Glutathionylated Lipid Aldehydes Are Products of Adipocyte Oxidative Stress and Activators of Macrophage Inflammation
- 1Department of Pediatrics, University of Minnesota, Minneapolis, MN
- 2Department of Biochemistry, Molecular Biology and Biophysics, University of Minnesota, Minneapolis, MN
- Corresponding author: David A. Bernlohr, .
B.I.F. and E.K.L. contributed equally to this work.
Obesity-induced insulin resistance has been linked to adipose tissue lipid aldehyde production and protein carbonylation. Trans-4-hydroxy-2-nonenal (4-HNE) is the most abundant lipid aldehyde in murine adipose tissue and is metabolized by glutathione S-transferase A4 (GSTA4), producing glutathionyl-HNE (GS-HNE) and its metabolite glutathionyl-1,4-dihydroxynonene (GS-DHN). The objective of this study was to evaluate adipocyte production of GS-HNE and GS-DHN and their effect on macrophage inflammation. Compared with lean controls, GS-HNE and GS-DHN were more abundant in visceral adipose tissue of ob/ob mice and diet-induced obese, insulin-resistant mice. High glucose and oxidative stress induced production of GS-HNE and GS-DHN by 3T3-L1 adipocytes in a GSTA4-dependent manner, and both glutathionylated metabolites induced secretion of tumor necrosis factor-α from RAW 264.7 and primary peritoneal macrophages. Targeted microarray analysis revealed GS-HNE and GS-DHN induced expression of inflammatory genes, including C3, C4b, c-Fos, igtb2, Nfkb1, and Nos2. Transgenic overexpression of GSTA4 in mouse adipose tissue led to increased production of GS-HNE associated with higher fasting glucose levels and moderately impaired glucose tolerance. These results indicated adipocyte oxidative stress results in GSTA4-dependent production of proinflammatory glutathione metabolites, GS-HNE and GS-DHN, which may represent a novel mechanism by which adipocyte dysfunction results in tissue inflammation and insulin resistance.
The effect of obesity on development of insulin resistance and cardiovascular risk has been associated with increased oxidative stress and a state of chronic low-grade inflammation in adipose tissue (1). Although pathologic states of oxidative stress and inflammation are clearly related in diseases spanning various biological tissues and systems, evidence for directionality and mechanism of interplay has remained elusive.
Overnutrition causes increased endothelial reticulum stress and adipose tissue mitochondrial dysfunction (2). This leads to decreased efficiency of oxygen consumption and electron transport, culminating in increased production of superoxide anion (3,4). Superoxide dismutase converts superoxide anion to hydrogen peroxide (H2O2) that can be further metabolized by catalase or glutathione peroxidases, forming oxygen and water (5–8). Alternatively, H2O2 is subject to nonenzymatic degradation via iron-mediated Fenton chemistry producing hydroxyl radical (9), the reactive oxygen intermediate responsible for lipid peroxidation of polyunsaturated fatty acids (10).
Oxidative stress–induced lipid peroxidation results in production of reactive α,β-unsaturated aldehydes (10). These react with cysteine, lysine, and histidine residues of proteins via Michael addition and Schiff base formation in a process termed protein carbonylation (11). Protein function and abundance is influenced by protein carbonylation (12,13), suggesting a mechanism by which oxidative stress may cause mitochondrial dysfunction or other changes in cell metabolism and signaling. Specifically, trans-4-hydroxy-2-nonenal (4-HNE) inhibits coupled respiration in isolated mitochondria and carbonylates mitochondrial proteins (2).
Protection against carbonylation-induced mitochondrial dysfunction is accomplished by a number of phase I and phase II enzymes that metabolize lipid aldehydes through oxidation, reduction, or glutathionylation. Glutathionylation via glutathione-S-transferase A4 (GSTA4) may play a particularly important role in the metabolism of lipid aldehydes in adipose tissue because obesity-induced alterations in adipose tissue oxidative stress and inflammatory status correlate strongly with downregulation of GSTA4 (14). Specifically, 4-HNE and other lipid aldehydes, such as trans-4-oxo-2-nonenal (4-ONE), are glutathionylated by GSTA4, exported rapidly in an ATP-dependent manner by RLIP76, and excreted in urine (15,16). Alternatively, GS-HNE (and GS-ONE) can be further reduced by aldoketoreductase to glutathionyl-1,4-dihydroxynonene (GS-DHN), which is also exported by RLIP76 (17).
