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Programmed suppression of oxidative phosphorylation and mitochondrial function by gestational alcohol exposure correlate with widespread increases in H3K9me2 that do not suppress transcription
Epigenetics & Chromatin volume 14, Article number: 27 (2021)
A critical question emerging in the field of developmental toxicology is whether alterations in chromatin structure induced by toxicant exposure control patterns of gene expression or, instead, are structural changes that are part of a nuclear stress response. Previously, we used a mouse model to conduct a three-way comparison between control offspring, alcohol-exposed but phenotypically normal animals, and alcohol-exposed offspring exhibiting craniofacial and central nervous system structural defects. In the cerebral cortex of animals exhibiting alcohol-induced dysgenesis, we identified a dramatic increase in the enrichment of dimethylated histone H3, lysine 9 (H3K9me2) within the regulatory regions of key developmental factors driving histogenesis in the brain. However, whether this change in chromatin structure is causally involved in the development of structural defects remains unknown.
Deep-sequencing analysis of the cortex transcriptome reveals that the emergence of alcohol-induced structural defects correlates with disruptions in the genetic pathways controlling oxidative phosphorylation and mitochondrial function. The majority of the affected pathways are downstream targets of the mammalian target of rapamycin complex 2 (mTORC2), indicating that this stress-responsive complex plays a role in propagating the epigenetic memory of alcohol exposure through gestation. Importantly, transcriptional disruptions of the pathways regulating oxidative homeostasis correlate with the emergence of increased H3K9me2 across genic, repetitive, and non-transcribed regions of the genome. However, although associated with gene silencing, none of the candidate genes displaying increased H3K9me2 become transcriptionally repressed, nor do they exhibit increased markers of canonical heterochromatin. Similar to studies in C. elegans, disruptions in oxidative homeostasis induce the chromatin looping factor SATB2, but in mammals, this protein does not appear to drive increased H3K9me2 or altered patterns of gene expression.
Our studies demonstrate that changes in H3K9me2 associate with alcohol-induced congenital defects, but that this epigenetic change does not correlate with transcriptional suppression. We speculate that the mobilization of SATB2 and increased enrichment of H3K9me2 may be components of a nuclear stress response that preserve chromatin integrity and interactions under prolonged oxidative stress. Further, we postulate that while this response may stabilize chromatin structure, it compromises the nuclear plasticity required for normal differentiation.
Dysregulation of chromatin structure underlies several neurodevelopmental disorders and cognitive impairments . However, emerging evidence reveals that histone H3 lysine 9 (H3K9), in particular, serves as a major hub in chromatin-based regulatory mechanisms important to central nervous system development and function. For example, disruption of acetylation on H3K9 leads to anxiety-related behavioral abnormalities [2,3,4] and blocking H3K9 deacetylation through pharmacological HDAC inhibitors serves as a powerful tool to counteract neurodegeneration-related cognitive decline [5, 6]. Similarly, inhibition of H3K9 methylation improves memory in the aged hippocampus [7, 8] and pharmacological inhibition of H3K9 methyltransferase activity restores alcohol-induced deficits in learning and memory [9,10,11]. Therefore, understanding the mechanisms driving the post-translational modifications of H3K9 is crucial to understanding central nervous system development and function.
We recently conducted a three-way comparison of chromatin structure between control offspring, alcohol-exposed but phenotypically normal animals (unaffected), and alcohol-exposed offspring exhibiting craniofacial and central nervous system structural defects (affected). In these studies, we focused on identifying changes in chromatin structure within the regulatory regions of genes directing the patterning of the brain that distinguish alcohol-exposed affected versus unaffected individuals. We identified a dramatic and widespread increase in the enrichment of dimethylated histone H3, lysine 9 (H3K9me2) in animals exhibiting alcohol-induced structural defects. At the same time, offspring in the alcohol-exposed unaffected group remained identical to the controls . Why regulatory regions within affected tissues become enriched for H3K9me2 and whether this change in chromatin structure is a passive symptom of dysgenesis or causally involved in the development of structural defects remains unknown.
While exposure to drugs of abuse, including cocaine, morphine, and alcohol, all increase global acetylation and influence H3K9 methylation, these changes in chromatin structure scarcely correlate with altered gene expression, especially on a genome-wide scale [13, 14]. In contrast, each of these toxicants also associates with the development of oxidative stress, which induces protective alterations in chromatin structure [15, 16]. Recent work in the nematode Caenorhabditis elegans indicates that changes in chromatin structure, increased H3K9me2 specifically, constitute an integral component of the metabolic stress response . Further, hypoxic stress can induce G9a-dependent increases in H3K9me2 across a range of cultured mammalian cells . Therefore, the increased methylation of H3K9 observed in these studies and our model may be a component of the cellular stress response, independent of programs controlling transcriptional regulation.
One of the critical emerging questions in the field of exposure biology is whether toxicant-induced changes in chromatin structure are causal in altering gene expression or are symptoms of exposure tied to transcription-independent nuclear changes promoting genome stability. Although H3K9me2-enriched regions of the genome associate with gene silencing, heterochromatin also protects chromosome integrity during cellular stress . Further, recent studies indicate that increased H3K9 methylation and formation of heterochromatin-like domains do not necessarily result in widespread gene repression . Work in multiple organisms, including C. elegans, have demonstrated that the effects of early-life mitochondrial dysfunction and oxidative stress persist throughout the lifespan [21, 22]. Patterns of H3K9 methylation transmit through the cell cycle, and therefore, may represent a heritable memory of the larger nuclear organization induced by early-life exposures [23,24,25,26]. However, whether stress-induced H3K9 methylation directly influences patterns of gene expression remains unanswered.
We hypothesized that the increased Histone H3 Lysine 9 dimethylation observed in alcohol-exposed tissues exhibiting dysgenesis represent a core element in a conserved genome-wide defense mechanism, one that may not directly influence gene transcription. Using deep-sequencing, we find tissue-specific disruptions in the genetic pathways controlling oxidative phosphorylation and mitochondrial function associate with widespread increases in H3K9me2. This increased H3K9me2 does not correlate with transcriptional suppression, appears in a non-transcribed region of the genome, and does not associate with increased markers of canonical heterochromatin. Similar to studies in worms, we also observe the induction of the mammalian homolog of the C. elegans chromatin looping protein DVE-1 (SATB2) . Importantly, our studies also implicate the mammalian target of rapamycin complex 2 (mTORC2) as one of the main drivers of this response, suggesting therapeutic interventions targeting this pathway may rescue alcohol-induced central nervous system patterning defects.
