microRNA-128a dysregulation in transgenic Huntington’s disease monkeys
- Jannet Kocerha†1, 2, 3,
- Yan Xu†1, 2,
- Melinda S Prucha1, 2,
- Dongming Zhao1, 2 and
- Anthony WS Chan1, 2Email author
© Kocerha et al.; licensee BioMed Central Ltd. 2014
Received: 24 March 2014
Accepted: 3 June 2014
Published: 13 June 2014
Huntington’s Disease (HD) is a progressive neurodegenerative disorder with a single causal mutation in the Huntingtin (HTT) gene. MicroRNAs (miRNAs) have recently been implicated as epigenetic regulators of neurological disorders, however, their role in HD pathogenesis is not well defined. Here we study transgenic HD monkeys (HD monkeys) to examine miRNA dysregulation in a primate model of the disease.
In this report, 11 miRNAs were found to be significantly associated (P value < 0.05) with HD in the frontal cortex of the HD monkeys. We further focused on one of those candidates, miR-128a, due to the corresponding disruption in humans and mice with HD as well as its intriguing lists of gene targets. miR-128a was downregulated in our HD monkey model by the time of birth. We then confirmed that miR-128a was also downregulated in the brains of pre-symptomatic and post-symptomatic HD patients. Additionally, our studies confirmed a panel of canonical HD signaling genes regulated by miR-128a, including HTT and Huntingtin Interaction Protein 1 (HIP1).
Our studies found that miR-128a may play a critical role in HD and could be a viable candidate as a therapeutic or biomarker of the disease.
KeywordsmicroRNAs Noncoding RNAs Huntington’s disease Brain miR-128a
Over the past decade, the microRNA (miRNA) class of noncoding RNAs (ncRNAs) has consistently been implicated in the neurogenesis, neurodegenerative, and synaptic plasticity functions of the central nervous system (CNS) [1–9]. Modulation of miRNA activity has been associated with a broad scope of CNS disorders, including schizophrenia, autism, Fragile X, addiction, Parkinson’s Disease (PD), Alzheimer’s Disease (AD), Frontotemporal Dementia (FTD), and Huntington’s Disease (HD) [10–17]. Indeed, the role of miRNA dysregulation in neurological diseases has come under increasingly intense study during recent years in the quest for novel therapeutic strategies [9, 18].
HD is characterized by progressive brain atrophy, particularly in the striatum and hippocampus, with associated deficits in cognitive, behavioral, and motor functions . Although the causative factor for HD is monogenic and results from expansion in the polyglutamine (polyQ) region of the Huntingtin (HTT) gene, there is wide variability in age of onset, polyQ length, and degree of symptoms [20, 21]. Published reports indicate that epigenetic factors, such as ncRNA regulation, work in union with the genetic anomalies to provoke pathogenic outcomes in HD [22–28].
MiRNA dysregulation has been reported in HD patients, transgenic HD mice, and in vitro experimental models [22–28]. Here we examine the miRNA expression profile of fetal and newborn frontal cortex from HD monkeys, with corresponding neuropathological analysis from a subset of those monkeys. The HD monkeys examined in this study carry the exon 1 of human HTT gene with an expanded polyQ tract of 27Q – 122Q (Additional file 1: Table S1), a range well above the polyQ repeat of 10-11Q in wild-type (WT) rhesus macaque [29, 30]. We identified a significant dysregulation of 11 miRNAs in the HD monkeys and a correlation of their gene targets with the HD canonical signaling pathway. Interestingly, through bioinformatic analysis and subsequent in vitro studies, miR-128a was found to regulate the 3’-untranslated regions (3’ UTRs) of the HTT and Huntingtin Interacting Protein 1 (HIP1) genes. Additionally, analysis of previously reported datasets revealed that miR-128a was also downregulated in the brain tissue of HD mice and humans [22–25]. We expand on these datasets to show that miR-128a is downregulated in a cohort of both pre-symptomatic and post-symptomatic HD patients.
Overall, we report miRNA dysregulation in the brains of HD monkeys, with parallel miRNA dysregulation in human patients. We find that neuronally-enriched miRNAs may play a fundamental role in HD pathogenesis. Additionally, we show that the miRNAs implicated in HD may regulate a significant network of genes within the HD canonical signaling pathway, providing a new paradigm approach for a disease with complex molecular dysregulation.
Genotyping and mRNA expression analysis of HD monkeys
In addition to confirming the genotype of each HD monkey, the expression of HTT mRNA in cortical tissues was also measured. All HD monkeys displayed significantly higher levels of HTT transcript levels than the controls, with HD7 displaying the highest expression (Figure 1B). Primers for the mRNA analysis were not designed to distinguish between the mutant and wild-type HTT transcripts, therefore, the relative expression of mHTT in the HD monkeys was determined by comparing with the endogenous transcript levels in the controls.
Expression of mHTT aggregates in HD monkey frontal cortex
Expression of activated caspase-3 and glial fibrillary acidic protein (GFAP) in HD monkey frontal cortex
miRNA array profiling
496 non-control transcripts (from rhesus macaque) were log2-transformed and normalized. Average probe intensities were filtered to generate a list of 352 rhesus miRNA probes with a fluorescence intensity exceeding threshold levels in at least 10% of the samples. Of the 352 detectable probes, 11 were significantly dysregulated in the HD monkeys with unpaired and unequal (Welch) t-test using Agilent GeneSpringGX 10.0 with condition P < 1 (Figure 1C and Additional file 3). Of the 11 miRNAs significantly (P < 0.05) correlated with HD pathogenesis, 9 were downregulated while 2 were upregulated compared to controls (Figure 1C).
