KIT, PDGFRA, NF1 and SDH mutations are alternate initiating events, fostering hyperplasia in gastrointestinal stromal tumours (GISTs), and additional genetic alterations are required for progression to malignancy. The most frequent secondary alteration, demonstrated in ∼70% of GISTs, is chromosome 14q deletion. Here we report hemizygous or homozygous inactivating mutations of the chromosome 14q MAX gene in 16 of 76 GISTs (21%). We find MAX mutations in 17% and 50% of sporadic and NF1-syndromic GISTs, respectively, and we find loss of MAX protein expression in 48% and 90% of sporadic and NF1-syndromic GISTs, respectively, and in three of eight micro-GISTs, which are early GISTs. MAX genomic inactivation is associated with p16 silencing in the absence of p16 coding sequence deletion and MAX induction restores p16 expression and inhibits GIST proliferation. Hence, MAX inactivation is a common event in GIST progression, fostering cell cycle activity in early GISTs.
Activating mutations of the receptor tyrosine kinases KIT1 or PDGFRA2 are initiating or early events in most gastrointestinal stromal tumours (GISTs) and indeed are present in micro-GISTs, which are asymptomatic subcentimetre GIST lesions found in one-third of the general population3. Genetic progression from micro-GIST to malignant GIST results from stepwise accumulation of deletions in chromosome arms 14q, 22q, 1p and 15q, together with cell cycle dysregulating events and dystrophin inactivation4,5,6,7,8. These highly recurrent chromosomal deletions implicate losses of yet-unidentified tumour suppressor mechanisms in GIST progression. Of these, the 14q deletions are most frequent, observed in 60–70% of GISTs (including neurofibromatosis type 1 (NF-1)-associated GIST) as an early event in genetic progression4,5,6,9,10.
Here we show that 14q deletions target the MAX transcriptional regulator gene in early GISTs of various molecular origins (KIT-mutant, PDGFRA-mutant or NF1-mutant). These MAX genomic-inactivating mutations are driver events, enabling GIST progression by loss of MAX expression, and consequent p16 silencing and cell cycle dysregulation.
Targeted sequencing of 812 cancer-associated genes demonstrated somatic homozygous inactivating MAX mutations in three of ten GISTs (Supplementary Data 1 and Supplementary Fig. 1a). The ten GISTs in this discovery set had KIT mutations (seven cases), PDGFRA mutations (two cases) and NF1 mutation (one case) (Supplementary Data 1). Apart from KIT and PDGFRA, MAX was the only other gene with demonstrable recurrent mutations in this discovery set. MAX evaluations by Ion AmpliSeq sequencing, Sanger sequencing (Supplementary Fig. 1b), quantitative PCR (Supplementary Fig. 1c) and single-nucleotide polymorphism (SNP) arrays (Supplementary Fig. 1d) were performed in the same 10 GISTs and in 66 additional GISTs (Supplementary Data 2). This total set of 76 GISTs was shown to have mutually exclusive mutations involving the KIT, PDGFRA, NF1 and SDH genes in 52 (68%), 8 (11%), 11 (14%) and 2 (3%) cases, respectively (Supplementary Data 2). These assays demonstrated somatic hemizygous or homozygous MAX-inactivating mutations in 16 of the 76 GISTs (21%), including 8 mononucleotide mutations and 8 larger-scale intragenic deletions (Fig. 1 and Supplementary Data 2). Non-neoplastic companion DNAs were MAX wild type for seven of eight GISTs with mononucleotide MAX mutations, showing that these were somatic mutations, and the MAX mutation allelic frequency in the remaining case (case 19) was 0.7, consistent with a hemizgyous or homozygous somatic mutation. The MAX mononucleotide mutations were nonsense (N=3), loss of start codon (N=1), frame-shift (N=1), splice site (N=2) and 5′-untranslated region (N=1). The two splice-site mutations (cases 7 and 59) destroyed invariant splicing motifs, creating inactive MAX transcripts with loss of exon 3 (case 7) or retention of intron 4 (case 59), as confirmed by reverse transcriptase–PCR, and—for case 7—also confirmed by genome RNA sequencing (Supplementary Fig. 2). The 5′-untranslated region mutation (case 19) was predicted to be functionally relevant by the PROMO.3 tool, with predicted disruption of transcription factor binding sites in the MAX promoter. Multiple anatomically distinct specimens were studied in five patients (pts) with MAX-mutant GISTs and all had identical mutations, as shown by comparisons of primary GIST and subsequent metastases in two pts, and by comparisons of multiple metastases (two–ten metastases analysed per pt) in three pts (Supplementary Data 2 and Supplementary Fig. 3).