Materials and methods
Ethanol treatments and tissue collection
All animal procedures were approved and conducted in accordance with the Institutional Animal Care and Use Committee at the University of North Carolina. This study utilized C57BL/6J mice (RRID:IMSR_JAX:000664). We administered intraperitoneal injections of EtOH (2.9 g/kg, cat# E7023; Millipore-Sigma) to pregnant dams on gestational day 7 (GD7), as described previously . Control dams were injected with a comparable volume of lactated Ringer’s solution. We terminated pregnancies on gestational day 17 (GD17) and then scored the offspring for ocular and cortical patterning defects using a previously described system [28, 29]. After assessment, we dissected the left and right cortices, cerebellum and heart, then immediately flash froze samples using liquid nitrogen.
DNA and RNA isolation, and sequencing analysis
We isolated total RNA from the GD17 cortex using the RNeasy Plus Mini Kit (catalog # 74134, Qiagen) according to the manufacturer’s instructions. Before RNASeq library preparation, we randomized samples and generated sequencing libraries using the TruSeq RNA Sample Preparation kit (catalog # RS-122-2001, Illumina). We sequenced pooled samples using an Illumina HiSeq 2500 at Whitehead Genomic Services (Cambridge, MA). The sequencing data were demultiplexed, aligned using STAR with default parameters , and referenced against the Mus musculus genome (UCSC version mm10).
RNA deep sequencing data analysis, selection of candidate mRNAs, and functional analysis
After obtaining 50-bp length paired-end reads, we used Bowtie and Tophat to align them into transcripts based on the Mouse Reference Genome (UCSC version mm10). We then used the Cufflinks suite to measure the relative abundance of each transcript. We quantified gene expression levels as the number of reads mapping to a gene divided by the gene length in kilobases and the total number of mapped reads in millions, and designated outputs as fragments per kilobase of exon per million fragments mapped (FPKM). To select differentially expressed transcripts, we generated volcano plots measuring statistical significance and magnitude of fold-change based on the log2 fold-change (X-axis) and − log10 p-value from the Cufflinks suite (Y-axis). We selected differentially expressed mRNAs based on a linear p-value cut off of 0.05, which was considered significant and highlighted by colored dots in the volcano plot. We conducted the Causal Network Analysis and Biological Pathway Enrichment analysis using the Ingenuity Pathway Analysis (IPA) software suite (QIAGEN Inc.) .
Neural stem cell culture and EtOH exposure
Derivation of primary mouse fetal cerebral cortical neuroepithelial stem cells is described here . We cultured free-floating neurospheres in T75 flasks containing a 50%/50% mixture by volume of Neurobasal media (Cat# 21103-049; Invitrogen) and DMEM F-12 (Cat# 11320-033; Invitrogen). This medium was supplemented with the N2-supplement (Cat# 17502-048; Invitrogen), B27 supplement (Cat# 17504-044; Invitrogen), 0.05% TC grade BSA in PBS (Cat# A1933 Sigma), 2 mM l-glutamine (Cat# 25030-081; Invitrogen), 1× penicillin/streptomycin (Cat# 15140-122; Invitrogen), 20 µg/mL FGF basic (Cat# PMG0034; Invitrogen), 20 µg/mL EGF (Cat# PHG0311; Invitrogen), and 0.85 units/mL heparin (Cat# H3149; Sigma). We cultured cells in medium containing either 160 mg/dL, 240 mg/dL, or 0 mg/dL (control) EtOH (cat# E7023; Millipore-Sigma). We cultured neurospheres in treated medium for 72 h, and collected samples for ChIP and RNA analysis after a 4-day recovery phase with no EtOH.
Chromatin immunoprecipitation (ChIP)
We thawed the cortices derived from a single brain and filtered the tissues into a single-cell suspension using gentle mechanical dissociation. We washed cells twice with PBS containing protease inhibitor cocktail (Cat# 78437; Thermo Scientific) and re-suspended them in medium (DMEM F-12 Cat# 11320-033; Invitrogen) containing 0.1 volume crosslinking solution . We carried out chromatin immunoprecipitation reactions following the previously published protocol . The specific antibodies used in this study include anti-H3K9me2 (Cat# 39239; Active Motif, RRID:AB_2793199), antiH3K9me3 (Cat# 05-1242; Millipore-Sigma, RRID:AB_1587136), antiH4K20me3 (Cat# 91107; Active Motif, RRID:AB_2793777), anti-SATB2 (Cat# ab34735; Abcam, RRID:AB_2301417) and the negative IgG control (Cat# SC-2027; Santa Cruz, RRID:AB_737197). We used antibodies for modified histones and the IgG control at a concentration of 1 µg/ChIP reaction and 4 µg/ChIP reaction for SATB2. We purified precipitated DNA using the QIAquick PCR Purification Kit (catalog # 28106, Qiagen) and assayed the enrichment of the indicated sequences using quantitative PCR. We performed qPCR using the Dynamo Flash supermix (Cat# F-415XL; Thermo Scientific) on a Bio-Rad CFX384 Touch PCR system. Primer sequences are listed in Additional file 1.
Analysis of gene expression
We isolated total RNA from the GD17 fetal cerebellum and heart using the AllPrep DNA/RNA/Protein Mini Kit (Catalog No. 80004; Qiagen) according to the manufacturer’s instructions. We then seeded 1 μg of RNA into a reverse transcription reaction using the High Capacity cDNA Reverse Transcription Kit (Catalog No. 4368814; Thermo Fisher) following the recommended protocol. We assayed gene expression using the DyNamo Flash SYBR qPCR kit (Catalog No. F-415; Thermo Fisher) on a Bio-Rad CFX384 Touch PCR system. Primer sequences are listed in Additional file 1. To normalize gene expression levels, we assayed the expression of the reference genes Glyceraldehyde 3-phosphate dehydrogenasetyrosine (Gapdh), 3-monooxygenase/tryptophan 5-monooxygenase activation protein zeta (Ywhaz), and H2A Histone family member Z (H2afz). For studies in the fetal cortex, we used Gapdh and Ywhaz. For studies in the cerebellum and heart, we replaced Gapdh with H2afz due to increased stability .