Although glutathione metabolism provides a protective clearance mechanism, recent studies suggest glutathionylated lipids have proinflammatory signaling properties. In studies examining the role of aldose reductase in inflammation, cells treated with a cell-permeable ethyl ester of GS-DHN induced nuclear factor-κB (NF-κB) signaling in RAW 264.7 macrophages (18). Further, injection of nonesterified GS-HNE into murine peritoneal cavities resulted in leukocyte infiltration and proinflammatory leukotriene production (19). Because nonesterified GS-HNE is poorly membrane soluble (20), there may be a receptor-mediated mechanism for its inflammatory properties.
To characterize glutathione metabolism in obesity-induced inflammation, GS-HNE and GS-DHN were quantified by liquid chromatography–tandem mass spectrometry (LC-MS/MS), and the inflammatory potential of each was measured using cell culture systems. In addition, a transgenic mouse model was produced whereby GSTA4 was overexpressed in adipose tissue and GS-HNE/GS-DHN evaluated. The results support the hypothesis that glutathione metabolites of lipid aldehydes provide a novel mechanistic link between adipocyte oxidative stress and local adipose tissue inflammation.
Research Design and Methods
Nonesterified GS-HNE, GS-HNE-d3, and leukotriene C4 (LTC4)-d5 were purchased from Cayman Chemical (Ann Arbor, MI). Glutathione, butylated hydroxytoluene, and sodium borohydride (NaBH4) were purchased from Sigma-Aldrich (St. Louis, MO).
Synthesis of GS-DHN
GS-HNE was incubated with 50 mmol/L NaBH4 in ethanol for 1 h at 23°C to reduce the aldehyde, dried under nitrogen, and resuspended in 0.1% acetic acid, eliminating excess NaBH4. Product was applied to a Strata-X solid-phase extraction cartridge, washed with water, and then eluted with methanol. Methanolic extract was dried under nitrogen and resuspended in water. GS-DHN was quantified spectrophotometrically using the GS-HNE calibration curve. Recovery was 33–67%, and product was >99% pure as determined by direct infusion MS.
3T3-L1 preadipocytes were cultured and differentiated into adipocytes as described previously (21,22) and used on day 8 after differentiation. For low-glucose experiments, cells were grown in low-glucose (5.5 mmol/L) Dulbecco’s modified Eagle’s medium (DMEM) or standard, high-glucose (25 mmol/L) DMEM from time of plating, with media changed daily. GSTA4-silenced (knockdown [KD]) and GSTA4 overexpressing (OE) 3T3-L1 adipocytes and their respective control cell lines were generated as described previously (12) and were grown and differentiated (21), with the addition of blasticidin (1 μg/mL) for GSTA4 KD and scrambled cells and geneticin (400 μg/mL) for OE and pcDNA cells from time of plating until time of cell confluence and addition of 1 μg/mL troglitazone to the differentiation cocktail. RAW 264.7 macrophages (American Type Culture Collection) were grown in DMEM containing 10% FBS.
Generation of GSTA4 Transgenic Mice
Male C57Bl/6J wild-type and ob/ob mice were purchased from The Jackson Laboratory (Bar Harbor, ME). GSTA4 transgenic mice were generated from C57Bl/6J mice at the University of Minnesota Mouse Genetics Laboratory (Minneapolis, MN). The HA-tagged GSTA4 transgene is under the FABP4 promoter (provided by Dr. Ormond MacDougald, Ann Arbor, MI). Mice were weaned at 3 weeks of age onto a high-fat diet (Bioserve Industries, Frenchtown, NJ; No. F3282: 20% protein, 35.5% fat, 36.3% carbohydrate by weight, 60% fat by calories) or standard chow (Teklad Global, Madison WI; 2018: 18.6% protein, 6% fat, 44% carbohydrate by weight), maintained at 70°F on a 14:10-h light-dark cycle, and fed ad libitum. At 15–20 weeks of age, animals were fasted for 4 h and underwent glucose tolerance testing (0.5 g glucose/kg) and insulin tolerance testing (1.0 unit/kg). Blood glucose was measured using the OneTouch Ultra glucometer (LifeScan, Inc.). Mice were killed 1 week later by CO2 asphyxiation. Epididymal fat pads were harvested, flash frozen in liquid nitrogen, and stored at −80°C. All procedures were reviewed and approved by University of Minnesota Institutional Animal Care and Use Committee.
