Thioesterase induction by 2,3,7,8-tetrachlorodibenzo-p-dioxin results in a futile cycle that inhibits hepatic β-oxidation

Abstract

2,3,7,8-Tetrachlorodibenzo-p-dioxin (TCDD), a persistent environmental contaminant, induces steatosis by increasing hepatic uptake of dietary and mobilized peripheral fats, inhibiting lipoprotein export, and repressing β-oxidation. In this study, the mechanism of β-oxidation inhibition was investigated by testing the hypothesis that TCDD dose-dependently repressed straight-chain fatty acid oxidation gene expression in mice following oral gavage every 4 days for 28 days. Untargeted metabolomic analysis revealed a dose-dependent decrease in hepatic acyl-CoA levels, while octenoyl-CoA and dicarboxylic acid levels increased. TCDD also dose-dependently repressed the hepatic gene expression associated with triacylglycerol and cholesterol ester hydrolysis, fatty acid binding proteins, fatty acid activation, and 3-ketoacyl-CoA thiolysis while inducing acyl-CoA hydrolysis. Moreover, octenoyl-CoA blocked the hydration of crotonyl-CoA suggesting short chain enoyl-CoA hydratase (ECHS1) activity was inhibited. Collectively, the integration of metabolomics and RNA-seq data suggested TCDD induced a futile cycle of fatty acid activation and acyl-CoA hydrolysis resulting in incomplete β-oxidation, and the accumulation octenoyl-CoA levels that inhibited the activity of short chain enoyl-CoA hydratase (ECHS1).

Introduction

Although the liver is the largest internal organ, it is second to adipose tissue in regard to lipid storage capacity. Approximately 15–25% (fasted vs fed state, respectively) are derived from chylomicron remnants, 5–30% (fasted vs fed state, respectively) from de novo lipogenesis, and 5–30% from visceral fat tissues¹. Under normal circumstances, lipid accumulation is coordinated by regulating uptake, utilization, and export (via very low-density lipoproteins [VLDL]) to ensure triacylglycerol (TAG) and cholesterol ester (CE) levels remain low. Excess fatty acids (FAs) are packaged into TAGs and CEs, not only for storage, but to reduce their potential lipotoxicity^2,3. Chronic simple, reversible, fat accumulation, or steatosis, may progress to steatohepatitis with fibrosis, as in the case of non-alcoholic fatty liver disease (NAFLD). NAFLD impairs liver function and increases the risk for more complex metabolic diseases such as: metabolic syndrome (MetS), diabetes, cardiovascular disease and hepatocellular carcinoma (HCC). NAFLD alone is estimated to affect ≥ 35% of the U.S. population and has become the second leading reason for requiring a liver transplant⁴.

NAFLD development is described by a ‘multi-hit hypothesis’ in which consecutive insults collectively promote the progression of liver pathologies such as steatosis, inflammation and fibrosis⁵. Diverse pharmaceuticals and xenobiotics induce hepatic fat accumulation. For example, pesticides and solvents are the most frequently identified chemicals to induce hepatic steatosis while 2,3,7,8-tetrachlorodibenzo-p-dioxin (TCDD) and related compounds exhibit the greatest potency^6,7. Previous studies have shown that male mice exhibit greater sensitivity to TCDD-elicited reductions in body weight gain compared to females, despite no change in daily food intake^8–10. Hepatic micro- and macro-steatosis, immune cell infiltration, fibrosis, and bile duct proliferation (males only) were dose-dependently induced following oral gavage with TCDD every 4 days for 28 days^11,12. Lipidomic analysis of hepatic steatosis induced by TCDD and related compounds reported marked increases in FAs, TAGs, phospholipids, and CEs^13–15. Fat accumulation has been attributed to increased hepatic uptake of dietary and mobilized peripheral fats, inhibition of VLDL export, and repression of FA oxidation^8,13,16,17. In humans, TCDD and related compounds are associated with altered lipid homeostasis, including steatosis with fibrosis and inflammation^6,18–20. Epidemiological studies also report elevated serum TAG and cholesterol levels in exposed workers^21,22. More recently, a study of second generation Seveso accident victims (age 2–39 years) suggested in utero TCDD exposure increased MetS risk in males²³. These data suggest that environmental contaminants may play an underappreciated role in the development of NAFLD and its associated metabolic diseases²⁴.

Most, if not all, of the effects of TCDD and related compounds are mediated by the aryl hydrocarbon receptor (AHR), a ligand-activated basic-helix-loop-helix Per-Arnt-Sim transcription factor. Mouse models deficient in AHR report no adverse effects following treatment with TCDD compared to wild-type animals^25–27. Although numerous endogenous metabolites, drugs, xenobiotics, and natural products bind to the AHR, its endogenous ligand(s) and role(s) remain elusive²⁸. Ligand binding to the cytosolic AHR causes dissociation of chaperone proteins, followed by translocation to the nucleus and heterodimerization with the aryl hydrocarbon receptor nuclear translocator (ARNT). In the canonical pathway, the AHR-ARNT complex interacts with dioxin response elements (DREs) within the promoter region of target genes, leading to recruitment of transcriptional co-regulators and differential gene expression²⁹. Studies also report binding to non-consensus DREs and DRE-independent mechanisms of differential gene expression^28,30. The dose-dependent species-, sex-, age-, tissue-, and cell-specific biochemical and toxicological responses are believed to be the result of aberrant differential gene expression mediated by the AHR^28,31. Despite our detailed understanding of AHR-mediated gene regulation, links between TCDD-elicited differential expression and adverse biological effects have not been fully elucidated.

Though FAs can undergo α- and ω-oxidation, β-oxidation is the primary pathway for FA oxidation to produce ATP, as well as intermediates for macromolecular and ketone biosynthesis. Binding proteins, such as diazepam binding inhibitor (DBI; aka acyl-CoA binding protein), fatty acid binding proteins (FABPs), and sterol carrier protein 2 (SCP2), not only shunt FAs to acyl-CoA synthetases for activation, but also protect acyl-CoAs from hydrolysis, channel acyl-CoAs to specific pathways, and protect against free FA and acyl-CoA toxicity^32–35. In β-oxidation, activated FAs are subjected to oxidation, hydration, a second oxidation, and finally coenzyme A (CoASH)-dependent thiolytic cleavage to complete the cycle, producing an acetyl-CoA and acyl-CoA that is two carbons shorter³⁶. Peroxisomal and mitochondrial β-oxidation employ similar strategies but exhibit different substrate preferences and use different enzymes encoded by distinct genes. Mitochondrial β-oxidation prefers long, medium, and short chain FAs (LCFAs, MCFAs and SCFAs, respectively), while peroxisomes metabolize very long chain FAs (VLCFAs), LCFAs, bile acid precursor side chains, and dicarboxylic acids (DCAs) produced via ω-oxidation, as well as branched chain FAs following α-oxidation³⁷. Under conditions of acyl-CoA accumulation that limits CoASH availability due to sequestration, cytosolic, peroxisomal, and mitochondrial thioesterases exert control by hydrolyzing β-oxidation substrates and end products, but not intermediates. This releases CoASH in order to support CoASH-dependent reactions in other pathways³⁸.

Despite studies reporting β-oxidation inhibition by TCDD and related compounds in rodents, the mechanism remains uncertain. In this study, we examined straight chain FA oxidation to test the hypothesis that TCDD dose-dependently represses gene expression at key steps in β-oxidation. Notably, TCDD decreased hepatic acyl-CoA levels except for the marked dose-dependent increase in octenoyl-CoA and non-monotonic increases in DCAs, consistent with the inhibition of β-oxidation. TCDD repressed genes associated with lipid hydrolysis, FA binding proteins, FA activation, and thiolytic cleavage while inducing thioesterases. These results suggest TCDD induced a futile cycle of FA activation by acyl-CoA synthetases followed by thioesterase-mediated acyl-CoA hydrolysis resulting in incomplete β-oxidation and the accumulation of octenoyl-CoA.

Results

MS analysis of acyl-CoA species

Untargeted metabolomics identified dose-dependent decreases in hepatic acyl-CoAs following oral gavage every 4 days for 28 days (Table 1). Octanoyl-, hexanoyl-, butyryl- and acetyl-CoA were annotated based on parent ion mass, isotope similarity, and theoretical fragmentation. Scores > 40 had features matching parent ion mass and isotope distribution and MSE fragmentation data matching in silico mass fragmentation, while most metabolite scores averaged ~ 35 based on parent ion mass and isotope distribution metrics. The presence of 426.1 m/z and 408.0 m/z coenzyme A fragment ions observed in the MS^E fragmentation mass spectra further confirmed the acyl-CoA identifications for octanoyl-, hexanoyl-, butyrl-, and acetyl-CoA³⁹. Hepatic levels of hexanoyl-, butyryl-, and acetyl-CoA were repressed 34.9-, 11.8-, and 6.3-fold at 30 μg/kg TCDD, respectively. Other β-oxidation metabolites also exhibited dose-dependent decreases including butenoyl-CoA, 3-hydroxyhexanoyl-CoA and 3-hydroxybutanoyl-CoA, while octenoyl-CoA was dose-dependently induced 138.9-fold (Table 1, Supplementary Table 1). These dose-dependent decreases in FA oxidation intermediates are consistent with β-oxidation inhibition^13,17.