Target analysis of dysregulated miRNAs in HD pathogenesis
We identified the predicted mRNA targets using TargetScan for all 11 of the significantly altered miRNAs in the HD monkeys. The list of predicted mRNA targets for each miRNA was then analyzed by Ingenuity Software for pathway associations. Ingenuity analysis revealed significant pathway associations for all of the 11 miRNAs, including CREB signaling in Neurons, Chemokine Signaling, IGF-1 Signaling, and Synaptic Long Term Depression. Furthermore, when examining for shared pathways for the 11 miRNAs, we discovered that 3 pathways were associated with 7 of the miRNAs, 12 pathways associated with 6 of the miRNAs, and 13 pathways associated with 5 of the miRNAs (Additional file 4: Table S3). Notably, the HD canonical signaling pathway was associated with the mRNA targets for 5 of the 11 miRNAs.For 4 of the 5 miRNAs with significant target association to the HD canonical pathway, we confirmed their expression by qPCR in the monkey cortical tissues (miR-940 did not have commercially available Taqman primers for qPCR) (Figure 1D). For the qPCR verification, we focused on the monkeys (HD4, HD7, and HD8) that had corresponding pathology. Quantitation by qPCR revealed a significant downregulation of miR-128a in the brains of the HD monkeys (Figure 1D), consistent with our microarray results. Additionally, miR-128a was also downregulated in the brains of pre-symptomatic and post-symptomatic HD patients (Figure 1E) when compared to controls (p < 0.05).
miR-128a regulates 3’-UTR activity of genes with known roles in HD canonical pathway
In this study, we examine ncRNA regulation in HD monkeys and identified 11 significant disease-associated miRNAs. This is the first study which analyzes miRNA regulation in a transgenic primate model of a human disease, with a goal of helping to bridge or expand on previous results in HD rodents and human patients. The HD monkeys offer a unique resource to identify pathogenic ncRNA mechanisms that are either conserved from lower vertebrates to humans or are primate specific. For example, miR-451, one of the 11 miRNAs we found modulated in the HD monkeys, is also upregulated in HD patients . However, miR-451 does not appear to be disrupted in HD mice models, suggesting the involvement of this miRNA in disease progression may be restricted to primates. On the contrary, we found miR-128a downregulated in the HD monkeys and human patients, and there are published reports also showing its corresponding downregulation in at least 2 distinct HD mice models . Additionally, our human data for miR-128a corresponds with other reported datasets in HD patients . The miR-128a results, however, were not previously highlighted in the previous publications.
Although it is important to identify both primate-specific and conserved molecular mechanisms in disease, we focused on miR-128a in this study due to the compelling list of genes it is predicted to target in HD, including; SP1, HIP1 as well as HTT itself. Our in vitro luciferase reporter assays revealed the binding sites for miR-128a in HIP1, SP1, and HTT are all regulated by miR-128a compared to stringent site-specific mutant controls. Although we experimentally examined a subset of the predicted miR-128a gene targets, there are likely more genes which miR-128a regulates within the HD pathway. Furthermore, a few of the other 11 miRNAs we identified to be associated with HD in this study are also likely to regulate genes within the HD pathway. A future point of interest could examine whether a distinct group of miRNAs work together as a network to govern the HD genes. MiR-940, one of the 11 HD-associated miRNAs in the transgenic monkeys, is also predicted to target HTT. Correspondingly, although we examined miR-128a regulation of the SP1 transcription factor, other miRNAS identified in this study also bioinformatically bind to SP1 (such as miR-320, miR-133, and miR-181). Overall, this report points to a collective miRNA targeting of HTT or genes which regulate HTT (i.e. SP1, HIP1, etc.). Furthermore, several of the dysregulated miRNAs in the HD monkeys are also predicted to target the insulin like growth factor −1 gene (IGF1) or its receptor (IGF1-R), including; miR-128a, miR940, miR-320, and miR133. It has previously been shown that IGF1 signaling is linked to HD and other neurodegenerative diseases [31–33]. Future studies of these other miRNAs and their target genes, along with miR-128a, could help develop a more complete understanding of ncRNA regulation in HD.
miR-128a is neuronally-enriched [34, 35] and one of the most abundantly expressed miRNAs in human and mouse brain . A recent report indicated a principal role for miR-128a in motor activity and neuronal excitability, and its downregulation can provoke epileptic seizures . HD is partly characterized by deficits in motor activity, leading to significant impact on associated movements and possible development of seizures in patients [37, 38]. Tan et al. showed that the seizures in mice with deficient miR-128a expression can be alleviated with treatment of an anti-convulsant drug . Moreover, the authors showed that the ablation of miR-128a specifically in the dopamine 1 receptor-expressing neurons (D1-neurons) leads to juvenile hyperactivity and seizures , consistent with other reports implicating D1-neurons in the symptoms of HD .