Western immunoblot analysis
We isolated protein from the GD17 fetal cortex using the AllPrep DNA/RNA/Protein Mini Kit (Catalog No. 80004; Qiagen) according to the manufacturer’s instructions. We then separated 5–10 µg of protein on 10–15% sodium dodecyl sulfate-polyacrylamide gels and transferred proteins to nitrocellulose membranes. The primary antibodies we used in this study are: anti-H3K9me2 (Cat# 39239; Active Motif, RRID:AB_2793199), anti-pan histone H3 (Cat# ab1791; Abcam, RRID:AB_302613), anti-SATB2 (Cat# ab34735; Abcam, RRID:AB_2301417) and anti-Tubulin (Cat# ab40742; Abcam, RRID:AB_880625). We visualized blots using secondary antibodies conjugated to horseradish peroxidase (catalog# sc-2004; RRID:AB_631746; Santa Cruz Biotechnology, Santa Cruz, CA, USA) and an enhanced chemiluminescence detection system (Pierce, Rockford, IL, USA). We calculated relative levels of H3K9me2 as a ratio to total histone H3, and relative levels of SATB2 as a ratio to Tubulin. We quantified band intensities by densitometry using ImageJ (RRID:SCR_003070; National Institutes of Health, Bethesda, MD, USA). Each experimental group contains protein extracts derived from 5 control, 3 unaffected, 4 affected animals.
For RT-qPCR analysis of gene expression, we imported the replicate cycle threshold (Ct) values for each transcript into Excel and normalized expression to the geometric mean of two validated reference genes . We then used the −∆∆CT method  to calculate the relative fold-change for each biological replicate. For studies using ChIP, we calculated the enrichment of each sequence using the published formula . After collating datasets in Excel, we then input the calculated values into the statistical analysis program GraphPad Prism 8 (RRID:SCR_002798; GraphPad Software, Inc., La Jolla, CA, USA) and set statistical significance set at alpha = 0.05. We then verified all datasets for normality using the Brown–Forsythe test. For the analysis of ChIP and RT-qPCR data, we conducted a one-way analysis of variance followed by an uncorrected Fisher’s LSD post hoc test. Data presented are mean ± standard error of the mean.
Transcriptome analysis of the alcohol-exposed, affected fetal cortex reveals deregulation of oxidative phosphorylation and mitochondrial pathways
To identify transcriptional differences distinguishing affected fetuses from unaffected offspring, we returned to our previously published, early gestational binge model of maternal alcohol exposure . Here, dams were intraperitoneally administered injections of either vehicle or alcohol on gestational day-7. On gestational day-17 (GD17), stage-matched control and alcohol-exposed fetuses were dissected and scored for both ocular and craniofacial congenital defects. After determining the sex of each fetus using PCR analysis targeting the Y-chromosome, we found that the majority of affected samples (13/17; 76%) were female. We then isolated RNA from the GD17 fetal cortex of three (n = 3) control, EtOH-exposed unaffected, and EtOH-exposed affected offspring and conducted deep-sequencing analysis of the cortex transcriptome. Our sequencing analyses identified a small number (88) of differentially expressed transcripts between the control and unaffected samples. In contrast, comparisons between control and affected, as well as unaffected and affected, identified 876 (412 downregulated, 522 upregulated) and 2281 (1432 downregulated, 1041 upregulated) differentially expressed genes, respectively (Fig. 1A, B).
The top three molecular pathways identified by Ingenuity Pathway Analysis  between unaffected: affected and control: affected comparisons were Oxidative Phosphorylation, Mitochondrial Dysfunction and EIF2 Signaling (Fig. 1B), all of which converge on the regulation of cellular respiration or the oxidative stress response [17, 38]. We validated the differential expression of the top genes in the Oxidative Phosphorylation and Mitochondrial Dysfunction pathways using RT-qPCR (Fig. 1C). These assays confirmed the downregulation of all candidates in the EtOH-exposed affected offspring. With a larger sample size, we also observed some differential expression of select candidate genes in the EtOH-exposed unaffected group. However, these samples tended to exhibit a lower fold-change than the affected offspring.
Alcohol-induced disruption of genes controlling cellular respiration and oxidative stress is tissue specific
In our model, gestational day-7 exposures predominantly impact cortical development, while sparing the cerebellum . In contrast, exposures on gestational day-8 induce significant cerebellar-specific reductions in volume, indicating stage-specific sensitivities of these subregions . To determine if the transcriptional signature identified in the cortices of EtOH-exposed affected offspring is present in morphologically normal tissues, we assayed the abundance of transcripts encoding the above candidate genes within the cerebellum. We also examined the heart, as the development of this organ is exquisitely sensitive to oxidative stress . As shown in Fig. 2A, we did not observe any differences in candidate gene expression in the cerebellum. At the same time, while hearts exhibited downregulation of Atp5e in tissues isolated from both unaffected and affected offspring, we did not detect differences in any other candidate gene (Fig. 2B). From these data, we conclude that the programmed suppression of the genetic pathways regulating Oxidative Phosphorylation, Mitochondrial Dysfunction, and EIF2 Signaling is unique to the cortex of EtOH-exposed affected brains.
Affected tissues display upregulation of mTORC2 and correlative increases in histone H3 lysine 9 dimethylation that do not associate with transcriptional repression
Out of the 109 identified candidate genes in the Oxidative Phosphorylation and Mitochondrial Dysfunction pathways, 105 are targets of the mammalian target of rapamycin complex 2 (mTORC2) (p-value = 9.19E−42). Consistent with these findings, we observed upregulation of multiple mTORC2 complex members in the alcohol-exposed affected offspring (p-value = 4.19E−09) and downregulation of targets known to be negatively regulated by mTORC2 . In mammals, mTORC2 has an established role in directing epigenetic changes in gene function, leading to enduring alterations in oxidative respiration and metabolism . However, how mTORC2 establishes and propagates this epigenetic memory is unknown. In yeast, the TOR2 complex is essential for establishing histone h3 lysine 9 dimethylation (H3K9me2) and promoting heterochromatin formation, stability, and spreading . Further, two independent studies using cultured mammalian cells and C. elegans identified a link between oxidative stress, the nuclear lamina, and increased global enrichment of H3K9me2 [17, 18].
Our previous experiments examining alcohol-induced epigenetic changes in the developing brain identified increased H3K9me2 in the promoter regions of several essential genes controlling cellular identity and proliferation . To determine if the differentially expressed genes we identified here also display this change, we selected a cohort of downregulated (Fig. 1C) and upregulated (Fig. 3A) candidate genes and assayed the enrichment of H3K9me2 within their promoter regions. As seen in Fig. 3B, only the promoter region of Prrc2a, an upregulated gene, displayed increased H3K9me2 compared to the control and unaffected offspring. We then turned to our RNA-seq dataset to examine transcript levels of the previously identified candidate genes exhibiting increased H3K9me2. Despite showing dramatic increases in H3K9me2 enrichment , only Ascl1 and Dlx2 were differentially expressed, and similar to Prrc2a, both of these candidates also displayed increased expression (Fig. 3C).