Table 1.

Effect of TCDD on acyl-CoA levels.

Compound ID	Description	Cn	Score	Fold-Change (TCDD vs. Veh.)
				0.3 µg/kg	1 µg/kg	3 µg/kg	10 µg/kg	30 µg/kg
HMDB01070	Octanoyl-CoA	8	36.8	1.77 ± 0.63	0.04 ± 0.01	0.28 ± 0.04	0.06 ± 0.03	0.01 ± 0.01
HMDB02845	Hexanoyl-CoA	6	37.2	1.43 ± 0.47	0.08 ± 0.02*	0.36 ± 0.05	0.08 ± 0.02	0.03 ± 0.02*
HMDB01088	Butyryl-CoA	4	44.3	1.24 ± 0.33	0.17 ± 0.05*	0.57 ± 0.10	0.09 ± 0.01*	0.08 ± 0.04*
HMDB01206	Acetyl-CoA	2	52.1	0.95 ± 0.12	0.30 ± 0.05*	0.53 ± 0.07*	0.04 ± 0.01*	0.16 ± 0.06*
HMDB03949	Octenoyl-CoA	8	34	1.66 ± 0.19	1.14 ± 0.23	26.16 ± 25.31	114.31 ± 4.89*	139.82 ± 6.88*

Acyl-CoA levels were assessed using untargeted liquid chromatography tandem mass spectrometry. Mice (n = 4–5) were orally gavaged every 4 days for 28 days with sesame oil vehicle or TCDD. Fold-changes were calculated for each treatment group relative to the vehicle control group. Bold font and asterisks (*) denote statistical significance (p ≤ 0.05) determined using a one-way ANOVA with a Dunnett’s post-hoc analysis. Scores were determined by Progenesis with 60 being the maximum value and 0 being the minimum value. Scores ranging from 30 to 40 are based on mass error and isotope distribution similarity, while score > 40 are based on mass error, isotope distribution and fragmentation score. All annotated compounds have a score distribution averaging ~ 35.

TAG and CE hydrolysis

Figure 1 summarizes the dose-dependent effects of TCDD on lipases, carboxylesterases, and a deacylase associated with TAG and CE hydrolysis. Note that because gene expression can vary significantly throughout the day due to circadian regulation, all fold-changes discussed in the text were derived from the circadian gene expression dataset to highlight the TCDD effects when controlled for diurnal rhythm (unless otherwise indicated). Despite similar trends, there may be fold-change discrepancies between the dose response and diurnal rhythmicity studies since the former study was not controlled for sample time collection.

Figure 1.

Effect of TCDD on lipid hydrolysis gene expression. Differential expression of genes associated with triacylglycerol hydrolysis assessed using RNA-seq. Mouse Genome Informatics (MGI) official gene symbols are used. (A) The presence of putative dioxin response elements (pDREs) and AHR genomic binding at 2 h. (B) Time-dependent expression following a single bolus dose of 30 μg/kg TCDD (n = 3). (C) Dose-dependent expression assessed following oral gavage every 4 days for 28 days with TCDD (n = 3). (D) Diurnal regulated gene expression denoted with a “Y”. An orange ‘X’ indicates abolished diurnal rhythm following oral gavage with 30 μg/kg TCDD every 4 days for 28 days. ZT indicates statistically significant (P1(t) > 0.8) time of maximum induction/repression. Counts represents the maximum number of raw aligned reads for any treatment group. Low counts (< 500 reads) are denoted in yellow with high counts (> 10,000) in pink. Differential gene expression with a posterior probability (P1(t)) > 0.80 is indicated by a black triangle in the top right tile corner. Protein subcellular locations were obtained from COMPARTMENTS and abbreviated as: cytosol (C), endoplasmic reticulum (ER), extracellular space (ES), Golgi apparatus (GA), lipid droplet (LD), lysosome (L), mitochondrion (M), nucleus (N), and plasma membrane (PM). The heatmap was created using R (v4.0.4).

Although TCDD induced gene expression of adipose triglyceride lipase (ATGL, Pnpla2) 4.3-fold, its paralog, Pnpla3, was repressed 37.7-fold. The requisite ATGL co-activator, CGI-58 (Abhydrolase Domain Containing 5, Abhd5) was also repressed 2.0-fold, as was G0s2 (10.9-fold), a potent ATGL inhibitor⁴⁰. In addition, other ATGL regulators including Faf2 (-1.6-fold), Cidec (8.7-fold), Plin2 (2.6-fold) and Plin5 (-3.1-fold) exhibited differential expression⁴¹. Lysosomal lipase A (Lipa, 2.3-fold), which deacylates endocytosed low-density lipoprotein TAGs and CEs, was dose-dependently repressed. Similarly, hormone sensitive lipase (Lipe, 3.3-fold), and hepatic lipase C (Lipc, 12.0-fold), which deacylate extracellular low-density lipoprotein TAGs and CEs, were also dose-dependently repressed. Highly expressed carboxylesterases, which serve important roles in lipid metabolism and VLDL assembly⁴², exhibited dose-dependent repression with the exception of Ces1b. Specifically, highly expressed Ces2a, Ces2e, Ces3a, and Ces3b were repressed 56.3-, 4.0-, 1,923-, and 1,333-fold, respectively. Ces mRNA, protein and/or enzymatic activity repression by TCDD and related compounds in mice and rats has been previously reported^43–45. Arylamide deacetylase (Aadac), another highly expressed gene associated with hepatic TAG metabolism⁴⁰ was dose-dependently repressed 28.6-fold. Both CESs and AADAC are localized to the extracellular region or endoplasmic reticulum. Interestingly, ATGL and monoglyceride lipase (Mgll, 2.7-fold), which are primarily located in the nucleus, cytosol, and plasma membranes, were both induced. In addition to substrate preferences based on fatty acid composition and cellular location, hydrolyases channel released FAs to specific fates such as β-oxidation, membrane formation, VLDL assembly or PPAR activation^40,42. Some lipases and carboxylesterases also exhibit cholesterol and retinyl ester hydrolysis activity.

The differential expression of genes associated with lipid hydrolysis was more pronounced at 28 days in mice treated with 30 μg/kg TCDD. Differential expression did not occur exclusively with genes exhibiting AHR enrichment. Although TCDD disrupted the diurnal rhythmicity of most lipid hydrolysis genes, this was not the case for highly expressed carboxylesterases which did not exhibit diurnal regulation. Ces genes are localized to a tandem cluster on chromosome 8 which may explain their collective repression by TCDD except for Ces1b⁴². Ces repression may also be due to the induction of proinflammatory cytokine signaling⁴³. Overall, the effect of TCDD on gene expression suggests lipid hydrolysis was repressed. However, cellular lipase mRNA levels do not always correlate with enzyme activity due to extensive post-translational regulation⁴⁶. Accordingly, hepatic levels of TAG, CEs, and bile acids were higher, as were free FAs suggesting esterification may be saturated^13,15.

FA and acyl-CoA binding proteins

We next examined the effect of TCDD on binding proteins that are important for lipid uptake, intra-/extra-cellular trafficking, and cytoprotection (Fig. 2)^34,35. In addition to channeling lipids to specific metabolic pathways, fatty acid binding proteins (FABPs), acyl-CoA binding protein (ACBP; aka diazepam binding inhibitor [DBI]), and sterol carrier protein 2 (SCP2) mitigate the toxicity, hydrolysis, and signaling potential of free acyl-CoAs. FABPs, DBI, and SCP2 also bind acyl-CoAs as well as other hydrophobic ligands including peroxisome proliferators, prostaglandins, bile acids, bilirubin, heme, fatty acid, and lipid metabolites. Highly expressed Fabp1, Dbi, and Scp2 encode for the majority of acyl-CoA buffering capacity and were repressed 5.9-, 7.1-, and 3.5-fold, respectively. Repression of the highly expressed DBI was consistent with gene expression patterns (Fig. 2E). Only Dbi exhibited an oscillating expression pattern that was abolished by TCDD (Fig. 2F). Despite AHR enrichment at 2 h in the presence of a putative DRE (pDRE), Fabp1, Dbi, and Scp2 exhibited minimal repression within 168 h of a single bolus gavage of 30 µg/kg TCDD. At 28 days, dose-dependent repression of Fabp1, Dbi, and Scp2 was observed with 10 and 30 µg/kg TCDD. Fabp2 and 5 were also repressed 4.5- and 1.9-fold, respectively. Despite the 6.6-, 14.0-, and 120.1-fold induction of Fabp4, 7, and 12, respectively, their induction would likely be insufficient to compensate for the loss of buffering capacity provided by FABP1, which showed expression levels ~ 125-fold higher than the other FABPs. FABP1, unlike other FABPs that only bind one FA, binds two FAs and accounts for 7–11% of the cytosolic protein in normal human liver³⁴. Fabp1, 5, and 12 all had multiple AHR enrichment sites but only Fabp2 and 12 exhibited differential expression at 168 h. Acyl-CoA binding domain containing proteins 4 and 5 (Acbd4 and 5), which facilitate acyl-CoA transfer to peroxisomes, were also repressed 2.7- and 3.1-fold, respectively. Consequently, decreased binding protein levels may impair FA and acyl-CoA channeling to specific pathways while increasing the potential for toxicity, signaling, and membrane disruption, as well as acyl-CoA susceptibility to hydrolysis.

