- Open Access
Restoration of histone acetylation ameliorates disease and metabolic abnormalities in a FUS mouse model
Acta Neuropathologica Communications volume 7, Article number: 107 (2019)
Dysregulation of epigenetic mechanisms is emerging as a central event in neurodegenerative disorders, including amyotrophic lateral sclerosis (ALS). In many models of neurodegeneration, global histone acetylation is decreased in the affected neuronal tissues. Histone acetylation is controlled by the antagonistic actions of two protein families –the histone acetyltransferases (HATs) and the histone deacetylases (HDACs). Drugs inhibiting HDAC activity are already used in the clinic as anti-cancer agents. The aim of this study was to explore the therapeutic potential of HDAC inhibition in the context of ALS. We discovered that transgenic mice overexpressing wild-type FUS (“Tg FUS+/+”), which recapitulate many aspects of human ALS, showed reduced global histone acetylation and alterations in metabolic gene expression, resulting in a dysregulated metabolic homeostasis. Chronic treatment of Tg FUS+/+ mice with ACY-738, a potent HDAC inhibitor that can cross the blood-brain barrier, ameliorated the motor phenotype and substantially extended the life span of the Tg FUS+/+ mice. At the molecular level, ACY-738 restored global histone acetylation and metabolic gene expression, thereby re-establishing metabolite levels in the spinal cord. Taken together, our findings link epigenetic alterations to metabolic dysregulation in ALS pathology, and highlight ACY-738 as a potential therapeutic strategy to treat this devastating disease.
Amyotrophic lateral sclerosis (ALS) is a fatal neurodegenerative disorder caused by the selective loss of motor neurons in the motor cortex, brainstem and spinal cord, leading to the paralysis of voluntary muscles . Motor symptoms usually appear in midlife and ultimately escalate to death, usually within 2 to 5 years after symptom onset . Approximately 90% of ALS cases are sporadic, while the remaining 10% are inherited . The most prevalent genetic causes of ALS are mutations in the genes encoding superoxide dismutase 1 (SOD1), TAR DNA-binding protein 43 (TDP-43) and fused in sarcoma (FUS), as well as hexanucleotide repeats in the ‘Chromosome 9 open reading frame 72’ (C9orf72) gene . Despite the identification of multiple genetic factors, the pathogenic mechanisms underlying the selective degeneration of motor neurons remain incompletely understood. At present, effective therapies are lacking for ALS patients [1, 9, 59]. As a consequence, there is a strong need for more effective therapies for ALS.
Mouse models manifesting the core symptoms of the disease, including a motor phenotype and motor neuron degeneration, remain crucial for the preclinical investigation of pathological mechanisms and novel therapeutic options. As all therapeutic strategies effective in the commonly used mutant SOD1 model subsequently failed in the clinic, other in vivo models to study ALS are urgently needed. One example is the PrP-hFUS-WT3 mouse model, which shows a strong ALS-like phenotype with severe motor neuron degeneration and a short lifespan, unlike many other FUS models [40, 62]. FUS is a DNA/RNA binding protein linked to ALS as well as to frontotemporal dementia (FTD), another neurodegenerative disorder belonging to the same disease spectrum as ALS [21, 69]. Mutations in the FUS gene account for approximately 4% of familial ALS cases and lead to neuronal and glial cytoplasmic mislocalization of the FUS protein [32, 70]. The majority of the identified mutations are found in the glycine-rich region and in the nuclear localization signal . However, mutations in the 3′ untranslated region causing a strong increase in FUS expression have also been identified in ALS patients [19, 57]. Moreover, FUS aggregates are found in the absence of mutations in the FUS gene in a subset of FTD cases [16, 42]. These findings strongly indicate that not only mutant, but also wild-type FUS can be detrimental to neurons. However, it remains unclear which pathogenic mechanisms contribute to the observed neurodegeneration .
Recently, aberrant homeostasis of epigenetic marks was detected in the nervous system of several models of neurodegenerative disorders, including ALS [31, 34, 53, 58, 68]. One of these deregulated marks is acetylation of lysine residues of histones. Acetylation of histones regulates high-order chromatin folding and thereby the accessibility of transcription factors to their target genes . Histone acetylation levels are regulated by the counteracting activities of two protein families –the histone acetyltransferases (HATs) and the histone deacetylases (HDACs) . Accumulating evidence indicates that decreased histone acetylation is a negative determinant for neuronal survival [34, 53, 58, 68]. A major indication is that global histone hypoacetylation in the nervous system is a feature of multiple neurodegenerative models [7, 31, 58]. This imbalance tremendously affects the global transcription profile [53, 54, 58, 68].
HDACs are druggable targets and compounds that inhibit this class of enzymes are used to treat several forms of cancer . The therapeutic potential of HDAC inhibitors was already studied in a wide range of neurodegenerative disorders, such as Alzheimer’s disease, Huntington’s disease, spinal muscular atrophy and ALS [5, 6, 37, 52, 54, 56, 64, 67, 76].
Many HDAC inhibitors were developed showing distinctive selectivity toward the 11 zinc-dependent HDACs identified in mammals. Genetic and pharmacological studies suggested that especially the class I HDACs (HDAC1, 2, 3 and 8) as well as the class IIb HDAC6 have the largest potential as treatment strategies for neurodegenerative diseases, including ALS [18, 34, 75]. Class I HDACs reside in the nucleus and their major targets are the histones. HDAC6 has distinct functions in the cytoplasm.
The therapeutic potential of pan-HDAC inhibitors has been investigated in SOD1 mice, showing modest effects. Principal determinants responsible for these limited outcomes could be the low HDAC inhibitory potency, poor blood-brain-barrier (BBB) permeability, lack of isoform selectivity or toxicity of the compounds used [54, 56, 64, 76]. These could also explain the negative results of phase II clinical trials with valproate and phenylbutyrate [13, 47]. Therefore, research on HDAC inhibition as a therapeutic strategy for ALS deserves further attention. Moreover, new HDAC inhibitors with improved characteristics were recently developed.
The aim of this study was to test the efficacy of the HDAC inhibitor ACY-738 in a transgenic FUS mouse model of ALS and to investigate the contribution of different types of HDACs to the disease phenotype. ACY-738 displays a selectivity profile towards class I HDACs and HDAC6 [8, 30, 41]. We used ACY-738 as it is unique amongst the HDAC inhibitors, having a high potency, tolerability, and capacity to penetrate the BBB [30, 37, 41]. ACY-738 treatment restored histone acetylation and slowed down disease progression of the Tg FUS+/+ mice. This treatment also corrected metabolic pathways in the spinal cord, which were already dysregulated at presymptomatic stage. Overall, our data suggest that global histone hypoacetylation is associated with metabolic dysregulation in FUS-mediated ALS pathology, and that histone deacetylases are potential therapeutic targets to delay disease progression by re-establishing metabolic homeostasis.
Material and methods
Tg FUS+/− breeding mice (stock no. 017916) were purchased from The Jackson Laboratory (Maine, USA). From the age of 28 to 30 days, crushed Teklad LM-485 (7912) sterilizable rodent chow (Envigo, Cambridgeshire, UK) containing 100 mg/kg ACY-738 (Regenacy Pharmaceuticals Inc., Waltham, USA) and mixed with water was provided ad libidum.
For genotyping, DNA was isolated from ear biopsies, and digested overnight in lysis buffer with 20 mg/ml proteinase K (Roche, Basel, Switzerland) at 55 °C. Genotyping of the mice was done using qPCR with a FAM-labelled probe recognizing the human FUS transgene (forward and reverse primers 5′-CAGCAAAGCTATGGACAGC-3′ and 5′-GTCTTGATTGCCATAACCGC-3′ and Taqman probe 5′-AGCAGAACCAGTACAACAGCAGCA-3′). β-actin was used as a housekeeping gene (forward and reverse primers 5′-CCCTACAGTGCTGTGGGTTT-3′ and 5′-GACATGCAAGGAGTGCAAGA-3′).
All mice were housed according to the guidelines of the KU Leuven. Mice were randomly selected for drug treatments and littermates were used as controls. Sample size and intermediate endpoints were based on the original study and a pilot experiment .
The concentration of ACY-738 in plasma and brain samples was determined by Liquid Chromatography/tandem Mass Spectrometry (LC-MS/MS). Plasma and brain were collected from mice killed after 5 days of ACY-738 therapy. ACY-738 was extracted from the samples by protein precipitation using 50:50 acetonitrile:methanol and analyzed using LC/MS/MS. The concentrations were then calculated using a standard curve.
Nerve conduction measurements were performed as described previously . Briefly, mice were anaesthetized under a 2.2 l/min oxygen flow containing 3% isoflurane and placed on a heating pad (Physitemp Instruments Inc., Clifton, USA) to maintain the body temperature. Motor nerve conduction studies were performed using sub-dermal platinum coated 0.4 mm needle electrodes (Technomed Europe, Maastricht, the Netherlands) for stimulating and recording and a UltraPro S100 monitoring set-up (Natus Medical Incorporated, Pleasanton, USA). Compound muscle action potentials (CMAPs) were determined by measuring the electrical response of the gastrocnemius muscle after stimulation of the sciatic notch. The stimulation intensity was gradually increased until the supramaximal CMAP amplitude was obtained. The amplitude and latency of the signal were quantified. The average of 3 measurements was determined.
Muscle force of the mice was measured using a Grip Strength Meter (Columbus Instruments, Columbus, USA) with a triangular bar as a probe to measure the grip strength in the forepaws. The average of five trials per animal was determined. To assess both fore- and hindlimb muscular strength, the hanging wire test was performed. Mice were placed on a wire cage lid. The lid was inverted and the latency to fall was recorded to a maximum of 60 s. The average of three trials per animal was determined. We evaluated motor performances and weight two times a week starting at 28 days of age. Disease onset was considered as the time point at which the mouse showed the highest value for forelimb grip strength. Survival was determined by the loss of righting reflex within 5 s after laying the mouse on its side. This time point was considered as disease end-stage, whereupon the mouse was sacrificed by intraperitonial injection with 200 mg/kg sodium pentobarbital (Dolethal, Vetoquinol) and used for histopathology.