Among the overall study group of 76 GISTs, the GIST primary site was known for 71 pts, whereas primary site could not be determined in the remaining 5 pts who presented with disseminated intra-abdominal disease. MAX genomic mutations were more common in non-gastric than gastric GISTs (P=0.001 for the 71 pts with known GIST primary sites, two-tailed Fisher’s exact test) and this association remained significant when GISTs with NF1 mutations—which are generally of small bowel origin—were removed from consideration (P=0.004 for 61 pts with NF1-wild type GISTs of known primary sites).
MAX was assessed in each of the 76 GISTs by immunoblotting (N=75) and/or immunohistochemistry (IHC) (N=22). MAX inactivation was demonstrated in 38 of 75 GISTs (51%) by immunoblotting (Fig. 2) and was associated with MAX genomic mutation (P<0.0001, two-tailed Fisher’s exact test). Likewise, MAX inactivation, as demonstrated by IHC in 14 of 22 GISTs (63%) (Fig. 3), was associated with MAX genomic inactivation (P=0.0062). Loss of MAX expression, when detected in any GIST metastasis, was detected in all others from the same pt (Supplementary Data 2 and Supplementary Fig. 4). Forty per cent of the GISTs with loss of MAX expression were classified, according to well-established clinicopathological criteria11, as ‘low-risk’ and ‘intermediate-risk’ cases (Fig. 4), which are stages of GIST development that precede transition to clinically aggressive ‘high-risk’ GIST. These findings show that MAX inactivation can be an early event in GIST biological and clinical progression. Further, MAX inactivation was detected in three of eight micro-GISTs, each of which had 14q deletion (Supplementary Fig. 5), confirming MAX dysregulation as an early event in GIST progression (Supplementary Table 1). Hemizygous or homozygous inactivating MAX mutations were demonstrated in sporadic GISTs (11 of 64=17%) and in syndromic GISTs in individuals with NF-1 (5 of 10=50%) (Fig. 4 and Supplementary Data 2). Likewise, loss of MAX protein expression was demonstrated in both sporadic (31 of 64=48%) and NF-1-associated GISTs (9 of 10=90%). GISTs occur in up to 25% of NF-1 pts, predominantly in the small intestine and often as multicentric tumours12,13,14. Our studies credential MAX inactivation, as an early step in GIST progression, associated with KIT and PDGFRA gain-of-function mutations and NF1 loss-of-function mutations.
The GIST48 cell line has MAX inactivation due to homozygous deletion of MAX exons 1 and 2, and has loss of p16 (p16INK4A) expression. This cell line shows a localized CDKN2A deletion, which affects the p14ARF coding sequence (Supplementary Fig. 6) but lacks genomic alterations of the p16 coding sequence in CDKN2A and lacks CDKN2A methylation. CDKN2A ranked in the top 0.1% of genes differentially expressed after MAX restoration in GIST48 and was the highest ranking cancer-associated gene (Supplementary Data 3). In keeping with this evidence, p16 protein expression was strong and diffuse in GISTs lacking MAX or p16INK4A coding sequence mutations, but was undetectable in MAX-mutant GISTs, even in the absence of p16 coding sequence mutation (Supplementary Fig. 7). Inducible restoration of MAX expression in GIST48 upregulated CDKN2A transcript expression, restored p16 protein expression and inhibited RB1 phosphorylation (pRB1Ser795) (Fig. 5a) and cell proliferation (Fig. 5b,c). MAX restoration in GIST48 was not associated with significant enrichment of MYC-related expression signatures or with altered sensitivity to MYC:MAX inhibitor drugs (Supplementary Fig. 8), suggesting that MAX tumour suppressor roles in GIST are not necessarily MYC dependent.
