and metabolic syndrome is more likely associated to obesity in men or postmenopausal women than in young fertile women. We hypothesized that obesity-induced metabolic syndrome is sex dependent due to a sex-specific regulation of the fatty acid (FA) synthesis pathways in liver and white adipose depots. We aimed to identify distinctive molecular signatures between sexes using a lipidomics approach to characterize lipid species in liver, perigonadal adipose tissue, and inguinal adipose tissue and correlate them to the physiopathological responses observed. Males had less total fat but lower subcutaneous on visceral fat ratio together with higher liver weight and higher liver and serum triglyceride (TG) levels. Males were insulin resistant compared to females. Fatty acid (FA) and TG profiles differed between sexes in both fat pads, with longer chain FAs and TGs in males compared to that in females. Remarkably, hepatic phospholipid composition was sex dependent with more abundant lipotoxic FAs in males than in females. This may contribute to the sexual dimorphism in response to obesity towards more metaflammation in males. Our work presents an exhaustive novel description of a sex-specific lipid signature in the pathophysiology of metabolic disorders associated with obesity in ob/ob mice. These data could settle the basis for future pharmacological treatment in obesity.
The liver is the main site for endogenous synthesis of fatty acids (FAs), and the adipose tissue (AT) is a major storage depot for excess lipids. In obesity, imbalance between energy intake and energy expenditure leads to storage of ectopic fat, as triglycerides (TGs) in non-adipose tissues including liver. Dysregulation of hepatic de novo lipogenesis (DNL) is a common feature of obesity and obesity-associated metabolic diseases such as insulin resistance (IR) and non-alcoholic fatty liver (NAFL). Hence, it is not surprising that extensive efforts have been committed to understand the link between obesity and these diseases. Fat metabolism is regulated by DNL/lipid uptake and lipolysis/oxidation of TGs and FAs. During a period of excess food intake, there is an imbalance between these two systems that drives towards more fat storage. Subcutaneous adipose tissue (SAT) acts as a powerful metabolic sink for FAs and TGs but, as adipocytes grow larger, they become dysfunctional and release FA metabolites that are the major cause of lipotoxicity and inflammation . IR is associated with an increased adipocyte lipolysis with abundant circulating free FAs . In addition, free FAs cause changes in membrane fluidity and availability of cell signaling molecules due to their effects on the lipid bilayer phospholipid (PL) molecular species composition . In obese mice, lipid accumulation and alteration of PL composition promote IR  being many PL molecular species pro- or anti-inflammatory .
Despite the numerous metabolic studies on obesity, sex specificity during obesity has been poorly investigated. Clinical studies showed that women are more responsive to stimuli that increase the drive to eat , more affected by obesity, and more resistant to weight loss . In humans, sexual dimorphism has been described not only related to body weight control, but also to body composition, fat distribution, and fuel metabolism [8,9,10]. Therefore, a sex-specific regulation on the expression of genes involved in lipid metabolism pathways is likely to occur. Interestingly, while obesity is more prevalent in women than in men , the latter are more prone to metabolic disorders . Visceral adipose tissue (VAT) is increased in males and is considered a more metabolically deleterious AT depot than SAT . The type of adipocytes, their endocrine function, lipolytic activity, response to insulin, and other hormones differ between the two fat depots.
We aimed to identify whether there is sexual dimorphism in lipid metabolism. For this purpose, we used the ob/ob mouse, a well-recognized model of human obesity . To better understand sex-dependent FA synthesis pathways leading to obesity, we aimed to identify distinctive molecular signatures between genders, using a lipidomics approach, to characterize lipid species in liver, perigonadal visceral adipose tissue (gAT), and subcutaneous inguinal adipose tissue (iAT), and to correlate them to the physio pathological responses observed. The use of ob/ob mouse model was motivated by the possibility to induce obesity on a chow diet where most of the differences in the lipid species found by lipidomic analysis are the result of de novo FA synthesis.
Research design and methods
Weight-matched 7–8-week-old ob/ob (B6.V-Lepob/J) female (F) and male (M) mice and, C57Bl/6J wild-type (WT) F and M mice, F estrogen receptor (ER) α knockout (ERαKO), and ERβ knockout (ERβKO)  mice were maintained in a temperature-controlled 12-h light/darkroom with free access to water and chow diet (R34, Lantmännen, Lantbruk, Sweden) or high-fat diet (HFD, research diet D12492). C57Bl/6 M mice have very low level of testosterone ; therefore, we used C57Bl/6 M mice to avoid to castrate males and stay in physiological conditions. Half of the WT M on HFD were treated IP, every other day, with estrogen (E2, 0.05 mg/kg body weight) for 3 weeks. For the ob/ob mice group, food intake was measured twice a week over the 5-week experimental period. Mice were anesthetised with 4% isoflurane at 9 AM, blood was immediately collected by heart puncture, and mice were euthanised by cervical dislocation. Liver, gAT (as a representative of visceral adipose tissue (VAT)), and iAT (as a representative of subcutaneous adipose tissue (SAT)) were collected and fixed in paraformaldehyde (PFA) or immediately frozen in liquid nitrogen for further analysis. The local Ethical Committee of the Swedish National Board of Animal Research approved all experiments.
Magnetic resonance imaging/body adiposity
Total body fat mass and lean mass were assessed using magnetic resonance imaging system (EchoMRI). Unanesthetized mice were placed in a restraint tube and inserted into the EchoMRI system. At killing, liver and individual fat pads were weighed.
Mice were fasted for 6 h prior to the glucose test and 4 h prior to the insulin test (n = 7 per sex). The tests were completed as explained in previous publications  and Homa-IR calculated as previously described . Matsuda index and direct measurement of hepatic insulin sensitivity (ISI) have been calculated as described [18, 19]. Briefly, the Matsuda index was calculated as follows: Matsuda index = 1000/(√[G0 × I0 × Gmean × Imean]), the suffix mean indicates the average value of glucose and insulin concentration measured during the whole length of the test. Hepatic insulin sensitivity index was calculated as ISI = k/(FPG × FPI).
Total RNA was extracted using TRIzol (Invitrogen AB) and mRNA expression levels were quantified as described  and normalized to female group. Relative gene expression changes were calculated using 36b4 gene for adipose tissue and Tf2b and β-actin for liver as internal references. List of the primers used for RT-PCR and their sequence can be find in Supplementary Table S3 (Additional file 1).
Histology and immunohistochemistry
Liver, gAT, and iAT were dissected, fixed in PFA, and embedded in paraffin . Sections (4 μm thickness) were stained with hematoxylin-eosin (H&E), Adipophilin (ADRP, PROGEN Biotechnik, Germany) and F4/80 (ab6640, Abcam) were detected according to standard histological procedures. The number of crown-like structures was determined from the mean value calculated on five different fields of one section for each animal, using a magnification of × 2 to cover the whole region.
Biochemical analysis of serum and liver
After blood collection, serum was aliquoted and stored at − 80 °C. ELISA kits were used to measure insulin (#EZRMI-13 K, Millipore), FGF21 (#MF2100, R&D systems), resistin (#MRSN00, R&D systems), and adiponectin (#MRP300, R&D systems) levels. For the measurement of the inflammatory cytokines in serum, a Bio-Plex Pro™ Mouse Cytokine Th17 Panel A 6-Plex was used (#M60-00007NY). Serum and liver TGs were measured by enzymatic assay using commercially available kits (Roche Diagnostics GmbH, Mannheim and mti Diagnostic GmbH, Idstein, Germany). The hepatic TG levels were corrected for the hepatic protein content, measured according to the Lowry method in the tissues digested with NaOH (1 M).