Mice were anaesthetized by intraperitonial injection with 200 mg/kg sodium pentobarbital (Dolethal, Vetoquinol) and transcardially perfused with PBS.
For spinal cord histology, the lumbar part of the spinal cord was harvested and post-fixed with 4% paraformaldehyde (PFA) overnight (4 °C) and dehydrated for 48 h in 30% sucrose (4 °C). To visualize the motor neurons in the ventral horn, cryosections (20 μm) were stained with a 2X thionin solution. Briefly, slides were washed twice with water for 15 s, stained with 2X thionin for 45 s, again washed twice with water and dehydrated in a three-step ethanol series of increasing concentrations (70, 90 and 100%) for 30 s each. Sections were cleared with Histoclear solution for 1 min and mounted with PerTex mounting medium (Histolab, Göteborg, Germany). Images were acquired with a Zeiss Imager M1 microscope (Carl Zeiss, Oberkochen, Germany) using a 10x objective. The area of neuron cell bodies in the ventral horn were analyzed using the AxioVision program and neurons larger than 400 μm2 were considered as motor neurons. To investigate FUS localization in the spinal cord, colocalization of FUS with neurons was assessed. Sections (20 μm) were blocked for 1 h with 10% Normal Donkey Serum (Sigma, St. Louis, USA) in PBS-T (0.1%) and incubated overnight (4 °C) with antibodies for FUS (Proteintech 11,570-A-1P, 1:100) and NeuN (Millipore, MAB377; 1:500). The sections were subsequently washed and incubated with appropriate secondary antibodies (ThermoFisher Scientific, 1:1000). Slides were mounted with DAPI-containing ProLong® Gold antifade reagent (Invitrogen - Life Technologies, Carlsbad, USA). To investigate astrocytosis and microgliosis, a similar protocol using antibodies against GFAP (Sigma, G3893; 1:200), CD11b (Serotex MCA74G; 1:200) was used. Images were acquired using the Leica SP8x confocal microscope.
For muscle histology, the legs were tied with a strip during perfusion. The gastrocnemius muscles were dissected and snap-frozen in isopentane cooled by immersion in liquid nitrogen. To visualize neuromuscular junctions, longitudinal cryosections (20 μm) were fixed with 4% PFA for 10 min and then washed with PBS and PBS-T (0.1% Triton X-100). Subsequently, sections were blocked for 1 h with 10% Normal Donkey Serum (Sigma) in PBS-T. To visualize the nerve axons, the sections were incubated overnight (4 °C) with Neurofilament-L conjugated to Alexa-488 antibody (Cell Signaling Technologies; 1:500), Synaptophysin antibody (Cell Signaling Technologies; 1:500) and Synaptic vesicle 2 (DSHB; 1:100). The sections were then washed and incubated with appropriate secondary antibodies (ThermoFisher Scientific, 1:1000) and α-bungarotoxin conjugated to Alexa-555 (Invitrogen; 1:1000) for 1 h at room temperature (RT). Slides were mounted with ProLong® Gold antifade reagent (Invitrogen - Life Technologies). At least 50 neuromuscular junctions were analyzed for innervation, as determined by the co-localization of the Neurofilament-L/Synaptophysin/Synaptic vesicle 2 and α-bungarotoxin labeling, on a Zeiss Axio Imager M1 microscope (Carl Zeiss) using a 10x objective. To visualize muscle fibers, transversal cryosections (20 μm) were blocked for 1 h with 1% BSA (Serva, Heidelberg, Germany) in PBS, after which they were incubated with WGA conjugated to Alexa-488 antibody (1/100 Invitrogen W11261) in 0.5% BSA in PBS for 1 h at room temperature. After washing three times with PBS, slides were mounted with ProLong® Gold antifade reagent (Invitrogen - Life Technologies).
Western blot analysis
For blotting of acetylated α-tubulin or FUS, tissue samples were lysed in RIPA buffer (50 mM Tris-HCl (pH 7.5), 150 mM NaCl, 1% NP-40, 0.5% Na-deoxycholic acid, 0.5% SDS), supplemented with Complete EDTA-free protease inhibitor cocktail (Roche, Basel, Switzerland). Tissues were homogenized using Lysing Matrix D beads (MP Biomedicals, Solon, USA) and a MagNa Lyser oscillator (Roche) at 6500 rpm for 30 s thrice with 1 min interval on ice. The samples were subsequently centrifuged at 14,000 rpm for 20 min, after which the supernatant was transferred to a pre-chilled tube.
For blotting of acetylated histones and for the subcellular fractionation experiment, tissue samples were extracted using the NE-PER Nuclear and Cytoplasmic Extraction kit (Pierce Biotechnology, Rockford, USA) following the Manufacturer’s instructions. Briefly, tissues were cut in small pieces, washed with PBS and homogenized with a pellet pestle motor in CER I buffer. Samples were vortexed thoroughly for 15 s and left on ice for 10 min. CER II buffer was added, after which the mixture was vortexed and centrifuged at 16,000 g for 5 min. The nuclear pellet was washed with CERI/II buffer, after which it was resuspended in NER buffer. Samples were left on ice for 40 min, vortexing thoroughly for 15 s every 10 min. All samples were sonicated quickly, centrifuged at 16,000 g for 10 min and the supernatant (nuclear extract) was transferred to a pre-chilled tube. For histone blotting, only the nuclear extract was used.
Protein concentrations were measured with the micro BCA kit (Pierce Biotechnology). Reducing sample buffer (ThermoFisher Scientific) was added to samples containing equal amounts of protein (2.5 μg for α-tubulin; 30 μg for FUS; 15 μg for histones) and heated for 10 min at 95 °C before separation on a SDS–polyacrylamide electrophoresis gel (12%, 90 V, 50 min for α-tubulin; 3 h for FUS). Proteins were transferred to a polyvinylidene difluoride (PVDF) membrane (Millipore, Massachusetts, USA) by a semi-dry transfer apparatus (Bio-Rad, Hercules, USA) (180 mA, 1 h 45 min). The membranes were blocked with 5% milk in TBS-T (10 mM Tris-HCl (pH 7.5), 150 mM NaCl and 1% Tween-20) for 1 h at RT. Immunoblots were then incubated with primary antibodies against FUS (rabbit, 1/1000, Bethyl A300–302), acetylated α-tubulin (mouse, 1/5000, Sigma T6793), calnexin (rabbit, 1/2000, Enzo Life Technologies ADI-SPA-860-F), acetyl histone 3 K9/14 (rabbit, 1/500, Cell Signaling 9677), histone 4 (rabbit, 1/500, Abcam ab10158) in TBS-T for 1 to 2 h at RT. The membranes were incubated with the appropriate secondary antibody conjugated with horseradish peroxidase (HRP) (1/5000; Agilent Technologies (Dako)) for 1 h at RT. Protein bands were visualized using enhanced chemiluminescence (ECL substrate, ThermoFisher Scientific) and an ImageQuant LAS 4000 Biomolecular Imager (GE Healthcare, Illinois, USA). For histone blotting, a mild reblotting buffer (Millipore) was applied to strip the blots. Band intensities were quantified using ImageQuant™ TL version 7.0 software (GE Healthcare) and normalized to the appropriate control (calnexin or histone 4).
In situ nuclear HDAC activity
For the determination of in situ nuclear HDAC activity, nuclei of tissue samples were extracted using the Epiquick Nuclear Extraction Kit (Epigentek, Farmingdale, USA), after which HDAC activity was determined using the Epigenase HDAC Activity/Inhibition Direct Assay Kit (Colorimetric) (Epigentek). In brief, tissues were homogenized in NE1 buffer using a motor-driven pestle. After 15 min incubation on ice, the samples were centrifuged for 10 min at 12,000 rpm, after which the supernatant was removed. Two volumes of NE2 containing PIC were added to the pellet, after which the samples were incubated on ice for 15 min. Samples were vortexed, sonicated and centrifuged for 10 min at 14,000 rpm. The supernatant was collected and the protein concentration was measured with the micro BCA kit (Pierce Biotechnology). The HDAC activity in the nuclear extracts was then determined using the HDAC activity assay kit, by adding equal amounts of protein of the nuclear extracts in the wells of a microplate, together with HO1 and HO2 in a final volume of 50 μl. The plate was then incubated at 37 °C for 90 min, after which the reactions were removed from the wells. After thorough washing, primary antibodies were added to the wells for 60 min at RT, after which the secondary antibodies were incubated for 30 min at RT. After thorough washing, DS buffer was added for 5 min, after which SS buffer was added to stop the enzymatic reaction. Signals were detected by absorbance at 450 nm. The amount of deacetylated histone product was extrapolated from a standard curve, after which the HDAC activity in OD/min/mg was calculated.
