Open Access

The GATA1s isoform is normally down-regulated during terminal haematopoietic differentiation and over-expression leads to failure to repress MYB, CCND2 and SKI during erythroid differentiation of K562 cells

  • Christina Halsey1, 2Email author,
  • Marie Docherty1,
  • Mhairi McNeill1,
  • Derek Gilchrist1,
  • Michelle Le Brocq1,
  • Brenda Gibson2 and
  • Gerard Graham1
Journal of Hematology & Oncology20125:45

DOI: 10.1186/1756-8722-5-45

Received: 4 May 2012

Accepted: 11 July 2012

Published: 1 August 2012

Abstract

Background

Although GATA1 is one of the most extensively studied haematopoietic transcription factors little is currently known about the physiological functions of its naturally occurring isoforms GATA1s and GATA1FL in humans—particularly whether the isoforms have distinct roles in different lineages and whether they have non-redundant roles in haematopoietic differentiation. As well as being of general interest to understanding of haematopoiesis, GATA1 isoform biology is important for children with Down syndrome associated acute megakaryoblastic leukaemia (DS-AMKL) where GATA1FL mutations are an essential driver for disease pathogenesis.

Methods

Human primary cells and cell lines were analyzed using GATA1 isoform specific PCR. K562 cells expressing GATA1s or GATA1FL transgenes were used to model the effects of the two isoforms on in vitro haematopoietic differentiation.

Results

We found no evidence for lineage specific use of GATA1 isoforms; however GATA1s transcripts, but not GATA1FL transcripts, are down-regulated during in vitro induction of terminal megakaryocytic and erythroid differentiation in the cell line K562. In addition, transgenic K562-GATA1s and K562-GATA1FL cells have distinct gene expression profiles both in steady state and during terminal erythroid differentiation, with GATA1s expression characterised by lack of repression of MYB, CCND2 and SKI.

Conclusions

These findings support the theory that the GATA1s isoform plays a role in the maintenance of proliferative multipotent megakaryocyte-erythroid precursor cells and must be down-regulated prior to terminal differentiation. In addition our data suggest that SKI may be a potential therapeutic target for the treatment of children with DS-AMKL.

Keywords

GATA1 transcription factor Humans Down syndrome/*genetics/physiopathology Leukaemia Megakaryoblastic Acute/genetics Dendritic cells Cell differentiation/*drug effects

Findings

GATA binding protein 1 (GATA1, GenBank ID: NM_002049) is a key haematopoietic transcription factor with a pivotal role in differentiation of the erythroid, megakaryocyte, eosinophil and mast cell lineages[1]. The GATA1 gene produces at least two protein isoforms—the well characterised GATA1 full-length (GATA1FL) isoform and a truncated isoform—GATA1 short (GATA1s). The GATA1FL protein comprises two zinc fingers (which interact with DNA and essential co-factors) a C-terminal tail (of mostly unknown function) and an N-terminal domain (originally thought to confer activation properties to the molecule, but which may also be involved in transcriptional repression [2]). GATA1s lacks the N-terminal domain but is otherwise identical.

The biological role of GATA1s in humans is unknown and this isoform received scant attention until the discovery that GATA1FL mutations were linked to a highly informative pair of disorders—transient abnormal myelopoiesis (TAM)[3] and acute megakaryoblastic leukaemia (AMKL) [4, 5]—seen in children with Down syndrome (constitutional trisomy 21, OMIM ID: 190685). In these disorders the GATA1FL mutations are always clustered within the N-terminus, allowing unhindered production of the GATA1s isoform. This finding has led to interest in the pathological and physiological role of GATA1s in haematopoiesis.

The biological effects of GATA1s have been studied using transgenic mice and in vitro rescue of GATA1 deficient cells [69]. These papers show that GATA1s expression, in the absence of GATA1FL, is associated with defects in lineage restriction, alternative cell fate decisions and proliferation/cell cycle control. In particular unopposed GATA1s expression is associated with outgrowth of primitive hyper-proliferative megakaryocytic progenitors with a limited capacity to undergo terminal differentiation [68]. However, concerns remain about translating results from murine systems into humans since mouse models do not recapitulate all the features of human disease [7, 10, 11]. In addition, whilst mice produce the two isoforms via alternative translation of a single GATA1 mRNA [12], humans use alternative splicing of a pre-mRNA to produce both GATA1FL and GATA1s transcript [13]. Alternative splicing provides a mechanism by which the isoforms could be individually regulated, raising the possibility that alternative isoform usage occurs in particular lineages or at specific stages of haematopoietic differentiation. For these reasons we chose to address three questions regarding the role of GATA1 isoforms in human haematopoiesis; 1) Do different lineages show different isoform usage? 2) Are isoform expression levels dynamically regulated during haematopoietic differentiation? 3) Do the two isoforms have different effects on the transcription of key target genes during in vitro differentiation?