TG content in gAT and iAT was quantified from total lipid extracts [21, 22] using the colorimetric kit LiquickCor-TG (Cormay) and related to tissue weight. TG fractions were recovered from total lipid extracts by solid phase extraction and analyzed by electrospray ionization mass spectrometry (ESI-MS) and MS/MSinaQ-ToF2 (Micromass) . In liver, phospholipid (PL) amounts were estimated from total phosphorus content . Identification of PL molecular species was carried out by LC-MS/MS analysis as in . The degree of saturation of the corresponding FAs was confirmed by analysis of FA methyl esters (FAME) obtained by transmethylation of the total lipid extract using gas chromatography with flame ionization detector (GC-FID) . Analysis was carried out in triplicate in at least three samples from each group.
Desaturase, elongase, and lipogenic activities were estimated from the product-to-precursor ratios of the percentage of individual FAs according to the following equations: Δ9 desaturation index = (C18:1 + C16:1)/(C18:0 + C16:0), Δ5 desaturation index = C18:2/C18:1, elongase activity index = C18:0/C16:0, SCD1 activity index = C18:1/C18:0, and the lipogenic index = C16:0/C18:2 as described [26, 27].
The between-sample normalization with TMM method  was performed to sample matrix, where each sample is as the column and each physical parameter is as the row. Unsupervised clustering was then performed to the normalized matrix by t-SNE plot with the R package Rtsne . The t-SNE is based on the most 50 variant dimensions of initial PCA plot. The speed/accuracy trade-off was set as 0.0 for the exact t-SNE distance matrix. The perplexity is set to 1 with optimal clusters shape. Plots showing all samples are based on the t-SNE field parameters V1 and V2 .
Values are expressed as mean ± sem. Differences between groups were determined by multiple t tests corrected for multiple comparison. Statistical significance was determined using the Holm-Sidak method, with alpha = 5.000% in GraphPad Prism (San Diego, CA). Each row was analyzed individually, without assuming a consistent SD. *, P < 0.05, **, P < 0.01, ***, P < 0.001 and ****, P < 0.0001 M vs F; #, P < 0.05, ##, P < 0.01, ###, P < 0.001 and ####, P < 0.0001 M HFD vs M HFD-E2 and &, P < 0.05, &&, P < 0.01, &&&, P < 0.001 and &&&&, P < 0.0001, F WT vs F ERKO were considered significant.
Sex-dependent fat distribution and metabolic response to weight gain
Chow-fed F and M ob/ob mice had similar body weight (BW) gain and food intake, but M had a lower percentage of fat mass (54% vs 57%, p < 0.01) and higher lean mass (42% vs 38%, p < 0.01) than F. Fat distribution differed between sexes with M accumulating more VAT and less SAT than F (Table 1 and Additional file 2: Figure S1A-B). F and M showed similar serum fasting glucose level but fasting insulin level was 60% higher in M (Table 1). To evaluate the ability of the whole body to glucose clearance, we challenged the mice with a glucose load given by gavage (OGTT). Glucose level in the circulation was similar between M and F; however, insulin level during the OGTT was significantly higher in M compared t F at all time points, except for time 120 (Fig. 1a). In line with these results, glucose uptake in response to insulin injection was higher in F than M (Fig. 1b). The Matsuda index and hepatic insulin sensitivity index were higher in F together with lower Homa-IR (Fig. 1c and Table 1).
The H&E staining and adipophylin immunostaining of the F and M livers revealed that both sexes showed lipid droplets accumulation; however, M livers showed more lipid droplet accumulation and a higher level of hepatic TGs than F (Fig. 1d–e and Additional file 2: Figure S1). In addition, liver weight and serum TGs were significantly higher in M (Table 1). Serum levels of insulin-sensitized adipokines, FGF21, and adiponectin were higher in F, whereas the level of resistin was 2.5-fold higher in M (Table 1). Hepatic mRNA levels of DNL genes Srepb1c and Fas were higher in M (Fig. 1f), and mRNA levels of Dgat2, which coordinates the last step of newly synthetized TGs, was similar between sexes. However, the expression level of Dgat1, involved in the re-esterification of diacylglycerol into TGs, was 6 times higher in M than F. Finally, expression levels of Plin, a cytosolic lipid droplet-coated protein, and hormone sensitive lipase (Hsl) were higher in M than F (Fig. 1f). These data are in line with the higher liver TG content in M compared to F. Taken together, these findings imply that, despite a higher fat mass, F displayed enhanced insulin sensitivity, associated with an improved lipid metabolic profile compared to M.
Sex-dependent inflammatory response to obesity in liver, gAT, and iAT
Results from Fig. 1 described a sex-dependent metabolic response to obesity, and lipid accumulation may result in an increased production of inflammatory mediators generated from FAs. Therefore, histological sections of F and M liver, gAT, and iAT were immunostained for F4/80, indicative of macrophage infiltration. Liver sections did not show differences between sexes in F4/80 positive staining (Fig. 2a). However, hepatic expression level of pro-inflammatory genes F4/80 and Clec4f were higher in F than in M. In gAT, adipocyte size was similar between sexes but the number of crown-like structures was higher in M together with a higher expression level of the pro-inflammatory genes Tnf-α, Il6, F4/80, Cd68, Ccl7, and Mcp1 except for Il1-β that was lower (Fig. 2b). In iAT, M showed a higher amount of crown-like structures together with a higher expression level of Tnf-α, Cd68, and Ccl7 and lower expression level of Il1-β, Il6, F4/80, and Mcp1 compared to F (Fig. 2c), and no differences between adipocyte sizes were observed. Circulating levels of pro-inflammatory cytokines (i.e., TNFα, IL1β and IL6) were similar between sexes. However, it is important to note that the serum level of the anti-inflammatory cytokine IL10 was 2.5-times higher in the F than in M (Table 1).
To conclude, F tend to present pro-inflammatory markers in liver despite a much less steatotic liver compared to M. In contrast, M are more prone to develop inflammation in gAT despite lower total fat content as compared to F. Together, our data show that each sex presents differential susceptibility to obesity-induced inflammation accompanied with a tissue-specific response.