Mice were euthanized with CO2 followed by cervical dislocation. Spinal cord was rapidly dissected and snap-frozen in liquid nitrogen. RNA was extracted using a combined protocol of TRIzol:chloroform and the RNeasy mini kit (Qiagen) and further processed according to the manufacturer’s protocol. For RNA sequencing, samples were sent to the Nucleomics Core (VIB, Leuven, Belgium) and analyzed for RNA integrity (≥ 8) by running on a Bioanalyzer (Agilent) before Trueseq total stranded RNA library preparation and sequencing on a Illumina NextSeq 500 system (Illumina, San Diego, USA). The libraries were sequenced using a high output paired end with 75 bp reads and ~ 50 million reads per sample. Reads were mapped using STAR aligner  on the latest mouse genome build (mm10). Reads were then counted using Salmon to estimate transcript and gene expression of every sample . Differential expression of coding genes and transcripts was performed with edgeR . Gene and transcripts with a FDR-adjusted P-value smaller than 0.05 and with an altered expression of 30% were deemed significantly differentially expressed. Differentially expressed genes were used as input for Panther gene ontology enrichment analysis to identify pathways associated with the differentially expressed genes [3, 39, 66]. Multiple testing correction was performed using FDR Benjamini-Hochberg correction. The most significant and promising genes were validated with qRT-PCR. For qRT-PCR analysis, first-strand cDNA was synthesized using SuperScript III (Invitrogen). PCR reactions were performed using SybrGreen reagents (ThermoFisher Scientific) with primers specific for the genes-of-interest (Additional file 1: Table S1) . Expression levels were normalized to two reference genes: AP3d1 (forward, 5′-CAAGGGCAGTATCGACCGC-3′; reverse, 5′-GATCTCGTCAATGCACTGGGA-3′) and Mon2 (forward, 5′-CTACAGTCCGACAGGTCGTGA-3′; reverse, 5′-CGGCACTGGAGGTTCTATATCTC-3′). Analysis was performed using qBase+ (v.3.0, Biogazelle, Zwijnaarde, Belgium).
Mice were anaesthetized by intraperitonial injection with 200 mg/kg sodium pentobarbital (Dolethal, Vetoquinol, UK) and transcardially perfused with PBS (Sigma). Spinal cord was rapidly dissected and snap-frozen in liquid nitrogen. Samples were sent to the Proteomics Core Facility (VIB, Ghent, Belgium) for Mass Spectrometry analysis. Liquid Chromatography - tandem Mass Spectrometry (LC-MS/MS) runs of all samples were searched together using the MaxQuant algorithm (version 184.108.40.206) with mainly default search settings including a false discovery rate set at 1% on both the peptide and protein level. Spectra were searched against the human protein sequences in the Swiss-Prot database (database release version of January 2018 containing 20,234 human protein sequences) (http://www.uniprot.org). Proteins that were identified in all replicates of at least one condition were kept. For statistical analysis, the missing values were imputed using a mixed approach. Missing not at random (MNAR) values were imputed using quantile regression-based left-censored function (MLE-QRILC), while missing at random values (MAR) were imputed using maximum-likelihood estimation (MLE). MNAR was assumed when the protein was not identified in all replicates of at least one condition. To reveal proteins of which the expression level was significantly regulated between the different conditions, the test_diff function of the DEP R-package was performed to compare intensities of the proteins between the three different conditions (non-Tg, Tg FUS+/+ vehicle, Tg FUS+/+ ACY-738) .
Mice were euthanized with CO2 followed by cervical dislocation. Spinal cord was rapidly dissected and snap-frozen in liquid nitrogen. Samples were sent to the Metabolomics core (VIB, Leuven, Belgium) to perform targeted metabolomic profiling by Liquid Chromatography - Mass Spectrometry (LC-MS). Separation of metabolites prior to MS measurement was performed using a Dionex UltiMate 3000 LC System (Thermo Scientific) in-line coupled to a Q Exactive Orbitrap mass spectrometer (Thermo Scientific). Practically, 10 μl of the extract was injected on a C18 column (Acquity UPLC®HSS T3 1.8 μm 2.1x100mm, Waters) using solvent A (H2O, 10 mM Tributyl-Amine, 15 mM acetic acid) and solvent B (100% Methanol). Chromatographic separation was achieved with a flowrate of 0.250 ml/min and the following gradient elution profile: 0 min, 0%B; 2 min, 0%B; 7 min, 37%B; 14 min, 41%B; 26 min, 100%B; 30 min, 100%B; 31 min, 0%B; 40 min, 0%B. The column was thermostatted at 40 °C throughout the analysis. The MS operated in full scan negative ion mode (m/z range: 70–1050 Th) using a spray voltage of 4.2 kV, capillary temperature of 320 °C, sheath gas at 50.0, auxiliary gas at 15.0. The AGC target was set at 3e6 and resolution at 140,000, with a maximum IT fill time of 512 ms. Data processing was performed using the Xcalibur Quan software (Thermo Scientific).
Statistical analyses were performed using GraphPad Prism software version 8.0.0 (GraphPad software Inc). For Kaplan-Meier survival curves, the log-rank test was used to determine the statistical significance. Unpaired two-tailed Student’s t-test was used for the comparison of two means. If needed, the results were corrected for multiple testing using the Holm-Sidak method, with Q = 1. One-way and two-way ANOVA were used for multiple group analyses. Data were tested for equal variances using Bartlett’s test, Brown-Forsythe test, F-test. Kruskal-Wallis and Mann-Witney were used when no equal variances were obtained in the data sets. Data are presented as means ± SEM. Statistical significance was set at P < 0.05. *P < 0.05, **P < 0.01, ***P < 0.001 ****P < 0.0001.
Progressive neurodegeneration in Tg FUS+/+ mice is associated with hypoacetylation of histones
To investigate the gradual deterioration of motor units in the Tg FUS+/+ mice, we assessed several characteristic neuropathological features before symptom onset (P28) and at late-symptomatic age (P60). Prior to the appearance of motor symptoms, there was no difference in the number of large α-motor neurons in the ventral horn of the lumbar spinal cord between Tg FUS+/+ mice and non-Tg littermate controls (Fig. 1a). At late-symptomatic age, approximately 60% of the α-motor neurons were lost in Tg FUS+/+ mice compared to age-matched controls (Fig. 1a). Assessment of the innervation of the gastrocnemius muscle showed a similar progressive neuromuscular denervation in Tg FUS+/+ animals compared to controls (Fig. 1b). Analysis of the myofiber size distribution in the gastrocnemius muscle showed a comparable profile as controls at pre-symptomatic age (Fig. 1c). However, a significant increase in small myofibers compared to controls was observed in Tg FUS+/+ animals at end-stage, indicating severe muscle atrophy (Fig. 1c). As a functional read-out of neuromuscular innervation, we performed in vivo nerve conduction studies in the sciatic nerve by measuring compound muscle action potentials (CMAPs). In line with our histological results, comparable amplitudes were measured at the gastrocnemius muscle in Tg FUS+/+ mice and controls at pre-symptomatic age, but these were significantly reduced at end-stage, complying with gradual axonal loss (Fig. 1d).
Interestingly, we found that the global acetylation levels of histones (lysine 9/14) were significantly reduced in spinal cord and cortical tissue of late-symptomatic (P60), but not of pre-symptomatic Tg FUS+/+ mice (P28) (Fig. 1e, f). To investigate whether the decreased histone acetylation was due to excessive activation of HDACs, we assessed the in situ enzymatic activity of nuclear HDACs in spinal cord homogenates of P60 mice (Fig. 1g). This assay revealed a 30% increase in nuclear HDAC activity in the spinal cord of Tg FUS+/+ mice compared to controls (Fig. 1g). Quantitative PCR and immunoblot analysis indicated no obvious expression changes of any of the class I HDACs, implying a post-transcriptional dysregulation of the HDACs (Fig. 1h, i and j).
HDAC inhibition mitigates the ALS disease phenotype in Tg FUS+/+ mice
In order to test whether nuclear HDAC hyperactivity might play a role in the phenotype observed in the Tg FUS+/+ mice, we tested the therapeutic potential of HDAC inhibition. ACY-738 increases histone acetylation in a concentration dependent manner. While it has the highest potency to inhibit HDAC6, class I HDACs are also targeted at higher concentrations. In N2a cells, 3 μM ACY-738 administration significantly increases the acetylation of both α-tubulin (lysine 40) and histone 3 (lysine 9/14) (Additional file 2: Figure S1A, B). To determine the concentration at which ACY-738 inhibits class I HDACs in vivo, nuclear fractions of mouse spinal cord lysates were treated with increasing concentrations of ACY-738, followed by measurement of HDAC enzymatic activity. The half maximal inhibitory concentration (IC50) of ACY-738 for nuclear HDACs was 0.59 μM in the spinal cord (Additional file 2: Figure S1C). We then treated Tg FUS+/+ mice with ACY-738 for 5 consecutive days, after which we measured the drug concentration in blood and brain samples using Liquid Chromatography/Mass Spectrometry (Additional file 2: Figure S1D). The concentrations ranged from ~ 0.25 to ~ 0.50 μM (Additional file 2: Figure S1D). This is in the concentration window where ACY-738 can inhibit class I HDACs (Additional file 2: Figure S1C). Western blot analyses of spinal cord lysates of Tg FUS+/+ mice treated with ACY-738 indeed revealed a two- to threefold increase in histone H3 acetylation (lysine 9/14), validating inhibition of class I HDACs in the central nervous system (CNS) (Fig. 2a, b). Consistent with Fig. 1f, histone acetylation was decreased in untreated Tg FUS+/+ mice compared to non-Tg controls (Fig. 2a, b).
