PPARγ-induced cardiolipotoxicity in mice is ameliorated by PPARα deficiency despite increases in fatty acid oxidation (original) (raw)
Generation of MHC-Pparg/Ppara–/– mice. To study the effects of PPARα deficiency in the PPARγ-mediated cardiomyopathy, we crossed the high-expressing MHC-Pparg mouse line (15) twice into the Ppara–/– background, which resulted in MHC-Pparg/Ppara–/– offspring. Overexpression of PPARγ and the absence of PPARα in the heart were confirmed in each genotype at the protein level (Supplemental Figure 1; supplemental material available online with this article; doi:10.1172/JCI40905DS1).
Circulating plasma metabolites. PPARα deficiency is associated with increased circulating FFAs (Table 1). In MHC-Pparg mice, FFA concentrations were similar to those in controls. In MHC-Pparg/Ppara–/– mice, FFAs were equivalent to those in Ppara–/– mice. TAG levels have been reported to be variable in the Ppara–/– mice (21, 22). In our mice, they were not significantly reduced compared with those in control or MHC-Pparg mice, but this reduction reached significance when the MHC-Pparg/Ppara–/– mice were compared with either control or MHC-Pparg animals. There were no statistical differences in plasma cholesterol among these mice. PPARα deficiency is associated with decreased circulating glucose. In MHC-Pparg mice, glucose concentrations were similar to those in controls; and in MHC-Pparg/Ppara–/– mice, glucose concentrations were equivalent to those in Ppara–/– mice.
PPARα deficiency increased plasma FA and decreased glucose levels in MHC-Pparg mice
PPARα deficiency ameliorates heart dysfunction and increases survival of MHC-Pparg mice. Heart weights of PPARγ mice were increased, and this increase was not reduced in MHC-Pparg/Ppara–/– mice (Figure 1A). However, echocardiography showed improved heart function in 3-month-old male MHC-Pparg/Ppara–/– compared with MHC-Pparg mice. As expected, MHC-Pparg mice exhibited reduced fractional shortening (FS) and increased systolic left ventricular dimensions (LVDs) compared with wild-type controls (Figure 1, B–D). In stark contrast, LV function of the MHC-Pparg/Ppara–/– mice was improved and was not different from that of the wild-type control mice. Consistent with the echocardiography data, the survival rate increased from 58% to 92% at 130 days in MHC-Pparg/Ppara–/– mice (P < 0.05, Figure 1E).
PPARα deficiency improved heart function and increased survival rates in MHC-Pparg mice. (A) Heart weight to body weight ratio in mice (n = 11–18). (B) Representative M-mode echocardiographic images of LVD in MHC-Pparg and MHC-Pparg/Ppara–/– mice. (C and D) Echocardiography showed increased FS and reduced LVDs in MHC-Pparg/Ppara–/– mice (n = 11–18). (E) Survival was increased in MHC-Pparg/Ppara–/– mice. Data are shown as mean ± SD. *P < 0.05 versus normal controls.
PPARα deficiency does not reduce cardiac lipid content. The finding of improved cardiac function with persistently increased cardiac size was surprising. To assess whether PPARα deficiency altered heart lipid accumulation, we stained heart tissues with oil red O. As shown in Figure 2A, MHC-Pparg hearts had more lipid than wild-type, whereas Ppara–/– hearts had less neutral lipid. Despite the improved cardiac function, loss of PPARα did not reduce lipid accumulation in the hearts of MHC-Pparg mice. Both MHC-Pparg and MHC-Pparg/Ppara–/– mice had copious amounts of stained lipids. Heart tissue TAG data was consistent with the oil red O staining pattern, demonstrating significantly higher TAG levels in both MHC-Pparg and MHC-Pparg/Ppara–/– mice (Figure 2B). Heart tissue FFA levels were significantly increased in MHC-Pparg/Ppara–/– mice compared with MHC-Pparg mice (10.03 ± 0.86 vs. 7.51 ± 1.01 mol/l, P < 0.01) (Figure 2C); FFA levels in Ppara–/– and control hearts were similar. MHC-Pparg hearts had a significant increase in palmitic acid (C16:0) and decrease in docosahexaenoic acid (C22:6n3) (DHA) and docosapentaenoic acid (C22:5n6) (DPA) concentrations compared with control, but MHC-Pparg and MHC-Pparg/Ppara–/– hearts had a similar FA distribution (Supplemental Figure 2). These data suggested that the improved function of MHC-Pparg/Ppara–/– hearts was not due to reduction in palmitate.