Figure 2.

Effect of TCDD on intracellular fatty acid trafficking proteins. Differential expression of genes associated with intracellular fatty acid trafficking assessed using RNA-seq. Mouse Genome Informatics (MGI) official gene symbols are used. (A) The presence of putative dioxin response elements (pDREs) and AHR genomic binding at 2 h. (B) Time-dependent gene expression following a single bolus dose of 30 μg/kg TCDD (n = 3). (C) Dose-dependent gene expression assessed following oral gavage every 4 days for 28 days with TCDD (n = 3). (D) Diurnal regulated gene expression denoted with a “Y”. An orange ‘X’ indicates abolished diurnal rhythm following oral gavage with 30 μg/kg TCDD every 4 days for 28 days. ZT indicates statistically significant (P1(t) > 0.8) time of maximum gene induction/repression. Counts represent the maximum number of raw aligned reads for any treatment group. Low counts (< 500 reads) are denoted in yellow with high counts (> 10,000) in pink. Differential gene expression with a posterior probability (P1(t)) > 0.80 is indicated by a black triangle in the top right tile corner. Protein subcellular locations were obtained from COMPARTMENTS and abbreviated as: cytosol (C), endoplasmic reticulum (ER), extracellular space (ES), Golgi apparatus (GA), mitochondrion (M), outer mitochondrial membrane (OMM), nucleus (N), peroxisome (P), and plasma membrane (PM). (E) Capillary electrophoresis was used to assess DBI protein levels in total lysate prepared from liver samples harvested between ZT0-3 (n = 3). Bar graphs denote the mean ± SEM. Statistical significance (*p ≤ 0.05) was determined using a one-way ANOVA followed by Dunnett’s post-hoc analysis. (F) Diurnal expression of Dbi was assessed by RNA-seq (n = 3). Asterisks denotes a posterior probability (P1(t) > 0.8) within the same timepoint comparing vehicle to TCDD. Diurnal rhythmicity (‡) was determined using JTK_CYCLE for each treatment. Circadian data are plotted twice along the x-axis to better visualize the gene expression rhythmicity. The heatmap was created using R (v4.0.4). Plots were created using GraphPad Prism (v8.4.3).

FA activation

Twenty-five mouse acyl-CoA synthetases (ACSs) catalyze the irreversible activation of FAs for β-oxidation or lipid biosynthesis. Each exhibits different tissue expression, subcellular locations, and substrate preferences while also channeling substrates to different pathways⁴⁷. Twenty-two ACS genes were detected in the mouse liver including short- (Acss1-2; carbons length (C) 2–4), medium- (Acsm1-5; C6-10), long- (Acsl1, 3–6; C12-18), and very long- (Slc27a1-6; C12-30) members. Of the 17 abundantly expressed ACS genes, 15 were repressed including highly expressed (> 10,000 counts) Acsm1 (-12.5-fold), Acsl1 (-9.1-fold), Acsl5 (-5.6-fold), Slc27a2 (-5.9-fold), and Slc27a5 (-16.9-fold) following TCDD treatment (Fig. 3). In general, repression was dose-dependently observed within 168 h of a single bolus gavage of 30 µg/kg TCDD. Most ACS loci exhibited AHR enrichment in the presence of a pDRE at 2 h and exhibited disrupted diurnal expression. Although ACS mRNA levels poorly correlate with protein and enzyme activity⁴⁸, TCDD-elicited gene repression was consistent with decreases in ACSM3 and ACSL1 protein levels (Fig. 3F,H). Collectively, these data point to ACS repression by TCDD being a direct target of AHR activation.

Figure 3.

Effect of TCDD on hepatic fatty acid activation. Differential expression of genes associated with fatty acid activation assessed using RNA-seq. (A) Fatty acid activation reaction catalyzed via acyl-CoA synthetases. Official gene symbol designated in the MGI database are listed. (B) The presence of putative dioxin response elements (pDREs) and AhR enrichment at 2 h. (C) Time-dependent gene expression was assessed following a single bolus dose of 30 μg/kg TCDD (n = 3). (D) Dose-dependent gene expression following oral gavaged every 4 days for 28 days with 0.01, 0.03, 0.1, 0.3, 1, 3, 10 or 30 μg/kg TCDD (n = 3). (E) Circadian regulated genes are denoted with a “Y”. An orange ‘X’ indicates abolished diurnal rhythm following oral gavage with 30 μg/kg TCDD every 4 days for 28 days. ZT indicates statistically significant (P1(t) > 0.8) time of maximum gene induction/repression. Counts represent the maximum number of raw aligned reads for any treatment group. Low counts (< 500 reads) are denoted in yellow with high counts (> 10,000) in pink. Differential expression with a posterior probability (P1(t)) > 0.80 is indicated with a black triangle in the top right tile corner. Protein subcellular locations were obtained from COMPARTMENTS and abbreviated as: cytosol (C), endoplasmic reticulum (ER), Golgi apparatus (GA), lipid droplet (LD), lysosome (L), mitochondrion (M), outer mitochondrial membrane (OMM), inner mitochondrial membrane (IMM), nucleus (N), peroxisome (P), and plasma membrane (PM). Capillary electrophoresis was used to assess (F) ACSM3 and (H) ACSL1 protein levels in total lysate prepared from liver samples harvested between ZT0-3 (n = 3). Bar graphs denote the mean ± SEM. Statistical significance (*p ≤ 0.05) was determined using a one-way ANOVA followed by Dunnett’s post-hoc analysis. Diurnal expression of (G) Acsm3 and (I) Acsl1 was assessed by RNA-seq (n = 3). Asterisks denotes a posterior probability (P1(t) > 0.8) within the same timepoint comparing vehicle to TCDD. Diurnal rhythmicity (‡) was determined using JTK_CYCLE for each treatment. Circadian data are plotted twice along the x-axis to better visualize the gene expression rhythmicity. The heatmap was created using R (v4.0.4). Plots were created using GraphPad Prism (v8.4.3). The biochemical reaction was created using Adobe Illustrator (v25.2).

Mitochondrial and peroxisomal transport

While SCFAs and MCFAs passively enter mitochondria, LCFAs and VLCFAS must be transported into the mitochondria⁴⁹. At the outer mitochondrial membrane, carnitine palmitoyltransferase I (Cpt1a; -2.7-fold) replaces CoASH in the activated FA with carnitine for transport of the acyl-carnitine (Fig. 4). Carnitine/acylcarnitine translocase (Slc25a20 aka CACT; -1.6-fold), transports acyl-carnitine species across the inner mitochondrial membrane into the matrix where carnitine palmitoyltransferase 2 (Cpt2; no change in gene expression) reactivates the acyl-carnitine into acyl-CoA in preparation for β-oxidation. Cpt1a and Slc25a20, which both possess pDREs, were also repressed within 168 h with evidence of AHR enrichment at 2 h.

Figure 4.

Mitochondrial and peroxisomal free fatty acid and acyl-CoA transport. Differential expression of genes associated with fatty acid transport assessed by RNA-seq. Mouse Genome Informatics (MGI) official gene symbols are used. (A) The presence of putative dioxin response elements (pDREs) and AHR genomic binding at 2 h. (B) Time-dependent expression following a single bolus dose of 30 μg/kg TCDD (n = 3). (C) Dose-dependent gene expression assessed following oral gavage every 4 days for 28 days with TCDD (n = 3). (D) Diurnal regulated gene expression denoted with a “Y”. An orange ‘X’ indicates abolished diurnal rhythm following oral gavage with 30 μg/kg TCDD every 4 days for 28 days. ZT indicates statistically significant (P1(t) > 0.8) time of maximum gene induction/repression. Counts represent the maximum number of raw aligned reads for any treatment group. Low counts (< 500 reads) are denoted in yellow with high counts (> 10,000) in pink. Differential gene expression with a posterior probability (P1(t)) > 0.80 is indicated by a black triangle in the top right tile corner. Protein subcellular locations were obtained from COMPARTMENTS and abbreviated as: cytosol (C), endoplasmic reticulum (ER), lysosome (L), mitochondrion (M), outer mitochondrial membrane (OMM), inner mitochondrial membrane (IMM), nucleus (N), peroxisome (P), and plasma membrane (PM). The heatmap was created using R (v4.0.4).