All MAX-inactivating point mutations in this series were hemizygous, with allelic frequencies typically ∼0.67 in GISTs known to have loss of the other MAX allele and containing ∼20% non-neoplastic cells. Similarly, all MAX intragenic deletions were homozygous. These findings indicate that GIST progression is best served by complete loss of MAX function. Although the Ion AmpliSeq and HaloPlex assays detect ≥5% mutant alleles15,16, we found no evidence for multiple MAX-mutant subclones within primary GISTs or between different metastases in a given pt. These observations indicate that a single KIT/PDGFRA-mutant/MAX-mutant or NF1-mutant/MAX-mutant subclone fosters biological and clinical progression in MAX-mutant GISTs. MAX is a helix-loop-helix leucine zipper transcription factor, which regulates cell proliferation, differentiation and apoptosis through heterodimerization with MYC-family proteins17,18,19, but MAX homodimers also regulate transcription in a MYC-independent manner20,21. MAX has tumour suppressor roles in a small subset of hereditary pheochromocytomas and in small cell lung cancer21,22, and a recent report demonstrated MAX mutation in one KIT/PDGFRA wild-type, NF1-mutant, GIST23. Our study demonstrates that MAX mutations are common alterations in GIST, occurring at early stages of GIST development. We detected hemizygous and homozygous MAX-inactivating mutations in 21% of the 76 GISTs in this study, thereby demonstrating that GIST is the neoplasia with the highest known frequency of MAX tumour suppressor mutations. Further, the true frequency of MAX mutations in GIST is likely to be >21%, given that homozygous deletions were a common mechanism of MAX inactivation. Homozygous deletions, particularly if small, will be difficult to detect in some early GISTs, where they are present in a subclone of the overall neoplastic proliferation.
We show MAX protein inactivation in ∼50% of GISTs, including micro and low-risk GISTs, which is additional evidence for MAX dysregulation as an early event in GIST development. MAX restoration in GIST48 cells inhibited GIST cell growth and upregulated CDKN2A expression, accompanied by p16 upregulation and inhibition of pRB1Ser795. These findings suggest that MAX inactivation causes cell cycle dysregulation at an early point in GIST progression, probably enabling progression to GIST stages with greater proliferative potential. Altogether, our studies demonstrate frequent disruption of MAX tumour suppressive roles during early progression of KIT-mutant, PDGFRA-mutant and NF1-mutant GISTs.
Tumour and tissue samples
Discarded, de-identified tumour specimens were obtained at Brigham and Women’s Hospital and Memorial Sloan-Kettering Cancer Center, under protocols approved by the Dana-Farber/Brigham and Memorial Sloan-Kettering Cancer Center Institutional Review Boards. Informed written consent was obtained from all human participants.
GIST cell lines were established in the Fletcher laboratory and were validated against the initial biopsy material by molecular cytogenetics and sequencing verification of known unique gene mutations. Daudi cells were obtained from ATCC (Manassus, VA, USA). All cultures were shown to be mycoplasma free.
Targeted sequencing was performed using the HaloPlex Target Enrichment System for Illumina sequencing (Agilent Technologies, Santa Clara, CA, USA) for a custom-designed set of 812 cancer-related genes. Data were analysed by SureCall software (version 126.96.36.199, Agilent Technologies) and Integrative Genomics Viewer (IGV) (version 2.3.25, Broad Institute). Targeted highly multiplexed PCR with semiconductor-based sequencing using the Ion AmpliSeq assay was performed as described previously15, analysing the MAX gene (NM_002382) coding sequence, an additional two nucleotides adjacent to each exon, and 1 kb of upstream sequence. Amplicon size ranged from 125 to 275 bp (including primers) with an average of 243 bp. Inserts ranged in size from 77 to 230 bp (excluding primers), with an average of 194 bp. Ion AmpliSeq detection for homozygous deletions was performed after normalization to non-neoplastic DNA sequences and establishing cutoffs based on estimated presence of 30% non-neoplastic cells in low-/intermediate-risk GISTs and 20% non-neoplastic cells in high risk/metastatic GISTs. Deletion of at least nine consecutive amplicons and/or a ratio of <0.4 for markers located at either the 3′- or 5′-end of the gene in relation to all markers in a given case were defined as criteria for homozygous deletion.
Genomic PCR and Sanger sequencing of MAX exons 1–5 (NM_002382) was performed using primers shown in Supplementary Table 2. Reverse transcription from tumour RNA was performed using the iScript cDNA Synthesis kit (Bio-Rad Laboratories, CA) and followed by PCR using Platinum PCR Super Mix (Life Technologies, Grand Island, NY, USA) with analysis by Sanger sequencing.