Accumulation of intracellular lipid in the heart of MHC-Pparg and MHC-Pparg/Ppara–/– mice. (A) Oil red O staining showed an abundance of neutral lipid droplets randomly scattered throughout the cytoplasm of cardiomyocytes in both MHC-Pparg and MHC-Pparg/Ppara–/– mice after overnight fasting (original magnification, ×200). (B) Heart TAG and (C) FFA content were significantly increased in both MHC-Pparg and MHC-Pparg/Ppara–/– mice compared with control mice (n = 7). Data are shown as mean ± SD. *P < 0.05 versus littermate controls; #P < 0.05 versus MHC-Pparg mice.
Ceramide levels were increased in MHC-Pparg mice compared with control mice (Figure 3A) but were not altered by crossing the MHC-Pparg transgene onto the Ppara–/– background. However, C24:1 and C24 ceramides, which have been shown to be more toxic (23, 24), were slightly but significantly decreased in MHC-Pparg/Ppara–/– mice (Figure 3B). DAG, measured using the DAG kinase method, was also increased, but neither the level nor the distribution correlated with the improved cardiac function (Supplemental Figure 3A).
Total ceramide, long-chain acyl-CoA, and acylcarnitine content in hearts of MHC-Pparg and MHC-Pparg/Ppara–/– mice. (A) Total ceramide and (B) individual ceramide species. Ceramide species data represent the content of each FA as a percentage of total ceramide and are shown as mean ± SD (n = 6–7 per group). (C) Total long-chain acyl-CoA and (D) acetylcarnitine content. Data are shown as mean ± SD. *P < 0.01, **P < 0.01, and §P < 0.001 versus controls; #P < 0.05, ##P < 0.01 versus MHC-Pparg mice.
Long-chain FA coenzyme A (LCCoA) and acylcarnitine are intermediates in lipid oxidation. PPARα deficiency significantly increased total intracellular LCCoA content in MHC-Pparg hearts (86.5 ± 10.4 nmol/g vs. 61.9 ± 9.7 nmol/g; P < 0.01) (Figure 3C and Supplemental Figure 3B), consistent with reduced FAO. LCCoAs are converted to acylcarnitines prior to mitochondrial FA β-oxidation; LCCoA can also be utilized for peroxisome β-oxidation and TAG synthesis (25, 26). Despite increased LCCoA content, acylcarnitine content was reduced in MHC-Pparg/Ppara–/– compared with MHC-Pparg mice (1,189.7 ± 163.5 nmol/g vs. 1,611.7 ± 98.6 nmol/g; P < 0.01) (Figure 3D), especially associated with a reduction in medium- and long-chain acylcarnitines (Supplemental Figure 3C). Because acylcarnitine is a toxic catabolite (27–29), reduction of acylcarnitine content and increased TAG storage might have, at least partially, contributed to amelioration of cardiac dysfunction in MHC-Pparg/Ppara–/– mice.