To investigate whether HDAC inhibition could improve the motor deficits of Tg FUS+/+ mice, ACY-738 was administered daily starting at symptom onset (P30) to mimic a clinically relevant time point. We monitored weight and motor function of ACY-738-treated and non-treated littermate Tg FUS+/+ mice twice a week during the disease course, as well as the survival. Strikingly, Kaplan-Meier survival analysis revealed that ACY-738-treatment led to a substantial 40 days increase in lifespan of Tg FUS+/+ mice, accounting for a 68% prolongation of survival (Fig. 3a). This was also reflected in the disease duration (defined as the time between disease onset and end-stage), which increased from a median of 29.5 days in non-treated to 73.5 days in ACY-738-treated Tg FUS+/+ mice (Fig. 3b). This beneficial effect on survival was seen both in males and females, with a larger effect in males (Additional file 3: Figure S2A, B). Treated mice also exhibited reduced weight loss compared to non-treated mice (Fig. 3c). Moreover, mice receiving ACY-738 showed improved motor performance, as evidenced by a significant increase in forelimb grip strength (Fig. 3d). Also a trend towards increased performance in the hanging wire test was detected (Fig. 3e). ACY-738 treatment likewise mitigated the reduction in CMAP amplitudes (Fig. 3f). Long-term follow up of ACY-738-treated mice revealed that end-stage treated mice acquired a comparable decrease in weight and forelimb grip strength as end-stage non-treated Tg FUS+/+ controls (Additional file 3: Figure S2C, D). To control for the compound treatment, we treated Tg FUS+/+ mice with ACY-1090, an inactive form of ACY-738. This drug has a very similar structure to ACY-738 but it is incapable of inhibiting its target HDACs as it has a modified zinc-binding group (Additional file 4: Figure S3A). Treatment with ACY-1090 did not demonstrate an effect on survival or on the motor performance of Tg FUS+/+ mice (Additional file 4: Figure S3B-E). All together, these findings show that HDAC inhibition by ACY-738 treatment ameliorated the disease phenotype and significantly extended the lifespan of the Tg FUS+/+ mice.
In order to explore the therapeutic effect of ACY-738 on the motor unit, we performed histological analyses at an early (P40) and late (P60) symptomatic age. We assessed the effect of ACY-738 on motor neuron degeneration by counting the number of α-motor neuron cell bodies in the ventral horn of the lumbar spinal cord. We observed that the ACY-738 treatment did not affect degeneration of motor neuron cell bodies at both time points (Fig. 4a). However, we found enhanced innervation of the gastrocnemius muscle in the ACY-738-treated mice compared to control Tg FUS+/+ mice at P40, which was less apparent at P60 (Fig. 4b). These findings suggest that ACY-738 treatment slowed down denervation.
We further evaluated the effect of ACY-738 treatment on muscle atrophy, as this reflects the functionality of the neuromuscular junctions (NMJs) [45, 55]. At both time points, the weight of the gastrocnemius muscle of ACY-738-treated Tg FUS+/+ mice was significantly higher than those of vehicle-treated controls (Fig. 4c). Analysis of the myofiber size distribution showed that ACY-738-treated Tg FUS+/+ animals had an increased number of myofibers with a large diameter compared to control animals at both time points, indicating a beneficial effect of the treatment on muscle atrophy (Fig. 4d, e). In addition to maintaining innervation, these results imply that ACY-738 treatment increased the functionality of the NMJs and/or directly supported muscle function.
Besides degeneration of the motor unit, reactive gliosis is a key pathological observation in ALS patients. We assessed the effect of ACY-738 on astrocytosis and microgliosis in the lumbar spinal cord of Tg FUS+/+ mice by immuno-stainings for GFAP and CD11b, respectively. These stainings confirmed gliosis in the spinal cord of Tg FUS+/+ mice, but could not demonstrate an obvious change of this process by ACY-738 (Additional file 5: Figure S4).
A typical pathological hallmark that is specific for FUS-mediated ALS is cytoplasmic mislocalization of FUS in motor neurons. To investigate the effect of HDAC inhibition on this core pathological alteration, we analyzed the levels of FUS in cytoplasmic and nuclear fractions of spinal cord tissues of late symptomatic mice by immunoblotting. We could confirm increased FUS levels in the cytoplasm and nucleus as was described in the initial study. (Fig. 5a, b) . Similar as in non-Tg mice, the majority of FUS still resided in the nucleus, although a slight decrease of the nuclear-to-cytoplasmic ratio was seen in Tg FUS+/+ mice (Fig. 5a, c). Strikingly, we observed that ACY-738-treatment significantly decreased transgene FUS levels in the cytoplasm and moderately increased its levels in the nucleus (Fig. 5a, b). This subcellular localization shift moderately increased the nuclear-to-cytoplasmic ratio (Fig. 5c). Importantly, the overall FUS levels were not affected by the treatment, which was confirmed by qPCR and Western blot analysis (Fig. 5d-f). Immunostainings for FUS in the ventral horn of the lumbar spinal cord confirmed a limited decrease in cytoplasmic FUS levels in ACY-738-treated Tg FUS+/+ mice compared to vehicle-treated controls (Fig. 5g).
Collectively, these results indicate that ACY-738 partially prevented cytoplasmic mislocalization of FUS in the remaining motor neurons, which could positively affect their function. This could preserve the innervation and hence improve the motor performance and survival of the Tg FUS+/+ mice.
HDAC6 is not involved in the therapeutic effect of ACY-738 in Tg FUS+/+ mice
Besides the class I HDACs, ACY-738 is capable of inhibiting the cytoplasmic class IIb HDAC6. To rule out the possibility that HDAC6 was mediating the therapeutic effect of ACY-738, we investigated whether the suppression of HDAC6 alone phenocopied the broad-acting HDAC inhibitor ACY-738, by combining genetic and pharmacological approaches. First, we investigated the consequences of genetic removal of Hdac6 on the disease phenotype by crossbreeding the Tg FUS+/+ mice with Hdac6 knock-out (KO) mice . Increased acetylation of α-tubulin can be used as a readout for HDAC6 inhibition or deletion . Indeed, we confirmed that Tg FUS+/+; Hdac6 KO mice showed hyperacetylated α-tubulin compared with their Tg FUS+/+; Hdac6 WT littermates (Fig. 6a). However, Kaplan-Meier survival analysis could not demonstrate a longer survival after genetic Hdac6 removal in the Tg FUS+/+ mice (Fig. 6b). Conversely, Tg FUS+/+; Hdac6 KO mice treated with ACY-738 showed a similar extension in life span of 41 days as treated Tg FUS+/+ mice (Fig. 6b). The treatment regimen in KO mice did not produce further increases in α-tubulin acetylation over KO baseline levels (Fig. 6a).
These findings strongly indicate that HDAC6 is not the key HDAC effector responsible for the beneficial effect of ACY-738 in the Tg FUS+/+ mouse model. Collectively, our data further substantiate that the therapeutic activity of ACY-738 is mediated by the inhibition of class I HDACs.
HDAC inhibition restores disease-associated pathways in Tg FUS+/+ mice
To elucidate the disease-causing pathways and possible treatment targets of ACY-738, we performed an integrative transcriptome and proteome analysis on spinal cord tissue of 60-day old non-Tg, vehicle- and ACY-738-treated Tg FUS+/+ mice.
Multidimensional scaling (MDS) of the transcriptomics dataset (15,203 detected genes) indicated a high degree of gene expression similarity between biological replicates (Additional file 6: Figure S5A). Statistical analysis showed that 2860 genes were significantly differentially expressed in vehicle-treated Tg FUS+/+ mice compared to non-Tg controls (Fig. 7a). Comparison of ACY-738-treated Tg FUS+/+ mice with non-Tg revealed 1576 differentially expressed genes (DEGs), indicating that ACY-738 therapy leads to a less severe effect on overall gene expression (Fig. 7a). Heat map analysis of all differentially expressed genes revealed that ACY-738 therapy rescued a large part of the disease-induced transcription aberrations, yielding a gene expression profile more similar to non-Tg controls (Additional file 6: Figure S5B). Besides the (partial) restoration of disease-induced expression changes, a moderate number of new transcriptomic changes (111 genes) were detected after ACY-738 therapy (Additional file 6: Figure S5C).
To determine the therapeutically relevant transcriptional changes, we focused on the intersection between disease- and drug-induced expression changes, which resulted in a list of 686 genes (Additional file 6: Figure S5C). The majority showed a trend towards the wild-type level after ACY-738 treatment. A subset of 417 genes demonstrated a complete restoration after treatment (Additional file 6: Figure S5C and Fig. 7b). As the beneficial effect of ACY-738 most likely results from reinstating histone acetylation, these fully restored genes might be considered as most relevant.
The proteomics dataset, containing 3491 detected proteins, was analyzed in a similar way. MDS revealed high similarity between the 3 biological replicates (Additional file 6: Figure S5D). Statistical analysis showed that the levels of 82 proteins were significantly altered in vehicle-treated Tg FUS+/+ mice compared to non-Tg controls (Fig. 7c). Also here, ACY-738-treated Tg FUS+/+ mice presented with less (37) differentially expressed proteins (DEPs) compared to non-Tg controls (Fig. 7c). Heat map analysis of all DEPs revealed that ACY-738 therapy rescued a large part of the disease-induced protein aberrations (Additional file 6: Figure S5E). The levels of 26 proteins were fully restored to wild-type levels (Additional file 6: Figure S5F and Fig. 7d).
Next, we performed a multi-omics correlation analysis to find out whether the same trends and patterns were found with transcriptomics and proteomics analyses. We compared differential expression based on the proteomic data with the differential expression of the corresponding mRNAs using the transcriptomic data. In vehicle-treated Tg FUS+/+ mice, 441 of the 3491 detected proteins were significantly altered on the mRNA level compared to controls (Additional file 6: Figure S5G). Overall, 33 of the 82 DEPs could not be explained by differences on the mRNA level (Additional file 6: Figure S5G). A possible explanation is that these proteins are regulated at the post-transcriptional level. Pearson correlation analysis showed a modest though significant correlation of the expression values for all found protein-transcript pairs (r2 = 0.31) (Additional file 6: Figure S5H). A consistent change at the mRNA and protein level was shown for a subset of 49 genes that were significantly differentially expressed in both datasets (r2 = 0.84) (Additional file 6: Figure S5I).