Quantitative PCR of MAX exons 1, 3 and 4, and the flanking genes FNTB and FUT8 was performed using 25 μl volume per reaction, containing 5 ng of genomic DNA, 100 nM forward primer, 100 nM reverse primer and 1 × iQ SYBR Green Supermix (Bio-Rad). The MyiQ single colour real-time detection system (Bio-Rad) was used for thermal cycling. Samples were run in triplicate with non-template control, human non-neoplastic cell DNA and GIST48 DNA with a known homozygous MAX deletion. Mixtures of non-neoplastic and MAX-mutant GIST48 DNA (30:70 and 20:80) were controls modelling detection of MAX homozygous deletions in human GIST biopsies (in which 10–30% of cells are nonneoplastic). Amplification accuracy was verified by melting curve analysis. The minimum threshold cycle (Ct value) generated by the MyiQ software (Bio-Rad) for each sample was used to calculate MAX copy number using Ct values for normal tissue and adjacent genes as reference.
High-molecular-weight gDNA was isolated using QIAamp DNA Mini Kit (Qiagen, Valencia, CA, USA) and analysed by Affymetrix Cytoscan HD 2,600 K SNP array (Affymetrix, Santa Clara, CA, USA) with Affymetrix Chromosome Analysis Suite 2.0.
Array comparative genomic hybridization
Micro-GIST gDNAs were obtained from microdissected tissues and extracted using QIAamp DNA FFPE Tissue kits (Qiagen) following the manufacturer’s protocol. Amplification was performed using a GenomePlex Tissue Whole Genome Amplification WGA5 kit (Sigma, Saint Louis, MO, USA). The post-WGA products were purified using a QIAquick PCR Purification Kit (Qiagen) and quantified using a NanoDrop ND-1000 Spectrophotometer. Comparative genomic hybridization was performed using a customized human array comparative genomic hybridization platform with 2 × 415 K coverage (Agilent Technologies). Four independent experiments were concurrently performed per template amplification and then mixed, to minimize amplification bias and allele dropout. Data were analysed using Agilent Technologies 10.5.1.1 Software.
Whole-cell lysates were prepared as described previously24 and protein concentrations were determined using the Bio-Rad protein assay (Bio-Rad). Electrophoresis, immunoblotting and chemiluminescence detection were as described previously8. Primary antibodies were directed against MAX (Santa Cruz Biotechnology, Dallas, TX, USA, C-17, 1:200 dilution), p16INK4A/CDKN2A (R&D Systems, Minneapolis, MN, USA, AF5779, 1:200 dilution), pRB1Ser795 (Cell Signaling Technology, Danvers, MA, USA, 9301, 1:1,000 dilution) and GAPDH (Sigma, GAPDH-71.1, 1:5,000 dilution). Full-length blottings can be viewed in Supplementary Fig. 9.
Immunohistochemical staining for MAX was performed with the MAX C-17 antibody (Santa Cruz) at dilution of 1:1,500 on 4 μm thin sections prepared from formalin-fixed, paraffin-embedded tissue blocks after antigen retrieval using a citrate buffer pressure cooker protocol. Staining for p16 (p16INK4A) was performed using a mouse monoclonal antibody (dilution 1:2; clone E6H4, Ventana Medical Systems, Tucson, AZ, USA).
Lentivirus preparations were produced by cotransfecting MAX construct (Broad Institute, clone ID BRDN0000560330, NM_002382.3) introduced into a destination vector pLXI_TRC401 (Alias pCW57.1 Dest, TRE-Gateway-No Tag) by LR Clonase (Thermo Fisher Scientific, Waltham, MA, USA) reaction and helper virus packaging plasmid pCMVΔR8.91 and pMD.G into 293T cells, as described previously25. Lentivirus was harvested at 24, 36, 48 and 60 h post transfection and virus titres were quantified and stored at −80 °C. GIST48 transductions were carried out overnight with polybrene 8 μg ml−1 (Sigma) and transduced cells were selected for 9 weeks with puromycin (0.125 μg ml−1), which was discontinued 7–10 days before analyses. MAX expression was induced in stably transduced cells with doxycycline (2.5 μg ml−1) every 36 h.
Gene expression profiling
RNA sequencing was performed 24 h after MAX restoration in GIST48 cells using an Illumina HiSeqTM 2000 platform (Beijing Genomics Institute, Hong Kong). Parental GIST48 cells treated with doxycycline for 24 h served as control. Data analyses were with BGI-Tech Pipeline Version 3.1 and differentially expressed genes were identified using criteria false discovery rate ≤0.001 and abs(log2(MAX-/MAX+))≥1.