Results and discussion

GATA1 isoforms are not separately expressed in different cell types

Both isoforms are known to be expressed in human CD34+ cells [14] and erythroblasts and megakaryocytes [10]. Here we extend these observations by using RT-PCR to detect isoform expression in other human primary cells (Figure 1a). Eosinophils expressed both isoforms whilst, as expected, the lymphoid B and T cells did not express either isoform. We also studied monocytes and dendritic cells since the role of GATA1 in dendritic cell (DC) maturation is currently debated [1517]. Human CD14+ cell preparations only weakly expressed both isoforms but maturation into DCs was associated with loss of expression of both transcripts both by RT-PCR (Figure 1a) and quantitative PCR (data not shown), arguing against a major role for GATA1 isoforms in DC development.
https://static-content.springer.com/image/art%3A10.1186%2F1756-8722-5-45/MediaObjects/13045_2012_Article_256_Fig1_HTML.jpg
Figure 1

Expression patterns of GATA1FL and GATA1 s in haematopoietic cells. (a) RT-PCR of human primary cell cDNA using GATA1 exon 1 and 3 primers (top panel) and GAPDH housekeeping gene primers (Bottom panel). Predicted size of GATA1FL = 430 bp and GATA1s = 192 bp (b) RT-PCR of human haematopoietic cell line cDNA using the same primers as (a).

To overcome concerns about possible contamination of primary preparations with other cell types, a number of cell lines were also studied (Figure 1b). An acute monocytic leukaemia cell line THP-1 and the histiocytic (monocyte/macrophage) cell line U937, did not express either isoform. Expression of both isoforms was seen in the megakaryocytic cell lines Meg-01 and MO7-E along with K562 (a chronic myeloid leukaemia cell line known to be capable of both megakaryocytic and erythroid differentiation in vitro). In addition the mast cell lines HMC-1 and LAD2 expressed both isoforms although, interestingly, they appeared to have a relatively weak GATA1s band compared to other cell types.

Importantly, in all the cells we examined the two isoforms appear to always be expressed together with no evidence of exclusive GATA1s or exclusive GATA1FL expression in any of the cell types. This observation argues against a primary role for the two isoforms in lineage specification.

GATA1 isoform expression is dynamically regulated during induction of haematopoietic differentiation

It is known that total GATA1 levels show initial up-regulation during erythroid commitment followed by terminal down-regulation [1, 18]. Whether the two GATA1 isoforms are independently regulated at the transcriptional level during this process is unknown. To investigate this, we used an established in vitro model of Haemin-induced erythroid differentiation in K562 cells [19]. Successful differentiation was confirmed by a visible haemoglobinised cell pellet as well as up-regulation of glycophorin A (Figure 2a). Quantitative PCR using GATA1 isoform specific primers and probes was performed at baseline and then 6 h, day 3 and day 6 following treatment (Figure 2b, c).
https://static-content.springer.com/image/art%3A10.1186%2F1756-8722-5-45/MediaObjects/13045_2012_Article_256_Fig2_HTML.jpg
Figure 2

GATA1s expression levels during haematopoietic differentiation of K562 cell lines by Haemin and TPA. (a) K562 surface glycophorin A expression measured by single colour FACS after 3 days of Haemin treatment (MFI = −Mean Fluorescence Intensity) (b, c) quantitative PCR analysis of (b) GATA1FL and (c) GATA1s, expression levels during the course of Haemin-induced erythroid differentiation (n = 3), results are expressed as fold change (log2) using day 0 as the calibrator (expression arbitrarily set at 1.0) (d) DNA ploidy analysis in K562 cells 0, 1, 2 and 3 days following treatment with the differentiating agent TPA (e, f) quantitative PCR analysis of (e) GATA1FL and (f) GATA1s, expression levels during the course of TPA-induced megakaryocytic differentiation (n = 3), results are expressed as fold change (log2) using day 0 as the calibrator (expression arbitrarily set at 1.0).