In ACY-738-treated Tg FUS+/+ mice, 163 of the 3491 detected proteins were differentially expressed on the mRNA level compared to controls (Additional file 6: Figure S5J). Fourteen of the 37 DEPs could not be validated on the mRNA level (Additional file 6: Figure S5J). Similarly, there was a moderate but significant correlation of the expression values for all found protein-transcript pairs (r2 = 0.24) (Additional file 6: Figure S5K). Again, the subset of 23 proteins overlapping between the DEGs and DEPs showed a strong correlation with their reciprocal transcript levels (r2 = 0.75) (Additional file 6: Figure S5L).
Using the Panther Gene Ontology (GO) enrichment analysis program on both omics datasets, we found that most genes and proteins that were changed in Tg FUS+/+ mice were associated with inflammation, metabolism, protein folding and cellular structures (Fig. 7e) [3, 39, 66]. Analysis of the subset of genes and proteins that were fully restored after ACY-738 therapy revealed an enrichment of GO terms related to metabolism (Fig. 7e).
The observed alterations in the expression of metabolic genes in the Tg FUS+/+ mouse model are interesting, as increasing evidence suggests that metabolic disturbances contribute to ALS pathogenesis . Targeted search of genes involved in metabolism showed decreased levels of genes associated with fatty acid and cholesterol biosynthesis and β-oxidation, and increased levels of genes associated with glycolysis, the pentose phosphate pathway (PPP) and lipid transport in Tg FUS+/+ mice (Additional file 7: Figure S6). ACY-738 treatment partially restored the expression levels of most of these genes, both on the mRNA and protein level (Additional file 7: Figure S6). The changes induced by the treatment include both up- and downregulated genes, suggesting an overall multifaceted restoration of these pathways.
HDAC inhibition reinstates metabolic homeostasis in the spinal cord
While transcriptomic and proteomic experiments took place on late-symptomatic Tg FUS+/+ mice, we investigated whether the observed metabolic abnormalities were critical for or rather a consequence of the disease. In order to do so, we performed qPCR experiments on spinal cord tissue of Tg FUS+/+ mice at pre-symptomatic age (P25), symptom onset (P30), early (P40) and late symptomatic (P60) age. Strikingly, we found that genes related to the breakdown of fatty acids were already significantly downregulated at pre-symptomatic age, whereas the downregulation of cholesterol and lipid synthesis, as well as the upregulation of lipid transport and glycolysis, were disturbed starting from symptom-onset or later (Fig. 8a). The upregulation of glycolysis and lipid transport pathways may therefore be a secondary mechanism compensating for primary defects in lipid metabolism. In P60 ACY-738-treated mice, the majority of the observed metabolic gene expression aberrations were less pronounced or even absent (Fig. 8a). These data indicate that alterations in the expression of metabolic genes are an initial and maybe critical event in the pathology of Tg FUS+/+ mice and suggest that ACY-738 therapy restores metabolic homeostasis.
To investigate the functional consequence of abnormalities in metabolic gene expression, we performed a metabolomic study at P60. Interestingly, several key glycolysis and PPP metabolites were significantly upregulated in the vehicle-treated Tg FUS+/+ mice, consistent with the observed upregulation of the enzymes that catalyze the corresponding reactions in this pathway (Fig. 8b, c and Additional file 7: Figure S6).
Collectively, these findings show that dysregulated metabolism is an early phenomenon correlating with progressive motor neuron pathology in Tg FUS+/+ mice and indicate that ACY-738 may act by reinstating metabolic homeostasis.
The pathological mechanisms underlying ALS remain incompletely understood, which could account for the numerous failed clinical trials in this patient population. We provide evidence for the contribution of aberrant histone acetylation in motor neuron pathology and discovered that HDAC inhibitors are an effective therapy in a preclinical model of ALS. Our data show that ACY-738, a potent HDAC inhibitor that crosses the BBB, restored global histone acetylation in the spinal cord, ameliorated the disease phenotype and significantly extended the lifespan of mice overexpressing wild-type FUS. We found that HDAC6 is not the key HDAC mediating this therapeutic effect. Our multi-omics approach revealed that dysregulated metabolism was an early phenomenon correlating with motor neuron pathology, which was largely restored by ACY-738 therapy.
Recent evidence points to a possible role of epigenetic mechanisms, including microRNAs, DNA methylation and histone modifications, in ALS pathology [7, 44]. Amongst these, we concentrated on the possible contribution of histone acetylation, a post-translational modification that regulates transcription, in a rodent model of ALS. Aberrant activation of HDACs, resulting in histone hypoacetylation, has been associated with several neurodegenerative disorders and with neuronal toxicity [7, 31, 58]. Pioneering work by Rouaux and collaborators reported evidence for a role of HDACs in ALS, demonstrating histone hypoacetylation in the SOD1 mouse model starting at the age of onset . In postmortem brain and spinal cord specimens of ALS patients, analysis of HDAC expression levels also revealed altered levels of HDAC2 and HDAC11 . While the various HDACs were classified and categorized, the role of particular HDACs in ALS pathogenesis has not been fully addressed yet. In more recent studies, it was shown that muscle HDAC4 plays a crucial role in muscle reinnervation in SOD1 mice and in patients with rapidly progressive ALS [11, 48, 49, 74].
One important question is the molecular mechanism underlying the decrease in histone acetylation observed in Tg FUS+/+ mice. ALS-causative genes have been associated with various epigenetic modifiers and epigenetic tags [7, 12]. For example, the DNA/RNA binding protein FUS directly interacts with CBP and p300, two histone acetyltransferases, as well as with HDAC1 [72, 73]. Therefore, the observed hyperactivity of nuclear HDACs and associated histone hypoacetylation in the Tg FUS+/+ mice could arise from such an interaction. Further studies are required to confirm this.
The role of HDACs in neurodegenerative diseases has largely been deduced from effects observed after inhibition of their enzymatic activity. In the context of ALS, several studies have shown a modest protective effect of three pan-HDAC inhibitors, trichostatin A (TSA), valproic acid (VPA) and phenyl butyrate (PB) in the SOD1 model [15, 46, 56, 76]. TSA is a very potent HDAC inhibitor, yet it can be used only in laboratory experiments due to its genotoxic effects . VPA is used as an antiepileptic drug, but has a low HDAC inhibitory potency, poor BBB permeability and cumbersome side effects. PB is currently used to treat hyperammonemia due to urea cycle disorders and is also known to have a low inhibitory potency. It may therefore not be surprising that phase II clinical trials in ALS patients showed negative results [13, 47]. In our study, we used ACY-738 to explore the therapeutic potential of HDAC inhibition in a preclinical FUS model of ALS. ACY-738 is a highly BBB permeable, potent HDAC inhibitor that primarily targets class I HDACs and HDAC6 [8, 30, 41]. Our data show that the inhibition of the class I HDACs, which corrects global histone acetylation and partially restores transcription, is responsible for the positive effect in the Tg FUS+/+ model. ACY-738 is an attractive drug candidate, as we could show robust class I HDAC inhibition in vivo with no obvious adverse effects on the treated animals.
The finding that genetic removal of Hdac6 did not have a beneficial effect in the Tg FUS+/+ mice is in contrast with our results observed in the SOD1 model, in which HDAC6 removal modestly extended their survival . This could be due to differences in the pathogenic mechanisms underlying both genetic forms of ALS. Another indication of this diversity is our previous observation that pharmacological inhibition as well as genetic silencing of HDAC6 in a different FUS-related model had positive effects . Motor neurons differentiated from induced pluripotent stem cells (iPSCs) from FUS-ALS patients developed axonal transport defects over time and inhibition of HDAC6 using tubastatin A or ACY-738 completely rescued these defects . In our current study, we excluded that HDAC6 inhibition by ACY-738 was responsible for the positive effect on the survival of the Tg FUS+/+ mice. One should keep in mind that these different effects of ACY-738 were obtained in two completely different models that both mimic relevant aspects of the ALS disease process. Whatever the exact contribution in ALS patients is of axonal transport defects due to decreased acetylation of α-tubulin or of aberrant transcription caused by hypoacetylation of histones, ACY-738 has the major advantage that it corrects both processes.
Furthermore, we noticed that ACY-738 therapy can significantly decrease cytoplasmic human FUS levels in the remaining motor neurons. It is possible that ACY-738 acts on this process by slowing down several key aspects of disease progression due to its effects on transcription. However, the partial restoration of FUS localization might also be independent from changes in histone acetylation or transcription. The synergistic correction of each of these different processes could contribute to the therapeutic activity of ACY-738.
Using an integrative transcriptomic, proteomic and metabolomic approach, we ultimately discovered that dysregulation of lipid metabolism was an early phenomenon correlating with progressive motor neuron pathology. These results are in line with a recent study that showed drastic morphological alterations in mitochondria at the synaptic terminals of pre-symptomatic Tg FUS+/+ mice . Furthermore, expression changes of genes related to (lipid) metabolism were noted in another wild-type FUS overexpression mouse model, as well as in a mutant FUS overexpression and FUS-ΔNLS-knock-in mouse model, suggesting a specific pathogenic mechanism contributing to FUS-mediated ALS [17, 50, 61]. It is possible that these other FUS models also present with histone acetylation changes that dysregulate the expression of metabolic genes. Strikingly, our multi-omics analysis revealed a substantial rescue of the observed metabolic disturbances by ACY-738 treatment. Although neurons and glial cells express many molecular components of lipid metabolic pathways, the importance of local regulation of lipid metabolism in the CNS has remained neglected for a long time. Only recently, several studies highlight central lipid metabolism homeostasis as a critical factor for neuronal function and survival [33, 35, 36]. Cholesterol is locally synthesized in the adult CNS, with little or no import from the periphery . It is synthesized mostly by astrocytes, after which it is transported by apolipoprotein E (APOE) and taken up by neurons via the low-density lipoprotein receptor. Fatty acids (FA) on the other hand are mainly transported into the CNS from the systemic circulation, although some FAs can be synthesized de novo by neurons and astrocytes [10, 23, 35]. Disturbances in either the synthesis, transport, or turnover of lipids were shown to trigger synapse loss and neurodegeneration [10, 23, 25, 35, 36]. The observed disturbances in lipid metabolic pathways in the Tg FUS+/+ mice could affect membrane biogenesis-dependent processes such as synaptogenesis, synapse maintenance, neurotransmitter release and mitochondrial function [26, 33, 36]. As these processes are all determinants of proper neuromuscular functionality, an early disturbance in central lipid homeostasis could contribute to ALS pathogenesis [4, 60]. Accordingly, the rescue of metabolic homeostasis by ACY-738 therapy could account for the preservation of neuromuscular junctions, as appreciated by an increased number of innervated junctions and increased compound muscle action potentials.