BrdU uptake and CellTiter-Glo analyses
Cells were plated in 96-well plates at 20,000 cells per well in growth medium and incubated overnight. Cells were treated with 2.5 μg ml−1 doxycycline for 24 h (MAX-restoration) and parental GIST48 was the untreated comparator. For 5-bromodeoxyuridine (BrdU) incorporation proliferation analyses, BrdU was added to the cells for 24 h. BrdU incorporation, fixation and detection were performed using a BrdU Cell Proliferation ELISA as per the manufacturer’s protocol (Roche Diagnostics, Indianapolis, IN, USA). BrdU incorporation was presented as % of untreated control. For CellTiter-Glo (Promega, Madison, WI, USA) viability analyses, MYC inhibitors versus dimethyl sulfoxide-only control were added for 3 days and ATP incorporation was then measured using a luminometer. All cell response assays were performed in triplicate wells, with the entire study replicated at least once.
Cells were trypsinized, resuspended in media and counted by haemocytometer.
Statistical analyses were performed using GraphPad Prism Software and Student’s t-test and two-tailed Fisher’s exact tests to compare two data sets.
Haloplex targeted DNA sequencing data of the discovery cohort, Ion Ampliseq MAX sequencing data of all cases and gene expression data have been deposited in the Sequence Read Archive (accession number SRP096291). Cytoscan HD SNP array data have been deposited in the Gene Expression Omnibus database (accession number GSE93077). All remaining data are available within the article and Supplementary Information files or available from the authors upon request.
How to cite this article: Schaefer, I.-M. et al. MAX inactivation is an early event in GIST development that regulates p16 and cell proliferation. Nat. Commun. 8, 14674 doi: 10.1038/ncomms14674 (2017).
Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Hirota, S. et al. Gain-of-function mutations of c-kit in human gastrointestinal stromal tumors. Science 279, 577–580 (1998).
Heinrich, M. C. et al. PDGFRA activating mutations in gastrointestinal stromal tumors. Science 299, 708–710 (2003).
Agaimy, A. et al. Minute gastric sclerosing stromal tumors (GIST tumorlets) are common in adults and frequently show c-KIT mutations. Am. J. Surg. Pathol. 31, 113–120 (2007).
El-Rifai, W., Sarlomo-Rikala, M., Andersson, L. C., Knuutila, S. & Miettinen, M. DNA sequence copy number changes in gastrointestinal stromal tumors: tumor progression and prognostic significance. Cancer Res. 60, 3899–3903 (2000).
Wozniak, A. et al. Array CGH analysis in primary gastrointestinal stromal tumors: cytogenetic profile correlates with anatomic site and tumor aggressiveness, irrespective of mutational status. Genes Chromosomes Cancer 46, 261–276 (2007).
Gunawan, B. et al. An oncogenetic tree model in gastrointestinal stromal tumours (GISTs) identifies different pathways of cytogenetic evolution with prognostic implications. J. Pathol. 211, 463–470 (2007).
Henze, J. et al. p53 modulation as a therapeutic strategy in gastrointestinal stromal tumors. PLoS ONE 7, e37776 (2012).
Wang, Y. et al. Dystrophin is a tumor suppressor in human cancers with myogenic programs. Nat. Genet. 46, 601–606 (2014).
Schaefer, I. M. et al. Chromosomal aberrations in primary PDGFRA-mutated gastrointestinal stromal tumors. Hum. Pathol. 45, 85–97 (2014).
Yamamoto, H. et al. Neurofibromatosis type 1-related gastrointestinal stromal tumors: a special reference to loss of heterozygosity at 14q and 22q. J. Cancer Res. Clin. Oncol. 135, 791–798 (2009).
Miettinen, M. & Lasota, J. Gastrointestinal stromal tumors: pathology and prognosis at different sites. Semin. Diagn. Pathol. 23, 70–83 (2006).
Agaimy, A., Vassos, N. & Croner, R. S. Gastrointestinal manifestations of neurofibromatosis type 1 (Recklinghausen’s disease): clinicopathological spectrum with pathogenetic considerations. Int. J. Clin. Exp. Pathol. 5, 852–862 (2012).
Miettinen, M., Fetsch, J. F., Sobin, L. H. & Lasota, J. Gastrointestinal stromal tumors in patients with neurofibromatosis 1: a clinicopathologic and molecular genetic study of 45 cases. Am. J. Surg. Pathol. 30, 90–96 (2006).
Mussi, C., Schildhaus, H. U., Gronchi, A., Wardelmann, E. & Hohenberger, P. Therapeutic consequences from molecular biology for gastrointestinal stromal tumor patients affected by neurofibromatosis type 1. Clin. Cancer Res. 14, 4550–4555 (2008).