Several studies have also linked miR-128a with tumor repression and apoptosis [40, 41]. Interestingly, apoptosis related signaling has consistently been implicated in HD pathogenesis [42–45]. One possibility is that the polyQ expansion in HTT of HD patients signals for apoptosis and neurodegenerative cascades through the regulation of miR-128a. Indeed, we found caspase-3, a component of the apoptosis pathway [44, 46, 47], was dysregulated in HD monkeys (Figure 2). It has also been reported that miR-128a is involved in the regulation of neuronal differentiation and survivability, including through the targeting of transcription factors and neurotrophins [48, 49]. Overexpressing miR-128a represses the levels of the neurotrophin-3 receptor (NTRK3) gene [48, 49] and the transcription factor E2F3A . Moreover, it has also been shown that miR-128a can target genes involved in neuronal differentiation and viability through the regulation of nonsense-mediated decay (NMD) [28, 51, 52]. NMD is an RNA surveillance pathway which can provoke the degradation of a subset of RNA transcripts. It has been suggested that increased expression of miR-128a can modulate the NMD pathway, resulting in elevated levels of important neuronal proteins [28, 51, 52].
Overall, our results suggest that miRNAs, and more specifically miR-128a, may play a pivotal role in HD pathogenesis. Epigenetic regulation of HD by miRNAs could provide a viable target for future therapeutics, particularly when one miRNA, such as miR-128a, regulates multiple genes within the HD signaling pathway.
HD monkeys and preparation of brain tissues
Brain tissues were collected from 11 monkeys (HD1-HD8 and C1-C3) (Additional file 1: Table S1). C2 and HD5 were miscarried at 3 months of gestation and C1, C3, HD1, HD2, HD3, HD4, and HD6 were miscarried at 4 months of gestation. HD7 and HD8 were delivered at full term and euthanized on the first day after birth because of severe involuntary movement and swallowing or respiratory difficulty, which was previously reported as rHD4 and rHD5, respectively . C1 and HD4 were twins, and HD7 and HD8 were also twins. C1-C3 carried green fluorescent protein (GFP) transgene, and HD1-HD8 carried the mHTT transgene (exon 1 driven by human polyubiquitin promoter with expanded polyQ) and GFP gene . Brain samples were prepared as soon as miscarried fetuses were retrieved or immediately after euthanasia. One hemisphere was post-fixed in 4% paraformaldehyde (PFA) and processed as described in the following section while the contralateral hemisphere was immediately dissected into small pieces (~0.5 cm3) according to distinct brain regions. The dissected brain regions were snap frozen in liquid nitrogen and stored at −80°C until analyzed. Sequence and copy analysis of all monkeys (Additional file 1: Table S1) was carried out according to previously published protocols .
Post-mortem brain tissues were fixed in 4% paraformaldehyde overnight and then saturated in 30% sucrose solution at 4°C. The brain was then cryo-sectioned coronally to 50 μm using a cryostat and preserved in cryoprotectant solution at −20°C. Because most monkeys were miscarried and their brains were immature and soft, some of the monkey brains were not adequate for sectioning and subsequent immunohistochemical studies. Thus, only sections of frontal cortex from C1, C3, HD4, HD7 and HD8 were used for neuropathological study. For DAB immunostaining, sections were incubated with 0.3% hydrogen peroxide for 15 minutes, blocked for 1 hour at room temperature, and incubated with primary antibody (mEM48 1:1000, caspase-3 1:1000, or GFAP 1:1000) at 4°C overnight. After thorough wash with DPBS, brain sections were incubated with avidin–biotin using the Vectastain Elite ABC kit (Vector Laboratories), and immediately stained with 3, 3’-diaminobezidine (DAB; Vector Laboratories) for 30–40 seconds until optimal signal was reached. The sections immunostained with caspase-3 were restained in hematoxylin (Richard-Allan scientific) for nuclear staining. Brain sections were then mounted on slides and examined by Olympus BX51 microscope.
Frontal cortex tissues from five individual monkeys (C1, C3, HD4, HD7 and HD8) were homogenized in RIPA buffer with protease cocktail inhibitor (Sigma). The tissue lysates were sonicated for 10 seconds and then centrifuged for 4 minutes at 1000 rpm at 4°C to pellet cellular debris. Protein concentrations were determined by protein assay. Equal amount (30–40 μg) of protein extract with loading dye was boiled for 5–10 minutes before loading into 9% (mEM8 and GFAP) polyacrylamide gels. After electrophoresis, proteins were transferred onto PVDF membrane (Bio-Rad) followed by blocking in 5% skim milk for 30 minutes. The membrane was incubated with the primary antibodies mEM48 (1:50 dilution) or GFAP (1:1000) overnight at 4°C, followed by the secondary peroxidase-conjugated antibodies for 1 h. Protein bands were detected with an Amersham ECL kit (PerkinElmer). Membrane was then labeled with γ-tubulin (1:2000) as internal control.
Primary antibodies used in this study are as follows: 1) mouse monoclonal antibody (mEM48) against the N-terminal region of human HTT with expanded polyQ was a gift from Dr. XJ Li lab ; 2) rabbit antibody against the activated form of caspase-3 (cleaved caspase-3 (Asp 175) antibody) was from Cell Signaling; 3) mouse anti-Glial Fibrillary Acidic Protein (GFAP) monoclonal antibody was purchased from Millipore; 4) the mouse anti-gamma-tubulin antibody was purchased from Sigma. Secondary antibodies for immunohistochemistry were biotinylated goat anti-rabbit IgG (caspase-3 immunohistochemistry) or biotinylated horse anti-mouse IgG (mEM48 and GFAP immunohistochemistry) from Vector Labs (Burlingame, CA). Secondary antibodies for Western blotting were peroxidase-conjugated donkey anti-rabbit or anti-mouse IgG from Jackson Immunoresearch Labs.