Isolation and Culture of Peritoneal Macrophages
C57Bl/6J mice were injected intraperitoneally with 3% thioglycollate (2 mL). After 4 days, peritoneal cells were collected by lavage and seeded in RPMI medium with 10% FBS. After 6 h, nonadherent cells were removed by rinsing with PBS. Adherent macrophages were grown in RPMI with 10% FBS and 1 μg/mL lipopolysaccharide (LPS) for 18 h, and then treated for 24 h with 10 μmol/L GS-HNE or 10 μmol/L GS-DHN in RPMI plus 10% FBS.
Adipose Tissue Glutathione Metabolite Content
Adipose tissue (∼100 mg) was homogenized and incubated with 1.5 pmol GS-HNE-d3 as the internal standard. Samples were vortexed, centrifuged at 3,800 rpm for 10 min at 4°C, and loaded on Strata-X solid-phase extraction cartridges preconditioned with methanol and equilibrated with water. Columns were washed with water. Glutathione metabolites were eluted with 100% methanol, dried under nitrogen, and resuspended in 25 μL methanol for LC-MS/MS analysis. GS-HNE was quantified by LC-MS/MS, similar to Long et al. (23).
Cellular Glutathione Metabolite Production
3T3-L1 adipocytes or RAW 264.7 macrophages were treated with 500 μmol/L H2O2 in Krebs-Ringer HEPES buffer (KRHB) containing 1% FBS for 1 h. Cell culture media was removed, spiked with 1 pmol GS-HNE-d3 and prepared identically to tissue samples.
Glutathione Metabolite–Induced Leukotriene C4 Production
Primary peritoneal macrophages were pretreated 18 h with 1 μg/mL LPS and were washed and treated with 10 μmol/L GS-HNE or GS-DHN in KRHB/0.1% FBS for 2 h. Cell culture media was removed and spiked with 1 pmol LTC4-d5 and then prepared, as described above, for LC-MS/MS analysis.
Glutathione Metabolite-Induced Tumor Necrosis Factor-α Production
RAW 264.7 or primary peritoneal macrophages were pretreated 24 h with 1 μg/mL LPS, followed by PBS wash. Macrophages were treated with GS-HNE or GS-DHN for 24 h in DMEM/0.1% FBS. Media was removed and frozen. Five microliters of media were assayed for tumor necrosis factor-α (TNF-α) content by ELISA kit from BD Biosciences (San Diego, CA).
RNA Preparations and RT-PCR
Total RNA was isolated from peritoneal macrophages by lysis in TRIzol (Invitrogen, Carlsbad, CA), according to the manufacturer’s directions. RNA was further purified using the RNeasy Mini Kit (Qiagen, Valencia, CA). cDNA was generated from ∼0.5 μg RNA using RT2 First Strand kit (Qiagen), followed by real-time PCR with 96-well RT2 profiler Mouse Inflammatory Response & Autoimmunity PCR array (Qiagen).
RNA was isolated from ∼0.2 g mouse epididymal adipose tissue using Trizol (Invitrogen), according to the manufacturer’s instructions. After DNase treatment, cDNA was synthesized using the iScript cDNA synthesis kit (BioRad). Relative quantification of mRNAs was performed by real-time PCR using iQ SYBR green Supermix and MyiQ detection system (BioRad). Primers for target genes were mGSTA4: forward: 5′-CGCTTTCAGGAGAGGGAAGTTG-3′ and reverse: 5′-AGGAACAAACCAGGAAACGTTAC-3′.