ATP binding cassette subfamily member D (ABCD) 1 and 2, and to a lesser extent ABCD3, transport long- and very long-chain acyl-CoAs into peroxisomes⁵⁰. ABCD1 (Abcd1), which prefers saturated and unsaturated 18-22C acyl-CoA substrates, and ABCD3 (Abcd3), with a preference for bile acid conjugated FAs⁵¹, were both repressed 2.2-fold (Fig. 4). Abcd1 and 3 exhibited negligible differential expression in the time course study despite AHR enrichment with pDREs. In contrast, Abcd2 showed disrupted oscillating expression in the time course and dose response studies. Although Abcd2 prefers C22:6- and C24:6-CoAs⁵¹, the level of very long unsaturated FAs in TAGs and CEs was increased by TCDD¹³.

Dehydrogenation of activated acyl-CoA species

Despite the repression of lipid hydrolases and decreased acyl-CoA binding capacity, Table 1 indicates ongoing β-oxidation in the presence of TCDD as evidenced by the presence of short- and medium-chain acyl-CoAs. The first step involves acyl-CoA dehydrogenation between C2 and C3 to produce trans-2-enoyl-CoA. In the mitochondria, this oxidation is catalyzed by acyl-CoA dehydrogenases (ACAD) which exhibit different tissue expression, subcellular locations, and substrate preferences. Highly expressed Acad11, which preferentially oxidizes saturated C22-CoA⁵², was repressed in the time course and dose response (3.8-fold at 30 µg/kg TCDD) studies with AHR enrichment at 2 h in the presence of a pDRE (Fig. 5). However, highly expressed Acadvl (induced 1.6-fold), which has overlapping substrate preferences, likely offsets the decreased expression of Acad11 while the effects on Acadm, which preferentially oxidizes medium-chain acyl-CoAs, were negligible. Overall, the effects of TCDD on mitochondrial acyl-CoA dehydrogenase gene expression were modest. In contrast, highly expressed acyl-CoA oxidase 1 (ACOX1), the rate-limiting step in peroxisomal β-oxidation, was repressed in the time course, dose response and circadian (3.9-fold at 30 µg/kg TCDD) studies in the presence of AHR enrichment at 2 h and pDREs (Fig. 5). Accordingly, ACOX1 protein levels were also repressed (Fig. 5F). The results suggests peroxisomal β-oxidation is impeded by TCDD, consistent with the accumulation of free and esterified very long- and long-chain FAs within TAGs, CEs, and phospholipids^13,15.

Figure 5.

Effect of TCDD on β-Oxidation of acyl-CoAs. Differential expression of genes associated with β-oxidation assessed by RNA-seq. (A) Fatty acid β-oxidation is sequentially catalyzed via acyl-CoA dehydrogenases, enoyl-CoA hydratases, hydroxyacyl-CoA dehydrogenases and thiolases. Official gene symbol designated in the MGI database are listed. (B) The presence of putative dioxin response elements (pDREs) and AHR enrichment at 2 h. (C) Time-dependent gene expression was assessed following a single bolus dose of 30 μg/kg TCDD (n = 3). (D) Dose-dependent gene expression following oral gavaged every 4 days for 28 days with TCDD (n = 3). (E) Circadian regulated genes are denoted with a “Y”. An orange ‘X’ indicates abolished diurnal rhythm following oral gavage with 30 μg/kg TCDD every 4 days for 28 days. ZT indicates statistically significant (P1(t) > 0.8) time of maximum gene induction/repression. Counts represent the maximum number of raw aligned reads for any treatment group. Low counts (< 500 reads) are denoted in yellow with high counts (> 10,000) in pink. Differential expression with a posterior probability (P1(t)) > 0.80 is indicated with a black triangle in the top right tile corner. Protein subcellular locations were obtained from COMPARTMENTS and abbreviated as: cytosol (C), mitochondrion (M), mitochondrial outer membrane (OMM), mitochondrial inner membrane (IMM), nucleus (N), peroxisome (P), and plasma membrane (PM). (F/H) Capillary electrophoresis was used to assess ACOX1 and ECHS1 protein levels in total lysate prepared from liver samples harvested between ZT0-3 (n = 3). Bar graphs denote the mean ± SEM. Statistical significance (*p ≤ 0.05) was determined using a one-way ANOVA followed by Dunnett’s post-hoc analysis. (G) Diurnal expression of Acox1 was assessed by RNA-seq (n = 3). Asterisks denotes a posterior probability (P1(t) > 0.8) within the same timepoint comparing vehicle to TCDD. Diurnal rhythmicity (‡) was determined using JTK_CYCLE for each treatment. Circadian data are plotted twice along the x-axis to better visualize the gene expression rhythmicity. (I) ECHS1 activity was assessed by monitoring the depletion of crotonyl-CoA which has an absorbance at 263 nm. Statistical significance (*p ≤ 0.05) was determined using a one-way ANOVA followed by Dunnett’s post-hoc analysis. The heatmap was created using R (v4.0.4). Plots were created using GraphPad Prism (v8.4.3). The biochemical reaction was created using Adobe Illustrator (v25.2).

Hydration of trans-2-enoyl-CoA

The hydration of trans-2-enoyl-CoA to 3-hydroxyacyl-CoA is catalyzed by enoyl-CoA hydratases depending on the number of carbons in the substrate (Fig. 5). In the mitochondria, long chain enoyl-CoAs are hydrated by the HADHA subunit of the mitochondrial trifunctional protein (MTP). HADHA exhibits the highest activity for C12-16 enoyl-CoAs with virtually no activity towards C4 enoyl-CoAs⁵³. The expression of Hadha was not affected by TCDD. In contrast, ECHS1, the short chain enoyl-CoA hydratase, prefers C4 enoyl-CoAs with diminishing activity towards C10 enoyl-CoAs⁵⁴. Although Echs1 transcript levels was repressed 2.0-fold in the presence of AHR enrichment and pDREs, protein levels were induced (Fig. 5H). Furthermore, Fig. 5I shows that octenoyl-CoA inhibited the hydration of crotonyl-CoA, the preferred C4-enoyl substrate of ECHS1. A tenfold higher concentration of octenoyl-CoA inhibited the hydration of crotonyl-CoA > 90% providing compelling evidence that octenoyl-CoA can inhibit ECHS1 activity. TCDD does not directly inhibit ECHS1 enzymatic activity at concentrations previously reported to repress HepG2 cell proliferation and colony formation (Supplementary Fig. S2)⁵⁵.

In peroxisomes, Ehhadh, which encodes for the enoyl-CoA hydratase subunit of the liver bifunctional enzyme (L-BPE), was induced 7.7-fold in the absence of AHR enrichment and pDREs. After several cycles, the resulting peroxisomal medium-chain acyl-CoAs are transported to the mitochondria for further β-oxidation. Despite the expression of multiple acyl-CoA dehydrogenases that produce medium-chain enoyl-CoAs, there is only one enoyl-CoA hydratase, ECHS1, with a preference for medium and short-chain acyl-CoAs. Consequently, Echs1 repression may contribute to the dose-dependent accumulation of octenoyl-CoA (Table 1, Fig. 5).

Eci1 and 2, and Decr1 and 2 isomerize mono- and poly-unsaturated acyl-CoA cis double bonds to the 2-trans configuration, and the reduction of 2,4-dienoyl-CoAs to trans-3-enoyl CoA, respectively (Supplementary Fig. 1). Eci1, Eci2 and peroxisomal Decr2 were repressed by TCDD (2.1-, 2.2-, and 2.9-fold, respectfully) while highly expressed mitochondrial Decr1 was unaffected by TCDD. All four genes exhibited AHR enrichment in the presence of a pDRE. Without appropriate standards, it was not possible to determine the presence of cis- versus trans-enoyl-CoA or 2- versus 3-enoyl-CoA or the existence of polyunsaturated enoyl-CoA species. Collectively, the data suggests Δ^2,3-octenoyl-CoA is present although other octenoyl-CoA species may also exist.