To determine how widespread this increase in H3K9me2 is, we measured the enrichment of this post-translational modification within the regulatory regions of IAP, LINE1 elements, and major satellite class repeats between control, EtOH-exposed unaffected, and EtOH-exposed affected brain cortex. In addition, we also determined the enrichment of H3K9me2 in an untranscribed region of chromosome 6 (Untr6), which provides a measure of genomic background in ChIP assays examining transcription factor binding . These experiments revealed increased enrichment of H3K9me2 in all three classes of repetitive DNA, as well as in the untranscribed region of chromosome 6 (Fig. 4A). Again, the increased H3K9me2 within repetitive sequences associated with increased transcription, not silencing (Fig. 4B). Unexpectedly, in EtOH-exposed unaffected cortices, we observed upregulation of LINE1 and major satellite class repeats, whereas IAP elements were only upregulated in EtOH-exposed affected samples. To determine if the enrichment in H3K9me2 reflects a global increase, we quantified H3K9me2 using western blotting and normalized measures to levels of total histone H3. As seen in Fig. 4C, we did not observe any differences in total cellular H3K9me2 between experimental groups. From these data, we conclude that EtOH-exposed affected tissues exhibit widespread increases in H3K9me2 that do not strictly associate with transcriptional suppression and are not reflective of a genome-wide increase in this post-translational modification.
Alcohol-induced enrichment of H3K9me2 does not associate with the formation of canonical heterochromatin
Di-methylation and tri-methylation of lysine nine are recognized components of heterochromatin that, along with HP1 and histone H4 lysine 20 methylation, play an essential role in transcriptional silencing and genome stability . To determine if alcohol selectively impacts only the dimethylated state of H3K9, we returned to our previously published primary neurosphere model of exposure [12, 13]. Here, we exposed cultured cells to 0, 160, and 240 mg/dL of alcohol for 3 days, then passaged exposed cells without alcohol for a 4-day recovery phase. Importantly, our cell culture experiments largely reproduced both the suppression of mTORC2 target genes (Atp5e and Atp5mf) and increases in H3K9me2 within repetitive sequences that we observed in our mouse model (Fig. 5A, B). Using ChIP, we next assayed the enrichment of trimethylated histone H3 lysine 9 (H3K9me3), as well as trimethylation of histone H4 lysine 20 (H4K20me3), which both co-localize during the formation of canonical heterochromatin . These experiments revealed decreased H3K9me3 in both IAP and major satellite repeats, while LINE1 elements and the untranscribed region of chromosome 6 both exhibited increases (Fig. 5C). In contrast, we observed no differences in H4K20me3 across any repeat regions or Untr6 (Fig. 5D).
To expand our analysis into protein-coding genes, we assayed the promoter region of the homeobox gene Nkx2.1, which exhibited a dramatic increase in H3K9me2 both in vitro and in vivo . The regulatory region of Nkx2.1 displayed a 75% decrease in H3K9me3, while the enrichment of H4K20me3 was not significantly different between treatments (Fig. 5E, F). Although the cortices of alcohol-exposed animals exhibiting congenital defects consistently display increased H3K9 dimethylation, H3K9me3 shows region-specific changes, while we did not observe any significant impact on H4K20me3 enrichment. From these data, we conclude that the observed ethanol-induced increases in H3K9me2 do not associate with the formation of canonical heterochromatin.
Increased expression SATB2 in alcohol-exposed affected tissues does not correlate with altered gene expression or increased H3K9me2
Previous studies using worms and mammalian cells demonstrate that mitochondrial dysfunction and oxidative stress induce global enrichment of H3K9me2 [17, 18]. In worms, upregulation, and nuclear localization of the chromatin looping protein DVE-1 precedes the global enrichment of H3K9me2, which together serve to stabilize chromatin interactions . The mammalian homologs of DVE-1 are SATB1 and SATB2, which also play major roles in organizing chromatin looping and stabilize interactions between gene enhancers and promoters [47,48,49,50,51,52]. Further, SATB2 function is critical for proper development of the cerebral cortex and normal craniofacial patterning [50, 53]. To determine if the DVE-1 homologs SATB1 and SATB2 are upregulated in our model, we assayed their expression in the cortices of control, EtOH-exposed unaffected, and EtOH-exposed affected offspring. Consistent with studies in c. elegans, we observed an increase in transcripts encoding Satb2 in the cortices of alcohol-exposed affected but not in control or alcohol-exposed unaffected offspring (Fig. 6A). Using Western blotting, we validated upregulation of SATB2 in alcohol-exposed affected offspring (Fig. 6B). We also observed a significant, although more minor, magnitude increase of SATB2 protein in cortices derived from EtOH-exposed unaffected offspring. Similar to candidate genes in the pathways regulating Oxidative Phosphorylation and Mitochondrial Dysfunction, we only identified Satb2 upregulation in the cortex and not the heart or cerebellum of EtOH-exposed, affected animals (Fig. 6C). We then assayed enrichment of H3K9me2 in the Satb1 and Satb2 regulatory regions. The Satb1 promoter displayed increased H3K9me2, and although the Satb2 promoter trended toward an increase, this did not reach statistical significance (p = 0.1) and was only different from samples derived from EtOH-exposed unaffected mice.
To determine if regions exhibiting enrichment in H3k9me2 also display increased occupancy of SATB2, we conducted ChIP-qPCR analysis using the previously validated antibody [53,54,55]. As a positive control, we assayed the enrichment of H3K9me2 and SATB2 at the SOX5 binding site within enhancer 434, upstream of the gene encoding Fezf2 [53, 56]. Although we identified both H3K9me2 and SATB2 within this region, neither displayed increased occupancy in EtOH-exposed affected samples (Fig. 6D). Further, although we could not identify SATB2 binding at any candidate gene regulatory regions, we did detect occupancy of SATB2 at repetitive sequences, and EtOH-exposed cortices displayed increased enrichment compared to controls (Fig. 6E). However, these primer sequences bind multiple genomic regions, and we cannot know if these sequences are common between H3K9me2 and SATB2. From these data, we conclude that although EtOH-exposed affected samples exhibit upregulation of the mammalian homolog of DVE-1, SATB2 does not bind the regulatory regions of any of our candidate genes nor strictly correlate with all instances of increased H3K9me2 enrichment.