Enzymatic Assay of GSTA4
Epididymal fat pads from GSTA4 transgenic or wild-type mice were homogenized and protein concentration determined by bicinchoninic acid assay Sigma-Aldrich. Homogenates were diluted to 0.1 mg/mL and incubated with 1 mmol/L glutathione and 1 μmol/L 4-HNE for 1 min. Reaction was stopped by acetic acid (1% final concentration) and incubated with GS-HNE-d3. Homogenates were subjected to solid-phase extraction and quantified by LC-MS/MS, as described above. Total GST activity was determined by the amount of GS-HNE produced per milligram of protein per minute (nmol/mg/min).
All analyses were performed using Prism 6.0 software (GraphPad Software, La Jolla CA). Data were graphed as means ± SEM. Comparisons among groups were made using the Student t test with equal variance.
GS-HNE/GS-DHN in Murine Adipose Tissue
Adipose tissue was assayed for GS-HNE/GS-DHN in chow-fed, high fat–fed, and ob/ob mice. GS-HNE was significantly increased in high fat–fed (6.9-fold) and ob/ob mice (6.2-fold) compared with chow-fed mice (Fig. 1A). GS-DHN was significantly increased in ob/ob mice (4.3-fold) and showed a trend toward increased levels in high fat–fed mice (14.8-fold) (Fig. 1B).
GS-HNE/GS-DHN Production in 3T3-L1 Cell Lines
To characterize cell-specific formation of GS-HNE and GS-DHN, 3T3-L1 adipocytes or RAW 264.7 macrophages were treated with H2O2 to induce oxidative stress. When 3T3-L1 adipocytes were used, GS-HNE (Fig. 2A) and GS-DHN (Fig. 2B) levels were increased (12-fold and 6-fold, respectively) in response to H2O2 treatment. In contrast, GS-HNE was not detected in control or treated RAW 264.7 macrophages, and GS-DHN levels did not increase in response to H2O2 (Fig. 2A). Furthermore, GS-HNE was not detected in primary peritoneal macrophages basally or in response to inflammatory stimuli (results not shown). These results suggested that adipocytes are the primary GS-HNE/GS-DHN–producing cells in adipose tissue.
Elevated serum glucose levels are associated with increased production of reactive oxygen species in a variety of tissues (24). In model systems, growth in high-glucose medium is associated with increased oxidative stress and insulin resistance (25). To test the effect of hyperglycemic conditions on lipid peroxidation in cultured adipocytes, 3T3-L1s were cultured in low- or high-glucose media from initial plating through differentiation. Adipocytes cultured in high-glucose media displayed larger and more abundant lipid droplets relative to those grown in low-glucose media, consistent with previous observations (Fig. 3A) (25). Adipocytes maintained in low- or high-glucose media were further challenged with H2O2 for 2 h on day 8 of differentiation. H2O2 treatment induced increased production of GS-HNE in low-glucose (9-fold, from 50 ± 8 to 460 ± 140 pg/mL; P < 0.05) and high-glucose (16-fold, from 65 ± 9 to 1,100 ± 200 pg/mL; P < 0.001) conditions (Fig. 3B). Production of GS-DHN increased with H2O2 treatment in low-glucose (4-fold, 150 ± 30 to 670 ± 270 pg/mL; but this was not significant, P = 0.11) and was significantly increased in high-glucose conditions (11-fold, 220 ± 90 to 2,500 ± 600 pg/mL; P < 0.05) (Fig. 3C). In untreated cells, high-glucose media generated slightly higher GS-HNE and GS-DHN relative to low-glucose media (65 ± 9 vs. 50 ± 8 pg/mL and 220 ± 90 vs. 150 ± 30 pg/mL, respectively); however, this was not significant. In combination with H2O2 treatment, however, high-glucose media resulted in increased GS-HNE production by 2.3-fold (1,100 ± 200 vs. 460 ± 140 pg/mL; P < 0.05) and GS-DHN was increased 3.7-fold (2,500 ± 600 vs. 670 ± 270 pg/mL; P < 0.05) relative to low-glucose media. These results demonstrate a synergistic effect of H2O2 treatment under high-glucose conditions (Fig. 3B and C).
