Canonical Wnt signaling in megakaryocytes regulates proplatelet formation

The Wingless (Wnt) family of secreted glycoproteins regulates diverse biologic processes, from embryonic development through to aspects of adult homeostasis and disease. The Wnt signaling pathways comprise 19 distinct Wnt ligands, a host of extracellular Wnt-modulating proteins and at least 10 members of the 7 transmembrane domain-containing Frizzled (FZD) receptor family.¹  After ligand-receptor binding, multiple pathways and downstream events are triggered in a context specific manner. The most studied Wnt signaling pathway, the canonical pathway, is mediated by the stabilization and nuclear translocation of β-catenin (see Figure 1A). Under unstimulated conditions, β-catenin is phosphorylated by casein kinase 1 (CK1) and glycogen synthase kinase-3β (GSK3β) in the axin/APC destruction complex, which tags β-catenin for ubiquitination and degradation. Stimulation with a canonical Wnt ligand (such as Wnt3a) inhibits this process, stabilizing cytoplasmic β-catenin which then migrates to the nucleus. There, it acts as a transcriptional coactivator in complex with transcription factors, such as T-cell factor/lymphoid enhancer factor (TCF/LEF) family members to regulate gene expression. The canonical Wnt pathway inhibitor dickkopf-1 (DKK1) binds to low-density lipoprotein receptor-related protein 5/6 (LRP5/6) and prevents signal transduction from occurring. Multiple “noncanonical” Wnt signaling pathways also exist.²  Although these pathways all function in a β-catenin independent manner, there is an interplay between canonical and noncanonical signaling in some contexts.^3,4 

Recently, Wnt signaling has been implicated in the development^5-7  and function of mature blood cells.^8,9  These have focused predominantly on the regulation of hematopoietic stem cell (HSC) function and T-cell development. Other effects of Wnt signaling on myeloid differentiation have been observed, yet its contribution to megakaryopoiesis and platelet formation remains unexplored.

We previously identified a role for the canonical Wnt signaling pathway in the regulation of platelet function,¹⁰  with Wnt3a modulating platelet adhesion and suppressing platelet activation to multiple platelet agonists (thrombin, collagen, ADP). More recently, noncanonical Wnt signaling via Wnt5a has also been described in platelets.¹¹  Whether the elements of Wnt signaling are expressed and functional in MKs is unknown, although roles for GSK3β have been proposed in MK development.^12,13  MKs differentiate from HSCs through a regulated hierarchy of changes in gene and receptor molecule expression, polyploidization, and cytoplasmic maturation. During differentiation, maturing MKs migrate from the osteoblastic niche to the vascular niche^14,15  where they extend cytoplasmic protrusions known as proplatelets into sinusoidal blood vessels, from which platelets are ultimately released in the circulation.^16-19  As several Wnts are expressed in hematopoietic niches,⁷  MKs probably encounter an array of Wnt ligands during this maturation process.

Here, we demonstrate that canonical and noncanonical Wnt signaling pathways are present and functional in MKs, and that Wnt signaling is essential for MK proliferation and maturation, and profoundly stimulate proplatelet formation from the mature MK.

CHRF288-11 cells were cultured in RPMI 1640, 10% fetal calf serum, 2mM l-glutamine in a humidified incubator with 5% CO₂. For Wnt treatments, cells (10⁶/mL) were cultured in serum free medium for 16 hours before treatment with recombinant mouse Wnt3a, Wnt5a or DKK1 (R&D Systems) at the stated doses. For protein analysis, the cells (which become weakly adherent after serum starvation) were gently scraped from the wells and washed twice in ice cold phosphate buffered saline (PBS). The cell pellet was then resuspended in PBS and lysed by addition of 2× reducing buffer (2% sodium dodecyl sulfate, 10% glycerol, 50mM dithiothreitol, 45mM Tris-HCl (pH 6.8), 0.1 g/L bromophenol blue). Subcellular fractionation was performed using the QProteome subcellular fractionation kit (Qiagen) following the manufacturer's instructions.