Lipid droplet morphology is altered in cardiomyocytes from MHC-Pparg/Ppara–/– mice. Electron microscopy showed distorted mitochondrial contours and more lipid droplets within the sarcoplasm of cardiomyocytes in the MHC-Pparg and MHC-Pparg/Ppara–/– mice. MHC-Pparg/Ppara–/– hearts showed a striking redistribution of lipid storage into large droplets (Figure 4A). In some areas of MHC-Pparg/Ppara–/– hearts, lipid droplets were surrounded by mitochondria (Figure 4A). In addition, as shown at higher power, disrupted cristae were seen in MHC-Pparg but not in MHC-Pparg/Ppara–/– hearts (Figure 4B). Lipid droplet size was significantly increased in MHC-Pparg/Ppara–/– mice compared with MHC-Pparg mice (1.93 ± 0.81 vs. 0.77 ± 0.32 μm, P < 0.001) (Figure 4C). MHC-Pparg mice had greater cardiac uptake of VLDL-TAG than wild-type or Ppara–/– mice (Figure 4D), and this was not reduced in MHC-Pparg/Ppara–/– mice. Cardiac 2-deoxyglucose uptake was increased in MHC-Pparg and Ppara–/– mice but was not further increased in MHC-Pparg/Ppara–/– mice (Figure 4E).
Increase in heart lipid droplet size and TG uptake in MHC-_Pparg/Ppara_–/– mice. (A) Increase in lipid droplets within the sarcoplasm of cardiomyocytes in both MHC-Pparg and MHC-_Pparg/Ppara_–/– mice (original magnification, ×5,000). Increase in lipid droplet size (right 2 panels) and larger lipid droplets in MHC-_Pparg/Ppara_–/– surrounded by mitochondria (far right). Scale bars: 2 μm. (B) In MHC-Pparg heart mitochondria, the cristae were disrupted (original magnification, ×50,000). (C) The lipid droplet size was determined by randomly counting 50 lipid droplets, and average size is shown. (D) Cardiac TG-VLDL uptake and (E) 2-deoxy-d-[3H]glucose uptake. LP, lipid droplet; M, mitochondria; N, nucleus. Data are shown as mean ± SD. *P < 0.05, ***P < 0.001 versus MHC-Pparg mice.
MHC-Pparg/Ppara–/– mice have increased cardiac lipid oxidation and DNA copy number. To further investigate the metabolism of these hearts, we determined palmitate oxidation and myocardial oxygen consumption (MVO2) in isolated working hearts (30). Rates of palmitate oxidation were not increased in MHC-Pparg mice (Figure 5A). However, palmitate oxidation rates were increased by 27.3% and 32.5% in MHC-Pparg/Ppara–/– mice versus controls and MHC-Pparg hearts, respectively (P < 0.05). MVO2 was reduced by 31% in Ppara–/– hearts relative to control hearts (P < 0.001, Figure 5B) and was unchanged in MHC-Pparg hearts. However, PPARα deficiency increased MVO2 by 18% in MHC-Pparg hearts compared with controls (P < 0.001). Cardiac efficiency, which reflects work performed per unit of oxygen consumed, was reduced in MHC-Pparg hearts because cardiac work was reduced despite “normal” levels of MVO2 (Figure 5C). In MHC-Pparg/Ppara–/– hearts, although cardiac efficiency was similar to that in MHC-Pparg hearts, cardiac power was increased by 49% relative to MHC-Pparg (P < 0.001, Figure 5D). Thus, MHC-Pparg/Ppara–/– hearts utilized more oxygen due to greater FAO but had improved function. And, at least under nonischemic conditions, MHC-Pparg/Ppara–/– mice had improved cardiac function associated with greater FAO. This was associated with increased mitochondrial mass as estimated by the ratio of the mitochondrially encoded gene ATPase6 to β_-actin_ and mitochondrial transcription factor A (mtTFA) to 18s (Figure 5, E and F). There was no change in mitochondrial function detected in permeabilized cardiac fibers (Supplemental Figure 4, A–C).
Determination of cardiac lipid oxidation and mitochondria DNA number. (A) Myocardial palmitate oxidation, (B) myocardial oxygen consumption, (C) cardiac efficiency, and (D) cardiac power in isolated working hearts (n = 4–5). (E) Heart mitochondrial DNA was quantified by calculating the ratio of mitochondrial gene copy number (ATPase6) to nuclear gene copy number (β_-actin_) (n = 7). (F) Heart mtTFA mRNA expression. Data are shown as mean ± SD. *P < 0.05, **P < 0.01, and ***P < 0.001 compared with littermate controls; ##P < 0.01, ###P < 0.001 compared with MHC-Pparg mice. HW, heart weight.