The enzyme primarily responsible for glutathionylation of 4-HNE, GSTA4, is implicated as an important factor in obesity-induced insulin resistance and metabolic dysfunction (2). To evaluate GSTA4-mediated production of GS-HNE/GS-DHN, GSTA4 KD and GSTA4 OE cell lines were challenged with H2O2. H2O2 treatment resulted in increased production of GS-HNE (6-fold, from 390 ± 50 to 2,400 ± 80 pg/mL; P < 0.0001) and GS-DHN (15-fold, from 530 ± 80 to 8,000 ± 1,400 pg/mL; P < 0.01) in GSTA4 KD (Fig. 4A and B). However, this increase was significantly less than the increased production of GS-HNE (20-fold, from 560 ± 20 to 11,000 ± 400 pg/mL; P < 0.0001) and GS-DHN (27-fold, from 510 ± 60 to 14,000 ± 400 pg/mL; P < 0.0001) by control cells (Fig. 4A and B). H2O2 stimulated production of GS-HNE and GS-DHN was 4.7-fold (P < 0.0001) and 1.7-fold (P < 0.01) higher in control cells relative to KD cells, respectively. Basally, control cells produced 1.4-fold higher levels of GS-HNE (P < 0.05) than GSTA4 KD cells; however, GS-DHN production did not differ between control and KD (Fig. 4A and B).
In GSTA4 OE cells, H2O2 treatment resulted in increased production of GS-HNE (9-fold, from 150 ± 3 to 1,300 ± 60 pg/mL; P < 0.0001) and GS-DHN (17-fold, from 300 ± 20 to 5,000 ± 500 pg/mL; P < 0.001) (Fig. 4C and D). Correlating with increased expression of GSTA4, this increase was significantly higher than the increase in GS-HNE (fivefold, from 110 ± 20 to 560 ± 60 pg/mL; P < 0.001) and GS-DHN (sixfold, from 350 ± 110 to 1,900 ± 180 pg/mL; P < 0.001) made by control cells. Compared with GSTA4 KD cells, GSTA4 OE cells had 2.3-fold (P < 0.001) and 2.6-fold (P < 0.01) higher production of GS-HNE and GS-DHN, respectively, in response to H2O2 relative to control cells (Fig. 4C and D). There was no significant difference between GSTA4 OE and control cells in basal formation of GS-HNE or GS-DHN (Fig. 4C and D).
Effect of GS-HNE/GS-DHN on Macrophage Inflammation
Because glutathione metabolites are produced by adipocytes and are hypothesized to induce inflammatory signaling cascades in macrophages, RAW 264.7 or primary peritoneal macrophages were pretreated with 1 μg/mL LPS and then incubated for 24 h with GS-HNE or GS-DHN to evaluate TNF-α secretion. Treatment of RAW 264.7 macrophages resulted in a dose-dependent increase in TNF-α secretion (Fig. 5A). Interestingly, treatment of primary peritoneal macrophages with GS-DHN, but not GS-HNE, resulted in increased TNF-α secretion (Fig. 5B). In contrast, neither GS-HNE nor GS-DHN treatment resulted in increased monocyte chemoattractant protein-1 or interleukin (IL)-6 production in macrophages (data not shown).
To further characterize the proinflammatory properties of glutathione metabolites, peritoneal macrophages were incubated with GS-HNE or GS-DHN for 2 h, and LTC4 production was measured by LC-MS/MS. LTC4 has been implicated as playing an inflammatory role in macrophage biology (26), and levels of LTC4 increase in visceral adipose tissue with obesity (27). GS-HNE and GS-DHN both induced an approximately threefold increase in production of LTC4 (Fig. 5C).
Given results showing GS-HNE and GS-DHN have proinflammatory signaling properties, a panel of proinflammatory genes was surveyed to provide a more complete evaluation of the role of glutathione metabolites in inflammation. Treatment of primary peritoneal macrophages with 10 μmol/L GS-HNE or GS-DHN after LPS stimulation resulted in significantly increased expression of C3, C4b, c-Fos, igtb2, Nfkb1, and Nos2. In addition, GS-HNE induced increased expression of Csf1 (macrophage colony–stimulating factor [MCSF]), IL23 receptor, Toll-like receptor (TLR) 6, and TLR9, whereas GS-DHN induced increased expression of CD40 (Fig. 6).