For RNA preparation, cells (10⁶/mL) were cultured in serum free medium for 16 hours before treatment with recombinant Wnt3a (150 ng/mL), Wnt5a (1200 ng/mL) or both Wnt3a and 5a in combination. Cells were collected as described above, lysed in 200 μL Trizol reagent (Invitrogen) and prepared according to the manufacturer's instructions.

MK cDNA was prepared as previously described²⁰  and analyzed using the Wnt signaling pathway PCR array (SABiosicences). Transcripts with a cycle threshold (C_t) value less than 35 were determined to be “present” in MKs, as per the manufacturer's instructions. The microarray data for in vitro differentiated MKs is available as supplemental material to Watkins et al.²¹ 

Western blotting was carried out as previously described.²²  Briefly, protein lysates were separated on an 8% to 20% gradient gel (Thermo), transferred to a nitrocellulose membrane and β-catenin was detected using mouse monoclonal antibodies (12F7, Santa Cruz or 610154, Millipore). Monoclonal antibodies against PTH2 (TIP39; [Z-24] sc-134089, Santa Cruz), EPAS1 (HIF-2; NB100-132, Novus Biologicals) and LRRC32 (GARP; IMG-6354A Imgenex) were also used where indicated. Where appropriate, blots were stripped using Restore Western stripping reagent (Thermo Scientific) and probed using anti-GAPDH (ab9485, Abcam) to ensure equal loading.

Total RNA (500 ng) was amplified using the Illumina Total Prep RNA amplification kit (Applied Biosystems) according to the manufacturer's instructions. The biotinylated cRNA (1500 ng per sample) was applied to Illumina HumanWG-6 v3 expression bead chips and hybridized overnight at 58°C. Chips were washed, detected, and scanned according to the manufacturer's instructions and the scanner output imported into BeadStudio Version 3 software (Illumina). Statistical analysis of the data were performed using the lumi package²³  for Bioconductor/R (www.r-project.org). Differentially expressed genes were identified as those showing > 1.5-fold change in expression relative to the control (untreated) sample with an adjusted P value < .005. Raw data have been deposited in the GEO database (accession no. GSE42071).

mRNA was reverse transcribed to cDNA in a reaction primed by oligo(dT)^12-18  using Superscript III following the manufacturer's protocols (Invitrogen). cDNA was diluted to the equivalent of 1 ng of input total RNA per reaction and amplified in 40 cycles of PCR on a Stratgene MX3000P using TaqMan Gene Expression probes and primers, following the manufacturer's instructions (Applied Biosystems). The assay IDs were as follows: endothelial PAS (PER-ARNT-SIM) domain containing protein 1 (EPAS1, Hs01026142_m1), glycoprotein A repetitions predominant (GARP/LRRC32, Hs00194136_m1), parathyroid hormone 2 (PTH2, Hs01094670_g1), vasohibin 1 (VASH1, Hs00208609_m1), and glyceraldehyde 3-phosphate dehydrogenase (GAPDH, Hs99999905_m1). C_t values were normalized to GAPDH to allow comparison between samples.

Littermate wild-type (WT) and LRP6^−/− mouse²⁴  fetuses were isolated between embryonic days 13 and 15 in accordance with guidelines approved by the Children's Hospital, Boston, animal care and use committee and the IACUC (protocol No. 08-05-1152). Single-cell suspensions, prepared by successive passage through 22- and 25-gauge needles, were cultured in Dulbecco modified Eagle medium (Gibco BRL) supplemented with 10% fetal bovine serum albumin, 2mM L-glutamax, 50 U/mL penicillin, 50 μg/mL streptomycin, and 0.1% tissue culture supernatant from a fibroblast cell line engineered to secrete recombinant human thrombopoietin (TPO).²⁵  Between days 4 and 6, these fetal liver cultures contained 50% to 60% acetylcholinesterase-positive cells. TPO was added only at the initiation of liquid cultures.²⁶  On the third day of MK culture, cells were placed on a 1.5% to 3.0% albumin step gradient and sedimented²⁷  to obtain enriched populations of MKs in the pellet. MKs homogeneity was verified before treatment, analyzed by MK/platelet-specific markers. The cultures were 97% positive for GPIIbIIIa and 87% positive for GPIX (data not shown). MKs were then resuspended in Dulbecco modified Eagle medium with 10% fetal bovine serum albumin, 1% antibiotic, and 0.1 μg/mL recombinant human TPO alone, and in the presence of Wnt3a or Wnt5a ± 5 μg/mL DKK1, and cultured at 37°C and 5% CO₂ before analysis.