Qualitative analysis of caspase-3 and mEM48
Immunostained sections were examined using a Leica DMRB microscope, photographed at a magnification of 10–100 (camera: Leica DC500; Varshaw Scientific, Atlanta, GA, USA) and captured with computer software (SPOT Basic). The percentage of caspase-3 positive neurons was calculated based on number of positive cells per total nuclei. Five randomly captured images at 40× magnification were used to determine the number of caspase-3 positive and total number of nuclei for each monkey. Brain sections were labeled with mEM48 and used to determine the percentage of the number of EM48 (mHTT) positive cells with intranuclear inclusions. Eight randomly captured images at 20× magnification were used to determine the number of total number of EM48 positive cells with intranuclear inclusion for each monkey. For quantitation of protein expression by densitometry with Western blot, bands were captured and the intensity of positive bands was quantified with ChemiDox (BIORAD Inc.). All data are presented as mean ± standard error of the mean (SEM), and analyzed by one-way ANOVA using Graphpad Prism software, and followed by Newman-Keuls method for comparisons between groups.
mHTT transgene characterization
The monkeys were genotyped and estimated copy number of the mHTT transgene were obtained following previous published protocols . Additionally, we detected the mutant transgene by gel electrophoresis after primer-specific PCR amplification. The genomic DNA (gDNA) was extracted from frontal cortex tissue using the Wizard Genomic DNA Purification Kit from Promega following the manufacturer’s protocol. For genomic amplification of the HTT transgene, 60 ng of gDNA for the 8 HD transgenics and 3 GFP controls was analyzed by PCR using SsoFast EvaGreen Supermix from BioRad at a 60.5°C annealing temperature. Primers were designed to specifically amplify the junction of the human polyubiquitin C promoter and 5’ region of the exon1 of the mHTT transgene (see Additional file 2: Table S2). qPCR was performed using the CFX96 BioRad CyclerAll amplified products were analyzed by 1.5% agarose gel and subsequently sequenced for transgene verification.
qPCR analysis of HTT mRNA in HD monkeys
Quantitation by qPCR was engaged to compare HTT mRNA levels between the HD and control monkeys. Total RNA from the cortical tissue was isolated using Trizol and subsequently treated with DNase to remove residual genomic DNA contamination. 200 ng of purified RNA was reverse-transcribed to cDNA (Applied Biosystems). To quantitate the mRNA levels of HTT, we custom designed Taqman assays (ABI) specific for the gene (see Additional file 2: Table S2). HTT transcript was amplified from the cDNA by qPCR using the Taqman assay with 1X final concentration of Taqman Universal PCR Master Mix (ABI). All data were normalized to 18S rRNA levels. The integrity of all RNA analyzed in this study was assessed by both a Bioanalyzer and RNA gel electrophoresis. All RNA was determined to be intact by the presence of distinct 28SRNA and 18SRNA ribosomal bands and a greater intensity of the 28SrRNA compared to the 18SrRNA (see Additional file 5 for RNA gel).
miRNA array profiling
Total RNA was isolated from the frontal cortex of all 3 control and all 8 HD transgenic Rhesus monkeys using Trizol reagent (Invitrogen) according to manufacturer’s recommendations. RNA samples were sent to Ocean Ridge Biosciences for analysis using custom multi-species microarrays containing 496 probes covering 505 mature miRNAs (rhesus) present in the Sanger 15.0 miRBase database. The microarrays were produced by Microarrays, Inc. (Huntsville, Alabama) and consisted of epoxide glass substrates with each probe spotted in triplicate. Quality of each total RNA sample was assessed using UV spectrophotometry and agarose gel electrophoresis. Low molecular weight (LMW) RNA (~0-200 nucleotides) was purified from total RNA by size fractionation and 3’-end labeled with Oyster-550 fluorescent dye using the Flash Tag RNA Labeling Kit (Genisphere Inc., Hatfield, PA). Labeled LMW RNA samples were hybridized to the arrays according to conditions recommended in the Flash Tag RNA labeling Kit manual. The microarrays were scanned on an Axon Genepix 4000B scanner and data were extracted from images using GenePix V4.1 software.
miRNA qPCR quantitation of in monkey and human brain
Dysregulated miRNAs which had predicted targets with significant HD pathway association, as determined by Ingenuity Pathways Analysis (p-value < 0.05), were subjected to further validation by qPCR. Taqman miRNA assays (ABI) were used to quantify levels of the selected candidates. The assay utilized miRNA-specific primers for both cDNA synthesis and qPCR, and all reactions were normalized to RNU48 as a small RNA endogenous control. Additionally, total RNA was prepared by Trizol-chloroform extractions from human samples for quantitation of miR-128a by qPCR. Human HD brain tissues were provided by Emory Alzheimer’s Disease Research Center and the Emory Neuroscience NINDS Core Facilities (ENNCF) Neuropathology Core Service at Emory University. The use of human tissues was followed and compiled with NIH guideline. All miR-128a qPCR values in the human tissues were normalized to the small RNA endogenous control, RNU6B.
TargetScan and Ingenuity pathway analysis of miRNA candidates
The predicted mRNA targets for all of the 11 miRNAs significantly dysregulated with HD by microarray (P value < 0.05) in our study were identified using the TargetScan prediction program. The predicted mRNA targets for each were then subjected to pathway analysis using the Ingenuity software to identify potential association with the HD signaling pathway (P value < 0.05).