GS-HNE/GS-DHN in GSTA4 OE Mice
To examine the effect of fat-specific GSTA4 overexpression on whole body metabolism, transgenic mice were generated expressing HA-tagged GSTA4 under FABP4 promoter and express the transgene in white and brown adipose tissue (Supplementary Fig. 1). As has been previously described, expression of GSTA4 in visceral adipose tissue was significantly downregulated (70% reduction; P < 0.05) on a high-fat diet (14). In contrast, adipose GSTA4 mRNA level in transgenic mice was not decreased by high-fat feeding (Fig. 7A). Owing to the differential effect of the high-fat diet on GSTA4 expression, transgenic mice had 15-fold and 42-fold higher levels of GSTA4 mRNA expression in low-fat and high-fat diet, respectively (Fig. 7A). In parallel to this, transgenic mice had a fivefold higher rate of GSTA4 enzymatic activity (Fig. 7B) and an ∼50% decrease in protein carbonylation in fat tissue (Fig. 7C). There was a trend toward higher levels of GS-HNE (P = 0.17) in epididymal adipose tissue of low fat–fed transgenic mice relative to wild-type mice but no difference in adipose GS-HNE content in high fat–fed transgenic mice relative to high fat–fed wild-type mice (data not shown). GS-DHN in epididymal adipose tissue was not different between transgenic and wild-type mice fed the low- or high-fat diet (data not shown).
GSTA4 transgenic mice fed a high-fat diet exhibited a significantly higher fasting blood glucose level (242 vs. 218 mg/dL, P < 0.05) but did not show a significant difference in weight compared with wild-type mice (data not shown). Glucose tolerance tests and insulin tolerance tests were performed on transgenic and wild-type mice fed a high-fat diet, and transgenic animals were mildly glucose-intolerant and had higher blood glucose on average at all time points (Fig. 8A and B). There was no difference in insulin tolerance tests between mouse strains.
Metabolism of α,β-unsaturated aldehydes by GST enzymes constitutes an important protective mechanism against oxidative damage to proteins, DNA, and lipids. Recent reports have characterized mitogenic and proinflammatory properties of GS-HNE and GS-DHN and their cell-permeable esters (19,20,28–30). Although these metabolites are products of the same pathway, GS-HNE, but not GS-DHN, induced peritoneal leukocyte infiltration and proinflammatory lipid and cytokine production (19,30). In contrast, GS-DHN formed via aldose reductase has been shown to induce inflammation (18,31) and mediate cytotoxic activity (28) in macrophages and induce mitogenic signaling in smooth muscle (30). A role for GS-HNE and GS-DHN in adipose biology is suggested by observations in RLIP76 knockout mice in which export of glutathione metabolites is blocked. These mice are protected against inflammation and, notably, from oxidative stress–induced insulin resistance (32,33).
To evaluate the role of GS-HNE and GS-DHN in obesity-induced metabolic syndrome, GS-HNE and GS-DHN were measured in visceral adipose tissue. GS-HNE levels were significantly increased in high fat–fed and ob/ob mice compared with chow-fed mice. GS-DHN was increased in ob/ob mice but lacked statistical significance for high fat–fed mice despite a very large effect size due to individual variability in GS-DHN. Expression of aldose reductase, which reduces GS-HNE to form GS-DHN, is upregulated by the antioxidant regulator KEAP (34). Thus, a possible explanation for variation in GS-DHN levels may be variable antioxidant response and, thus, variable expression of this enzyme. Interestingly, these increases occurred despite the observation that GSTA4, the primary enzyme responsible for glutathionylation of 4-HNE, is downregulated ∼90% during chronic overnutrition (14). This may represent a dramatic increase in lipid peroxidation with greater nonenzymatic formation of GS-HNE and GS-DHN and suggests these metabolites have the potential to maintain obesity-induced inflammation despite downregulation of GSTA4.