In this study, we found that alcohol-exposed tissues isolated from fetuses exhibiting structural defects exhibit disruptions in the genetic pathways controlling cellular respiration and oxidative phosphorylation, the majority of which are regulated by mTORC2. Although acute alcohol exposure is known to induce mTORC2 activation in the CNS , our study is the first to identify prolonged programming of this complex, long after the removal of the toxicant. In glioblastoma multiforme, the acetyl-CoA-dependent acetylation of RICTOR, a core component of the mTORC2 signaling complex, promotes an autoactivation loop, even when the upstream growth factor driving this signaling pathway is removed [58, 59]. Prenatal alcohol exposure associates with the ACSS2-dependent formation of acetate within the gestating brain . Consistent with this study and adult models of alcohol exposure , we also observe transient increases in H3K9 acetylation but only during the exposure phase and not after alcohol is removed . As increased acetate drives increased cellular levels of acetyl-CoA, we speculate that during gestation, binge exposures program an acetate-driven increase in mTORC2 activity, resulting in a lasting suppression of the genetic pathways driving cellular respiration and the oxidative stress response. Additional experiments are required to determine if prenatal alcohol exposure is associated with the acetyl-CoA-dependent acetylation of RICTOR.
Consistent with our previous in vitro studies  and prior publications that examine chronic models of adult alcohol exposure , our RNA-seq analysis of the affected transcriptome revealed a broad suppression of transcriptional pathways that counter oxidative stress, while alcohol-exposed unaffected tissues do not. Similar to adult tissues, these signatures of differential gene expression and altered H3K9me2 are tissue-specific . Interestingly, in our model, female offspring appear more prone to dysregulation of these pathways and overt dysgenesis. These data are consistent with recent studies indicating female offspring are more susceptible to the teratogenic impacts of intrauterine alcohol exposures . Future studies are needed to determine if this mTORC2 signature is present in other models of exposure, is sex-specific, and if pharmacological interventions that target this pathway rescue EtOH-induced patterning defects.
In our model, affected tissues consistently display widespread increases in the enrichment of H3K9me2, which appear in genic, repetitive, and non-transcribed regions of the genome. Despite an established role of H3K9me2 in the formation of heterochromatin , we do not observe widespread silencing of gene expression. As specific examples, we previously reported a 500% increase in the enrichment of H3K9me2 at both the Nkx2.1 and Wnt5b promoters . Notwithstanding this dramatic increase, we find that the expression of both of these genes increased in alcohol-exposed affected cortices. In contrast, the other 14 H3K9me2-enriched candidate genes we previously identified did not display any significant changes in gene expression. Further, despite the widespread increase in H3K9me2, our RNA-seq analysis identified a near equivalent number of candidate genes that were up- and down-regulated. Although we acknowledge that increased H3K9me2 may correlate with the suppression of genes we did not assay here, the fact that some of our top upregulated candidate genes exhibited increased enrichment and that we observed augmented H3K9me2 in a non-transcribed region of the genome, we conclude that this change in chromatin structure does not always silence gene expression. Importantly, these observations are consistent between both our mouse and cell culture models.
Although H3K9 methylation predominantly associates with transcriptional silencing, similar to DNA methylation, this modification is also found in gene bodies and associates with transcriptional elongation [64,65,66]. Further, microscopy-based studies employing FISH have revealed that while deposition of H3K9me2 correlates with the localization of gene sequences into large domains at the nuclear periphery, this does not always associate with transcriptional silencing [67,68,69,70]. As an example, during both muscle and T-cell development, key homeobox genes driving progressive changes in cell identity need to be released from the nuclear periphery in order to achieve optimal transcriptional activation. However, most genes moving to or from the nuclear periphery display little to no change in expression, despite dynamic alterations in H3K9me3 [71,72,73]. Importantly, if a gene locus that becomes relocated to the nuclear periphery and silenced during differentiation is artificially moved to the nuclear periphery outside of a differentiation context, it does not become silenced [72, 74]. Similarly, although CAS9-mediated increases in H3K9 methylation across a large region of human chromosome 19 can induce the formation of heterochromatin-like domains, this large-scale change in chromatin structure did not result in widespread gene repression . From these various studies, it appears that although increased H3K9 methylation may associate with transcriptional suppression, direct regulation of gene expression falls to protein factors (activators/repressors) located in the various nuclear compartments during specific developmental windows; not by a change in histone methylation. Given the association between H3K9 methylation and DNA methylation , future studies will determine if DNA methylation changes also associate with dysgenesis of the fetal cortex.
The induction of Satb2 in the cortices of EtOH-exposed affected offspring, combined with the disruption of the transcriptional programs regulating mitochondrial function, prompted us to consider that similar to worms , mammalian cells also induce a chromatin-based stress response to stabilize nuclear interactions. Consistent with this idea, in osteoblasts, SATB2 messenger RNA and protein upregulate in response to oxidative stress, and loss of SATB2 disrupts chromatin structure and causes nuclear damage . SATB2 interacts with the H3K9me2 methyltransferase EHMT2 (G9a), which promotes the association of target loci with the nuclear lamina [67, 77, 78]. However, outside of transposable elements and repetitive sequences, we could not identify SATB2 binding at any candidate region exhibiting altered expression or increased H3K9me2. Thus, from these data, we conclude that although gestational alcohol exposure may induce SATB2, this protein does not appear to drive the altered H3K9me2 or transcriptional changes observed in EtOH-exposed affected tissues.
One of the major confounding elements in the study of fetal alcohol spectrum disorders (FASDs) is the enormous variation observed in phenotypes and incidence . FASD-associated defects have a wide range of severity, and while many women who drink have affected children, a significant subset of alcohol-exposed babies remain unaffected . However, the vast majority of animal model-based studies have ignored this variation and have contrasted measures between control and alcohol-exposed tissues. Thus, we have a very poor understanding of what molecular changes distinguish affected versus unaffected individuals. Our studies indicate that changes in histone H3 lysine 9 dimethylation associate with alcohol-induced defects but that this epigenetic change may not directly influence the transcriptional programs driving development.
Availability of data and materials
The datasets generated and/or analyzed during the current study are available in the Gene Expression Omnibus (GEO) repository, GSE163300.
Fetal alcohol spectrum disorders
Dimethylated histone H3, lysine 9
Trimethylated histone H3, lysine 9
Trimethylated histone H4, lysine 20
Mammalian target of rapamycin complex 2
Special AT-Rich Sequence Binding Protein 1
Special AT-Rich Sequence Binding Protein 2
- Ehmt2 (G9a):
Euchromatic Histone Lysine Methyltransferase 2
Acyl-CoA Synthetase Short Chain Family Member 2
ATP Synthase F1 Subunit Epsilon
ATP Synthase Membrane Subunit F
ATP Synthase Membrane Subunit G
Achaete-Scute Family BHLH Transcription Factor 1
Cytochrome C Oxidase Subunit 7B
Distal-Less Homeobox 2
Eukaryotic Translation Initiation Factor 2A
NADH dehydrogenase [ubiquinone] 1 alpha subcomplex subunit 7
NK2 Homeobox 1
Long interspersed nuclear elements
Untranscribed region of chromosome 6
FEZ Family Zinc Finger 2
Medrano-Fernández A, Barco A. Nuclear organization and 3D chromatin architecture in cognition and neuropsychiatric disorders. Mol Brain. 2016;9(1):83.