GATA1FL expression remained relatively constant during differentiation but GATA1s showed a significant up-regulation at 6 h and down regulation by day 3 compared to baseline expression levels.

We went on to see whether similar dynamic changes are seen during in vitro megakaryocytic differentiation of K562 using TPA [20]. Successful differentiation was confirmed by an increase in DNA ploidy (Figure 2d) and by induction of expression of the megakaryocytic genes ITGA2B and GPB1A (data not shown). Analysis of GATA1 isoform expression levels (Figure 2e, f) showed an initial reduction in both isoforms at 6 h. Again, GATA1s transcripts remained suppressed at later time-points whilst GATA1FL transcripts rose to above baseline.

Although the effects are modest, the fact that levels of the two isoforms can move in opposite directions suggests that their expression can be independently and dynamically regulated. Our observation of GATA1s down-regulation from day 3 onwards fits into the prevailing model of GATA1s function which suggests that GATA1s is important for maintenance of a suitable primed highly proliferative progenitor compartment but that a switch to predominant GATA1FL usage may be needed to enact terminal differentiation.

GATA1FL and GATA1s transfectants show distinct transcriptional profiles during haemin induced in vitro differentiation

To extend these observations further we looked at the impact of isoform expression on transcriptional profiles during erythroid differentiation. K562 cells were stably transfected with a GATA1s-IRESGFP or GATA1FL-IRESGFP expressing plasmid or an empty vector control and high GFP expressers were sorted and used in all subsequent experiments. Details of the construction and validation of these vectors are given in the materials and methods section and outlined in Figure 3. The presence of empty vector had no effect on growth characteristics compared to the parental cell line (p = 0.6, 2-way ANOVA untransfected K562 vs. empty vector). Both GATA1FL and GATA1s transfection conferred a modest but significant growth advantage to the K562 cells (GATA1FL vs. empty vector p = 0.03, GATA1s vs. empty vector p = 0.02, student’s 2 tailed t-test), but there was no difference between the two isoforms (p = 0.40 GATA1FL vs. GATA1s). Since the lower proliferation in the empty vector transfectants could confound comparison of transcriptional profiles it was decided to directly compare GATA1FL vs. GATA1s transfectants in subsequent analysis. Although this cannot completely rule out off-target effects related to the presence of the vector the two transfectants should be equally affected by this. We used this system to answer the question of whether the GATA1s and GATA1FL isoforms produce differential effects on transcription when over-expressed in the same cellular context. All experiments were performed in triplicate.

Using data from microarray studies in Down syndrome AMKL [21, 22] and GATA1 transgenic mice [7] we identified eight potentially informative genes and examined their response to in vitro erythroid differentiation in our engineered cell lines. Results of gene expression levels were compared between the GATA1FL and GATA1s transfectants at day 0 (baseline), day 1 and day 3 of differentiation using ΔΔCT relative quantification (n = 3, Figure 4). GATA1FL expressing cells formed a well haemoglobinised cell pellet by day 1 of differentiation whereas GATA1s cells formed a haemoglobinsed pellet by day 3 indicating a potential slowing but no absolute block to differentiation.
https://static-content.springer.com/image/art%3A10.1186%2F1756-8722-5-45/MediaObjects/13045_2012_Article_256_Fig3_HTML.jpg
Figure 3

Production and validation of GATA1 isoform specific expression vectors. (a) production of GATA1s and GATA1FL transcripts from wild type (WT) HEK293 cDNA black arrows represent the position of the GATA1WT/FL primers, white arrows mark GATA1s primers. (b) Map of the pEF6 GATA1-IRESGFP expression plasmid. (c) Western blot of GATA1 protein expression from GATA1FL (lane 1) and GATA1s (lane 2) plasmids respectively, using Santa Cruz GATA1 M20 antibody. Arrows show the position of the 40 and 50 kDa size markers, the expected protein sizes are 47 kDa GATA1FL and 40 kDa GATA1s, a loading control is also shown. (d) Luciferase assay using a GATA1 reporter plasmid showing fold induction of luminescence with expression of the WT GATA1 plasmid versus the mutated GATA1FL plasmid (84 Met-Thr).

Two genes—Ikaros and NFE2—were down regulated in GATA1FL transfectants but to a lesser extent in GATA1s transfectants. Inadequate repression of Ikaros (a master regulator of lymphoid differentiation [23]) has already been described in the GATA1s transgenic mice [7] and is thought to be consistent with maintenance of a primed multipotent progenitor state. The reduced repression of NFE2, an important megakaryocytic transcription factor [24], may partially explain the strong association of GATA1s with acute megakaryoblastic leukaemia [4].