Luciferase reporter assays
3’-UTR sequence information was obtained for the rhesus genes HIP-1, HTT, SP-1 and GRM5 using TargetScan (Release 5.2: June 2012), UCSC Genome Browser, and NCBI databases. Sense and anti-sense oligos spanning the predicted miR-128a binding sites in each gene’s 3’UTR were custom ordered (Eurofin Operon) (see Additional file 2: Table S2 for oligo sequences). Additionally, sense and anti-sense oligos with point mutations in 4 of the 6 nucleotides of the seed region for the miR-128a binding sites were generated for use as mutant (MUT) controls. Sense and anti-sense strands for each site were annealed and ligated into the pmirGLO Dual-Luciferase miRNA Target Expression Vector (Promega). Constructs were transformed into High Efficiency JM109 Competent Cells (Promega). Annealing, ligation, and transformations were performed according to manufacturer’s recommendations. Selected clones were mini-prepped using a QIAGEN Plasmid mini-prep kit, and inserts/sequences were confirmed using restriction digests and sequencing.
HEK-293FT cells were used for 3’UTR Luciferase reporter transfections. Lipofectamine 2000 (Invitrogen) was used to transfect plasmids/miR-128a into 293FT cells according to manufacturer’s recommendations in 96-well plates (coated with 0.1% gelatin, 14,000 cells/well). Each well was transfected with 40 ng of plasmid alone (controls), or in combination with 10 nM pre-miR-128a (Ambion, catalog AM17100) or Negative Control #2 (Ambion). Following transfection, cells were grown for 24 hours at 37ºC and luciferase levels were quantified using the Dual-Glo Luciferase Assay (Promega) according to vendor instructions; measurements were read using a Synergy H4 plate reader (BioTek Instruments, Inc.). All Firefly luciferase data were normalized to Renilla luciferase levels; experiments were run in quadruplicate and individual experiments were replicated at least once.
All protocols involving animal care and handling were approved by Emory University’s IACUC. All experimental researches described in this study were approved by the Emory environmental health and biosafety committee EHSO. Study using human tissues was complied with NIH guideline. Human HD brain tissues were provided by Emory Alzheimer’s Disease Research Center and the Emory Neuroscience NINDS Core Facilities (ENNCF) Neuropathology Core Service at Emory University. We thank Yerkes National Primate Research Center (YNPRC) veterinarian and animal care staff for providing outstanding services. We also thank all former and current members of the Chan’s lab who have contributed immensely to the development of HD monkeys. The YNPRC is supported by the base grant P51RR165 awarded by the Animal Resources Program of the NIH. This work was supported by grants awarded to AWSC by ORIP/NIH (RR018827) and the American Recovery and Reinvestment Act (ARRA) Fund).
- Bartel DP: MicroRNAs: target recognition and regulatory functions. Cell. 2009, 136: 215-233. 10.1016/j.cell.2009.01.002.PubMedPubMed CentralView ArticleGoogle Scholar
- Beveridge NJ, Cairns MJ: MicroRNA dysregulation in schizophrenia. Neurobiol Dis. 2012, 46: 263-271. 10.1016/j.nbd.2011.12.029.PubMedView ArticleGoogle Scholar
- Shi Y, Zhao X, Hsieh J, Wichterle H, Impey S, Banerjee S, Neveu P, Kosik KS: MicroRNA regulation of neural stem cells and neurogenesis. J Neurosci. 2010, 30: 14931-14936. 10.1523/JNEUROSCI.4280-10.2010.PubMedPubMed CentralView ArticleGoogle Scholar
- Gao FB: Context-dependent functions of specific microRNAs in neuronal development. Neural Dev. 2010, 5: 25-10.1186/1749-8104-5-25.PubMedPubMed CentralView ArticleGoogle Scholar
- Fiore R, Khudayberdiev S, Saba R, Schratt G: MicroRNA function in the nervous system. Prog Mol Biol Transl Sci. 2011, 102: 47-100.PubMedView ArticleGoogle Scholar
- Vo NK, Cambronne XA, Goodman RH: MicroRNA pathways in neural development and plasticity. Curr Opin Neurobiol. 2010, 20: 457-465. 10.1016/j.conb.2010.04.002.PubMedView ArticleGoogle Scholar
- Li X, Jin P: Roles of small regulatory RNAs in determining neuronal identity. Nat Rev Neurosci. 2010, 11: 329-338. 10.1038/nrn2739.PubMedView ArticleGoogle Scholar
- Im HI, Kenny PJ: MicroRNAs in neuronal function and dysfunction. Trends Neurosci. 2012, 35: 325-334. 10.1016/j.tins.2012.01.004.PubMedPubMed CentralView ArticleGoogle Scholar