Bahari-Javan S, Maddalena A, Kerimoglu C, Wittnam J, Held T, Bähr M, et al. HDAC1 regulates fear extinction in mice. J Neurosci. 2012;32(15):5062–73.
Sakharkar AJ, Zhang H, Tang L, Shi G, Pandey SC. Histone deacetylases (HDAC)-induced histone modifications in the amygdala: a role in rapid tolerance to the anxiolytic effects of ethanol. Alcohol Clin Exp Res. 2012;36(1):61–71.
Moonat S, Sakharkar AJ, Zhang H, Tang L, Pandey SC. Aberrant histone deacetylase2-mediated histone modifications and synaptic plasticity in the amygdala predisposes to anxiety and alcoholism. Biol Psychiatry. 2013;73(8):763–73.
Fischer A, Sananbenesi F, Wang X, Dobbin M, Tsai L-H. Recovery of learning and memory is associated with chromatin remodelling. Nature. 2007;447(7141):178–82.
Rudenko A, Tsai L-H. Epigenetic modifications in the nervous system and their impact upon cognitive impairments. Neuropharmacology. 2014;80:70–82.
Gupta S, Kim SY, Artis S, Molfese DL, Schumacher A, Sweatt JD, et al. Histone methylation regulates memory formation. J Neurosci. 2010;30(10):3589–99.
Snigdha S, Prieto GA, Petrosyan A, Loertscher BM, Dieskau AP, Overman LE, et al. H3K9me3 inhibition improves memory, promotes spine formation, and increases BDNF levels in the aged hippocampus. J Neurosci. 2016;36(12):3611–22.
Subbanna S, Basavarajappa BS. Pre-administration of G9a/GLP inhibitor during synaptogenesis prevents postnatal ethanol-induced LTP deficits and neurobehavioral abnormalities in adult mice. Exp Neurol. 2014;261:34–43.
Subbanna S, Shivakumar M, Umapathy NS, Saito M, Mohan PS, Kumar A, et al. G9a-mediated histone methylation regulates ethanol-induced neurodegeneration in the neonatal mouse brain. Neurobiol Dis. 2013;54:475–85.
Subbanna S, Joshi V, Basavarajappa BS. Activity-dependent signaling and epigenetic abnormalities in mice exposed to postnatal ethanol. Neuroscience. 2018;392:230–40.
Veazey KJ, Parnell SE, Miranda RC, Golding MC. Dose-dependent alcohol-induced alterations in chromatin structure persist beyond the window of exposure and correlate with fetal alcohol syndrome birth defects. Epigenet Chromatin. 2015;8(1):1–19.
Veazey KJ, Wang H, Bedi YS, Skiles WM, Chang RCA, Golding MC. Disconnect between alcohol-induced alterations in chromatin structure and gene transcription in a mouse embryonic stem cell model of exposure. Alcohol. 2017;60:121–33.
Walker DM, Nestler EJ. Neuroepigenetics and addiction. Handb Clin Neurol. 2018;148:747–65.
Hayes JD, Dinkova-Kostova AT. Epigenetic control of NRF2-directed cellular antioxidant status in dictating life-death decisions. Mol Cell. 2017;68(1):5–7.
Kreuz S, Fischle W. Oxidative stress signaling to chromatin in health and disease. Epigenomics. 2016;8(6):843–62.
Tian Y, Garcia G, Bian Q, Steffen KK, Joe L, Wolff S, et al. Mitochondrial stress induces chromatin reorganization to promote longevity and UPR(mt). Cell. 2016;165(5):1197–208.
Chen H, Yan Y, Davidson TL, Shinkai Y, Costa M. Hypoxic stress induces dimethylated histone H3 lysine 9 through histone methyltransferase G9a in mammalian cells. Cancer Res. 2006;66(18):9009–16.
Janssen A, Colmenares SU, Karpen GH. Heterochromatin: guardian of the genome. Annu Rev Cell Dev Biol. 2018;34(1):265–88.
Feng Y, Wang Y, Wang X, He X, Yang C, Naseri A, et al. Simultaneous epigenetic perturbation and genome imaging reveal distinct roles of H3K9me3 in chromatin architecture and transcription. Genome Biol. 2020;21(1):1–24.
Dillin A, Hsu AL, Arantes-Oliveira N, Lehrer-Graiwer J, Hsin H, Fraser AG, et al. Rates of behavior and aging specified by mitochondrial function during development. Science. 2002;298(5602):2398–401.
Feng J, Bussière F, Hekimi S. Mitochondrial electron transport is a key determinant of life span in Caenorhabditis elegans. Dev Cell. 2001;1(5):633–44.
Alabert C, Barth TK, Reverón-Gómez N, Sidoli S, Schmidt A, Jensen ON, et al. Two distinct modes for propagation of histone PTMs across the cell cycle. Genes Dev. 2015;29(6):585–90.
Audergon PNCB, Catania S, Kagansky A, Tong P, Shukla M, Pidoux AL, et al. Epigenetics. Restricted epigenetic inheritance of H3K9 methylation. Science. 2015;348(6230):132–5.
Ragunathan K, Jih G, Moazed D. Epigenetics. Epigenetic inheritance uncoupled from sequence-specific recruitment. Science. 2015;348(6230):1258699.
Reverón-Gómez N, González-Aguilera C, Stewart-Morgan KR, Petryk N, Flury V, Graziano S, et al. Accurate recycling of parental histones reproduces the histone modification landscape during DNA replication. Mol Cell. 2018;72(2):239–49.
Godin EA, O’Leary-Moore SK, Khan AA, Parnell SE, Ament JJ, Dehart DB, et al. Magnetic resonance microscopy defines ethanol-induced brain abnormalities in prenatal mice: effects of acute insult on gestational day 7. Alcohol Clin Exp Res. 2010;34(1):98–111.
Gilbert MT, Sulik KK, Fish EW, Baker LK, Dehart DB, Parnell SE. Dose-dependent teratogenicity of the synthetic cannabinoid CP-55,940 in mice. Neurotoxicol Teratol. 2015;58:15–22.
Parnell SE, Dehart DB, Wills TA, Chen S-Y, Hodge CW, Besheer J, et al. Maternal oral intake mouse model for fetal alcohol spectrum disorders: ocular defects as a measure of effect. Alcohol Clin Exp Res. 2006;30(10):1791–8.