Sex-dependent FA profile in liver
Dysfunctions in one of the metabolic pathways involved in synthesis, transport, or removal of FAs and TGs are the basis for the development of liver steatosis. On a regular chow diet, the liver is the main organ that contributes to lipid production. To investigate whether F and M livers present different molecular species in their FA and PL profiles, a lipidomic analysis was carried out on total lipid extract from F and M livers. The proportion of C16, C18, and C20 FAs chains was similar between sexes (Additional file 2: Figure S1C) GC-FID identified a total of 11 FAs, with oleic acid (C18:1) > palmitic acid (C16:0) > palmitoleic acid (C16:1) > linoleic acid (C18:2) being the most abundant relative to the total amount of FAs in both F and M (Fig. 3a). The reduced multi-dimension plot (tSNE) of the FAs classes identified a high level of FAs homogeneity in the F group, while within the M group FAs classes were heterogenous (Additional file 3: Figure S2A). F livers had a higher relative amount of C18:1 (60.1% vs 56.3%, p < 0.01) whereas relative C18:2 > C18:0 > C20:4 > C17:1 content was higher in M compared to F (6.1% vs 2.7%, 2.3% vs 0.7%, 0.3 vs 0.9%, and 0.11% vs 0.03%, respectively, p ≤ 0.01) (Fig. 3a). To explore the mechanisms behind these sex-related FA profiles, the mRNA expression levels of genes involved in the elongation (Elovl3, Elovl4, Elovl5, Elovl6, Elovl7) and desaturation (Scd1, Scd2) of FAs were measured. M showed a higher expression level of Elovl3, Elovl4, and Elovl7 (Fig. 3b). On the other hand, Scd1 expression was significantly lower, thereby supporting a lower C18:1 relative content in M (Fig. 3a, b). Further supporting these results, the ratio C18:0/C16:0, a marker of elongase activity, was five times higher; whereas the C18:1/C18:0 ratio, indicative of desaturation, was six times reduced in M compared to F (Table 2). Finally, C16:0/C18:2 ratio, a marker of hepatic DNL activity, was 2.4 times higher in F than M. Moreover, the saturated FA (SFA) relative content was similar between sexes, but M showed respectively lower and higher relaive amount of mono-saturated FA (MUFA) poly-unsaturated FA (PUFA) compared to F. Therefore, MUFA/PUFA ratio was 2.3 times lower and PUFA/SFA 3 times higher in M (Table 2).
To further investigate the potential role of female sex hormones on hepatic expression levels of the main genes that drive the FA pathways described above, we investigated the expression levels of several genes from the same lipid pathways in C57Bl/6J F and M wild-type (WT), estrogen receptor (ER) α knockout (KO), and ERβKO F mice. Gene expressions pattern within the WT (F and M) and ERαKO and ERβKO (F) mice groups was highly dependent of the sex and/or the loss of ERα or ERβ as shown in Additional file 4: Figure S4. Srebp1c, Fas, and Acc1 expression levels were enhanced in ERβKO, Srebp1c in ERαKO F mice, and Fas in M WT, as compared to F WT, while Hsl and Plin expression levels were induced in ERβKO F only, with similar expression as M WT (Additional file 4: Figure S4A). Elovl3, Elovl4, and Elovl7 hepatic expression levels were upregulated, and Scd1 downregulated in M WT compared to F WT as observed in ob/ob model. ERαKO F mice displayed a higher expression level of Elovl3 and Elovl6 but downregulation of Elov7 and Scd2 as compared to WT F. On the contrary, ERβKO F mice had a higher expression level of Elovl4 and lower of Elovl5 compared to WT F (Additional file 4: Figure S4B).
In addition, we measured the expression level of these genes in liver of M and F WT mice on a high-fat induced obesity model. In HFD, most of the FAs are taken up by the liver from the circulation as opposed to chow diet where FAs are mainly synthetized by the liver. After uptake, non-esterified FAs are esterified into neutral lipid and packaged for secretion or stored. M had higher expression levels of Fas and Acc1 and of all the elongases family compared to F and respectively higher and lower expression levels of Scd1 and Scd2 (Additional file 4: Figure S4C-D). Interestingly, M treated with E2 for 3 weeks rescued their expression level to the F level for all these genes except for Elov3 and scd2. These data would support a transcriptional regulation of the FA synthesis by estrogens in liver and suggest that both ERs are involved in these regulations, as summarized in Fig. 5a. However, further studies will be necessary to unravel the mechanism by which sex hormones act as key regulators of lipid partitioning and hereby participate in the sexual dimorphism in obesity related diseases.
Sex-dependent PL profile in liver
PLs comprise the most abundant class of membrane lipids and are a key component of the cellular membrane integrity that can behave as signaling molecules; thus, their levels are tightly regulated. We analyzed the two major hepatic PL classes phosphatidylcholine (PC) and phosphatidylethanolamine (PE), as well as lysophosphatidylcholine (LPC) and lysophosphatidylethanolamine (LPE), in order to identify a sex-specific signature of their molecular profiles. The reduced multi-dimension plot (tSNE) of these PL classes successfully cluster F and M groups (Additional file 3: Figure S2B). Most interestingly, reduced multi-dimension plot (tSNE) of each PL class identified, i.e., PC, LPC, PE, and LPE, clearly distinguished F and M specific PL profiles (Additional file 3: Figure S2C-D). Even though the proportion of each PC class (PC32 to PC40) did not differ between M and F, except for PC32 (Additional file 2: Figure S1D), among the 21 PC molecular species identified, six of them were statistically different between F and M when using a multiple t test corrected for multiple comparisons. PC34:1 (~ 13.5%), PC38:4 (~ 10.2%), PC38:6 (~ 9.7%), and PC36:4 (~ 9.1%) were the most abundant PC species in both sexes, compared to the rest of the PC species identified (Fig. 3c and Additional file 5: Table S1). The relative content of PC34:1 > PC34:0 > PC32:0 ≥ PC32:1 species to total PC were higher in F compared to M (16% vs 11%, 2.7% vs 1.9%, 1.9% vs 1.3% and 1.6% vs 0.9%, respectively, p < 0.01); in contrast, the relative content of PC38:4 > PC38:4-O species to total PC were higher in M than in F (12% vs 8% and 1.5% vs 0.8%, respectively, p < 0.01). Therefore, F PC profile showed enrichment of shorter acyl-chains as compared to M. In addition, M showed higher relative levels of the alkyl-substituted PC resulting in an overall higher level of total plasmalogen species within the PC class.
PC conversion by LP-PLA2 raises lysoPC (LPC) species. No differences into the LPC classes were observed (Additional file 2: Figure S1F); however, among the eight LPC molecular species identified, six of them were statistically different between F and M. LPC16:0 and LPC18:0 were the most present in both M and F livers (Fig. 3d and Additional file 5: Table S1). The percentage of LPC18:1 > LPC18:2 > LPC16:1 species was much higher in F compared to M (22% vs 11%, 17% vs 2% and 2.2% vs 0.9%, respectively, p < 0.0001); whereas the amount of LPC18:0 > LPC18:0-O ≥ LPC16:0-O species relative to total LPC was higher in M compared to F (37.2% vs 18.1%, 6.1% vs 2.6%, 5.2% vs 3.5%, respectively, p < 0.0001). These results indicate that M have higher proportion of saturated LPC and plasmalogen species whereas F show higher proportion of mono- and poly-unsaturated LPC species.
Among the PE classes, no difference between sexes were observed into the distribution (Additional file 2: Figure S1E) and 14 PE species were identified. When using a multiple t test corrected for multiple comparisons, only two of these were statistically different between sexes. However, the reduced multi-dimension plot (tSNE) of each PE class clearly distinguished F and M specific PE profiles (Additional file 3: Figure S2D). PE38 species were the most abundant PE species compared to the rest of the PE species identified in both sexes, total PE38 (~ 61%) with PE38:4 (~ 30%) > PE38:6 (~ 16%) > PE38:5 (~ 11%) > PE38:3 (~ 2.5%) and total PE40 (~ 13.5%) ≥ PE34 (~ 12.4%) ≥ PE36 (~ 11.7%). The proportion of PE40:7 > PE34:1-o were significantly higher in M compared to F (5.6% vs 3.5% and 0.6% vs 0.2%, respectively, p < 0.05) (Fig. 3e and Additional file 5: Table S1).