- Kocerha J, Kauppinen S, Wahlestedt C: microRNAs in CNS disorders. Neuromolecular Med. 2009, 11: 162-172. 10.1007/s12017-009-8066-1.PubMedView ArticleGoogle Scholar
- Beveridge NJ, Gardiner E, Carroll AP, Tooney PA, Cairns MJ: Schizophrenia is associated with an increase in cortical microRNA biogenesis. Mol Psychiatry. 2010, 15: 1176-1189. 10.1038/mp.2009.84.PubMedPubMed CentralView ArticleGoogle Scholar
- Kocerha J, Faghihi MA, Lopez-Toledano MA, Huang J, Ramsey AJ, Caron MG, Sales N, Willoughby D, Elmen J, Hansen HF, Orum H, Kauppinen S, Kenny PJ, Wahlestedt C: MicroRNA-219 modulates NMDA receptor-mediated neurobehavioral dysfunction. Proc Natl Acad Sci U S A. 2009, 106: 3507-3512. 10.1073/pnas.0805854106.PubMedPubMed CentralView ArticleGoogle Scholar
- Kocerha J, Kouri N, Baker M, Finch N, DeJesus-Hernandez M, Gonzalez J, Chidamparam K, Josephs KA, Boeve BF, Graff-Radford NR, Crook J, Dickson DW, Rademakers R: Altered microRNA expression in frontotemporal lobar degeneration with TDP-43 pathology caused by progranulin mutations. BMC Genomics. 2011, 12: 527-10.1186/1471-2164-12-527.PubMedPubMed CentralView ArticleGoogle Scholar
- Hollander JA, Im HI, Amelio AL, Kocerha J, Bali P, Lu Q, Willoughby D, Wahlestedt C, Conkright MD, Kenny PJ: Striatal microRNA controls cocaine intake through CREB signalling. Nature. 2010, 466: 197-202. 10.1038/nature09202.PubMedPubMed CentralView ArticleGoogle Scholar
- Mouradian MM: MicroRNAs in Parkinson’s disease. Neurobiol Dis. 2012, 46: 279-284. 10.1016/j.nbd.2011.12.046.PubMedView ArticleGoogle Scholar
- Hebert SS, Horre K, Nicolai L, Papadopoulou AS, Mandemakers W, Silahtaroglu AN, Kauppinen S, Delacourte A, De Strooper B: Loss of microRNA cluster miR-29a/b-1 in sporadic Alzheimer’s disease correlates with increased BACE1/beta-secretase expression. Proc Natl Acad Sci U S A. 2008, 105: 6415-6420. 10.1073/pnas.0710263105.PubMedPubMed CentralView ArticleGoogle Scholar
- Jin P, Alisch RS, Warren ST: RNA and microRNAs in fragile X mental retardation. Nat Cell Biol. 2004, 6: 1048-1053. 10.1038/ncb1104-1048.PubMedView ArticleGoogle Scholar
- Mellios N, Sur M: The Emerging Role of microRNAs in Schizophrenia and Autism Spectrum Disorders. Front Psychiatry. 2012, 3: 39-PubMedPubMed CentralView ArticleGoogle Scholar
- Chan AW, Kocerha J: The Path to microRNA Therapeutics in Psychiatric and Neurodegenerative Disorders. Front Genet. 2012, 3: 82-PubMedPubMed CentralView ArticleGoogle Scholar
- Ross CA, Tabrizi SJ: Huntington’s disease: from molecular pathogenesis to clinical treatment. Lancet Neurol. 2011, 10: 83-98. 10.1016/S1474-4422(10)70245-3.PubMedView ArticleGoogle Scholar
- Cajavec B, Herzel H, Bernard S: Death of neuronal clusters contributes to variance of age at onset in Huntington’s disease. Neurogenetics. 2006, 7: 21-25. 10.1007/s10048-005-0025-x.PubMedView ArticleGoogle Scholar
- Squitieri F, Frati L, Ciarmiello A, Lastoria S, Quarrell O: Juvenile Huntington’s disease: does a dosage-effect pathogenic mechanism differ from the classical adult disease?. Mech Ageing Dev. 2006, 127: 208-212. 10.1016/j.mad.2005.09.012.PubMedView ArticleGoogle Scholar
- Gaughwin PM, Ciesla M, Lahiri N, Tabrizi SJ, Brundin P, Bjorkqvist M: Hsa-miR-34b is a plasma-stable microRNA that is elevated in pre-manifest Huntington’s disease. Hum Mol Genet. 2011, 20: 2225-2237. 10.1093/hmg/ddr111.PubMedView ArticleGoogle Scholar
- Lee ST, Chu K, Im WS, Yoon HJ, Im JY, Park JE, Park KH, Jung KH, Lee SK, Kim M, Roh JK: Altered microRNA regulation in Huntington’s disease models. Exp Neurol. 2011, 227: 172-179. 10.1016/j.expneurol.2010.10.012.PubMedView ArticleGoogle Scholar
- Marti E, Pantano L, Banez-Coronel M, Llorens F, Minones-Moyano E, Porta S, Sumoy L, Ferrer I, Estivill X: A myriad of miRNA variants in control and Huntington’s disease brain regions detected by massively parallel sequencing. Nucleic Acids Res. 2010, 38: 7219-7235. 10.1093/nar/gkq575.PubMedPubMed CentralView ArticleGoogle Scholar
- Packer AN, Xing Y, Harper SQ, Jones L, Davidson BL: The bifunctional microRNA miR-9/miR-9* regulates REST and CoREST and is downregulated in Huntington’s disease. J Neurosci. 2008, 28: 14341-14346. 10.1523/JNEUROSCI.2390-08.2008.PubMedPubMed CentralView ArticleGoogle Scholar