Dehydrogenation of 3-hydroxyacyl-CoA

The oxidation of 3-hydroxyacyl-CoA to 3-ketoacyl-CoA is catalyzed by 3-hydroxyacyl-CoA dehydrogenase (Fig. 5). In the mitochondria, long-chain 3-hydroxyacyl-CoAs are oxidized by the highly expressed alpha subunit (Hadha) of MTP which was not affected by TCDD. In peroxisomes, the highly expressed Ehhadh subunit, which was induced 7.7-fold, preferentially oxidizes very long- and long-chain 3-hydroxyacyl-CoAs. Medium- and short-chain 3-hydroxyacyl-CoAs are then oxidized by Hadh and Hsd17b4 which were repressed 1.5- and 1.8-fold, respectively. Hadh and Hsd17b4 both exhibited AHR enrichment in the presence of a pDRE while Ehhadh induction occurred in the absence of AHR enrichment or pDREs.

Thiolysis of 3-ketoacyl-CoA

Thiolytic cleavage of 3-ketoacyl-CoA requires an additional CoASH to generate acetyl-CoA and an acyl-CoA that is two carbons shorter (Fig. 5). In the mitochondria, the MTP beta subunit (Hadhb), which exhibited no change, catalyzes the cleavage of long-chain 3-ketoacyl-CoAs. In peroxisomes, ACAA1A (Acaa1a), ACAA1B (Acaa1b) and SCP2 (Scp2), which preferentially catalyze very long 3-ketoacyl-CoA thiolysis, were repressed 1.8-, 3.9- and 3.5-fold, respectively. Long-, medium- and short-chain 3-ketoacyl-CoAs undergo thiolytic cleavage catalyzed by ACAA2 (Acaa2) and ACAT1 (Acat1) which were repressed 4.2- and 3.0-fold. All six genes with thiolytic cleavage activity exhibited AHR enrichment in the presence of a pDRE. Collectively, 5 of 6 genes associated with thiolase activity were repressed by TCDD.

Acyl-CoA deactivation

Excess FAs can overload β-oxidation causing mitochondrial stress that reduces flux and depletes free CoASH needed for other metabolic pathways including the TCA cycle and FA metabolism. In response, acyl-CoA thioesterases (ACOTs) hydrolyze acyl-CoAs releasing the CoASH from activated FAs (Fig. 6)⁵⁶. Therefore, we examined the effect of TCDD on cytosolic and mitochondrial thioesterase expression. Acot1 and Acot2, which exhibit a preference for long-chain acyl-CoAs, were induced 8.9- and 21.2-fold, respectively. ACOT2 is the primary mitochondrial thioesterase with little activity for < 10C acyl-CoAs. In contrast, Acot7 and Acot13, are enzymatically inhibited by CoASH, and were repressed 2.4- and 2.8-fold, respectively. Peroxisomal thioesterase Acot4, which prefers very long- and long-chain acyl-CoAs was induced 3.7-fold, while CoASH sensitive Acot8 that exhibits broad substrate preferences (C2-20 acyl-CoAs), was repressed 1.5-fold. Unlike the mitochondria, which catalyzes complete FA oxidation, peroxisomes only complete 2–5 β-oxidative cycles producing medium-chain acyl-CoAs that are hydrolyzed by ACOT3 (Acot3; induced 12.5-fold) and readily taken up by the mitochondria. Alternatively, they are transported to the mitochondria following conversion to medium-chain acylcarnitine by carnitine O-octanoyltransferase (Crot) (Fig. 7). Mitochondrial Acot9, which preferentially hydrolyzes medium- and short-chain acyl-CoAs, and is inhibited by CoASH, was also induced 6.0-fold (Fig. 6). Accumulating mitochondrial CoASH could then either be used to reactivate free FAs in the matrix or be exported to the cytosol via PMP34 (Slc25a17, no expression change) initiating a futile cycle (Fig. 7)⁵⁶. Nudt7 which preferentially cleaves medium-chain acyl-CoAs to acyl-phosphopantetheines and 3',5'-ADP, was repressed 8.0-fold⁵⁷. This futile cycle may be exacerbated by the 23.3-fold induction of Ucp2 which would not only facilitate the mitochondrial export of liberated FAs and FA peroxides, but dissipate the proton gradient and uncouple oxidative phosphorylation^58,59. In summary, TCDD-elicited differential gene expression of thioesterases favors the hydrolysis of very long- and long-chain acyl-CoAs freeing CoASH required for other reactions while leaving medium-chain acyl-CoAs intact for peroxisomal and mitochondrial β-oxidation.

Figure 6.

Hydrolysis of acyl-CoAs. Differential expression of genes associated with fatty acid deactivation assessed by RNA-seq. (A) Fatty acid deactivation reaction catalyzed via acyl-CoA thioesterases. Official gene symbol designated in the MGI database are listed. (B) The presence of putative dioxin response elements (pDREs) and AHR enrichment at 2 h. (C) Time-dependent gene expression was assessed following a single bolus dose of 30 μg/kg TCDD (n = 3). (D) Dose-dependent gene expression following oral gavaged every 4 days for 28 days with 0.01, 0.03, 0.1, 0.3, 1, 3, 10 or 30 μg/kg TCDD (n = 3). (E) Circadian regulated genes are denoted with a “Y”. An orange ‘X’ indicates abolished diurnal rhythm following oral gavage with 30 μg/kg TCDD every 4 days for 28 days. ZT indicates statistically significant (P1(t) > 0.8) time of maximum gene induction/repression. Counts represents the maximum number of raw aligned reads for any treatment group. Low counts (< 500 reads) are denoted in yellow with high counts (> 10,000) in pink. Differential expression with a posterior probability (P1(t)) > 0.80 is indicated with a black triangle in the top right tile corner. Protein subcellular locations were obtained from COMPARTMENTS and abbreviated as: cytosol (C), mitochondrion (M), nucleus (N), and peroxisome (P). The heatmap was created using R (v4.0.4). The biochemical reaction was created using Adobe Illustrator (v25.2).

Figure 7.

Mitochondria and peroxisomal fatty acid and CoASH transport. Differential expression of genes associated with mitochondrial and peroxisomal fatty acid and CoASH transport assessed by RNA-seq. Mouse Genome Informatics (MGI) official gene symbols are used. (A) The presence of putative dioxin response elements (pDREs) and AHR genomic binding at 2 h. (B) Time-dependent expression following a single bolus dose of 30 μg/kg TCDD (n = 3). (C) Dose-dependent gene expression assessed following oral gavage every 4 days for 28 days with TCDD (n = 3). (D) Diurnal regulated gene expression denoted with a “Y”. An orange ‘X’ indicates abolished diurnal rhythm following oral gavage with 30 μg/kg TCDD every 4 days for 28 days. ZT indicates statistically significant (P1(t) > 0.8) time of maximum gene induction/repression. Counts represent the maximum number of raw aligned reads for any treatment group. Low counts (< 500 reads) are denoted in yellow with high counts (> 10,000) in pink. Differential gene expression with a posterior probability (P1(t)) > 0.80 is indicated by a black triangle in the top right tile corner. Protein subcellular locations were obtained from COMPARTMENTS and abbreviated as: cytosol (C), mitochondrion (M), nucleus (N), peroxisome (P), and plasma membrane (PM). The heatmap was created using R (v4.0.4).

Omega(ω)-oxidation of fatty acids

FAs can also undergo ω-hydroxylation with subsequent metabolism by alcohol and aldehyde dehydrogenases to produce dicarboxylic acids (DCAs) when β-oxidation is impeded. Consequently, we examined our metabolomics data for the presence of DCAs. Dose-dependent changes in short-, medium- and long-chain DCAs were identified (Table 2). MCFAs (C10:0 and C12:0) are reported to have the greatest affinity for ω-oxidation⁶⁰. Sebacic (C10:0) and dodecanedioic (C12:0) acids were induced 20.4- and 1.5-fold. Both can undergo further peroxisomal β-oxidation to produce shorter DCAs. Suberic (C8:0), azelaic (C9:0) and undecanedioic (C11:0) acids were induced 2.8-, 2.7-, and 8.9-fold, respectively, between 1 and 10 µg/kg TCDD with decreasing levels at higher doses. The detection of azelaic acid has been previously reported in TCDD treated mice⁴³.

Table 2.

Induction of dicarboxylic acid levels by TCDD.