Gene expression in MHC-Pparg/Ppara–/–mice. We determined whether reduction of PPARα expression would reduce PPARα target gene expression in the MHC-Pparg mice. We unexpectedly found an increase in PPAR target gene expression in MHC-Pparg/Ppara–/– mice (Figure 6 and Supplemental Table 1); mRNAs were increased for genes mediating lipid uptake, synthesis, oxidation, lipolysis, and storage, such as fatty acid translocase (Cd36), fatty acid synthase (Fasn), acyl-CoA oxidase (AOX), adipose TAG lipase (Atgl), adipose differentiation related protein (Adrp), and diacylglycerol acyltransferase1 (Dgat1). The increase in LCCoA content was associated with increased mRNA expression of long-chain fatty acyl-CoA synthetase (Acsl4), an enzyme expressed in the heart peroxisome (31). However mitochondrial acyl-CoA thioesterase 2 (Acate2), an enzyme that catalyzes the hydrolysis of acyl-CoAs to the FFA and coenzyme A (CoASH), was also increased in MHC-Pparg/Ppara–/– mice (Supplemental Table 1). Expression of PPARγ coactivator 1α (_Pgc-1_α) and oxidative phosphorylation–related (OXPHOS) genes were unchanged by crossing with Ppara–/– mice (Supplemental Table 1). Additionally, PPARα deficiency dramatically increased cellular retinol-binding protein III (CRBPIII) expression in MHC-Pparg mice (5.91-fold, P < 0.05). In contrast, there was no change in genes regulating glucose metabolism. Thus, the absence of PPARα appeared to increase the efficacy of the MHC-Pparg transgene in driving expression of PPAR target genes in the cardiomyocyte. PPARα deficiency did not alter endogenous PPARδ and PPARγ expression (Supplemental Figure 5).
Heart tissue mRNA expression. (A) qRT-PCR analysis of mRNA expression using gene-specific primers. Data were normalized to 18s rRNA. Values represent fold change relative to wild-type controls, which was set as 1 (n = 5–8). Data are shown as mean ± SD. *P < 0.05, **P < 0.01, and §P < 0.001 compared with controls; #P < 0.05, ##P < 0.01, and ‡P < 0.001 compared with MHC-Pparg mice. (B) Clustering of gene expression in MHC-Pparg and MHC-Pparg/Ppara–/– mice. Clustering was performed using centered correlation as distance measure and average linkage as method. For the color bar scale, the numeric value is the gene-specific log10 difference in probe intensity from median probe intensity of all 6 samples.
Because loss of PPARα was, curiously, associated with greater expression of several PPARγ downstream genes, we tested the hypothesis that PPARα blocked the actions of MHC-Pparg by treating MHC-Pparg mice with the potent PPARα agonist WY-14,643. Ten days of WY-14,643 treatment decreased plasma TAG without altering FFA or glucose levels (Figure 7A). Heart tissue oil red O staining showed reduced heart neutral lipid in WY-14,643–treated MHC-Pparg mice (Figure 7B). Expression of PPARγ downstream targets Cd36, Fasn, and CRBPIII (32) was reduced compared with that in nontreated MHC-Pparg mice. FAO and mitochondrial biogenesis genes, such as Lcad, Ucp3, and _Pgc-1_α, were also reduced with WY-14,643 treatment. However, expression of Cpt1, AOX, and Dgat1 was not altered by WY-14,643 treatment in MHC-Pparg mice (Figure 7C). These data suggested that PPARγ activity may be regulated by PPARα.
MHC-Pparg mice with or without WY-14,643 treatment. (A) Plasma TG, FFA, and glucose concentrations in the mice. (B) Oil red O staining of hearts from 3-month-old MHC-Pparg mice with or without WY-14,643 treatment (original magnification, ×200). (C) qRT-PCR analysis of cardiac mRNA expression in MHC-Pparg mice with or without WY-14,643 treatment (n = 6–7 per group). The results were repeated in 2 independent experiments. Data are shown as mean ± SD. *P < 0.05, **P < 0.01, §P < 0.001 compared with nontreated MHC-Pparg mice.