- Jovicic A, Zaldivar Jolissaint JF, Moser R, Silva Santos Mde F, Luthi-Carter R: MicroRNA-22 (miR-22) overexpression is neuroprotective via general anti-apoptotic effects and may also target specific Huntington’s disease-related mechanisms. PLoS One. 2013, 8: e54222-10.1371/journal.pone.0054222.PubMedPubMed CentralView ArticleGoogle Scholar
- Soldati C, Bithell A, Johnston C, Wong KY, Stanton LW, Buckley NJ: Dysregulation of REST-regulated coding and non-coding RNAs in a cellular model of Huntington’s disease. J Neurochem. 2013, 124: 418-430. 10.1111/jnc.12090.PubMedView ArticleGoogle Scholar
- Jin J, Cheng Y, Zhang Y, Wood W, Peng Q, Hutchison E, Mattson MP, Becker KG, Duan W: Interrogation of brain miRNA and mRNA expression profiles reveals a molecular regulatory network that is perturbed by mutant huntingtin. J Neurochem. 2012, 123: 477-490. 10.1111/j.1471-4159.2012.07925.x.PubMedPubMed CentralView ArticleGoogle Scholar
- Kocerha J, Liu Y, Willoughby D, Chidamparam K, Benito J, Nelson K, Xu Y, Chi T, Engelhardt H, Moran S, Yang SH, Li SH, Li XJ, Larkin K, Neumann A, Banta H, Yang JJ, Chan AW: Longitudinal transcriptomic dysregulation in the peripheral blood of transgenic Huntington’s disease monkeys. BMC Neurosci. 2013, 14: 88-10.1186/1471-2202-14-88.PubMedPubMed CentralView ArticleGoogle Scholar
- Putkhao K, Kocerha J, Cho IK, Yang J, Parnpai R, Chan AW: Pathogenic cellular phenotypes are germline transmissible in a transgenic primate model of Huntington’s disease. Stem Cells Dev. 2013, 22: 1198-1205. 10.1089/scd.2012.0469.PubMedPubMed CentralView ArticleGoogle Scholar
- Pouladi MA, Xie Y, Skotte NH, Ehrnhoefer DE, Graham RK, Kim JE, Bissada N, Yang XW, Paganetti P, Friedlander RM, Leavitt BR, Hayden MR: Full-length huntingtin levels modulate body weight by influencing insulin-like growth factor 1 expression. Hum Mol Genet. 2010, 19: 1528-1538. 10.1093/hmg/ddq026.PubMedPubMed CentralView ArticleGoogle Scholar
- Sadagurski M, Cheng Z, Rozzo A, Palazzolo I, Kelley GR, Dong X, Krainc D, White MF: IRS2 increases mitochondrial dysfunction and oxidative stress in a mouse model of Huntington disease. J Clin Invest. 2011, 121: 4070-4081. 10.1172/JCI46305.PubMedPubMed CentralView ArticleGoogle Scholar
- Cohen E, Dillin A: The insulin paradox: aging, proteotoxicity and neurodegeneration. Nat Rev Neurosci. 2008, 9: 759-767. 10.1038/nrn2474.PubMedPubMed CentralView ArticleGoogle Scholar
- Evangelisti C, Florian MC, Massimi I, Dominici C, Giannini G, Galardi S, Bue MC, Massalini S, McDowell HP, Messi E, Gulino A, Farace MG, Ciafrè SA: MiR-128 up-regulation inhibits Reelin and DCX expression and reduces neuroblastoma cell motility and invasiveness. FASEB J. 2009, 23: 4276-4287. 10.1096/fj.09-134965.PubMedView ArticleGoogle Scholar
- Papagiannakopoulos T, Friedmann-Morvinski D, Neveu P, Dugas JC, Gill RM, Huillard E, Liu C, Zong H, Rowitch DH, Barres BA, Verma IM, Kosik KS: Pro-neural miR-128 is a glioma tumor suppressor that targets mitogenic kinases. Oncogene. 2012, 31: 1884-1895. 10.1038/onc.2011.380.PubMedPubMed CentralView ArticleGoogle Scholar
- Tan CL, Plotkin JL, Veno MT, Von Schimmelmann M, Feinberg P, Mann S, Handler A, Kjems J, Surmeier DJ, O’Carroll D, Greengard P, Schaefer A: MicroRNA-128 governs neuronal excitability and motor behavior in mice. Science. 2013, 342: 1254-1258. 10.1126/science.1244193.PubMedPubMed CentralView ArticleGoogle Scholar
- Cloud LJ, Rosenblatt A, Margolis RL, Ross CA, Pillai JA, Corey-Bloom J, Tully HM, Bird T, Panegyres PK, Nichter CA, Higgins DS, Helmers SL, Factor SA, Jones R, Testa CM: Seizures in juvenile Huntington’s disease: frequency and characterization in a multicenter cohort. Mov Disord. 2012, 27: 1797-1800. 10.1002/mds.25237.PubMedView ArticleGoogle Scholar
- Franciosi S, Shim Y, Lau M, Hayden MR, Leavitt BR: A systematic review and meta-analysis of clinical variables used in Huntington disease research. Mov Disord. 2013, 28: 1987-1994. 10.1002/mds.25663.PubMedView ArticleGoogle Scholar
- Gantois I, Fang K, Jiang L, Babovic D, Lawrence AJ, Ferreri V, Teper Y, Jupp B, Ziebell J, Morganti-Kossmann CM, O'Brien TJ, Nally R, Schütz G, Waddington J, Egan GF, Drago J: Ablation of D1 dopamine receptor-expressing cells generates mice with seizures, dystonia, hyperactivity, and impaired oral behavior. Proc Natl Acad Sci U S A. 2007, 104: 4182-4187. 10.1073/pnas.0611625104.PubMedPubMed CentralView ArticleGoogle Scholar