It will be important to validate our findings on disturbed histone acetylation and metabolism in other ALS models. In fact, none of the ALS rodent models, including the Tg FUS+/+ mouse model used in our study, fully recapitulates human disease. Therefore, it is reasonable that only the combined knowledge obtained from each of these models will enable us to understand the deleterious processes underlying the selective motor neuron death in ALS.
Overall, our hypothesis illustrated in Fig. 8d is that ALS-associated proteins such as FUS can influence the epigenetic code. These epigenetic alterations, in combination with cytoplasmic accumulation of ALS-associated proteins, will have tremendous implications on the global transcription profile. This will affect different processes, such as metabolic pathways, that are essential for motor neurons, ultimately leading to degeneration. We propose that inhibition of class I HDACs by ACY-738 can partially overcome these transcriptional defects by restoring histone acetylation and FUS mislocalization, thereby ultimately improving the ALS phenotype. It will be important to define which HDAC family member is most crucial for the observed effect, so that safe, selective and potent HDAC inhibitors can be developed.
In summary, our findings confirm that epigenetic mechanisms contribute to ALS pathology in a FUS animal model that recapitulates many aspects of the disease. Moreover, our study provides evidence that class I HDACs are promising pharmacological targets for ALS. ACY-738 showed the most significant beneficial effects of all HDAC inhibitors tested in ALS models so far, probably due to its superior pharmacokinetic features. Therefore, this drug should be further evaluated for its clinical efficacy in the context of ALS.
Availability of data and materials
The datasets generated during and/or analysed during the current study are available from the corresponding author on reasonable request.
Amyotrophic lateral sclerosis
Chromosome 9 open reading frame 72
Compound muscle action potential
Central nervous system
Differentially expressed gene
Differentially expressed protein
Fused in sarcoma
Pentose phosphate pathway
Superoxide dismutase 1
TAR DNA-binding protein 43
Abe K, Aoki M, Tsuji S, Itoyama Y, Sobue G, Togo M et al (2017) Safety and efficacy of edaravone in well defined patients with amyotrophic lateral sclerosis: a randomised, double-blind, placebo-controlled trial. Lancet Neurol 16:505–512
Al-Chalabi A, Jones A, Troakes C, King A, Al-Sarraj S, van den Berg LH (2012) The genetics and neuropathology of amyotrophic lateral sclerosis. Acta Neuropathol 124:339–352
Ashburner M, Ball CA, Blake JA, Botstein D, Butler H, Cherry JM et al (2000) Gene ontology: tool for the unification of biology. Nat Genet 25:25–29
Aufschnaiter A, Kohler V, Diessl J, Peselj C, Carmona-Gutierrez D, Keller W et al (2017) Mitochondrial lipids in neurodegeneration. Cell Tissue Res 367:125–140
Avila AM, Burnett BG, Taye A, Gabanella F, Knight MA, Hartenstein P et al (2007) Trichostatin a increases SMN expression and survival in a mouse model of spinal muscular atrophy. J Clin Invest 117:659–671
Benito E, Urbanke H, Ramachandran B, Barth J, Halder R, Awasthi A et al (2015) HDAC inhibitor-dependent transcriptome and memory reinstatement in cognitive decline models. J Clin Invest 125:3572–3584
Bennett SA, Tanaz R, Cobos SN, Torrente MP (2018) Epigenetics in amyotrophic lateral sclerosis: a role for histone post-translational modifications in neurodegenerative disease. Transl Res 204:19–30
Benoy V, Vanden Berghe P, Jarpe M, Van Damme P, Robberecht W, Van Den Bosch L (2017) Development of improved HDAC6 inhibitors as pharmacological therapy for axonal Charcot–Marie–Tooth disease. Neurotherapeutics 14:417–428.
Bensimon G, Lacomblez L, Meininger V (1994) A controlled trial of Riluzole in amyotrophic lateral sclerosis. N Engl J Med 330:585–591
Bouyakdan K, Taïb B, Budry L, Zhao S, Rodaros D, Neess D et al (2015) A novel role for central ACBP/DBI as a regulator of long-chain fatty acid metabolism in astrocytes. J Neurochem 133:253–265
Bruneteau G, Simonet T, Bauché S, Mandjee N, Malfatti E, Girard E et al (2013) Muscle histone deacetylase 4 upregulation in amyotrophic lateral sclerosis: potential role in reinnervation ability and disease progression. Brain 136:2359–2368
Chen K, Bennett SA, Rana N, Yousuf H, Said M, Taaseen S et al (2017) Neurodegenerative disease Proteinopathies are connected to distinct histone post-translational modification landscapes. ACS Chem Neurosci 9:838–848
Cudkowicz ME, Andres PL, Macdonald SA, Bedlack RS, Choudry R, Brown RH Jr et al (2009) Phase 2 study of sodium phenylbutyrate in ALS. Amyotroph Lateral Scler 10:99–106
d’Ydewalle C, Krishnan J, Chiheb DM, Van Damme P, Irobi J, Kozikowski AP et al (2011) HDAC6 inhibitors reverse axonal loss in a mouse model of mutant HSPB1–induced Charcot-Marie-tooth disease. Nat Med 17:968–974
Del Signore SJ, Amante DJ, Kim J, Stack EC, Goodrich S, Cormier K et al (2009) Amyotrophic lateral sclerosis combined riluzole and sodium phenylbutyrate therapy in transgenic amyotrophic lateral sclerosis mice. Amyotroph Lateral Scler 10:85–94
Deng HX, Zhai H, Bigio EH, Yan J, Fecto F, Ajroud K et al (2010) FUS-immunoreactive inclusions are a common feature in sporadic and non-SOD1 familial amyotrophic lateral sclerosis. Ann Neurol 67:739–748
Devoy A, Kalmar B, Stewart M, Park H, Burke B, Noy SJ et al (2017) Humanized mutant FUS drives progressive motor neuron degeneration without aggregation in ‘FUSDelta14’ knockin mice. Brain 140:2797-2805
Didonna A, Opal P (2014) The promise and perils of HDAC inhibitors in neurodegeneration. Ann Clin Transl Neurol 2:79–101
Dini Modigliani S, Morlando M, Errichelli L, Sabatelli M, Bozzoni I (2014) An ALS-associated mutation in the FUS 3′-UTR disrupts a microRNA–FUS regulatory circuitry. Nat Commun 5:4335
Dobin A, Davis CA, Schlesinger F, Drenkow J, Zaleski C, Jha S et al (2013) STAR: ultrafast universal RNA-seq aligner. Bioinformatics 29:15–21
Dormann D, Haass C (2013) Fused in sarcoma (FUS): an oncogene goes awry in neurodegeneration. Mol Cell Neurosci 56:475–486
Eberharter A, Becker PB (2002) Histone acetylation: a switch between repressive and permissive chromatin. EMBO Rep 3:224–229
Ebrahimi M, Yamamoto Y, Sharifi K, Kida H, Kagawa Y, Yasumoto Y et al (2016) Astrocyte-expressed FABP7 regulates dendritic morphology and excitatory synaptic function of cortical neurons. Glia 64:48–62
Eckschlager T, Plch J, Stiborova M, Hrabeta J (2017) Histone deacetylase inhibitors as anticancer drugs. Int J Mol Sci 18:1414
Ferris HA, Perry RJ, Moreira GV, Shulman GI, Horton JD, Kahn CR (2017) Loss of astrocyte cholesterol synthesis disrupts neuronal function and alters whole-body metabolism. Proc Natl Acad Sci U S A 114:1189–1194
Frank C, Rufini S, Tancredi V, Forcina R, Grossi D, D’Arcangelo G (2008) Cholesterol depletion inhibits synaptic transmission and synaptic plasticity in rat hippocampus. Exp Neurol 212:407–414
Guo W, Naujock M, Fumagalli L, Vandoorne T, Baatsen P, Boon R et al (2017) HDAC6 inhibition reverses axonal transport defects in motor neurons derived from FUS-ALS patients. Nat Commun 8:861
Hubbert C, Guardiola A, Shao R, Kawaguchi Y, Ito A, Nixon A et al (2002) HDAC6 is a microtubule-associated deacetylase. Nature 417:455–458
Janssen C, Schmalbach S, Boeselt S, Sarlette A, Dengler R, Petri S (2010) Differential Histone Deacetylase mRNA Expression Patterns in Amyotrophic Lateral Sclerosis. J Neuropathol Exp Neurol 69:573–581
Jochems J, Boulden J, Lee BG, Blendy JA, Jarpe M, Mazitschek R et al (2014) Antidepressant-like properties of novel HDAC6-selective inhibitors with improved brain bioavailability. Neuropsychopharmacology 39:389–400
Konsoula Z, Barile FA (2012) Epigenetic histone acetylation and deacetylation mechanisms in experimental models of neurodegenerative disorders. J Pharmacol Toxicol Methods 66:215–220
Kwiatkowski TJ, Bosco DA, Leclerc AL, Tamrazian E, Vanderburg CR, Russ C et al (2009) Mutations in the FUS/TLS gene on chromosome 16 cause familial amyotrophic lateral sclerosis. Science 323:1205–1208
Lauwers E, Goodchild R, Verstreken P (2016) Membrane lipids in presynaptic function and disease. Neuron 90:11–25
Lazo-Gómez R, Ramírez-Jarquín UN, Tovar-y-Romo LB, Tapia R (2013) Histone deacetylases and their role in motor neuron degeneration. Front Cell Neurosci 7:243
Liu L, MacKenzie KR, Putluri N, Maletić-Savatić M, Bellen HJ (2017) The glia-neuron lactate shuttle and elevated ROS promote lipid synthesis in neurons and lipid droplet accumulation in glia via APOE/D. Cell Metab 26:719–737
Liu Q, Trotter J, Juan Z, Melinda MP, Cheng H, Jianxin B et al (2010) Neuronal LRP1 knockout in adult mice leads to impaired brain lipid metabolism and progressive, age-dependent synapse loss and neurodegeneration. J Neurosci 30:17068–17078