In vitro experimentation with macrophage and cultured adipocytes showed GS-HNE and GS-DHN production was increased in adipocytes, but not macrophages, in response to oxidative stress, suggesting adipocytes are responsible for oxidative stress–induced production of GS-HNE and GS-DHN in adipose tissue. To elucidate the oxidative stress response to overnutrition, 3T3-L1 adipocytes were grown in low- or high-glucose conditions. High glucose induced greater lipid accumulation in adipocytes, mirroring lipid accumulation in adipose tissue during chronic overnutrition. Growing 3T3-L1 adipocytes in high-glucose conditions alone did not result in increased GS-HNE or GS-DHN production. However, H2O2 with high glucose synergistically increased GS-HNE and GS-DHN, suggesting high glucose exposure potentiates cells toward increased oxidative stress and lipid peroxidation. The mechanism for this potentiation is not clear and may be due to increased reactive oxygen species production, increased lipid substrate for lipid peroxidation, or both. Experiments with GSTA4-silenced and OE 3T3-L1 adipocytes demonstrated oxidative-stress induced production of GS-HNE and GS-DHN was dependent on GSTA4 expression, supporting the conclusion that GSTA4 is the primary enzyme responsible for the regulation of production of GS-HNE and GS-DHN.
Although both glutathionyl lipid aldehydes induced dose-dependent increases in TNF-α production by macrophages in culture, GS-DHN was effective at lower concentrations than GS-HNE. Primary peritoneal macrophages produced TNF-α in response to GS-DHN, but response to GS-HNE was weaker and not statistically significant. The more potent induction of the inflammatory cytokine TNF-α by GS-DHN is consistent with previous studies showing GS-DHN, but not GS-HNE, is responsible for inducing macrophage production of inflammatory mediators (31). In contrast, production of LTC4 by peritoneal macrophages was similar in response to GS-HNE or GS-DHN. Differential activity of GS-HNE and GS-DHN may indicate differences in their role in acute inflammatory response, as characterized by LTC4 production (35) versus chronic inflammation as characterized by TNF-α (36). Induction of macrophage production of TNF-α (37,38) by GS-DHN represents a potential direct mechanism by which adipocyte oxidative stress may induce macrophage inflammation via intercellular cross talk. The role and relative importance of GS-HNE are less clear, but one possibility is an indirect chemotactic mechanism as LTC4 induces vascular permeability, contributing to immune cell infiltration (39), consistent with previously identified chemotactic activity of GS-HNE in the peritoneum (19).
Increased TNF-α and LTC4 production provide evidence that glutathionyl lipid aldehydes display chronic and acute proinflammatory properties. To broaden characterization of these inflammatory properties, RNA from primary peritoneal macrophages treated with GS-DHN or GS-HNE was assessed by proinflammatory microarray analysis. GS-HNE and GS-DHN both increase C3, C4b, Nos2 (inducible nitric oxide synthase), NF-κB1, Igtb2, and c-FOS. C3 and C4b are important in the complement cascade and contribute to the innate immune response (40). Nos2 and NF-κB1 are involved in increasing proinflammatory gene expression (41,42). Igtb2 is found in myeloid cells and is associated with the innate immune response of macrophages (43). Fos interacts with TLR signaling pathways, contributing to inflammatory response (44). In addition, GS-HNE, but not GS-DHN, induced increased expression of MCSF, IL23R, TLR6, and TLR9. MCSF is involved in differentiation of peripheral monocytes into macrophages and is important in M1 polarization of macrophages, a proinflammatory phenotype (45). IL23R is associated with a number of autoimmune disorders (46). TLR6 and TLR9 are involved in pathogen recognition and innate immune response (47). GS-DHN, but not GS-HNE, induced increased expression of CD40, which is found on antigen-presenting cells and is a member of the TNF receptor superfamily that binds interferon-γ (48). Taken together, these array data indicate that GS-HNE and GS-DHN induce an inflammatory response via expression of a number of genes involved in the innate immune response and infiltration and polarization of macrophages to a proinflammatory phenotype.