A second set of genes—EKLF, PU.1 and GATA2 show some alterations at baseline but no significant differences in response to differentiation. In the GATA1s transgenic mouse model [7] PU.1 and GATA2 showed inadequate repression during in vitro megakaryocytic differentiation. The different result seen here may be due to differences between erythroid and megakaryocytic differentiation regimes, expression of a dominant GATA1FL isoform from the endogenous K562 allele or it may reflect differences in the transcriptional response to GATA1s between mice and humans.

Perhaps the most interesting genes were those that showed persistent up-regulation in the presence of GATA1s; MYB, CCND2 and SKI. MYB is a key haematopoietic transcription factor involved in stem cell self-renewal and lineage decisions [25]. In the GATA1s transfectants MYB persisted at higher levels than undifferentiated GATA1FL cells consistent with maintenance of a primitive progenitor state. Interestingly one of the key findings from GATA1s transgenic mice is that fetal liver derived megakaryocytic precursors failed to down-regulate MYB when differentiated in vitro[7]. These results confirm these findings in a completely different (and human) experimental system. Our second gene of interest was CCND2, a cell cycle regulator. Since CCND2 is associated with megakaryocytic differentiation [26] down-regulation would be expected during terminal erythroid differentiation. This is seen with the GATA1FL transfectants but not GATA1s consistent with its proposed role in bipotent meg-erythroid and megakaryocytic cells. Finally SKI is known to show peak expression in murine bipotent meg-erythroid progenitors (MEP) with much lower or undetectable levels in earlier precursors or unipotent megakaryocytic or erythroid precursors [27]. It has been shown to block erythroid differentiation by a direct interaction with GATA1 involving the C-terminal Zinc finger [28]. SKI is an important component of the histone deacetylase complex, and over-expression of SKI has been implicated in the pathogenesis of acute myeloid leukaemia [2931]. These observations suggest that a GATA1s-SKI interaction may be important for the maintenance of an expanded MEP compartment with a block to terminal differentiation as seen in transient abnormal myelopoiesis. The precise role of SKI in Down syndrome transient abnormal myelopoiesis needs further investigation particularly as this raises the possibility that these children may respond well to relatively non-toxic HDAC inhibitors currently in development [32].

Conclusions

The data presented here show that the two GATA-1 isoforms can be independently regulated at the transcriptional level during haematopoietic differentiation but we were unable to find any evidence that they are used to specify different lineages. When overexpressed during human erythroid differentiation the two isoforms produce distinct transcriptional profiles which largely mirror those seen in murine models. Finally our observation of sustained SKI up-regulation by GATA1s suggests a potential target gene which may play an important role in the development of DS-AMKL and is a tractable therapeutic target.

Methods

Cell lines

THP-1, U937, K562, and Meg01 cell lines were grown in complete RPMI 1640 with 10% fetal bovine serum (FBS). MO7E were grown in RPMI supplemented with 20% FBS and 10 ng/ml GM-CSF (StemCell Technologies). HMC-1 cells were grown in IMDM supplemented with 10% FBS, 25 mM HEPES, and α-thioglycerol. LAD2 cells were grown in Stem pro-34 SFM media supplemented with stem pro-34 nutrient supplement (Invitrogen) plus 10 ng/ml human Stem Cell Factor (StemCell Technologies).

Primary cells

Human peripheral blood (PB) eosinophils, T and B cell populations were isolated from human PB as previously described [16]. Cell purities were verified by staining for CD4 (T cells >95%) and CD19 (B cells >95%). Monocytes were isolated using human buffy coats layered over Ficoll-Paque (GE Healthcare). The mononuclear cell fraction was washed and CD14+ cells separated using microbeads and an autoMACS Pro separator, following the manufacturer’s protocol (Miltenyi Biotec). Cell purities were consistently >90% by flow cytometry. To generate immature dendritic cells (DCs) (CD14-HLA-DRmidCD86mid) the CD14+ cells were grown for 6 days in RPMI 1640, supplemented with HEPES, L-glut (Invitrogen), 5% AB serum, gentamicin (Sigma), 50 ng/mL GM-CSF and 15 ng/mL IL-4 (Miltenyi Biotec). Immunophenotype was confirmed by flow cytometry (MACSQuant, Miltenyi Biotec). Mature DCs (CD14-HLA-DRhighCD83+CD86+CD80+CD25+) were generated by resuspension of the immature DC fraction in RPMI 1640 supplemented with 5% AB serum, gentamicin, HEPES, L-glut, 50 ng/mL GM-CSF, 15 ng/mL IL-4, 12.5 μg/mL PolyI:C (Sigma) and 1 μg/mL PGE2 (Sigma) for 48 h. Again identity was confirmed by flow cytometry.