Dobin A, Davis CA, Schlesinger F, Drenkow J, Zaleski C, Jha S, et al. STAR: ultrafast universal RNA-seq aligner. Bioinformatics. 2013;29(1):15–21.
Jiménez-Marín A, Collado-Romero M, Ramirez-Boo M, Arce C, Garrido JJ. Biological pathway analysis by ArrayUnlock and ingenuity pathway analysis. BMC Proc. 2009;3(Suppl 4):S6.
Miranda RC, Santillano DR, Camarillo C, Dohrman D. Modeling the impact of alcohol on cortical development in a dish: strategies from mapping neural stem cell fate. Methods Mol Biol. 2008;447:151–68.
Kondo Y, Shen L, Yan PS, Huang TH-M, Issa JP-J. Chromatin immunoprecipitation microarrays for identification of genes silenced by histone H3 lysine 9 methylation. Proc Natl Acad Sci USA. 2004;101(19):7398–403.
Chang RC, Thomas KN, Bedi YS, Golding MC. Programmed increases in LXRα induced by paternal alcohol use enhance offspring metabolic adaptation to high-fat diet induced obesity. Mol Metab. 2019;30:161–72.
Carnahan MN, Veazey KJ, Muller D, Tingling JD, Miranda RC, Golding MC. Identification of cell-specific patterns of reference gene stability in quantitative reverse-transcriptase polymerase chain reaction studies of embryonic, placental and neural stem models of prenatal ethanol exposure. Alcohol. 2013;47(2):109–20.
Schmittgen TD, Livak KJ. Analyzing real-time PCR data by the comparative C(T) method. Nat Protoc. 2008;3(6):1101–8.
Mukhopadhyay A, Deplancke B, Walhout AJM, Tissenbaum HA. Chromatin immunoprecipitation (ChIP) coupled to detection by quantitative real-time PCR to study transcription factor binding to DNA in Caenorhabditis elegans. Nat Protoc. 2008;3(4):698–709.
Harding HP, Zhang Y, Zeng H, Novoa I, Lu PD, Calfon M, et al. An integrated stress response regulates amino acid metabolism and resistance to oxidative stress. Mol Cell. 2003;11(3):619–33.
Godin EA, Dehart DB, Parnell SE, O’Leary-Moore SK, Sulik KK. Ventromedian forebrain dysgenesis follows early prenatal ethanol exposure in mice. Neurotoxicol Teratol. 2011;33(2):231–9.
Parnell SE, O’Leary-Moore SK, Godin EA, Dehart DB, Johnson BW, Allan Johnson G, et al. Magnetic resonance microscopy defines ethanol-induced brain abnormalities in prenatal mice: effects of acute insult on gestational day 8. Alcohol Clin Exp Res. 2009;33(6):1001–11.
Morgan SC, Relaix F, Sandell LL, Loeken MR. Oxidative stress during diabetic pregnancy disrupts cardiac neural crest migration and causes outflow tract defects. Birth Defects Res A Clin Mol Teratol. 2008;82(6):453–63.
Lamming DW, Demirkan G, Boylan JM, Mihaylova MM, Peng T, Ferreira J, et al. Hepatic signaling by the mechanistic target of rapamycin complex 2 (mTORC2). FASEB J. 2014;28(1):300–15.
Masui K, Harachi M, Cavenee WK, Mischel PS, Shibata N. mTOR complex 2 is an integrator of cancer metabolism and epigenetics. Cancer Lett. 2020;478:1–7.
Cohen A, Habib A, Laor D, Yadav S, Kupiec M, Weisman R. TOR complex 2 in fission yeast is required for chromatin-mediated gene silencing and assembly of heterochromatic domains at subtelomeres. J Biol Chem. 2018;293(21):8138–50.
Sofronescu AG, Detillieux KA, Cattini PA. FGF-16 is a target for adrenergic stimulation through NF-kappaB activation in postnatal cardiac cells and adult mouse heart. Cardiovasc Res. 2010;87(1):102–10.
Schotta G, Lachner M, Sarma K, Ebert A, Sengupta R, Reuter G, et al. A silencing pathway to induce H3-K9 and H4-K20 trimethylation at constitutive heterochromatin. Genes Dev. 2004;18(11):1251–62.
Cai S, Lee CC, Kohwi-Shigematsu T. SATB1 packages densely looped, transcriptionally active chromatin for coordinated expression of cytokine genes. Nat Genet. 2006;38(11):1278–88.
Yasui D, Miyano M, Cai S, Varga-Weisz P, Kohwi-Shigematsu T. SATB1 targets chromatin remodelling to regulate genes over long distances. Nature. 2002;419(6907):641–5.
Dobreva G, Dambacher J, Grosschedl R. SUMO modification of a novel MAR-binding protein, SATB2, modulates immunoglobulin mu gene expression. Genes Dev. 2003;17(24):3048–61.
Dobreva G, Chahrour M, Dautzenberg M, Chirivella L, Kanzler B, Fariñas I, et al. SATB2 is a multifunctional determinant of craniofacial patterning and osteoblast differentiation. Cell. 2006;125(5):971–86.
Liang YC, Wu P, Lin GW, Chen CK, Yeh CY, Tsai S, et al. Folding keratin gene clusters during skin regional specification. Dev Cell. 2020;53(5):561.e9-576.e9.
Savarese F, Dávila A, Nechanitzky R, De La Rosa-Velazquez I, Pereira CF, Engelke R, et al. Satb1 and Satb2 regulate embryonic stem cell differentiation and Nanog expression. Genes Dev. 2009;23(22):2625–38.
McKenna WL, Ortiz-Londono CF, Mathew TK, Hoang K, Katzman S, Chen B. Mutual regulation between Satb2 and Fezf2 promotes subcerebral projection neuron identity in the developing cerebral cortex. Proc Natl Acad Sci USA. 2015;112(37):11702–7.
Jaitner C, Reddy C, Abentung A, Whittle N, Rieder D, Delekate A, et al. Satb2 determines miRNA expression and long-term memory in the adult central nervous system. Elife. 2016;5:e17361.
Zhang L, Song N-N, Zhang Q, Mei W-Y, He C-H, Ma P, et al. Satb2 is required for the regionalization of retrosplenial cortex. Cell Death Differ. 2020;27(5):1604–17.
Kwan KY, Lam MMS, Krsnik Ž, Kawasawa YI, Lefebvre V, Šestan N. SOX5 postmitotically regulates migration, postmigratory differentiation, and projections of subplate and deep-layer neocortical neurons. Proc Natl Acad Sci. 2008;105(41):16021–6.