LPE class analysis showed clear sex-dependent distribution (Additional file 2: Figure S1D) with all LPE molecular species differently expressed between M and F (Additional file 2: Figure S1G). LPE species analysis showed that three out of the four species identified were drastically different between F and M, being more than ~ 20% higher in either F or M. Whereas, the proportion of LPE18:0 to total LPE was the most present in both sexes, in M, it was 70% higher than in F (51% vs 30%, respectively, p < 0.0001). In addition, M showed higher proportion of LPE16:0 than F (28% vs 18%, respectively, p < 0.0001). Interestingly, the percentage of LPE20:4 to total LPE was 22 times higher in F than in M (23% vs 1%, respectively, p < 0.0001) (Fig. 3f and Additional file 5: Table S1). Altogether, our data clearly reveal sex differences in hepatic PL and LPL composition, suggesting a sex-specific regulation of PL synthesis in mouse liver that may contribute to the sexual dimorphism observed during obesity.
To examine the mechanisms behind these sex-related PL pattern in mouse-livers, we measured the expression level of the main enzymes of the PL synthesis pathways (i.e., choline kinase (Ck), CTP:phosphocholine cytidylyltransferase (Ct), ethanolamine kinase (Ek), CTP:phosphoethanolamine cytidylytransferase (Et), PE N-methyltransferase (Pemt), and Lipoprotein-associated phospholipase A2 (Lp-Pla2)). In liver, PC species are synthesized via the choline pathway (Ck and Ct) or by methylation of PE via PE N-methyltransferase (Pemt) while PE species are synthesized by the ethanolamine pathway (Ek and Et). Interestingly, M showed a reduced Ck and Pemt mRNA expression level; whereas, the mRNA expression levels of Ek, Et, and Lp-Pla2 were induced compared to F (Fig. 3g). These results suggest that in obese mouse livers, PC biosynthesis is favored in F, while PE and LPE biosynthesis are promoted in M. In line with these findings, M showed a decreased relative PC/PE ratio compared to F (1.73 vs 2.33, respectively, p < 0.01), that has been shown to adversely affect membrane integrity and result in liver damage . Further supporting the sex-dependent enzyme activity of the PL synthesis, Ck and Pemt were less expressed, and Ct and Lp-Pla2 were more expressed in WT M as well as in ERβKO F mice compared to WT F (Additional file 3: Figure S4E). ERαKO showed similar expression as WT F mice. On HFD, where most of the FAs are taken-up from circulation, M showed an overexpression of all genes of the PL pathway as compared to F but this expression was rescued to F level in M treated with estrogen (E2) for 3 weeks except for Lp-Pla2 that stayed high (Additional file 4: Figure S4F). These data imply that the sex-dependent PL composition in liver could be partly driven by sex hormones both for synthesis and uptake as summarized in Fig. 5b.
Sex-dependent FA species in gAT and iAT
AT expansion is a key component of lipid homeostasis during overfeeding. Free FAs have been demonstrated as important mediators in the development of metaflammation in obesity. Adipocytes from VAT and SAT have different lipolytic and lipogenic properties. In our study, the ratio between total SAT and total VAT (SAT/VAT) was 32% higher in F (Table 1). Differences in fat distribution have been directly associated to different susceptibilities to metabolic diseases in human-obesity. However, little is known about sex-differences in lipid composition in these depots. Therefore, gAT and iAT were subjected to lipidomic analysis to characterize FAs composition and TG molecular species in F and M adipose depots. A relative amount of C16 FA species was significantly higher in gAT only and C18 lower in both gAT and iAT of F compared to M (Fig. 4a–d and Table 2). The reduced multi-dimension plot (tSNE) of the FAs classes identified high level of FAs homogeneity in the F group in the iAT as opposed to M, which showed high homogeneity in gAT (Additional file 6: Figure S3A).
GC-FID identified seven FAs in both fat pads (Fig. 4b and e) where palmitic acid (C16:0), palmitoleic acid (C16:1), oleic acid (C18:1n9c), and linoleic acid (C18:2n6t) were the most abundant FAs identified in all groups. In gAT, the proportion of C16:1 FA specie was higher in F than in M, in line with the higher C16:1/C16:0 ratio in F (Fig. 4b and Table 2). Interestingly, the relative content of the trans-FA C18:1n9t and C18:2n6t were lower in F in gAT and iAT, respectively (Fig. 4b, e). M and F showed comparable SFA and MUFA relative content in both adipose depots, but in iAT, M had higher relative PUFA content than F. Therefore, in iAT, as in liver, M presented a lower MUFA/PUFA ratio and higher PUFA/SFA than F (Table 2).
Lipid metabolism gene expression was studied to evaluate if the FA species revealed by lipidomic analysis were related to sex-dependent regulation at the transcriptional level. In gAT, de novo lipogenic gene Srebp1c, the desaturase Scd1, and the elongase Elovl5 were significantly downregulated in M; as opposed to Elovl7 that was upregulated compared to F (Fig. 4c). These findings support the lower C16:1 relative content and the higher C18 species content in M compared to F found in gAT. Oppositely, in iAT, Srebp1c and Elovl5 expressions were upregulated in M compared to F in line with the longer chain FAs in M (Fig. 4f).
Sex-dependent TG species in gAT and iAT
In AT, FAs undergo re-esterification into TGs and TG species have different metabolic properties; therefore, lipidomic analysis for TG molecular species in gAT and iAT have been performed. The reduced multi-dimension plot (tSNE) of the TG classes identified a high level of TG homogeneity in the F group in the gAT with one M showing similarity to F. The three other M showed high TGs homogeneity in gAT (Additional file 5: Figure S3B). In iAT, we found three clusters, with one F showing heterogeneity with the rest of the F group that was homogeneous in their TGs classes. Moreover, M did not show homogeneity in their TG classes. F gAT was, in percent, enriched in shorter chain TGs (C48 and C50) and had lower long chain TGs (C52 and C54) independently of their saturation degree, compared to M (Fig. 4g). 21 TG molecular species were identified by ESI-MS and MS/MS in all groups. Among them, in gAT six and in iAT five TG molecular species out of the 21 identified showed statistical differences between F and M when using a multiple t test corrected for multiple comparisons (Fig. 4h, k and Additional file 7: Table S2). In gAT, F displayed a higher percentage of TGs 50:2 > 50:3 > 48:1 ≥ 48:2 > 48:0 ≥ 48:3 compared to M (12.4% vs 10.2%, 7.0% vs 5.5%, 3.4% vs 2.1%, 2.9% vs 1.7%, 1.6% vs 1.0%, 1.0% vs 0.6%, respectively, p < 0.001). In iAT, F had a higher percentage of TGs 50:1 > 54:2 > 52:1 ≥ 50:0 (5.6% vs 4.4%; 3.2% vs 2.0%; 2.5% vs 2.1%; 1.4% vs 0.9%; F vs M respectively, p ≤0.01), whereas, TG54:5 was lower (3.6% vs 6.3%, respectively, p ≤0.01) in F than in M (Fig. 4h, k and Additional file 3: Table S2). These data indicate a sex-specific composition in TG species in both gAT and iAT. At the transcriptional level, the expression level of genes involved in the TGs synthesis showed significant differences between sexes especially in the gAT. In gAT, Dgat1 and AgPat2 were downregulated in M whereas Cd36, coding for the FAs transport in the adipocyte, and adipose triglyceride lipase (Atgl) were over expressed in M compared to F (Fig. 4i). In contrast, in iAT the mRNA level of Dgat1 and Plin was higher in M with no differences in Dgat2, AgPat2, Cd36 and Atgl expression levels (Fig. 4l). These data revealed a sex-specific TG species and synthesis in both adipose depots as presented in Fig. 5.