Expression plasmids

GATA1FL and GATA1s isoforms were amplified from a GATA1-BFT4 expression plasmid using exon 2 (gttccatggattttcctg) and exon 3 (caacagtatggagggaattcc) primers respectively along with a common exon 6 reverse primer (gctattctgtgtaccttcaagaac) (Figure 3a) and cloned into pcDNA3.1 expression plasmids (Invitrogen). The GATA1FL plasmid then underwent site directed mutagenesis (QuikChangeII, Stratagene) of the second start codon at position 84 (ATG to ACA), to prevent alternative translation of GATA1s from the same transcript (Figure 3a). Products were subcloned into the pEF6V5hisTOPO expression vector (Invitrogen) and an IRES GFP sequence was ligated into a downstream NotI site to produce the vectors GATA1s-IRESGFP, GATA1FL-IRESGFP and an Empty vector control containing all vector sequences but no GATA1 insert: Empty-IRESGFP (Figure 3b). Protein expression from the GATA1s and GATA1FL vectors was confirmed by western blotting of transfected HEK293 cells (GATA1 M20 antibody, Santa Cruz) (Figure 3c). Transactivation of a GATA1 luciferase reporter vector was used to confirm that the amino-acid 84 (Met-Thr) change, introduced by site directed mutagenesis, did not produce a functional change in the GATA1FL protein (Figure 3d).
https://static-content.springer.com/image/art%3A10.1186%2F1756-8722-5-45/MediaObjects/13045_2012_Article_256_Fig4_HTML.jpg
Figure 4

Gene expression changes in GATA1 isoform expressing K562 transgenic cell lines treated with Haemin. Levels of expression of eight target genes (a)-(h) in response to Haemin treatment in GATA1FL- IRESGFP (black bars) and GATA1s- IRESGFP (white bars) transfected K562 cells. Results are expressed as fold change (log2) using day 0 K562 GATA1FL- IRESGFP cells as the calibrator (expression arbitrarily set at 1.0). * p ≤ 0.05, ** p ≤ 0.01 and *** p ≤ 0.001.

The vectors were stably transfected into K562 cells using Fugene6 (Promega) and maintained in selective Blasticidin containing media. Following several weeks in culture high GFP expressors were isolated using a BD FACSAria cell sorter before use in in vitro differentiation experiments.

Haemin and TPA differentiation

Differentiation of K562 cells was achieved by plating 1 × 106 cells in each well of a 6-well plate and treating for up to 4 days with 100 nM 12-O-tetradecanoyl phorbol-13-acetate (TPA) [33] or 10 μM Haemin (from a 4 mM stock dissolved in NaOH 0.5 M, Tris (pH 7.8))[19]. All experiments were preformed in triplicate.

Flow cytometry

Cells were washed and treated with human Fc receptor Blocking agent (Miltenyi Biotec) followed by mouse anti-human PE-Cy5 conjugated anti-CD235a (glycophorin A) (BD Pharmingen). Data was acquired from 20,000 gated events on a FACSCalibur instrument (Becton Dickinson) and analyzed using BD CellQuest Pro software.

DNA ploidy analysis

Cells were washed in cold PBS and added drop-wise to ice-cold ethanol. Following overnight incubation at 4°C cells were spun down and resuspended in 2 ml of Propidium Iodide (PI) mastermix (1xPBS, PI 40 μg/ml, RNase (DNAse-free) 100 μg/ml) and incubated at 37°C for 30 min. Cells were filtered through a 40–70 μm cell strainer and analysed on the flow cytometer as detailed above. A known 2N cell line (Raji) was used as a control and run alongside test samples.