MK cultures were examined on day 5 by phase contrast microscopy using a Nikon eclipse TS100 benchtop microscope (Nikon Instruments) at 40× magnification, digital images were collected on a Hamamatsu C2400 CCD camera (Hamamatsu) and analyzed using ImageJ Version 1.42q software. Mature MKs were identified by size (> 10 μm diameter) and distinguished from proplatelet-producing MKs because of the presence or absence of long proplatelet elongations (circularity ≥ 0.7). Our laboratory has invested a large effort to identify methods to quantitate proplatelet production. We recently established that round MKs do not adhere to coverslips at the same rate as proplatelet-producing MKs, leading to inaccurate quantitation with immunofluorescence microscopy. Thus, we focused our efforts on a live cell assay. For quantification of the percentage of proplatelet-producing MKs, 10 representative pictures were taken at 40× magnification per sample, and 4 separate samples were analyzed per condition tested. An average number of ∼35 cells were counted per sample and categorized as either round MKs or proplatelet-producing MKs. Quantifications from sample replicates were pooled such that ∼ 140 cells were counted in total per condition tested. Total cell counts were comparable across all conditions tested. Statistical significance was determined by 1-way ANOVA followed by Dunnett multiple comparison test to compare test samples with the control experiments.

Mouse fetal livers were prepared as previously described, and single-cell suspensions were cultured for 4 days either alone or in the presence of Wnt3a (600 ng/mL), Wnt5a (600 ng/mL), or DKK1 (5 μg/mL). Round MKs were then placed on a 1.5% to 3.0% albumin step gradient, sedimented, and resuspended in 100 μL citrate buffer (40mM Na-Citrate pH 7.4, 0.25mM sucrose). Coloring buffer (400 μL; 0.5% NP-40, 0.5mM EDTA) supplemented with 0.5 mg/mL RNase A and 20 μg/mL propidium iodide were added to the MK suspension and cells were measured for ploidy by flow cytometry (FACSCalibur, Becton Dickinson). Experiments were performed in triplicate. Error bars represent ± 1 SD.

To determine the specific components of the Wnt signaling pathway present in human MKs differentiated from umbilical cord blood-derived CD34⁺ progenitor cells, we used data from our previously published microarray analyses of the MK transcriptome and other mature blood cell lineages.^21,22  Transcripts encoding the main components of the canonical and several components of the noncanonical Wnt signaling effectors were present in MKs (supplemental Figure 1, available on the Blood Web site; see the Supplemental Materials link at the top of the online article). These were confirmed using a PCR array specific for the Wnt signaling pathway (Figure 1B). Of note, DKK1, disheveled-associated activator of morphogenesis 1 (DAAM1), NEMO-like kinase (NLK), prickle-like protein 1 (PRICKLE1), and Van Gogh-like 1 and 2 (VANGL1, VANGL2) were identified as having MK-restricted expression in our previous microarray studies (Figure 1C).²¹  Together these analyses confirm that the main components of the canonical pathway are expressed in MKs, along with several noncanonical pathway components.