This study is an extensive characterization of a sex-specific regulation of lipid species composition in mouse liver, gAT and iAT, which may contribute to the sexual dimorphism in obesity. Despite differences in AT distribution as well as in liver and serum lipid composition between sexes, the biological role of lipid species in metabolic response is still unknown. In order to gain more insight into the sex-dependent lipid profile in obesity, our study focused on the characterization of the most abundant lipid classes and molecular species in liver (PC and PE) and in AT (TGs). This work unveils molecular signatures, which are markedly different between sexes. In addition, we showed that estrogen plays a key role in the regulation of the lipid synthesis in liver at the transcriptional level through both ERα and ERβ signaling pathways. This novel characterization could be of interest to identify sex-specific functional differences in the metabolic response observed in F and M obesity.
Although no differences in BW gain and food intake were found, physiological response to weight gain was sex dependent. F showed higher TF content and SAT/VAT ratio together with better insulin sensitivity and lower fasting insulin level compared to M. A higher plasma insulin concentration is positively correlated to the degree of AT inflammation . The circulating levels of cytokines, which play a main role in the inflammation and IR in obesity, has been shown to be sex dependent [30,31,32,33]. In line with this, we found that resistin, which possesses pro-inflammatory effects and contributes to IR and inflammation [32, 33], was reduced in F. Oppositely, FGF21 and adiponectin, two anti-inflammatory adipokines with insulin sensitizing properties and negatively correlated to obesity, were higher in F. Conversely, M showed a high level of pro-inflammatory markers and crown-like structure in both AT compared to F, despite a lower proportion of total body fat. Therefore, our data show that M metabolic response to overfeeding a chow diet is altered compared to F which seems to be protected despite a higher total fat content.
When diet contains low content of lipids (chow diet), FAs composition reflects, in most part, DNL pathway activity in the liver rather than FA uptake. De novo FAs composition is dependent of the activity of the elongase (Elovl) and the desaturase (Scd) enzyme family in the liver . As proposed in the model in Fig. 6a, the DNL pathway in the liver for the synthesis of SFA, MUFA, and PUFA is sex dependent. Our results show that MUFAs biosynthesis was favored in F compared to M due to elevated desaturase Δ9D transcript level whereas long-chain PUFA (C20:4 and C18:2) and SFA (C18:0) were more abundant in M than in F. C18:0/C16:0 ratio, a marker of elongase activity in the liver, was ten times higher in M than F and has been recently identified as the most important factor that was correlated with the steatosis score in humans . Our results suggest that liver steatosis observed in M livers could be the consequence of the sex-dependent regulation of key genes of the FAs pathways in the liver. Whether or not these genes are directly controlled by sex hormones remains to be discovered. However, previous data imply that Elovl3 expression level in liver is under circadian variation in sexually mature males . The authors conclude that androgens are essential for diurnal Elovl3 expression in liver. Another study found that hepatic Elovl3 gene expression level was induced 16 fold and Scd1 induced 2 fold, in ERαKO F mice compared to WT F mice , in line with our study. F ob/ob mice treated for 3 weeks with E2 decreased the expression level of the hepatic lipogenic genes . These data support a tight regulation of key genes of the lipid pathway by sex hormones at the transcriptional level that could initiate the sex dimorphism observed in metabolic disorders associated to obesity.
The biological implications of the changes in lipid composition are likely complex and difficult to predict simply on the basis of the FA or the PL compositions. The physiological outcomes of lipid composition depend on their locations (membrane, cytosolic, or nuclear)  and amounts . For instance, arachidonic acid (AA, C20:4 n-6) is released from membrane PLs by phospholipase A2; cyclooxygenase then rapidly converts AA into a pro-inflammatory metabolite that accelerates the progression of hepatotoxicity [40, 41]. M livers had higher Δ5D activity, estimated by the 20:4/20:3 ratio, together with higher relative content of AA and a higher level of PC species containing AA. AA increases the risk for cardiovascular disease, and eicosanoids derived from AA may contribute to the development of inflammatory disorders . In addition, increase of n6PUFA has been demonstrated to be linked to inflammation and, C18:2n-6trans FA is in higher proportion in M WAT than F. Although presently, we cannot directly relate sex-dependent FAs composition to inflammation, our results suggest that M intake of AA could be more detrimental than in F. Inflammatory response observed in obese M adipose depot could be the consequence of increased de novo synthesis of pro-inflammatory lipid species as compared to F.
The ratio between PC and PE reflects membrane integrity  and, a decrease in PC/PE ratio perturbs membrane integrity. This imbalance has been associated with liver failure . M showed a decrease in the PC biosynthesis enzyme activity as summarized in Fig. 5b. Additionally, PC are required for very low-density lipoproteins (VLDL) secretion, as PC are the major lipids of the surface monolayer of the VLDL particles. A sex-dependent regulation of Pemt in the regulation of plasma high-density lipoproteins and VLDL has been demonstrated in mice , and estrogen has been shown to induce Pemt gene expression in human and mouse primary hepatocytes . In addition, PEMT-deficient male mice had higher liver TG level as compared to WT-control males . Additionally, diabetic patients with metabolic syndrome and cardiovascular diseases have higher Lp-PLA2 activity than those without the diseases [46, 47]. In line with these findings, ob/ob as well as WT M and ERβKO F mice showed lower hepatic Pemt together with higher Lp-Pla2 expression levels compared to ob/ob F. On HFD, where most of the FAs are taken-up from circulation, M overexpressed, as compared to F, all genes of the PL, and E2 rescued this expression to the F level except for Lp-Pla2 that stayed high. It is thus likely that M showed severe imbalance between PC and PE production due to PEMT and LP-PLA2 malfunction and that may imply liver dysfunctions (increased steatosis and TGs level) during obesity. Further studies should be performed to unravel the direct role of estrogens in these regulations.
AT and its stored lipid species are primarily derived from exogenous sources and endogenously synthesized via DNL, which are part of the lipid metabolism. In obesity, DNL capacity of adipocytes is substantially reduced and this may contribute to the associated metabolic perturbations. Studies have documented the possible connection between an increased DNL, particularly of palmitoleate (C16:1), in AT and systemic beneficial outcomes, such as an increased insulin sensitivity . F gAT accumulated TAGs enriched in palmitic acid (C16:0) and myristic acid (C14:0), the direct products of DNL, with higher expression of the DNL genes (Srebp1c and Fas) and better insulin sensitivity than M. Increase of n6 PUFA levels has been demonstrated to be linked to inflammation and, C18:2n-6trans FA was found in higher proportion in M than F together with increased crown-like structures in M and a two-fold induction of Tnfα expression in both fat pads. Therefore, as in the liver, sex -specific response to obesity is likely to occur in adipose depots and could be different between iAT and gAT in M and F as suggested by recent studies [49, 50]. However, much remains to be learned about the factors that influence adipogenesis in the different depots and their contribution to metabolic health and diseases. Evidences raised from recent studies suggested that the differential regulation of FAs release and uptake in SAT and VAT modify their depot-specific metabolic properties [51, 52]. A possible role of sex hormones, especially estrogens, in white adipose function controlled by genes in development and pattern specification has been revealed in the last decade [50, 51].