RT and qPCR

Total RNA was extracted from cell lysates using RNeasy columns (Qiagen) with on-column DNase digestion (RNase-free DNase, Qiagen). RNA (2 μg) was reverse-transcribed using random primers and AffinityScript multiple temperature Reverse Transcriptase (Stratagene). The resulting cDNA was diluted 1:5 and standard RT-PCR was performed using a commercial PCR mastermix (ReddyMix, Abgene) with the following primers: GATA1 5′ ctccgcaaccaccagcccag 3′ tatggtgagccccctgggatc. The identity of PCR products was confirmed by excision of bands from the agarose gel, purification of DNA using a commercial QIAquick gel extraction method (Qiagen), followed by TOPO cloning into a pCR4TOPO vector (Invitrogen). Plasmid preparations containing insert were then sent for commercial sequencing (http://www.agowa.de).

Quantitative PCR (qPCR) was performed on a 7900HT (Applied Biosystems (ABI)) thermal cycler using Taqman technology (ABI). Previously published GATA1 isoform primers and probes were used [14]. GATA1 transcript levels were normalized to 18s rRNA (one of several reference genes analyzed and found to be unaffected by experimental conditions). Gene expression signatures were analyzed on 384 well microfluidic plates (Taqman low density array (TLDA®plates), ABI) using Universal PCR Mastermix (ABI). Results were analyzed using Sequence Detection Systems (SDS) Software v2.1 and statistical analysis was performed using a two-tailed student’s t-test with a p value of ≤0.05 being considered significant.

Declarations

Acknowledgements

This work was supported by a Leukemia and Lymphoma Research Clinical Training Fellowship (CH). We thank Dr Paresh Vyas, Weatherall Institute of Molecular Medicine, University of Oxford for the kind gift of the Luciferase reporter vector and Dr Oliver Tunstall-Pedoe and Prof Irene Roberts, Imperial College, London for the GATA1 isoform qPCR primers and probes.

Authors’ Affiliations

(1)
Institute of Infection, Immunity and Inflammation, Level 3, Glasgow Biomedical Research Centre
(2)
Department of Paediatric Haematology, Royal Hospital for Sick Children