We investigated the function of the Wnt signaling pathway using the CHRF288-11 cell line as a model for MKs.^28,29  When treated with Wnt3a for 24 hours, at doses between 50 and 800 ng/mL, β-catenin accumulation was observed in whole cell lysates, with a maximal effect observed at 150 ng/mL (Figure 2A). The response to Wnt3a (150 ng/mL) was time-dependent (Figure 2B), with an increase in β-catenin abundance after 1 hour and the response peaking after 8 hours. Analysis of the subcellular fractions of the CHRF288-11 cells showed that the canonical Wnt signal caused β-catenin to accumulate not only in the nucleus, but also in the cytoplasmic, membrane, and cytoskeletal fractions of the cell in a time-dependent manner (Figure 2C), indicating that β-catenin's activity in MKs may not limited to the regulation of gene expression. Again, β-catenin accumulation reached a maximum at 8 hours, after which a slight reduction was observed in the cytoplasm and nucleus, and a complete reduction in the membrane fraction. In contrast, β-catenin continued to accumulate in the cytoskeletal fraction over time. Nuclear accumulation of β-catenin suggests that it may function in its traditional role as a transcriptional regulator. Consistent with the observations of Soda et al in the TPO/UT7 cell line,¹³  we observed a detectable level of nuclear β-catenin in the untreated cell, indicating that there may be a minimal level of endogenous Wnt signaling in operation in these cells. Interestingly, costimulation of the noncanonical Wnt signaling pathway with low amounts of Wnt5a (50 ng/mL) inhibited the Wnt3a-mediated accumulation of β-catenin, suggesting that in MKs there may be crosstalk between these 2 pathways (Figure 2D). Inhibition by Wnt5a was also dose responsive, with maximal inhibition observed when Wnt3a-treated cells (150 ng/mL) were coincubated with higher doses of Wnt5a (600 and 1200 ng/mL). The canonical Wnt antagonist, DKK1, also showed a dose-dependent inhibition of Wnt3a-mediated β-catenin accumulation, confirming that the signaling observed is dependent on a canonical mechanism (Figure 2E).

To determine whether Wnt3a and Wnt5a could elicit a transcriptional response in CHRF288-11 cells, we performed whole genome microarray analysis of cells treated with Wnt3a (150 ng/mL) or Wnt5a (1200 ng/mL), doses that we showed above induced or inhibited cellular β-catenin accumulation, respectively. To determine whether the crosstalk between the 2 ligands regulates gene transcription, we analyzed the transcriptional response of the cells when coincubated with both Wnt3a and Wnt5a. These studies identified that both Wnt3a and Wnt5a regulate the expression of a small number of genes in these cells (Figure 3A, supplemental Table 1), and revealed distinct, overlapping and antagonistic effects of Wnt3a and Wn5a.

Using a cut-off of 1.5-fold change in gene expression with an adjusted P value less than .005, 36 genes were identified, which responded positively or negatively to treatment with Wnt3a, Wnt5a, or a combination of the 2 (supplemental Table 1). Cluster analysis identified distinct patterns of Wnt responses among these genes (Figure 3A), several of which are known to be responsive to Wnt3a in other cells, including hypoxia inducible factor 2α/Hif2α (EPAS1),³⁰  monocyte to macrophage differentiation factor (MMD),³¹  sprouty homologue (SPRY),³¹  ephrin B1 (EFNB1),³² TMEM2,³¹  and TMEM158.³³  Of note is the observation that the platelet receptor, LRRC32 (also known as GARP)^22,34  was up-regulated after Wnt3a treatment. To date there has been little characterization of the genes regulated by Wnt5a. Here we show several genes respond to this noncanonical Wnt signal, including Vasohibin-1 (VASH1).

Consistent with the observations in Figure 2, many of the genes up-regulated by Wnt3a, including EPAS1, were inhibited by coincubation with Wnt5a. Others, including LRRC32, were unaffected. Conversely, all genes up-regulated by Wnt5a were either unaffected by coincubation with Wnt3a, or, as in the case of parathyroid hormone 2 (PTH2), were up-regulated by both. Several genes were found to be down-regulated by Wnt5a (> 1.5-fold); for most of these genes, weak down-regulation (< 1.5-fold) was also observed in the Wnt3a treated samples.