We cannot exclude that in the ob/ob model with a C57BL/6 background, the absence of leptin production could be a limitation in the exploration of sex-dependent lipid profile in obesity and its translation to humans. However, recent studies have emphasized the need to develop gender appropriate medicine in lipid homeostasis especially in obesity and associated disorders [53,54,55,56]; and studies comparing different animal species agreed that the mouse is a suitable species for the study of human hepatic lipid metabolism [57, 58]. Although the transgenic model we used herein may not represent the exact lipid changes observed in humans, it has clearly demonstrated that alterations in lipid homeostasis in response to overfeeding are sex dependent. Central effect of leptin on food intake and lipid homeostasis has been largely explored and many groups showed the implication of leptin, insulin, and sex hormones in these regulations, at the central level [59,60,61] in both M and F . However, to get more insight into the implication of sex hormones in these regulations, we also used two other models, (1) the high-fat diet induced obesity and (2) the ERKO mice for gene expression analysis. In both models, we observed sex-dependent and/or ER-dependent hepatic regulation in lipid gene expression that support our hypothesis. ERKO F mice brought crucial information on the potential implication of both ERs in these regulations, and WT M treated with E2 indicate that E2 treatment in M mice drives gene expression pattern towards the F one. Further studies should be performed to unravel the mechanism by which estrogen can affect lipid distribution and composition in obesity.
Altogether these findings provide more evidence to understand the sex-dependent metabolic response towards obesity. In the current work, we demonstrate that there is a characteristic lipid molecular profile in obesity in each sex, and we propose that this may drive sexual dimorphism associated to metabolic dysfunctions between M and F. The functional analysis of such changes is important but not simple and merits a study in its own. More research is needed to understand the functional significance of each PL species in disease progression, to assess whether PL and LPL metabolisms represent a promising target for the sex-dependent treatment of obesity-associated diseases. This work characterizes sex-specific lipid molecular species with active roles in metabolic homeostasis and has paved the way for recognizing uncharted avenues for potential therapies. Our studies reveal a fine sex-specific regulation of hepatic PL composition and TGs synthesis in WAT in obese mice. Knowing the importance of the high regulation of PLs in the cell membranes, this investigation opens a new field to unravel if the sex dimorphism observed in both sexes and the concomitant obesity-associated diseases are due to alterations in the PL pathway. Moreover, these sex-dependent molecular signatures found in obesity raise new questions, such as whether pharmacological treatment of obesity modifies these lipid molecular signatures in a sex-specific manner and whether these differences are driven by sex-specific hormones such as estrogens and/or androgens. Finally, we suggest that manipulating FA composition with diets and/or treatment could potentially be a new strategy in the treatment of metabolic diseases.
Adipose triglyceride lipase
C-C motif chemokine ligand
Cluster of differentiation
C-type lectin domain family 4 member F
Fibroblast growth factor
Perigonadal adipose tissue
Hormone sensitive lipase
Inguinal adipose tissue
Et, Lipoprotein-associated phospholipase A2
Monocyte chemoattractant protein
Monounsaturated fatty acids
Oral glucose tolerance test
Polyunsaturated fatty acids
Subcutaneous adipose tissue
Saturated fatty acids
Sterol regulatory element-binding protein
Tumor necrosis factor
Visceral adipose tissue
Cheung O, Sanyal AJ. Abnormalities of lipid metabolism in nonalcoholic fatty liver disease. Semin Liver Dis. 2008;28:351–9.
Bechmann LP, Hannivoort RA, Gerken G, Hotamisligil GS, Trauner M, Canbay A. The interaction of hepatic lipid and glucose metabolism in liver diseases. J Hepatol. 2012;56:952–64.
Lordan R, Tsoupras A, Zabetakis I. Phospholipids of animal and marine origin: structure, function, and anti-inflammatory properties. Molecules. 2017;22. https://doi.org/10.3390/molecules22111964.
Fu S, Yang L, Li P, Hofmann O, Dicker L, Hide W, Lin X, Watkins SM, Ivanov AR, Hotamisligil GS. Aberrant lipid metabolism disrupts calcium homeostasis causing liver endoplasmic reticulum stress in obesity. Nature. 2011;473:528–31.
Rodriguez-Cuenca S, Pellegrinelli V, Campbell M, Oresic M, Vidal-Puig A. Sphingolipids and glycerophospholipids - the “ying and yang” of lipotoxicity in metabolic diseases. Prog Lipid Res. 2017;66:14–29.
Croll J, Neumark-Sztainer D, Story M, Ireland M. Prevalence and risk and protective factors related to disordered eating behaviors among adolescents: relationship to gender and ethnicity. J Adolesc Health. 2002;31:166–75.
Legato MJ. Gender-specific medicine--should it change the way we are doing business? J Gend Specif Med. 1999;12(15):2.
Blaak E. Gender differences in fat metabolism. Curr Opin Clin Nutr Metab Care. 2001;4:499–502.
Bjorntorp P. The regulation of adipose tissue distribution in humans. Int J Obes Relat Metab Disord. 1996;20:291–302.
Wajchenberg BL, Giannella-Neto D, da Silva ME, Santos RF. Depot-specific hormonal characteristics of subcutaneous and visceral adipose tissue and their relation to the metabolic syndrome. Horm Metab Res. 2002;34:616–21.
Regitz-Zagrosek V, Lehmkuhl E, Weickert MO. Gender differences in the metabolic syndrome and their role for cardiovascular disease. Clin Res Cardiol. 2006;95:136–47.
Cheung O, Kapoor A, Puri P, Sistrun S, Luketic VA, Sargeant CC, Contos MJ, Shiffman ML, Stravitz RT, Sterling RK, Sanyal AJ. The impact of fat distribution on the severity of nonalcoholic fatty liver disease and metabolic syndrome. Hepatology. 2007;46:1091–100.
Clement K, Vaisse C, Lahlou N, Cabrol S, Pelloux V, Cassuto D, Gourmelen M, Dina C, Chambaz J, Lacorte JM, et al. A mutation in the human leptin receptor gene causes obesity and pituitary dysfunction. Nature. 1998;392:398–401.
Antonson P, Omoto Y, Humire P, Gustafsson JA. Generation of ERalpha-floxed and knockout mice using the Cre/LoxP system. Biochem Biophys Res Commun. 2012;424:710–6.
Brouillette J, Rivard K, Lizotte E, Fiset C. Sex and strain differences in adult mouse cardiac repolarization: importance of androgens. Cardiovasc Res. 2005;65:148–57.
Archer A, Laurencikiene J, Ahmed O, Steffensen KR, Parini P, Gustafsson JA, Korach-Andre M. Skeletal muscle as a target of LXR agonist after long-term treatment: focus on lipid homeostasis. Am J Physiol Endocrinol Metab. 2014;306:E494–502.
Archer A, Venteclef N, Mode A, Pedrelli M, Gabbi C, Clement K, Parini P, Gustafsson JA, Korach-Andre M. Fasting-induced FGF21 is repressed by LXR activation via recruitment of an HDAC3 corepressor complex in mice. Mol Endocrinol. 2012;26:1980–90.