References

  1. Ferreira R, Ohneda K, Yamamoto M, Philipsen S: GATA1 function, a paradigm for transcription factors in hematopoiesis. Mol Cell Biol. 2005, 25: 1215-1227. 10.1128/MCB.25.4.1215-1227.2005.PubMed CentralView ArticlePubMedGoogle Scholar
  2. Crispino JD: GATA1 in normal and malignant hematopoiesis. Semin Cell Dev Biol. 2005, 16: 137-147. 10.1016/j.semcdb.2004.11.002.View ArticlePubMedGoogle Scholar
  3. Greene ME, Mundschau G, Wechsler J, McDevitt M, Gamis A, Karp J, Gurbuxani S, Arceci R, Crispino JD: Mutations in GATA1 in both transient myeloproliferative disorder and acute megakaryoblastic leukemia of Down Syndrome. Blood Cells Mol Dis. 2003, 31: 351-356. 10.1016/j.bcmd.2003.08.001.View ArticlePubMedGoogle Scholar
  4. Wechsler J, Greene M, McDevitt MA, Anastasi J, Karp JE, Le Beau MM, Crispino JD: Acquired mutations in GATA1 in the megakaryoblastic leukemia of Down Syndrome. Nat Genet. 2002, 32: 148-152. 10.1038/ng955.View ArticlePubMedGoogle Scholar
  5. Zipursky A: Transient leukaemia–a benign form of leukaemia in newborn infants with trisomy 21. Br J Haematol. 2003, 120: 930-938. 10.1046/j.1365-2141.2003.04229.x.View ArticlePubMedGoogle Scholar
  6. Kuhl C, Atzberger A, Iborra F, Nieswandt B, Porcher C, Vyas P: GATA1-mediated megakaryocyte differentiation and growth control can be uncoupled and mapped to different domains in GATA1. Mol Cell Biol. 2005, 25: 8592-8606. 10.1128/MCB.25.19.8592-8606.2005.PubMed CentralView ArticlePubMedGoogle Scholar
  7. Li Z, Godinho FJ, Klusmann JH, Garriga-Canut M, Yu C, Orkin SH: Developmental stage-selective effect of somatically mutated leukemogenic transcription factor GATA1. Nat Genet. 2005, 37: 613-619. 10.1038/ng1566.View ArticlePubMedGoogle Scholar
  8. Muntean AG, Crispino JD: Differential requirements for the activation domain and FOG-interaction surface of GATA-1 in megakaryocyte gene expression and development. Blood. 2005, 106: 1223-1231. 10.1182/blood-2005-02-0551.PubMed CentralView ArticlePubMedGoogle Scholar
  9. Muntean AG, Ge Y, Taub JW, Crispino JD: Transcription factor GATA-1 and Down Syndrome leukemogenesis. Leuk Lymphoma. 2006, 47: 986-997. 10.1080/10428190500485810.View ArticlePubMedGoogle Scholar
  10. Hollanda LM, Lima CS, Cunha AF, Albuquerque DM, Vassallo J, Ozelo MC, Joazeiro PP, Saad ST, Costa FF: An inherited mutation leading to production of only the short isoform of GATA-1 is associated with impaired erythropoiesis. Nat Genet. 2006, 38: 807-812. 10.1038/ng1825.View ArticlePubMedGoogle Scholar
  11. Alford KA, Slender A, Vanes L, Li Z, Fisher EM, Nizetic D, Orkin SH, Roberts I, Tybulewicz VL: Perturbed hematopoiesis in the Tc1 mouse model of Down Syndrome. Blood. 2010, 115: 2928-2937. 10.1182/blood-2009-06-227629.PubMed CentralView ArticlePubMedGoogle Scholar
  12. Calligaris R, Bottardi S, Cogoi S, Apezteguia I, Santoro C: Alternative translation initiation site usage results in two functionally distinct forms of the GATA-1 transcription factor. Proc Natl Acad Sci U S A. 1995, 92: 11598-11602. 10.1073/pnas.92.25.11598.PubMed CentralView ArticlePubMedGoogle Scholar
  13. Halsey C, Tunstall O, Gibson B, Roberts I, Graham G: Role of GATA-1s in early hematopoiesis and differences between alternative splicing in human and murine GATA-1. Blood. 2010, 115: 3415-3416. 10.1182/blood-2010-02-267930.View ArticlePubMedGoogle Scholar
  14. Tunstall-Pedoe O, Roy A, Karadimitris A, de la Fuente J, Fisk NM, Bennett P, Norton A, Vyas P, Roberts I: Abnormalities in the myeloid progenitor compartment in down syndrome fetal liver precede acquisition of GATA1 mutations. Blood. 2008, 112: 4507-4511. 10.1182/blood-2008-04-152967.View ArticlePubMedGoogle Scholar
  15. Gutierrez L, Nikolic T, van Dijk TB, Hammad H, Vos N, Willart M, Grosveld F, Philipsen S, Lambrecht BN: Gata1 regulates dendritic-cell development and survival. Blood. 2007, 110: 1933-1941. 10.1182/blood-2006-09-048322.View ArticlePubMedGoogle Scholar
  16. McKimmie CS, Fraser AR, Hansell C, Gutierrez L, Philipsen S, Connell L, Rot A, Kurowska-Stolarska M, Carreno P, Pruenster M: Hemopoietic cell expression of the chemokine decoy receptor D6 is dynamic and regulated by GATA1. J Immunol. 2008, 181: 8171-8181.View ArticlePubMedGoogle Scholar
  17. Shimokawa N, Nishiyama C, Nakano N, Maeda K, Suzuki R, Hara M, Fukai T, Tokura T, Miyajima H, Nakao A: Suppressive effects of transcription factor GATA-1 on cell type-specific gene expression in dendritic cells. Immunogenetics. 2010, 62: 421-429. 10.1007/s00251-010-0444-1.View ArticlePubMedGoogle Scholar