Compound ID	Description	Cn	Score	Fold-Change (TCDD vs. Veh.)
				0.3 µg/kg	1 µg/kg	3 µg/kg	10 µg/kg	30 µg/kg
HMDB00672	Hexadecanedioic acid	16	46.1	1.00 ± 0.03	0.93 ± 0.04	1.10 ± 0.14	1.33 ± 0.17	1.90 ± 0.41*
HMDB00872	Tetradecanedioic acid	14	43.5	0.99 ± 0.02	1.10 ± 0.07	0.91 ± 0.11	0.38 ± 0.04*	0.57 ± 0.10*
HMDB00623	Dodecanedioic acid	12	37.9	0.95 ± 0.01	1.13 ± 0.05	1.12 ± 0.05	1.18 ± 0.07	1.53 ± 0.11*
HMDB00888	Undecanedioic acid	11	42.7	0.36 ± 0.02	2.05 ± 0.21	3.01 ± 1.38	8.79 ± 0.67*	5.40 ± 1.96*
HMDB00792	Sebacic acid	10	36.5	0.44 ± 0.06	3.67 ± 0.53	6.54 ± 3.33	20.39 ± 3.53*	12.79 ± 5.62*
HMDB00784	Azelaic acid	9	45.9	0.90 ± 0.09	2.73 ± 0.26*	2.32 ± 0.57*	1.66 ± 0.12	2.22 ± 0.20*
HMDB00893	Suberic acid	8	37.9	0.83 ± 0.02	1.54 ± 0.13	1.50 ± 0.32	2.82 ± 0.38*	2.06 ± 0.31*

Dicarboxylic acid levels were assessed in mice using untargeted liquid chromatography tandem mass spectrometry. Mice (n = 4–5) were orally gavaged every 4 days for 28 days with sesame oil vehicle or TCDD. Fold-changes were calculated for each treatment group relative to the vehicle control group. Bold font and asterisks (*) denote statistical significance (p ≤ 0.05) determined using a one-way ANOVA with Dunnett’s post-hoc analysis. Scores were determined by Progenesis with 60 being the maximum value and 0 being the minimum value. Scores ranging from 30—40 are based on mass error and isotope distribution similarity, while score > 40 are based on mass error, isotope distribution and fragmentation score. All annotated compounds have a score distribution averaging ~ 35.

In ω-oxidation, SCFAs, MCFAs, LCFAs and VLCFAs are first ω-hydroxylated by the CYP4Bs, CYP4As, CYP4Fs or CYP4Us. However, most cytochrome P450, ADH, and ALDH genes associated with ω-oxidation were repressed (Fig. 8). Specifically, Cyp4a12a, Cyp4a12b and Cyp4a32 which preferentially ω-hydroxylate MCFAs were repressed 150.9-, 23.6 and 1.9-fold, respectively. Similarly, Cyp4f13 (-3.2-fold), Cyp4f14 (-387.6-fold), Cyp4f15 (-12.2-fold), Cyp4f17 (-3.1-fold) and Cyp4v3 (-4.5-fold) that preferentially ω-hydroxylate LCFAs were all repressed. Cyp2u1 which mediates the ω-hydroxylation of LCFAs was also repressed 10.2-fold. However, the principal genes that mediate FA ω-hydroxylation, Cyp4a10 and Cyp4a14, were induced 4.2-, and 6.7-fold, respectively. Cyp4a10 and Cyp4a14 induction is primarily mediated by PPARA (Ppara), which was repressed 8.7-fold, with AHR enrichment in the presence of a pDRE. Cyp4a31 and Cyp4f16 were also induced 25.9- and 4.1-fold. Of these induced genes, only Cyp4a31 exhibited AHR enrichment with a pDRE by TCDD at 2 h. Poorly defined alcohol and aldehyde dehydrogenases are responsible for the oxidation of ω-hydroxylated FAs. Adh4 and Adh5 expression was repressed 14.8- and 2.2-fold, respectively, consistent with other reports^61,62. TCDD did not affect Adh7 which is reported to oxidize long ω-hydroxylated FAs⁶³. Highly expressed Aldh1a1 was repressed 1.9-fold, while Aldh3a2 showed negligible changes. However, Aldh3b1 and Aldh18a1 were induced 41.1- and 19.0-fold, respectively. Despite most genes being repressed, key ω-oxidation genes were induced by TCDD consistent with increased DCA levels.

Figure 8.

ω-Oxidation of fatty acids into dicarboxylic acids. Differential expression of genes associated with ω-oxidation assessed by RNA-seq. (A) Fatty acid ω-oxidation is sequentially catalyzed via CYP450s, alcohol dehydrogenases and aldehyde dehydrogenases. Official gene symbol designated in the MGI database are listed. (B) The presence of putative dioxin response elements (pDREs) and AHR enrichment at 2 h. (C) Time-dependent gene expression was assessed following a single bolus dose of 30 μg/kg TCDD (n = 3). (D) Dose-dependent gene expression following oral gavaged every 4 days for 28 days with TCDD (n = 3). (E) Circadian regulated genes are denoted with a “Y”. An orange ‘X’ indicates abolished diurnal rhythm following oral gavage with 30 μg/kg TCDD every 4 days for 28 days. ZT indicates statistically significant (P1(t) > 0.8) time of maximum gene induction/repression. Counts represent the maximum number of raw aligned reads for any treatment group. Low counts (< 500 reads) are denoted in yellow with high counts (> 10,000) in pink. Differential expression with a posterior probability (P1(t)) > 0.80 is indicated with a black triangle in the top right tile corner. Protein subcellular locations were obtained from COMPARTMENTS and abbreviated as: cytosol (C), endoplasmic reticulum (ER), extracellular space (ES), mitochondrion (M), inner mitochondrial membrane (IMM), nucleus (N), peroxisome (P), and plasma membrane (PM). The heatmap was created using R (v4.0.4). The biochemical reaction was created using Adobe Illustrator (v25.2).

Discussion

In this study, TCDD is used as a prototypical AHR ligand and represents the cumulative burden of all AHR agonists. The dose range and regimen approached steady state levels while inducing full dose response curves for many genes in the absence of (i) necrosis or apoptosis, (ii) significant serum ALT increases, (iii) changes in food consumption and (iv) body weight loss > 15%^8,9. To provide perspective, 30 µg/kg TCDD resulted in mouse hepatic tissue levels comparable to serum levels reported in Viktor Yushchenko following intentional poisoning, while 0.03–0.1 μg/kg resulted in serum levels comparable to the Seveso cohort of women following the 1976 chemical release accident. At 0.01 µg/kg, hepatic levels were comparable to control hepatic levels, and to dioxin-like compound levels in US, German, Spanish and British serum samples^8,64,65. Consequently, the dose range and regimen are relevant to human exposures, and the elicited effects cannot be attributed to overt toxicity. Conservation of the AHR, and similarities in AHR-mediated dyslipidemia and metabolic disease between rodents and humans, suggest a common mechanism that may identify novel therapeutic interventions for NAFLD which currently has limited treatment options⁶⁶.

TCDD dose-dependently induced steatosis in mice with marked increases in TAGs, CEs, phospholipids, and free FAs in the absence of acute toxicity^13,15. This steatosis is attributed, in part, to the accumulation of dietary lipids and the inhibition of VLDL export^13,67. Previous metabolomic analysis suggested TCDD disruptedd β-oxidation based increased palmitoylcarnitine¹⁵, with more targeted functional assays demonstrating repression of hepatic β-oxidation^13,17, which was confirmed by dose-dependent decreases in shorter chain acyl-CoAs. This is consistent with reported decreases of acyl-CoAs by 2,3,7,8-tetrachlorodibenzo-p-furan (TCDF) in mice and in human liver Huh-7 cells following TCDD treatment^68,69. We further investigated this inhibition by integrating metabolomics, ChIP-seq, and RNA-seq datasets to determine the effects of TCDD on FA oxidation, focusing on differential gene expression associated with lipid hydrolysis, FA activation, binding proteins, β-oxidation, and acyl-CoA hydrolysis.

RNA-seq analysis identified seven of nine lipid hydrolases repressed by TCDD with only Pnpla2 and Lpl showing induction. Yet, TCDD increased hepatic free FA levels which could serve as substrate for β-oxidation. The increase in FA levels is attributed not only to increased hepatic uptake of dietary FAs and mobilized peripheral lipids following CD36 induction, but also reduced ACS levels^13,15,17. ACSs catalyze a two-step, ATP-dependent, reaction producing activated FAs required for β-oxidation to proceed. In addition, genes encoding the predominant FA binding proteins FABP1, DBI, and SCP2, which also bind acyl-CoAs, heme, bile acids, retinoids, and other hydrophobic ligands, were repressed by TCDD, therefore reducing cytosolic, peroxisomal, and mitochondrial acyl-CoA binding capacity and trafficking. Furthermore, FABPs, DBI, and SCP2 buffer the toxicity, block the signaling potential of free ligands, and protect acyl-CoAs from hydrolysis^34,70. For example, long-chain acyl-CoAs are powerful disruptors of membrane bilayers, inhibit diverse enzyme activities, and alter ion channel function⁷¹. Consequently, decreases in ACS and binding proteins would impede FA metabolism by reducing activated FA levels, and increasing acyl-CoA susceptibility to hydrolysis.