- Adlakha YK, Saini N: miR-128 exerts pro-apoptotic effect in a p53 transcription-dependent and -independent manner via PUMA-Bak axis. Cell Death Dis. 2013, 4: e542-10.1038/cddis.2013.46.PubMedPubMed CentralView ArticleGoogle Scholar
- Adlakha YK, Saini N: MicroRNA-128 downregulates Bax and induces apoptosis in human embryonic kidney cells. Cell Mol Life Sci. 2011, 68: 1415-1428. 10.1007/s00018-010-0528-y.PubMedView ArticleGoogle Scholar
- Almeida S, Sarmento-Ribeiro AB, Januario C, Rego AC, Oliveira CR: Evidence of apoptosis and mitochondrial abnormalities in peripheral blood cells of Huntington’s disease patients. Biochem Biophys Res Commun. 2008, 374: 599-603. 10.1016/j.bbrc.2008.07.009.PubMedView ArticleGoogle Scholar
- Teles AV, Rosenstock TR, Okuno CS, Lopes GS, Bertoncini CR, Smaili SS: Increase in bax expression and apoptosis are associated in Huntington’s disease progression. Neurosci Lett. 2008, 438: 59-63. 10.1016/j.neulet.2008.03.062.PubMedView ArticleGoogle Scholar
- Yang D, Wang CE, Zhao B, Li W, Ouyang Z, Liu Z, Yang H, Fan P, O’Neill A, Gu W, Yi H, Li S, Lai L, Li XJ: Expression of Huntington’s disease protein results in apoptotic neurons in the brains of cloned transgenic pigs. Hum Mol Genet. 2010, 19: 3983-3994. 10.1093/hmg/ddq313.PubMedPubMed CentralView ArticleGoogle Scholar
- Bhattacharyya NP, Banerjee M, Majumder P: Huntington’s disease: roles of huntingtin-interacting protein 1 (HIP-1) and its molecular partner HIPPI in the regulation of apoptosis and transcription. FEBS J. 2008, 275: 4271-4279. 10.1111/j.1742-4658.2008.06563.x.PubMedView ArticleGoogle Scholar
- D’Amelio M, Cavallucci V, Cecconi F: Neuronal caspase-3 signaling: not only cell death. Cell Death Differ. 2010, 17: 1104-1114. 10.1038/cdd.2009.180.PubMedView ArticleGoogle Scholar
- Mazumder S, Plesca D, Almasan A: Caspase-3 activation is a critical determinant of genotoxic stress-induced apoptosis. Methods Mol Biol. 2008, 414: 13-21.PubMedGoogle Scholar
- Muinos-Gimeno M, Guidi M, Kagerbauer B, Martin-Santos R, Navines R, Alonso P, Menchon JM, Gratacos M, Estivill X, Espinosa-Parrilla Y: Allele variants in functional MicroRNA target sites of the neurotrophin-3 receptor gene (NTRK3) as susceptibility factors for anxiety disorders. Hum Mutat. 2009, 30: 1062-1071. 10.1002/humu.21005.PubMedView ArticleGoogle Scholar
- Guidi M, Muinos-Gimeno M, Kagerbauer B, Marti E, Estivill X, Espinosa-Parrilla Y: Overexpression of miR-128 specifically inhibits the truncated isoform of NTRK3 and upregulates BCL2 in SH-SY5Y neuroblastoma cells. BMC Mol Biol. 2010, 11: 95-10.1186/1471-2199-11-95.PubMedPubMed CentralView ArticleGoogle Scholar
- Zhang Y, Chao T, Li R, Liu W, Chen Y, Yan X, Gong Y, Yin B, Qiang B, Zhao J, Yuan J, Peng X: MicroRNA-128 inhibits glioma cells proliferation by targeting transcription factor E2F3a. J Mol Med. 2009, 87: 43-51. 10.1007/s00109-008-0403-6.PubMedView ArticleGoogle Scholar
- Nguyen LS, Wilkinson MF, Gecz J: Nonsense-mediated mRNA decay: inter-individual variability and human disease. Neurosci Biobehav Rev. 2013, doi:10.1016/j.neubiorev.2013.10.016. [Epub ahead of print]Google Scholar
- Bruno IG, Karam R, Huang L, Bhardwaj A, Lou CH, Shum EY, Song HW, Corbett MA, Gifford WD, Gecz J, Pfaff SL, Wilkinson MF: Identification of a microRNA that activates gene expression by repressing nonsense-mediated RNA decay. Mol Cell. 2011, 42: 500-510. 10.1016/j.molcel.2011.04.018.PubMedPubMed CentralView ArticleGoogle Scholar
- Yang SH, Cheng PH, Banta H, Piotrowska-Nitsche K, Yang JJ, Cheng EC, Snyder B, Larkin K, Liu J, Orkin J, Fang ZH, Smith Y, Bachevalier J, Zola SM, Li SH, Li XJ, Chan AW: Towards a transgenic model of Huntington’s disease in a non-human primate. Nature. 2008, 453: 921-924. 10.1038/nature06975.PubMedPubMed CentralView ArticleGoogle Scholar
- Wang CE, Tydlacka S, Orr AL, Yang SH, Graham RK, Hayden MR, Li S, Chan AW, Li XJ: Accumulation of N-terminal mutant huntingtin in mouse and monkey models implicated as a pathogenic mechanism in Huntington’s disease. Hum Mol Genet. 2008, 17: 2738-2751. 10.1093/hmg/ddn175.PubMedPubMed CentralView ArticleGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/4.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly credited. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.