  18. Suzuki N, Suwabe N, Ohneda O, Obara N, Imagawa S, Pan X, Motohashi H, Yamamoto M: Identification and characterization of 2 types of erythroid progenitors that express GATA-1 at distinct levels. Blood. 2003, 102: 3575-3583. 10.1182/blood-2003-04-1154.View ArticlePubMedGoogle Scholar
  19. Andersson LC, Jokinen M, Gahmberg CG: Induction of erythroid differentiation in the human leukaemia cell line K562. Nature. 1979, 278: 364-365. 10.1038/278364a0.View ArticlePubMedGoogle Scholar
  20. Tetteroo PA, Massaro F, Mulder A, Schreuder-van Gelder R, von dem Borne AE: Megakaryoblastic differentiation of proerythroblastic K562 cell-line cells. Leuk Res. 1984, 8: 197-206. 10.1016/0145-2126(84)90143-7.View ArticlePubMedGoogle Scholar
  21. Bourquin JP, Subramanian A, Langebrake C, Reinhardt D, Bernard O, Ballerini P, Baruchel A, Cave H, Dastugue N, Hasle H: Identification of distinct molecular phenotypes in acute megakaryoblastic leukemia by gene expression profiling. Proc Natl Acad Sci U S A. 2006, 103: 3339-3344. 10.1073/pnas.0511150103.PubMed CentralView ArticlePubMedGoogle Scholar
  22. Ge Y, Dombkowski AA, LaFiura KM, Tatman D, Yedidi RS, Stout ML, Buck SA, Massey G, Becton DL, Weinstein HJ: Differential gene expression, GATA1 target genes, and the chemotherapy sensitivity of Down Syndrome megakaryocytic leukemia. Blood. 2006, 107: 1570-1581. 10.1182/blood-2005-06-2219.PubMed CentralView ArticlePubMedGoogle Scholar
  23. Georgopoulos K, Moore DD, Derfler B: Ikaros, an early lymphoid-specific transcription factor and a putative mediator for T cell commitment. Science. 1992, 258: 808-812. 10.1126/science.1439790.View ArticlePubMedGoogle Scholar
  24. Shivdasani RA: Molecular and transcriptional regulation of megakaryocyte differentiation. Stem Cells. 2001, 19: 397-407. 10.1634/stemcells.19-5-397.View ArticlePubMedGoogle Scholar
  25. Sakamoto H, Dai G, Tsujino K, Hashimoto K, Huang X, Fujimoto T, Mucenski M, Frampton J, Ogawa M: Proper levels of c-Myb are discretely defined at distinct steps of hematopoietic cell development. Blood. 2006, 108: 896-903. 10.1182/blood-2005-09-3846.View ArticlePubMedGoogle Scholar
  26. Matsumura I, Tanaka H, Kawasaki A, Odajima J, Daino H, Hashimoto K, Wakao H, Nakajima K, Kato T, Miyazaki H, Kanakura Y: Increased D-type cyclin expression together with decreased cdc2 activity confers megakaryocytic differentiation of a human thrombopoietin-dependent hematopoietic cell line. J Biol Chem. 2000, 275: 5553-5559. 10.1074/jbc.275.8.5553.View ArticlePubMedGoogle Scholar
  27. Pearson-White S, Deacon D, Crittenden R, Brady G, Iscove N, Quesenberry PJ: The ski/sno protooncogene family in hematopoietic development. Blood. 1995, 86: 2146-2155.PubMedGoogle Scholar
  28. Ueki N, Zhang L, Hayman MJ: Ski negatively regulates erythroid differentiation through its interaction with GATA1. Mol Cell Biol. 2004, 24: 10118-10125. 10.1128/MCB.24.23.10118-10125.2004.PubMed CentralView ArticlePubMedGoogle Scholar
  29. Teichler S, Illmer T, Roemhild J, Ovcharenko D, Stiewe T, Neubauer A: MicroRNA29a regulates the expression of the nuclear oncogene Ski. Blood. 2011, 118: 1899-1902. 10.1182/blood-2010-09-306258.View ArticlePubMedGoogle Scholar
  30. Ritter M, Kattmann D, Teichler S, Hartmann O, Samuelsson MK, Burchert A, Bach JP, Kim TD, Berwanger B, Thiede C: Inhibition of retinoic acid receptor signaling by Ski in acute myeloid leukemia. Leukemia. 2006, 20: 437-443. 10.1038/sj.leu.2404093.View ArticlePubMedGoogle Scholar
  31. Nomura T, Khan MM, Kaul SC, Dong HD, Wadhwa R, Colmenares C, Kohno I, Ishii S: Ski is a component of the histone deacetylase complex required for transcriptional repression by mad and thyroid hormone receptor. Genes Dev. 1999, 13: 412-423. 10.1101/gad.13.4.412.PubMed CentralView ArticlePubMedGoogle Scholar
  32. Quintas-Cardama A, Santos FP, Garcia-Manero G: Histone deacetylase inhibitors for the treatment of myelodysplastic syndrome and acute myeloid leukemia. Leukemia. 2011, 25: 226-235. 10.1038/leu.2010.276.View ArticlePubMedGoogle Scholar
  33. Alitalo R: Induced differentiation of K562 leukemia cells: a model for studies of gene expression in early megakaryoblasts. Leuk Res. 1990, 14: 501-514. 10.1016/0145-2126(90)90002-Q.View ArticlePubMedGoogle Scholar

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© Halsey et al.; licensee BioMed Central Ltd. 2012

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/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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