Matsuda M, DeFronzo RA. Insulin sensitivity indices obtained from oral glucose tolerance testing: comparison with the euglycemic insulin clamp. Diabetes Care. 1999;22:1462–70.
Pacini G, Omar B, Ahren B. Methods and models for metabolic assessment in mice. J Diabetes Res. 2013;2013:986906.
Archer A, Stolarczyk E, Doria ML, Helguero L, Domingues R, Howard JK, Mode A, Korach-Andre M, Gustafsson JA. LXR activation by GW3965 alters fat tissue distribution and adipose tissue inflammation in ob/ob female mice. J Lipid Res. 2013;54:1300–11.
Folch J, Lees M, Sloane Stanley GH. A simple method for the isolation and purification of total lipides from animal tissues. J Biol Chem. 1957;226:497–509.
Bligh EG, Dyer WJ. A rapid method of total lipid extraction and purification. Can J Biochem Physiol. 1959;37:911–7.
Doria ML, Cotrim Z, Macedo B, Simoes C, Domingues P, Helguero L, Domingues MR. Lipidomic approach to identify patterns in phospholipid profiles and define class differences in mammary epithelial and breast cancer cells. Breast Cancer Res Treat. 2012;133:635–48.
Doria ML, Cotrim CZ, Simoes C, Macedo B, Domingues P, Domingues MR, Helguero LA. Lipidomic analysis of phospholipids from human mammary epithelial and breast cancer cell lines. J Cell Physiol. 2013;228:457–68.
Aued-Pimentel S, Lago JH, Chaves MH, Kumagai EE. Evaluation of a methylation procedure to determine cyclopropenoids fatty acids from Sterculia striata St. Hil. Et Nauds seed oil. J Chromatogr A. 2004;1054:235–9.
Ntambi JM, Miyazaki M, Dobrzyn A. Regulation of stearoyl-CoA desaturase expression. Lipids. 2004;39:1061–5.
Guillou H, Zadravec D, Martin PG, Jacobsson A. The key roles of elongases and desaturases in mammalian fatty acid metabolism: insights from transgenic mice. Prog Lipid Res. 2010;49:186–99.
Robinson MD, Oshlack A. A scaling normalization method for differential expression analysis of RNA-seq data. Genome Biol. 2010;11:R25.
Krijthe JH. Rtsne: T-distributed stochastic neighbor embedding using a Barnes-hut implementation; 2015.
Li Z, Agellon LB, Allen TM, Umeda M, Jewell L, Mason A, Vance DE. The ratio of phosphatidylcholine to phosphatidylethanolamine influences membrane integrity and steatohepatitis. Cell Metab. 2006;3:321–31.
Pedersen DJ, Guilherme A, Danai LV, Heyda L, Matevossian A, Cohen J, Nicoloro SM, Straubhaar J, Noh HL, Jung D, et al. A major role of insulin in promoting obesity-associated adipose tissue inflammation. Mol Metab. 2015;4:507–18.
Qatanani M, Szwergold NR, Greaves DR, Ahima RS, Lazar MA. Macrophage-derived human resistin exacerbates adipose tissue inflammation and insulin resistance in mice. J Clin Invest. 2009;119:531–9.
Park HK, Kwak MK, Kim HJ, Ahima RS. Linking resistin, inflammation, and cardiometabolic diseases. Korean J Intern Med. 2017;32:239–47.
Yamada K, Mizukoshi E, Sunagozaka H, Arai K, Yamashita T, Takeshita Y, Misu H, Takamura T, Kitamura S, Zen Y, et al. Characteristics of hepatic fatty acid compositions in patients with nonalcoholic steatohepatitis. Liver Int. 2015;35:582–90.
Brolinson A, Fourcade S, Jakobsson A, Pujol A, Jacobsson A. Steroid hormones control circadian Elovl3 expression in mouse liver. Endocrinology. 2008;149:3158–66.
Bryzgalova G, Gao H, Ahren B, Zierath JR, Galuska D, Steiler TL, Dahlman-Wright K, Nilsson S, Gustafsson JA, Efendic S, Khan A. Evidence that oestrogen receptor-alpha plays an important role in the regulation of glucose homeostasis in mice: insulin sensitivity in the liver. Diabetologia. 2006;49:588–97.
Gao H, Bryzgalova G, Hedman E, Khan A, Efendic S, Gustafsson JA, Dahlman-Wright K. Long-term administration of estradiol decreases expression of hepatic lipogenic genes and improves insulin sensitivity in ob/ob mice: a possible mechanism is through direct regulation of signal transducer and activator of transcription 3. Mol Endocrinol. 2006;20:1287–99.
Schievella AR, Regier MK, Smith WL, Lin LL. Calcium-mediated translocation of cytosolic phospholipase A2 to the nuclear envelope and endoplasmic reticulum. J Biol Chem. 1995;270:30749–54.
Simopoulos AP. Evolutionary aspects of diet, the omega-6/omega-3 ratio and genetic variation: nutritional implications for chronic diseases. Biomed Pharmacother. 2006;60:502–7.
Das UN. Essential fatty acids: biochemistry, physiology and pathology. Biotechnol J. 2006;1:420–39.
Di Marzo V. Arachidonic acid and eicosanoids as targets and effectors in second messenger interactions. Prostaglandins Leukot Essent Fatty Acids. 1995;53:239–54.
Li Z, Agellon LB, Vance DE. Phosphatidylcholine homeostasis and liver failure. J Biol Chem. 2005;280:37798–802.
Noga AA, Vance DE. A gender-specific role for phosphatidylethanolamine N-methyltransferase-derived phosphatidylcholine in the regulation of plasma high density and very low density lipoproteins in mice. J Biol Chem. 2003;278:21851–9.
Resseguie M, Song J, Niculescu MD, da Costa KA, Randall TA, Zeisel SH. Phosphatidylethanolamine N-methyltransferase (PEMT) gene expression is induced by estrogen in human and mouse primary hepatocytes. FASEB J. 2007;21:2622–32.
Watkins SM, Zhu X, Zeisel SH. Phosphatidylethanolamine-N-methyltransferase activity and dietary choline regulate liver-plasma lipid flux and essential fatty acid metabolism in mice. J Nutr. 2003;133:3386–91.
Allison MA, Denenberg JO, Nelson JJ, Natarajan L, Criqui MH. The association between lipoprotein-associated phospholipase A2 and cardiovascular disease and total mortality in vascular medicine patients. J Vasc Surg. 2007;46:500–6.
Noto H, Chitkara P, Raskin P. The role of lipoprotein-associated phospholipase a(2) in the metabolic syndrome and diabetes. J Diabetes Complicat. 2006;20:343–8.
Yilmaz M, Claiborn KC, Hotamisligil GS. De novo lipogenesis products and endogenous Lipokines. Diabetes. 2016;65:1800–7.
Belanger C, Luu-The V, Dupont P, Tchernof A. Adipose tissue intracrinology: potential importance of local androgen/estrogen metabolism in the regulation of adiposity. Horm Metab Res. 2002;34:737–45.
Pedersen SB, Bruun JM, Hube F, Kristensen K, Hauner H, Richelsen B. Demonstration of estrogen receptor subtypes alpha and beta in human adipose tissue: influences of adipose cell differentiation and fat depot localization. Mol Cell Endocrinol. 2001;182:27–37.