CoASH is an obligate cofactor for > 100 different metabolic reactions. It does not passively diffuse across membranes, and therefore distinct cytosolic, peroxisomal, and mitochondrial CoASH and acyl-CoA pools exist. Hereditary or acquired conditions involving CoA ester accumulation, often referred to as CoASH sequestration, toxicity, or redistribution (CASTOR) disease, lead to the accumulation of one or more acyl-CoA species that reduce free CoASH levels causing adverse effects⁷². Deficiencies in short-, medium-, long-, and very long-chain acyl-CoA dehydrogenase, trifunctional protein, and carnitine shuttle activities are associated with CASTOR disease⁷². This phenomena is also associated with the toxicity of valproic, salicylic, pivalic, phenylbutyric, and benzoic acids and does not solely arise from free CoASH depletion^72,73.

In response to CoASH sequestration, thioesterases prevent acyl-CoA levels from reaching toxic levels³⁸. TCDD dose-dependently induced cytosolic, peroxisomal, and mitochondrial thioesterases including Acot9 which prefers medium-chain acyl-CoAs, but is strongly inhibited by CoASH favoring octanoyl-CoA accumulation. Furthermore, Nudt7 which hydrolyzes free CoASH and acyl-CoAs to (acyl)phosphopantetheines and 3’,5’-ADP, was repressed⁵⁷. Nudt7 repression and thioesterase induction would increase free CoASH levels and de-activate FAs in an ATP-consuming futile cycle that inhibits β-oxidation. Collectively, (i) ACS repression and thioesterase induction would reduce activated FA levels required for β-oxidation, while (ii) decreased FABPs, DBI, and SCP2 binding capacity would increase acyl-CoA susceptibility to hydrolysis and compromise trafficking substrates to metabolic pathways. Moreover, Ucp2 induction would export liberated FAs from the matrix, uncoupling oxidative phosphorylation and further compromise energy production. The accumulation of TAGs and CEs containing long-chain FAs¹³, the dose-dependent decrease in acyl-CoA levels (Table 1), and the detection of palmitoylcarnitine in serum, all suggest TCDD impaired FA oxidation¹⁵. Increased palmitoyl (C16)-, tetradecanoyl (C14)-, and decanoyl (C10)-carnitine levels are also reported in factory workers with 29.49–765.35 pg TEQs/g lipid levels⁷⁴. Elevated serum acylcarnitine levels are associated with NAFLD⁷⁵, suggesting the effects of TCDD in mice may have relevance in humans.

An unexpected result was the dose-dependent increase in octenoyl-CoA. In the mitochondria, long-chain acyl-CoAs are oxidized by multiple dehydrogenases that were minimally affected by TCDD. The trifunctional protein (MTP), encoded by Hadha and Hadhb, carries out the enoyl-CoA hydratase, hydroxyacyl-CoA dehydrogenase, and 3-ketothiolase activities. Hadha expression was not affected by TCDD, Hadhb was modestly induced, and thiolases (Acaa1b, Acaa2) were repressed. Enoyl-, 3-hydroxy- and 3-keto-acyl-CoA intermediates are not substrates for thioesterases. Very long- and long-chain acyl-CoAs that escape thioesterase hydrolysis and complete several β-oxidation spirals would result in the production of medium-chain acyl-CoAs. TCDD induced thioesterases with a preference for very long- and long-chain acyl-CoAs. Acot9 which prefers medium-chain acyl-CoAs was also induced but is strongly inhibited by CoASH³⁸. Peroxisomal MCFAs produced by peroxisomal β-oxidation would be ferried into the mitochondrial matrix via carnitine O-octanoyltransferase (Crot) which prefers medium-chain acyl-CoAs^36,57, MCFA trafficking is not dependent on binding proteins and tend to be metabolized by hepatic mitochondrial β–oxidation following activation as opposed to being incorporated into TAGs, CEs or phospholipids⁴⁹. We posit that accumulating peroxisomal and mitochondrial octanoyl-CoAs are oxidized to octenoyl-CoA by ACADM which was largely unaffected by TCDD. Accumulating octenoyl-CoA levels represent a metabolic conundrum since the HADHA enoyl-CoA hydratase subunit prefers substrate chain lengths of C12-16 with virtually no activity⁵³. ECHS1, the short chain enoyl-CoA hydratase, prefers C4 enoyl-CoAs with diminishing activity towards C10 enoyl-CoAs, although ECHS1 has been reported hydrate enoyl-CoA species up to C10^54,76. This is somewhat analogous to ACADM deficient mice where octanoyl-CoA oxidation is not compensated by other acyl-CoA dehydrogenases⁷⁷. Moreover, in addition to being a poor substrate for hydration, we showed octenoyl-CoA inhibited the hydration of crotonyl-CoA, the preferred substrate of ECHS1.

When β-oxidation is hindered, FAs can undergo ω-hydroxylation, primarily by CYP4A10 and CYP4A14, with subsequent oxidation by poorly defined cytosolic alcohol and aldehyde dehydrogenases to produce DCAs⁷⁸. In humans, ω-oxidation is a secondary pathway responsible for 5–10% of FA metabolism under normal conditions. During fasting, starvation, or when β-oxidation is impeded due to an inborn error of metabolism, ω-oxidation is considered a rescue pathway producing DCAs that undergo peroxisomal β-oxidation to produce TCA cycle and gluconeogenesis intermediates⁷⁹. Conversely, DCAs are also associated with oxidative stress, lipotoxicity and PPAR activation that induces β-oxidation⁸⁰. However, TCDD repressed Ppara expression and inhibits PPARα-mediated gene expression⁸¹, thus compromising β-oxidation induction by DCAs.

Long-chain DCAs can be reactivated to the corresponding CoA ester and undergo chain shortening by peroxisomal β-oxidation to produce DCAs of varying length following hydrolysis by thioesterases⁸². For example, dodecanedioic acid (12C) can be oxidized to sebacic (C10) and suberic acids (C8) while undecanedioic acid (11C) is rarely detected since it is partially oxidized in peroxisomes before further mitochondrial metabolism. Interestingly, TCDD decreased serum azelaic (C9) acid levels due to the repression of CES3 that hydrolyzes monoesters to release azelaic acid⁴³. By extrapolation, we surmise that decreasing DCA levels (Table 2) at higher TCDD doses is inversely correlated with the repression of Ces genes that exhibit different DCA monoester preferences as reported for other carboxylesterase substrates^43,83.

In summary (Fig. 9), we propose that β-oxidation inhibition by TCDD is due to the differential expression of genes peripheral to the spiral itself. More specifically, TCDD represses lipid hydrolysis, FA activation, and binding protein expression, while inducing thioesterases. However, most of the effects reported here are limited to gene expression and selected proteins, and do not consider post-translational modifications that can also regulate enzyme activity. Nevertheless, the data suggest TCDD induces a futile cycle of FA activation by ACSs and de-activation by thioesterases that inhibits complete oxidation of FAs, uncouples oxidative phosphorylation, and depletes ATP levels. Consequently, FAs underwent ω-oxidation producing PPAR ligands in an attempt to induce β-oxidation. However, Ppara and Fabp1, the encoded proteins, of which, deliver ligands to PPARα, were repressed thwarting efforts to induce β-oxidation. This would not only further deplete energy levels but also increase free FA and DCA levels that likely exacerbate TCDD toxicity. The inhibition of ECHS1 activity and accumulation of mitochondrial octenoyl-CoA may also contribute to toxicity by precipitating metabolic decompensation due to the exhaustion of free CoASH required by enzymes in other pathways. Moreover, octenoyl-CoA may itself be toxic by inappropriately inducing signaling, and/or possess lytic (detergent-like) properties that disrupt membranes. Although many of these effects are consistent with the development and progression of NAFLD, as well as AHR-mediated hepatotoxicity following activation by TCDD and related compounds, their relevance in human models warrants further investigation. This should include complementary metabolomic analyses of other fractions and compartments such as serum and urine for metabolites associated with impaired β-oxidation and NAFLD.

Figure 9.

Summary of the effects of TCDD on fatty acid oxidation. Inhibition of β-oxidation in TCDD-induced hepatic steatosis involves the (i) repression of FA binding proteins, (ii) repression of FA activation, and (iii) induction of thioesterase activity. Acyl-CoA synthetase repression reduces activated FAs available for β-oxidation while the repression of binding proteins increases acyl-CoA susceptibility to hydrolysis by induced thioesterases. VLCFAs and LCFAs were partially metabolized in peroxisomal β-oxidation (green box) to medium-length chain FAs (MCFAs) due to peroxisomal specific thioesterase activity which deactivates acyl-CoAs. Peroxisomal CROT transports MCFAs out of peroxisomes to the mitochondria (orange box). MCFAs, such as octanoic acid, could also diffuse out of peroxisomes and into mitochondria where they undergo oxidation following activation by acyl-CoA synthetases. In the canonical pathway, acyl-CoAs are first oxidized by acyl-CoA dehydrogenases that were minimally affected by TCDD. Two enzymes catalyze the subsequent step of mitochondrial β-oxidation; HADHA (which prefers long chain acyl-CoAs) and ECHS1 which prefers short and medium chain acyl-CoAs. Peroxisomal and mitochondrial medium chain acyl-CoA species would accumulate, specifically octenoyl-CoA, due to substrate overload and inhibition of ECHS1 activity by accumulating octenoyl-CoA levels. Octenoyl-CoA accumulation also sequesters free CoASH inhibiting other CoASH-dependent reactions including the thiolytic cleavage of the ketoacyl-CoA into acetyl-CoA and an acyl-CoA that is 2 carbons shorter. Therefore, TCDD dose-dependently induced a futile cycle of FA activation and acyl-CoA hydrolysis leading to octenoyl-CoA accumulation that inhibits ECHS1 activity and depletes free coenzyme A required by enzymes in other pathways leading to the inhibition of β-oxidation and energy depletion. With β-oxidation impaired, accumulating FFAs undergo ω-oxidation leading to increases in DCAs. Proteins are denoted with an oval. Red arrows indicate induction and blue arrows indicate repression. Solid lines denote reactions while dashed lines denote substrate trafficking. The figure was created using Adobe Illustrator (v25.2).