Evidence that lipid redistribution alters intracellular lipid signaling and reduces apoptosis and ROS. The pattern of intracellular lipid storage relates to the metabolic characteristics of cells; larger droplets have reduced total surface area and are likely to reflect more inert lipid storage (33). We then studied the reasons for the redistribution of cellular lipids. Adrp, perilipin 4, and cell death–inducing DFFA-like effector c (Fsp27) are associated with the surface of intracellular lipid droplets and regulate their formation and mobilization (33–35) and are regulated by PPARγ (36). mRNA expression of Adrp, perilipin 4, and Fsp27 was upregulated in MHC-Pparg mice by crossing with Ppara–/– mice (Figure 6, Supplemental Table 1, and Supplemental Figure 6).
Several intracellular lipids are potent signaling molecules and are thought to function as activators of classical PKCs (37, 38). To determine whether lipid redistribution led to altered intracellular lipid activation, we measured heart PKC activation. MHC-Pparg increased membrane PKCα and PKCδ. This increase was ameliorated in the MHC-Pparg/Ppara–/– mice (Figure 8A). Thus, the altered lipid distribution changed lipid activation of this potentially toxic pathway.
Cardiac PKC content and apoptosis-related proteins. (A) Representative Western blot image of membrane PKCα and PKCδ content. (B) BAX and p-JNK proteins in the heart. Pan-cadherin, Gapdh, and total JNK are shown as controls. (C) Cardiac ventricular tissues were stained for DNA fragmentation by TUNEL protocol (original magnification, ×200). Apoptotic cardiomyocytes containing fragmented nuclear chromatin exhibited dark brown nuclear staining (arrows). (D) The TUNEL-positive myocytes were counted and expressed as the number of TUNEL-positive myocytes per millimeter squared tissue area. Data are shown as mean ± SD. ###P < 0.0001 compared with MHC-Pparg mice.
Greater FAO is associated with more ROS production (39) and in some situations cellular apoptosis (40). However, TUNEL-positive myocytes were reduced in MHC-Pparg/Ppara–/– compared with MHC-Pparg mice, and expression of the apoptosis-related protein Bax and p-JNK was decreased in the heart of MHC-Pparg/Ppara–/– mice (Figure 8, B–D). Heart tissue intracellular O2– levels measured using dihydroethidium and fluorescence staining were increased in MHC-Pparg mice, but this was markedly attenuated in MHC-Pparg/Ppara–/– mice (Figure 9A). Mitochondrial and ER stress markers prohibitin and protein disulfide isomerase (PDI) (41, 42) were also decreased in the MHC-Pparg/Ppara–/– hearts (Figure 9, B and C). This was associated with increased expression of Sod2 but no differences in expression of Gpx1, catalase, Sod1, and Ucp2 between MHC-Pparg and MHC-Pparg/Ppara–/– mice. Expression of cardiac hypertrophic markers and apoptosis-related genes, such as natriuretic peptide precursor type B (BNP), serine hydrolase-like (Serh1), DNA damage–inducible transcript 3 (chop), and caspase-6, was significantly decreased in MHC-Pparg/Ppara–/– mouse hearts (Figure 6B, Figure 9D, and Supplemental Table 1).
Detection of ROS production and of mitochondrial and ER stress in heart tissues. (A) Histological analysis of heart tissues using dihydroethidium staining to detect ROS (original magnification, ×100). (B) Mitochondrial stress was detected by immunohistochemical staining of heart tissue sections with antibodies against prohibitin protein (original magnification, ×400). (C) Immunofluorescence analysis of the heart tissues using disulfide isomerase antibody (original magnification, ×400). (D) qRT-PCR analysis of heart gene expression. Data were normalized to 18s RNA. Values represent fold change relative to wild-type controls, which was set as 1 (n = 5–8). Data are shown as mean ± SD. *P < 0.05, **P < 0.01, and ***P < 0.01 compared with littermate controls; #P < 0.05 compared with MHC-Pparg mice.