Majid T, Griffin D, Criss Z, Jarpe M, Pautler RG (2015) Pharmocologic treatment with histone deacetylase 6 inhibitor (ACY-738) recovers Alzheimer’s disease phenotype in amyloid precursor protein/presenilin 1 (APP/PS1) mice. Alzheimer’s Dement Transl Res Clin Interv 1:170–181
McCarthy DJ, Chen Y, Smyth GK (2012) Differential expression analysis of multifactor RNA-Seq experiments with respect to biological variation. Nucleic Acids Res 40:4288–4297
Mi H, Huang X, Muruganujan A, Tang H, Mills C, Kang D et al (2017) PANTHER version 11: expanded annotation data from gene ontology and Reactome pathways, and data analysis tool enhancements. Nucleic Acids Res 45:D183–D189
Mitchell JC, McGoldrick P, Vance C, Hortobagyi T, Sreedharan J, Rogelj B et al (2013) Overexpression of human wild-type FUS causes progressive motor neuron degeneration in an age- and dose-dependent fashion. Acta Neuropathol 125:273–288
Mithraprabhu S, Khong T, Jones SS, Spencer A (2013) Histone deacetylase (HDAC) inhibitors as single agents induce multiple myeloma cell death principally through the inhibition of class I HDAC. Br J Haematol 162:559–562
Neumann M, Rademakers R, Roeber S, Baker M, Kretzschmar HA, Mackenzie IRA (2009) A new subtype of frontotemporal lobar degeneration with FUS pathology. Brain 132:2922–2931
Olaharski AJ, Ji Z, Woo J-Y, Lim S, Hubbard AE, Zhang L et al (2006) The histone deacetylase inhibitor Trichostatin a has genotoxic effects in human Lymphoblasts in vitro. Toxicol Sci 93:341–347
Paez-Colasante X, Figueroa-Romero C, Sakowski SA, Goutman SA, Feldman EL (2015) Amyotrophic lateral sclerosis: mechanisms and therapeutics in the epigenomic era. Nat Rev Neurol 11:266–279
Pansarasa O, Rossi D, Berardinelli A, Cereda C (2014) Amyotrophic lateral sclerosis and skeletal muscle: an update. Mol Neurobiol 49:984–990
Petri S, Kiaei M, Kipiani K, Chen J, Calingasan NY, Crow JP et al (2006) Additive neuroprotective effects of a histone deacetylase inhibitor and a catalytic antioxidant in a transgenic mouse model of amyotrophic lateral sclerosis. Neurobiol Dis 22:40–49
Piepers S, Veldink JH, De Jong SW, Van Der Tweel I, Van Der Pol W-L, Uijtendaal EV et al (2009) Randomized sequential trial of valproic acid in amyotrophic lateral sclerosis. Ann Neurol 66:227–234
Pigna E, Renzini A, Greco E, Simonazzi E, Fulle S, Mancinelli R et al (2018) HDAC4 preserves skeletal muscle structure following long-term denervation by mediating distinct cellular responses. Skelet Muscle 8:6
Pigna E, Simonazzi E, Sanna K, Bernadzki KM, Proszynski T, Heil C et al (2019) Histone deacetylase 4 protects from denervation and skeletal muscle atrophy in a murine model of amyotrophic lateral sclerosis. EBioMedicine. https://doi.org/10.1016/J.EBIOM.2019.01.038
Qiu H, Lee S, Shang Y, Wang WY, Au KF, Kamiya S et al (2014) ALS-associated mutation FUS-R521C causes DNA damage and RNA splicing defects. J Clin Invest 124:981–999
Renton AE, Chiò A, Traynor BJ (2014) State of play in amyotrophic lateral sclerosis genetics. Nat Neurosci 17:17–23
Riessland M, Ackermann B, Förster A, Jakubik M, Hauke J, Garbes L et al (2010) SAHA ameliorates the SMA phenotype in two mouse models for spinal muscular atrophy. Hum Mol Genet 19:1492–1506
Rouaux C, Jokic N, Mbebi C, Boutillier S, Loeffler J-P, Boutillier A-L (2003) Critical loss of CBP/p300 histone acetylase activity by caspase-6 during neurodegeneration. EMBO J 22:6537–6549
Rouaux C, Panteleeva I, René F, Gonzalez de Aguilar J-L, Echaniz-Laguna A, Dupuis L et al (2007) Sodium valproate exerts neuroprotective effects in vivo through CREB-binding protein-dependent mechanisms but does not improve survival in an amyotrophic lateral sclerosis mouse model. J Neurosci 27:5535–5545
Rudolf R, Deschenes MR, Sandri M (2016) Neuromuscular junction degeneration in muscle wasting. Curr Opin Clin Nutr Metab Care 19:177–181
Ryu H, Smith K, Camelo SI, Carreras I, Lee J, Iglesias AH et al (2005) Sodium phenylbutyrate prolongs survival and regulates expression of anti-apoptotic genes in transgenic amyotrophic lateral sclerosis mice. J Neurochem 93:1087–1098
Sabatelli M, Moncada A, Conte A, Lattante S, Marangi G, Luigetti M et al (2013) Mutations in the 3′ untranslated region of FUS causing FUS overexpression are associated with amyotrophic lateral sclerosis. Hum Mol Genet 22:4748–4755
Saha R, Pahan K (2006) HATs and HDACs in neurodegeneration: a tale of disconcerted acetylation homeostasis. Cell Death Differ 13:539–550
Sawada H (2017) Clinical efficacy of edaravone for the treatment of amyotrophic lateral sclerosis. Expert Opin Pharmacother 18:735–738
Schmitt F, Hussain G, Dupuis L, Loeffler J-P, Henriques A (2014) A plural role for lipids in motor neuron diseases: energy, signaling and structure. Front Cell Neurosci 8:25
Sephton CF, Tang AA, Kulkarni A, West J, Brooks M, Stubblefield JJ et al (2014) Activity-dependent FUS dysregulation disrupts synaptic homeostasis. Proc Natl Acad Sci U S A 111:E4769–E4778
So E, Mitchell JC, Memmi C, Chennell G, Vizcay-Barrena G, Allison L et al (2018) Mitochondrial abnormalities and disruption of the neuromuscular junction precede the clinical phenotype and motor neuron loss in hFUSWTtransgenic mice. Hum Mol Genet 27:463–474
Spandidos A, Wang X, Wang H, Seed B (2010) PrimerBank: a resource of human and mouse PCR primer pairs for gene expression detection and quantification. Nucleic Acids Res 38:792–799
Sugai F, Yamamoto Y, Miyaguchi K, Zhou Z, Sumi H, Hamasaki T et al (2004) Benefit of valproic acid in suppressing disease progression of ALS model mice. Eur J Neurosci 20:3179–3183
Taes I, Timmers M, Hersmus N, Bento-Abreu A, Van Den Bosch L, Van Damme P et al (2013) Hdac6 deletion delays disease progression in the SOD1G93A mouse model of ALS. Hum Mol Genet 22:1783–1790
The Gene Ontology Consortium (2017) Expansion of the gene ontology knowledgebase and resources. Nucleic Acids Res 45:D331–D338
Thomas EA, Coppola G, Desplats PA, Tang B, Soragni E, Burnett R et al (2008) The HDAC inhibitor 4b ameliorates the disease phenotype and transcriptional abnormalities in Huntington’s disease transgenic mice. Proc Natl Acad Sci U S A 105:15564–15569
Valle C, Salvatori I, Gerbino V, Rossi S, Palamiuc L, René F (2014) Tissue-specific deregulation of selected HDACs characterizes ALS progression in mouse models: pharmacological characterization of SIRT1 and SIRT2 pathways. Cell Death Dis 5:1296
van Langenhove T, van der Zee J, van Broeckhoven C (2012) The molecular basis of the frontotemporal lobar degeneration–amyotrophic lateral sclerosis spectrum. Ann Med 44:817–828
Vance C, Rogelj B, Hortobágyi T, De Vos KJ, Nishimura AL, Sreedharan J et al (2009) Mutations in FUS, an RNA processing protein, cause familial amyotrophic lateral sclerosis type 6. Science 323:1208–1211
Vandoorne T, De Bock K, Van Den Bosch L (2018) Energy metabolism in ALS: an underappreciated opportunity? Acta Neuropathol 135:489–509
Wang W-Y, Pan L, Su SC, Quinn EJ, Sasaki M, Jimenez JC et al (2013) Interaction of FUS and HDAC1 regulates DNA damage response and repair in neurons. Nat Neurosci 16:1383–1391
Wang X, Arai S, Song X, Reichart D, Du K, Pascual G et al (2008) Induced ncRNAs allosterically modify RNA-binding proteins in cis to inhibit transcription. Nature 454:126–130
Williams AH, Valdez G, Moresi V, Qi X, McAnally J, Elliott JL et al (2009) MicroRNA-206 delays ALS progression and promotes regeneration of neuromuscular synapses in mice. Science 326:1549–1554
Yang S-S, Zhang R, Wang G, Zhang Y-F (2017) The development prospection of HDAC inhibitors as a potential therapeutic direction in Alzheimer’s disease. Transl Neurodegener 6:19
Yoo Y-E, Ko C-P (2011) Treatment with trichostatin a initiated after disease onset delays disease progression and increases survival in a mouse model of amyotrophic lateral sclerosis. Exp Neurol 231:147–159
Zhang J, Liu Q (2015) Cholesterol metabolism and homeostasis in the brain. Protein Cell 6:254–264
Zhang X, Smits AH, van Tilburg GB, Ovaa H, Huber W, Vermeulen M (2018) Proteome-wide identification of ubiquitin interactions using UbIA-MS. Nat Protoc 13:530–550
Zhang Y, Kwon S, Yamaguchi T, Cubizolles F, Rousseaux S, Kneissel M et al (2008) Mice lacking histone deacetylase 6 have hyperacetylated tubulin but are viable and develop normally. Mol Cell Biol 28:1688–1701
Rob Patro, Geet Duggal, Michael I Love, Rafael A Irizarry, Carl Kingsford, (2017) Salmon provides fast and bias-aware quantification of transcript expression. Nature Methods 14 (4):417-419
We thank Caroline Eykens, Veronick Benoy and Tijs Vandoorne for scientific discussions. We wish to acknowledge Wendy Scheveneels and Stijn Verschoren for technical assistance. We are grateful to Begga Schevenels and Séraphina Penninckx for mouse colony maintenance.