Methods

Animal treatment

Postnatal day 25 (PND25) male C57BL/6 mice weighing within 10% of each other were obtained from Charles River Laboratories (Kingston, NY). Mice were housed in Innovive Innocages (San Diego, CA) containing ALPHA-dri bedding (Shepherd Specialty Papers, Chicago, IL) in a 23 °C environment with 30–40% humidity and a 12 h/12 h light/dark cycle. Aquavive water (Innovive) and Harlan Teklad 22/5 Rodent Diet 8940 (Madison, WI) was provided ad libitum. TCDD (AccuStandard, New Haven, CT) was dissolved in acetone and diluted in sesame oil to a working stock. The acetone from the working stock was then evaporated off using nitrogen gas. On PND28, mice were orally gavaged at the start of the light cycle (zeitgeber [ZT] 0) with 0.1 ml sesame oil vehicle (Sigma-Aldrich, St. Louis, MO) or 0.01, 0.03, 0.1, 0.3, 1, 3, 10, and 30 μg/kg body weight TCDD every 4 days for 28 days for a total of 7 treatments. The first gavage was administered on day 0, while the final gavage was on day 24 of the 28-day study. This dosing regimen was selected to approach steady state levels given the 8–12 day half-life of TCDD in mice⁸⁴. Comparable treatment has been used in previous studies^{8,9,13,16,17,43}. Mice were fasted six hours prior to the end of the study. On day 28, vehicle- and TCDD-treated mice were weighed and euthanized. Liver samples were immediately flash frozen in liquid nitrogen and stored at − 80 °C until analysis. This study was conducted in accordance with relevant guidelines and regulations. All animal procedures were approved by the Michigan State University (MSU) Institutional Animal Care and Use Committee (IACUC; PROTO201800043) and meet the ARRIVE guidelines.

Liquid chromatography tandem mass spectrometry

Samples were extracted using methanol:water:chloroform as previously described with slight modifications⁹. Briefly, untargeted extractions were reconstituted with 400 µl tributylamine with no dilutions for analysis. Analysis was performed using a Xevo G2-XS QTOF attached to a Waters UPLC (Waters, Milford, MA) with negative-mode electrospray ionization run in MS^E continuum mode. LC phases, gradient rates, and columns were used as previously published⁹. For untargeted acyl-CoA analysis, MS^E continuum data was processed with Progenesis QI (Waters) to align features, peaks, deconvolute, and annotate metabolite peaks. Metabolite annotations were scored based on a mass error < 12 ppm to Human metabolome Database entries⁸⁵, isotopic distribution similarity, and theoretical fragmentation comparisons to MS^E high-energy mass spectra using the MetFrag option with each metric contributing a max of 20 points towards a max score of 60. Raw signals for each compound abundances were normalized to a correction factor calculated using a median and mean absolute deviation approach by Progenesis QI. Significance was determined by a one-way ANOVA adjusted for multiple comparisons with a Dunnett’s post-hoc test.

Protein quantification and capillary electrophoresis protein analysis

Frozen samples (~ 50 mg) were homogenized in RIPA buffer with protease inhibitor (Sigma-Aldrich) using a Polytron PT2100 homogenizer (Kinematica, Lucerne, Switzerland) and sonicated on ice. Samples were centrifuged and protein concentration measured using a bovine serum albumin standard curve and a bicinchoninic acid (BCA) assay (Sigma-Aldrich). The WES capillary electrophoresis system (ProteinSimple, San Jose, CA) was used following standard manufacturer protocols with the following antibodies and dilutions from Proteintech (Rosemont, IL): ACOX1 (1:50; 10,957–1-AP), ACSM3 (1:50; 10,168–2-AP), ACSL1 (1:50; 13,989–1-AP), DBI (1:50; 14,490–1-AP). Primary antibodies were detected using an anti-rabbit detection module (ProteinSimple). Chemiluminescence signal intensity was analyzed with Compass Software v4.0.0 (ProteinSimple). Representative spectra for each protein in each treatment group can be found in Figure S3. GraphPad Prism v8.4.3 (La Jolla, CA, USA) was used to conduct a one-way ANOVA followed by a Dunnett’s post-hoc analysis to determine statistical significance (p ≤ 0.05).

ECHS1 enzymatic activity assay

Enoyl-CoA hydratase, short chain 1 (ECHS1) activity was measured spectrophotometrically as previously described^86,87. Hepatic extracts were prepared from control mice treated with sesame oil vehicle every 4 days for 28 days using crotonyl-CoA (Sigma-Aldrich) and trans-2,3-octenoyl-CoA (Toronto Research Chemicals, Toronto, Canada) as substrates. Total protein lysates were isolated from frozen samples with NP-40 cell lysis buffer (Thermo Fisher Scientific, Waltham, MA) with protease inhibitor using a Polytron PT2100 homogenizer (Kinematica). Incubations were performed in 100 mM Tris buffer (pH 8.0) supplemented with 0.1 mg/ml bovine serum albumin at 37 °C for 5 min. Reactions were started with 0.02 mg/ml total protein lysate and one of the following substrate ratios: 0.025 mM crotonyl-CoA (1:0 ratio), 0.025 mM crotonyl-CoA:0.025 mM octenoyl-CoA (1:1 ratio), or 0.025 mM crotonyl-CoA:0.25 mM octenoyl-CoA (1:10 ratio). ECHS1 activity was measured by following the decrease in absorbance over time at 263 nm using a SpectraMax ABS Plus (Molecular Devices, San Jose, CA). Enzymatic activity was calculated using 6700 cm⁻¹ M⁻¹ as the extinction coefficient.

Protein location data

COMPARTMENTS (accessed September 30, 2020) was used for cytosol (C), endoplasmic reticulum (ER), extracellular space (ES), Golgi apparatus (GA), lipid droplet (LD), lysosome (L), mitochondrion (M), mitochondrial outer membrane (OMM), mitochondrial inner membrane (IMM), nucleus (N), peroxisome (P), and plasma membrane (PM) mouse protein localizations⁸⁸. COMPARTMENTS is a database that integrates evidence on protein subcellular localization from multiple sources including curated literature, high-throughput screens, automatic text mining, and sequence-based prediction methods.

Author contributions

G.N.C., R.R.F. and T.R.Z. designed the project. R.R.F., K.A.F., N.A.Z. and R.N. performed the animal work. G.N.C., R.R.F., N.A.Z., and K.A.F. performed the experiments. R.R.F. developed the LC–MS workflow for untargeted metabolomics. G.N.C., R.R.F. and N.A.Z. compiled all the data and produced the figures and tables. G.N.C., R.R.F. and T.R.Z. wrote the manuscript. All authors reviewed the manuscript.

Data availability

Hepatic RNA-seq data sets were previously published^9,10,89. Differentially expressed genes (|fold-change|≥ 1.5 and posterior probability (P1(t)) ≥ 0.8) were determined by empirical Bayes analysis⁹⁰. Time course (GSE109863), dose response (GSE87519), and diurnal rhythmicity (GSE119780) sequencing data are available at the Gene Expression Omnibus. Diurnal rhythmicity was determined using JTK_CYCLE as previously described⁹. AHR ChIP-seq (GSE97634) and computationally identified putative dioxin response elements (pDREs, https://doi.org/10.7910/DVN/JASCVZ) data were previously published¹⁰. ChIP-seq analysis used a false discovery rate (FDR) ≤ 0.05. pDREs were considered functional with a matrix similarity score (MSS) ≥ 0.856 and associated with genes when located 10 kb upstream of the transcription start site (TSS) to the transcription end site (TES). Raw metabolomic data is deposited in the NIH Metabolomics Workbench (ST001379).

Competing interests

The authors declare no competing interests.

Supplementary Information

The online version contains supplementary material available at 10.1038/s41598-021-95214-0.