To study the role of GSTA4 in the development of insulin resistance, transgenic mice OE GSTA4 were fed a high-fat diet. Although transgenic mice became similarly obese and activity of GSTA4 was higher in transgenic fat, actual levels of GS-HNE and GS-DHN were not significantly higher in their adipose tissue, relative to wild-type mice. Because glutathionyl lipid aldehydes are actively transported out of the cell into the bloodstream, further metabolized in the kidney, and excreted, the content of tissue at any given time likely largely represents steady-state levels in the extracellular matrix and local tissue vasculature, with a relatively small intracellular content. This may explain the discrepancy between increased GSTA4 capacity and unchanged levels of its product in transgenic mice relative to wild-type mice. Another possibility is limitation of GS-HNE and GS-DHN production by the precursor 4-HNE, which may be equally elevated in wild-type and transgenic mice. In contrast, the differences seen in GS-HNE content in mice fed a high-fat diet relative to mice fed chow is consistent with both increased 4-HNE production and increased fat tissue mass.
Despite unchanged tissue GS-HNE and GS-DHN content, fasting blood glucose was significantly higher in transgenic mice. This difference may indicate that although adipose GS-HNE and GS-DHN levels are unchanged, increased GSTA4 activity results in increased efflux of glutathionyl lipid aldehydes from adipocytes and increased exposure of tissue-resident macrophages to these inflammatory mediators. Action of GS-HNE on chemotaxis of inflammatory cells or GS-DHN on activation of macrophages may contribute to the development of insulin resistance.
Interestingly, GSTA4-null mice, although showing an increased steady-state level of 4-HNE in their tissues (49), were noted to have an extended life span (50) that was attributed to an associated increase in antioxidant response (50). Studies described here suggest decreased inflammation may be an alternate explanation, supported by the observation that GSTA4-null mice show greater susceptibility to bacterial infection (49), an indication of reduced immune function.
These results suggest a novel mechanism for development of obesity-induced metabolic syndrome in which oxidative stress in adipocytes results in increased production of GS-HNE and GS-DHN, inducing a macrophage inflammatory response. Induction of inflammatory cytokines and lipids then feeds forward to adipocytes, inducing insulin resistance and metabolic dysfunction. This model provides a plausible mechanism for oxidative stress-induced inflammation via intercellular cross talk. Furthermore, obesity-induced decreases in GSTA4 expression may be a compensatory response, supporting the concept that downregulation of GSTA4 is an adaptive mechanism designed to decrease the inflammatory cascade induced by GS-HNE and GS-DHN.
Acknowledgments. The authors thank the members of the Bernlohr laboratory for helpful suggestions during the preparation of this manuscript and the members of the University of Minnesota Center for Mass Spectrometry and Proteomics (Minneapolis, MN) for their assistance with lipid analysis.
Funding. Research reported in this study was supported by the National Institutes of Health (NIH) under grants DK-084669 and DK-053189 to D.A.B., P30-DK-050456 to B.I.F., and F32-DK-091004 to E.K.L. The content is solely the responsibility of the authors and does not necessarily represent the official views of the NIH.
Duality of Interest. No potential conflicts of interest relevant to this article were reported.
Author Contributions. B.I.F. and E.K.L. researched data, performed analysis and interpretation, and wrote the manuscript. W.S.H. developed the mouse model, researched data, performed analysis and interpretation, contributed to discussion, and reviewed and edited the manuscript. D.A.B. developed the overall research plan, contributed to analysis and interpretation, and reviewed and edited the manuscript. D.A.B. is the guarantor of this work, and, as such, had full access to all the data in the study and takes responsibility for the integrity of the data and the accuracy of the data analysis.
Prior Presentation. Parts of this study were presented in abstract form at the Joint Meeting of Pediatric Endocrinology, Milan, Italy, 20 September 2013.
This article contains Supplementary Data online at http://diabetes.diabetesjournals.org/lookup/suppl/doi:10.2337/db13-0777/-/DC1.
- Received May 15, 2013.
- Accepted September 15, 2013.
- © 2014 by the American Diabetes Association.
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