Laguesse S, Morisot N, Phamluong K, Sakhai SA, Ron D. mTORC2 in the dorsomedial striatum of mice contributes to alcohol-dependent F-Actin polymerization, structural modifications, and consumption. Neuropsychopharmacology. 2018;43(7):1539–47.
Masui K, Tanaka K, Ikegami S, Villa GR, Yang H, Yong WH, et al. Glucose-dependent acetylation of Rictor promotes targeted cancer therapy resistance. Proc Natl Acad Sci USA. 2015;112(30):9406–11.
Masui K, Harachi M, Ikegami S, Yang H, Onizuka H, Yong WH, et al. MTORC2 links growth factor signaling with epigenetic regulation of iron metabolism in glioblastoma. J Biol Chem. 2019;294(51):19740–51.
Mews P, Egervari G, Nativio R, Sidoli S, Donahue G, Lombroso SI, et al. Alcohol metabolism contributes to brain histone acetylation. Nature. 2019;574(7780):717–21.
Hoek JB, Cahill A, Pastorino JG. Alcohol and mitochondria: a dysfunctional relationship. Gastroenterology. 2002;122(7):2049–63.
Berkel TDM, Zhang H, Teppen T, Sakharkar AJ, Pandey SC. Essential role of histone methyltransferase G9a in rapid tolerance to the anxiolytic effects of ethanol. Int J Neuropsychopharmacol. 2018;22(4):292–302.
Kwan STC, Presswood BH, Helfrich KK, Baulch JW, Mooney SM, Smith SM. An interaction between fetal sex and placental weight and efficiency predicts intrauterine growth in response to maternal protein insufficiency and gestational exposure window in a mouse model of FASD. Biol Sex Differ. 2020;11(1):40.
Mikkelsen TS, Ku M, Jaffe DB, Issac B, Lieberman E, Giannoukos G, et al. Genome-wide maps of chromatin state in pluripotent and lineage-committed cells. Nature. 2007;448(7153):553–60.
Vakoc CR, Mandat SA, Olenchock BA, Blobel GA. Histone H3 lysine 9 methylation and HP1gamma are associated with transcription elongation through mammalian chromatin. Mol Cell. 2005;19(3):381–91.
Vakoc CR, Sachdeva MM, Wang H, Blobel GA. Profile of histone lysine methylation across transcribed mammalian chromatin. Mol Cell Biol. 2006;26(24):9185–95.
Guelen L, Pagie L, Brasset E, Meuleman W, Faza MB, Talhout W, et al. Domain organization of human chromosomes revealed by mapping of nuclear lamina interactions. Nature. 2008;453(7197):948–51.
Kind J, Pagie L, Ortabozkoyun H, Boyle S, de Vries SS, Janssen H, et al. Single-cell dynamics of genome-nuclear lamina interactions. Cell. 2013;153(1):178–92.
Peric-Hupkes D, Meuleman W, Pagie L, Bruggeman SWM, Solovei I, Brugman W, et al. Molecular maps of the reorganization of genome-nuclear lamina interactions during differentiation. Mol Cell. 2010;38(4):603–13.
Zhao H, Sifakis EG, Sumida N, Millán-Ariño L, Scholz BA, Svensson JP, et al. PARP1- and CTCF-mediated interactions between active and repressed chromatin at the lamina promote oscillating transcription. Mol Cell. 2015;59(6):984–97.
Gonzalez-Sandoval A, Towbin BD, Kalck V, Cabianca DS, Gaidatzis D, Hauer MH, et al. Perinuclear anchoring of H3K9-methylated chromatin stabilizes induced cell fate in C. elegans embryos. Cell. 2015;163(6):1333–47.
Robson MI, de Las Heras JI, Czapiewski R, Lê Thành P, Booth DG, Kelly DA, et al. Tissue-specific gene repositioning by muscle nuclear membrane proteins enhances repression of critical developmental genes during myogenesis. Mol Cell. 2016;62(6):834–47.
Robson MI, de Las Heras JI, Czapiewski R, Sivakumar A, Kerr ARW, Schirmer EC. Constrained release of lamina-associated enhancers and genes from the nuclear envelope during T-cell activation facilitates their association in chromosome compartments. Genome Res. 2017;27(7):1126–38.
Wijchers PJ, Krijger PHL, Geeven G, Zhu Y, Denker A, Verstegen MJAM, et al. Cause and consequence of tethering a SubTAD to different nuclear compartments. Mol Cell. 2016;61(3):461–73.
Rothbart SB, Krajewski K, Nady N, Tempel W, Xue S, Badeaux AI, et al. Association of UHRF1 with methylated H3K9 directs the maintenance of DNA methylation. Nat Struct Mol Biol. 2012;19(11):1155–60.
Wei J-D, Lin Y-L, Tsai C-H, Shieh H-S, Lin P-I, Ho W-P, et al. SATB2 participates in regulation of menadione-induced apoptotic insults to osteoblasts. J Orthop Res. 2012;30(7):1058–66.
Ma Y-N, Zhang H-Y, Fei L-R, Zhang M-Y, Wang C-C, Luo Y, et al. SATB2 suppresses non-small cell lung cancer invasiveness by G9a. Clin Exp Med. 2018;18(1):37–44.
Wen B, Wu H, Shinkai Y, Irizarry RA, Feinberg AP. Large histone H3 lysine 9 dimethylated chromatin blocks distinguish differentiated from embryonic stem cells. Nat Genet. 2009;41(2):246–50.
Schaefer GB, Deere D. Recognition, diagnosis and treatment of fetal alcohol syndrome. J Ark Med Soc. 2011;108(2):38–40.
Kesmodel US, Bertrand J, Støvring H, Skarpness B, Denny CH, Mortensen EL, et al. The effect of different alcohol drinking patterns in early to mid pregnancy on the child’s intelligence, attention, and executive function. BJOG. 2012;119(10):1180–90.
This work was supported by National Institute on Alcohol Abuse and Alcoholism, Grant Nos. R01 AA028219-01 (MCG) and U01 AA021651 (SEP).
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Chang, R.C., Thomas, K.N., Mehta, N.A. et al. Programmed suppression of oxidative phosphorylation and mitochondrial function by gestational alcohol exposure correlate with widespread increases in H3K9me2 that do not suppress transcription. Epigenetics & Chromatin 14, 27 (2021). https://doi.org/10.1186/s13072-021-00403-w
- Developmental programming
- Fetal alcohol spectrum disorders (FASDs)
- Epigenetic programming
- Oxidative phosphorylation
- Chromatin looping
- Birth defects