Gesta S, Bluher M, Yamamoto Y, Norris AW, Berndt J, Kralisch S, Boucher J, Lewis C, Kahn CR. Evidence for a role of developmental genes in the origin of obesity and body fat distribution. Proc Natl Acad Sci U S A. 2006;103:6676–81.
Heid IM, Jackson AU, Randall JC, Winkler TW, Qi L, Steinthorsdottir V, Thorleifsson G, Zillikens MC, Speliotes EK, Magi R, et al. Meta-analysis identifies 13 new loci associated with waist-hip ratio and reveals sexual dimorphism in the genetic basis of fat distribution. Nat Genet. 2010;42:949–60.
Mauvais-Jarvis F. Sex differences in metabolic homeostasis, diabetes, and obesity. Biol Sex Differ. 2015;6:14.
Mittendorfer B. Sexual dimorphism in human lipid metabolism. J Nutr. 2005;135:681–6.
Palmisano BT, Zhu L, Eckel RH, Stafford JM. Sex differences in lipid and lipoprotein metabolism. Mol Metab. 2018;15:45–55.
Varlamov O, Bethea CL, Roberts CT Jr. Sex-specific differences in lipid and glucose metabolism. Front Endocrinol (Lausanne). 2014;5:241.
Bergen WG, Mersmann HJ. Comparative aspects of lipid metabolism: impact on contemporary research and use of animal models. J Nutr. 2005;135:2499–502.
Gordon SM, Li H, Zhu X, Shah AS, Lu LJ, Davidson WS. A comparison of the mouse and human lipoproteome: suitability of the mouse model for studies of human lipoproteins. J Proteome Res. 2015;14:2686–95.
Clegg DJ, Brown LM, Woods SC, Benoit SC. Gonadal hormones determine sensitivity to central leptin and insulin. Diabetes. 2006;55:978–87.
Wade GN, Gray JM, Bartness TJ. Gonadal influences on adiposity. Int J Obes. 1985;9(Suppl 1):83–92.
Gao Q, Horvath TL. Cross-talk between estrogen and leptin signaling in the hypothalamus. Am J Physiol Endocrinol Metab. 2008;294:E817–26.
Dubuc PU. Effects of estrogen on food intake, body weight, and temperature of male and female obese mice. Proc Soc Exp Biol Med. 1985;180:468–73.
We thank Dr. Myriam Aouadi for excellent comments and suggestions on the manuscript. We thank the SRP Diabetes animal phenotyping platform for giving access to the phenotyping facility for EchoMRI in the framework of “The Strategic Research Programme in Diabetes at Karolinska Institutet”.
This work was supported by the Swedish Science Council, Emil och Wera Cornells Stiftelse and the Emerging Technology Fund of Texas under agreement 300–9-1958. J.A.G. was supported by the Robert A. Welch Foundation (E-0004). The contribution from the University of Aveiro, Portuguese Science and Technology Foundation (FCT, Portugal), European Union, QREN, COMPETE and co-financed by the FEDER, within the PT2020 Partnership Agreement to QOPNA Project PEst-C/QUI/UI0062/2013, the project REDE/1504/REM/2015 (that concerns the Portuguese Mass Spectrometry Network). LAH acknowledges the support from national funds through the Institute for Biomedicine (UID/BIM/04501/2013 and POCI-01-0145-FEDER-007628). Eliana Alves is grateful to FCT for her grant (BPD/UI51/5441/2015 from RNEM/2013/UA).
Availability of data and materials
The local Ethical Committee of the Swedish National Board of Animal Research approved all experiments. Ethical number N230/15.
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Table S3. List of the primers used for RT-PCR and their sequence. (DOCX 19 kb)
Figure S1. (A) F and (B) M representative photograph depicting the liver and the distribution of gAT and iAT (n = 7) and; representative histological sections immunostained for adipophylin in liver (n = 3–4); pie charts presenting the relative content of (C) FA classes; (D) PC classes; (E) PE classes; (F) LPC classes; (G) LPE classes. Abbreviations: FA: fatty acid, PC: phosphatidylcholine, PE: phosphatidylethanolamine, LPC: lysophosphatidylcholine and LPE: lysophosphatidylethanolamine. *, P < 0.05 M vs F were considered significant. (PDF 128080 kb)
Figure S2. Sex-dependent hepatic FAs and phospholipid profile in liver of ob/ob mice. Relative hepatic t-SNE plot of (A) FAs; (B) phospholipids; (C) phosphatidylcholine (PC) and lysophosphatidylcholine (LPC); and (D) phosphatidylethanolamine (PE) and lysophospatidylethanolamine (LPE) species clusters in liver of ob/ob F (♀ pink bullets, n = 3) and M (♂ blue triangles, n = 4) mice. (PDF 168 kb)
Figure S4. Hepatic gene expression levels in F WT (♀ pink bullets), M WT (♂ blue triangles), F ERαKO (♀ pink open diamonds) and F ERβKO (♀ pink filled diamonds) mice (n = 3–6) of (A) lipogenic pathway; (B) elongases and desaturases and (E) PL pathway. Hepatic gene expression levels in HFD fed mice (n = 8): F WT (♀ pink bullets, black bar), M WT (♂ blue triangles, filled gray bar) and M WT treated with estrogen (E2) (♂ blue triangles, stripped bar) of (C) lipogenic pathway; (D) elongases and desaturases and (F) PL pathway. Values are expressed as mean ± sem. Differences between groups were determined by Multiple t tests corrected for multiple comparison. Statistical significance was determined using the Holm-Sidak method, with alpha = 5.000% in GraphPad Prism (San Diego, CA). Each row was analyzed individually, without assuming a consistent SD. *, P < 0.05, **, P < 0.01, ***, P < 0.001 and ****, P < 0.0001 M vs F; #, P < 0.05, ##, P < 0.01, ###, P < 0.001 and ####, P < 0.0001 M HFD vs M HFD-E2 and &, P < 0.05, &&, P < 0.01, &&&, P < 0.001 and &&&&, P < 0.0001, F WT vs F ERKO were considered significant. (PDF 306 kb)
Table S1. Most probable phospholipid species (FAME measure by GC-FID) identified in liver. Relative amount of phosphatidylcholine (PC), lysophosphatidylcholine (LPC), phosphatidylethanolamine (PE) and lysophosphatidylethanolamine (LPE) molecular species. Data are presented as mean ± sem, n = 3–4. *p < 0.05 male (M) vs female (F) mice; ns = not significant. (DOCX 21 kb)
Figure S3. Sex-dependent FAs and TGs profile in gAT and iAT of ob/ob mice. Relative t-SNE plot of (A) FAs; (B) TGs clusters in gAT and iAT of ob/ob F (♀ pink bullets, n = 4) and M (♂ blue triangles, n = 4). Abbreviations: gAT: perigonadal adipose tissue and iAT: inguinal adipose tissue. (PDF 129 kb)
Table S2. Triglyceride molecular species identified in fat depots by MS/MS. Data are presented as mean ± sem. n = 4. *p < 0.05 male (M) vs female (F) mice; ns: not significant. Abbreviations: TG: triglycerides; gAT: perigonadal adipose tissue and iAT: inguinal adipose tissue. (DOCX 24 kb)