Beadling, C. et al. Combining highly multiplexed PCR with semiconductor-based sequencing for rapid cancer genotyping. J. Mol. Diagn. 15, 171–176 (2013).
Stoddard, J. L., Niemela, J. E., Fleisher, T. A. & Rosenzweig, S. D. Targeted NGS: a cost-effective approach to molecular diagnosis of PIDs. Front Immunol. 5, 531 (2014).
Blackwood, E. M. & Eisenman, R. N. Max: a helix-loop-helix zipper protein that forms a sequence-specific DNA-binding complex with Myc. Science 251, 1211–1217 (1991).
Prendergast, G. C., Lawe, D. & Ziff, E. B. Association of Myn, the murine homolog of max, with c-Myc stimulates methylation-sensitive DNA binding and ras cotransformation. Cell 65, 395–407 (1991).
Blackwood, E. M., Luscher, B. & Eisenman, R. N. Myc and Max associate in vivo. Genes Dev. 6, 71–80 (1992).
Nair, S. K. & Burley, S. K. X-ray structures of Myc-Max and Mad-Max recognizing DNA. Molecular bases of regulation by proto-oncogenic transcription factors. Cell 112, 193–205 (2003).
Comino-Mendez, I. et al. Exome sequencing identifies MAX mutations as a cause of hereditary pheochromocytoma. Nat. Genet. 43, 663–667 (2011).
Romero, O. A. et al. MAX inactivation in small cell lung cancer disrupts MYC-SWI/SNF programs and is synthetic lethal with BRG1. Cancer Discov. 4, 292–303 (2014).
Belinsky, M. G. et al. Somatic loss of function mutations in neurofibromin 1 and MYC associated factor X genes identified by exome-wide sequencing in a wild-type GIST case. BMC Cancer 15, 887 (2015).
Rubin, B. P. et al. KIT activation is a ubiquitous feature of gastrointestinal stromal tumors. Cancer Res. 61, 8118–8121 (2001).
Ou, W. B., Zhu, M. J., Demetri, G. D., Fletcher, C. D. & Fletcher, J. A. Protein kinase C-theta regulates KIT expression and proliferation in gastrointestinal stromal tumors. Oncogene 27, 5624–5634 (2008).
We thank Raymond DiDonato, PhD, from Agilent Technologies, for HaloPlex targeted cancer gene panel design and for other helpful advice with the HaloPlex analyses, and Jason Hornick, MD, PhD for assistance with the p16 IHC studies. This work was supported by grants from the US National Institutes of Health, including 1P50CA127003 (J.A.F. and G.D.D.), 1P50CA168512 (J.A.F. and A.M.-E.), the GIST Cancer Research Fund (J.A.F., M.C.H., C.L.C., C.R.A.), the Life Raft Group (J.A.F., M.v.d.R., M.C.H., C.L.C, S.B.), the Deutsche Krebshilfe (I.-M.S.), the VA Merit Review Grants 1I01BX000338-01 and 2I01BX000338-05 (M.C.H.) and the V Foundation Translational Research Grant (M.C.H.).
C.L.C. has received consulting fees from ThermoFisher. The remaining authors declare no competing financial interests.
Supplementary Information and Supplementary Tables (PDF 966 kb)
Haloplex sequencing results in a discovery cohort of 10 GISTs. (XLSX 19 kb)
. Clinicopathologic characteristics of 76 GISTs. (XLSX 16 kb)
Differentially expressed genes by RNA sequencing 24 hours after inducible MAX restoration in MAX-deficient/MAX-mutant GIST48 cells. (XLSX 19 kb)
About this article
Cite this article
Schaefer, IM., Wang, Y., Liang, Cw. et al. MAX inactivation is an early event in GIST development that regulates p16 and cell proliferation. Nat Commun 8, 14674 (2017). https://doi.org/10.1038/ncomms14674
Journal of Cancer Research and Clinical Oncology (2022)
Nature Reviews Disease Primers (2021)
Decreased MYC-associated factor X (MAX) expression is a new potential biomarker for adverse prognosis in anaplastic large cell lymphoma
Scientific Reports (2020)
Genetic alterations in cell cycle regulation-associated genes may promote primary progression of gastrointestinal stromal tumors
Laboratory Investigation (2020)
Genomic aberrations in cell cycle genes predict progression of KIT-mutant gastrointestinal stromal tumors (GISTs)
Clinical Sarcoma Research (2019)