This work was supported by grants from the Fund for Scientific Research Flanders (FWO-Vlaanderen, G.0431.12 N and G.0440.12 N), the Interuniversity Attraction Poles Programme P7/16 initiated by the Belgian Science Policy Office, the Muscular Dystrophy Association (MDA, 577668), the ALS Liga, the European Community’s Health Seventh Framework Programme (FP7/2007–2013 under grant agreement 259867), the ALS Therapy Alliance, the ALS Association (14-LGCA-181) and the Thierry Latran Foundation. PVD and LVDB are supported by the ‘Opening the Future’ Fund (KU Leuven). PVD holds a clinical investigatorship of FWO-Vlaanderen and is supported by ‘Een Hart voor ALS’ and Laevers Fund for ALS Research. ER and LVH are supported by the ‘Agency for Innovation by Science and Technology in Flanders’ (IWT-Vlaanderen). EP is supported by Saastamoinen foundation, Instrumentarium Science foundation and Finnish Cultural foundation.
Ethics approval and consent to participate
All animal experiments were approved by the ethical committee of the KU Leuven, Belgium (P055–2014) and comply with the current laws of Belgium.
Consent for publication
MJ is a shareholder of Acetylon Pharmaceuticals, a subsidiary of Celgene. The other authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Table S1. Primer sequences for the determination of expression of metabolic genes. Primers for quantitative PCR analysis of expression levels of metabolic genes. (DOCX 14 kb)
Figure S1. In vitro and in vivo pharmacokinetic properties of ACY-738. (A) Western blots showing the effects of different concentrations of ACY-738 on acetylation of α-tubulin and histone 3 in N2a cells. (B) Dose-response curves of the effect of ACY-738 based on the quantification of Western blots. The ratio of acetylated α-tubulin is normalized to calnexin (top) and acetylation of histone 3 is normalized to histone 4 (bottom). Values were normalized to vehicle (n = 2). (C) Dose-response curve showing the effect of ACY-738 on acetylation of histone 3 in nuclear fractions of spinal cord lysates of non-Tg mice using a colorimetric HDAC activity kit. The orange band depicts the concentration range of the compound as measured in tissues of treated Tg FUS+/+ mice. (D) Concentrations of ACY-738 in the plasma and brain of Tg FUS+/+ mice measured by mass spectrometry. Half maximal inhibitory concentration (IC50) (n = 4). (PDF 73 kb)
Figure S2. ACY-738 therapy ameliorates ALS disease phenotype both in male and female Tg FUS+/+ mice. (A) Kaplan-Meier survival analysis of vehicle- and ACY-738-treated Tg FUS+/+ mice split up by gender. (B) Overview of median life span of vehicle-treated Tg FUS+/+ mice and ACY-738-treated Tg FUS+/+ mice by gender. n = 23-25, of which 12 males and 11 females in the vehicle-treated group and 10 males and 15 females in the ACY-738-treated group, Log-rank test. (C) Longitudinal follow-up of weight and (D) forelimb grip strength, test of vehicle- and ACY-738-treated Tg FUS+/+ mice. n = 10–14, mice were followed up twice a week, Student’s t-test with Holm Sidak method to correct for multiple testing. **P < 0.01, ***P < 0.001, ****P < 0.0001. Data are presented as means ± SEM. (PDF 47 kb)
Figure S3. Therapy with an ACY-1090, an inactive form of ACY-738, does not have any effect on ALS disease progression in Tg FUS+/+ mice. (A) Chemical structure of ACY-738 (left) and ACY-1090 (right). The active zinc-binding group of ACY-738 and the inactive form of ACY-1090 are marked in red boxes. (B) Kaplan-Meier survival analysis of vehicle- and ACY-1090-treated Tg FUS+/+ mice. (C) Longitudinal follow-up of weight, (D) forelimb grip strength, and (E) compound muscle action potential (CMAP) amplitudes of vehicle- and ACY-1090-treated Tg FUS+/+ mice. n = 8–10, mice were followed up twice a week, Student’s t-test with Holm-Sidak method to correct for multiple testing. Data are presented as means ± SEM. (PDF 50 kb)
Figure S4. ACY-738 does not affect gliosis in the spinal cord of Tg FUS+/+ mice. Immunostaining for astrogliosis and microgliosis in the ventral horn of the lumbar spinal cord of P60 non-Tg controls, vehicle- and ACY-738-treated Tg FUS+/+ mice. GFAP was used as a marker for astrogliosis, CD11b as a marker for microgliosis. Scale bar = 100 μm. (PDF 4055 kb)
Figure S5. Transcriptomics and proteomics analyses show a high degree of similarity. (A) Multidimensional scaling (MDS) of transcriptomics data. (B) Heat map by hierarchical clustering of all differentially expressed genes. (C) Venn diagram representing the overlap of differentially expressed genes between vehicle-treated Tg FUS+/+ mice and non-Tg controls (blue), between ACY-738-treated Tg FUS+/+ mice and non-Tg controls (light orange) and between vehicle- and ACY-738-treated Tg FUS+/+ mice (dark orange). (D) MDS of proteomics data. (E) Heat map by hierarchical clustering of all differentially expressed proteins. (F) Venn diagram representing the overlap of differentially expressed proteins between vehicle-treated Tg FUS+/+ mice and non-Tg controls (blue), between ACY-738-treated Tg FUS+/+ mice and non-Tg controls (light orange) and between vehicle- and ACY-738-treated Tg FUS+/+ mice (dark orange). (G) Venn diagram comparing differential expression in vehicle-treated Tg FUS+/+ mice compared to non-Tg controls on the mRNA- (blue grid) and protein-level (blue lines) of all identified mRNA-protein pairs. (H) Correlation plot of all identified mRNA-protein pairs, comparing the expression values on the mRNA and protein level in vehicle-treated Tg FUS+/+ mice compared to non-Tg controls. (I) Correlation plot of genes that were differentially expressed in both data sets, comparing the expression values on the mRNA and protein level in vehicle-treated Tg FUS+/+ mice compared to non-Tg controls. (J) Venn diagram comparing differential expression in ACY-738-treated Tg FUS+/+ mice compared to non-Tg controls on the mRNA- (orange grid) and protein-level (orange lines) of all identified mRNA-protein pairs. (K) Correlation plot of all identified mRNA-protein pairs, comparing the expression values on the mRNA and protein level in ACY-738-treated Tg FUS+/+ mice compared to non-Tg controls. (L) Correlation plot of genes that were differentially expressed in both datasets, comparing the expression values on the mRNA and protein level in ACY-738-treated Tg FUS+/+ mice compared to non-Tg controls. (PDF 225 kb)
Figure S6. The expression of metabolic genes is partially restored by ACY-738 therapy. Heatmap of expression changes of a subset of metabolic genes at the mRNA and protein level based on transcriptomics and proteomics experiments. Hexokinase 2 (Hk2), pyruvate dehydrogenase kinase 4 (Pdk4), Acyl-CoA synthetase long-chain family member 6 (Acsl6), acyl-CoA dehydrogenase family member 11 (Acad11), 3-oxoacid CoA-transferase (Oxct1), 7-Dehydrocholesterol reductase (7-Dhcr), squalene epoxidase (Sqle), Elongation of very long chain fatty acids protein 7 (Elovl7), 1-acylglycerol-3-phosphate O-acyltransferase 4 (Agpat4), Apolipoprotein D (Apod), Apolipoprotein E (Apoe), Fatty acid binding protein 4 (Fabp4). (PDF 62 kb)
About this article
Cite this article
Rossaert, E., Pollari, E., Jaspers, T. et al. Restoration of histone acetylation ameliorates disease and metabolic abnormalities in a FUS mouse model. acta neuropathol commun 7, 107 (2019). https://doi.org/10.1186/s40478-019-0750-2
- Amyotrophic lateral sclerosis
- Histone deacetylases
- HDAC inhibitors