The microarray expression patterns for EPAS1 (Wnt3a up-regulated, inhibited by Wnt5a), VASH1 (Wnt5a up-regulated), and LRRC32 (Wnt3a up-regulated, not inhibited by Wnt5a) were replicated by RT-PCR (Figure 3B), and in the case of EPAS1 and LRRC32, by Western blotting (Figure 3C). In the case of LRRC32, up-regulation of the protein in response to Wnt3a appeared to be inhibited by Wnt5a, whereas the mRNA expression was unchanged. The expression pattern for PTH2, which was up-regulated in response to Wnt3a and Wnt5a, was confirmed at the protein level in both CHRF cells (Figure 3C) and in MKs derived from murine fetal liver (Figure 3D-F). Elevated β-catenin levels were also observed in response to Wnt signaling in these primary cells (Figure 3E-F). We also examined global gene expression in human cord blood derived MKs and found that the majority of genes regulated by Wnt signaling in the CHRF-288-11 cell line are also similarly regulated in response to Wnt signaling in primary MKs (supplemental Figure 2).

To establish the importance of canonical Wnt signaling in MK maturation, fetal liver megakaryopoiesis from LRP6^−/− mice was compared with WT littermate controls. LRP6^−/− mice are embryonic lethal and frequently die during late gestation (E15-E18), reflecting the predominant role of this receptor in transducing canonical Wnt signaling in embryonic development.²⁴  Mouse fetal liver cells were isolated on embryonic day 13 and cultured in the presence of TPO to direct MK differentiation. Interestingly, LRP6^−/− fetal liver cells generated significantly fewer MKs in culture (Figure 4A-C) and these were of lower ploidy (Figure 4D) than WT control fetal liver cells (Figure 4B-D). These results demonstrate a role for canonical Wnt signaling through LRP6 for MK maturation in culture. LRP6^+/− embryos, by comparison, develop normally and circulating blood counts are not affected in adult mice, suggesting that a single copy of this gene is sufficient for normal hematopoietic development (data not shown). LRP5^−/− mice have a WT phenotype,³⁵  further underscoring the importance of LRP6 signaling in hematopoietic stem-cell development.

MKs generate platelets by remodeling their cytoplasm into long proplatelet extensions, which serve as assembly lines for platelet production. To establish which Wnt signaling factors are involved in this process, we analyzed the effect of Wnts on proplatelet production in a mouse fetal liver MK model (Figure 5A). Wnt3a was shown to significantly (P < .05) increase the number of MKs extending proplatelets at all concentrations tested, from a mean of 62% ± 6.7% (mean ± SD) in untreated to 80.75% ± 7.1%, 87.6% ± 6.02%, and 90.33% ± 3.78% when treated with 150 ng/mL, 600 ng/mL, and 1200 ng/mL Wnt3a, respectively. Representative data from control and Wnt3a treated samples are shown in panels 5B and 5C, respectively. The canonical antagonist DKK1 had no independent effect on proplatelet formation at 5 μg/mL (52.67% ± 12%), but did ablate the effect of Wnt3a (600 ng/mL), reducing the number of MKs extending proplatelets to levels observed in control samples (53.3% ± 16.2%; Figure 5A-D). The finding that Wnt3a can promote proplatelet formation coupled with the fact that this response can be abrogated by DKK1, demonstrate that canonical Wnt signaling controls proplatelet formation ex vivo and represents the first identification of extrinsic regulators of proplatelet formation.

We previously demonstrated a role for canonical Wnt signaling in the regulation of platelets, acting to inhibit activation.¹⁰  Here we demonstrate for the first time the presence and functional effects of the Wnt signaling pathways in MKs and identify the Wnt ligands Wnt3a and DKK1 as extrinsic regulators of proplatelet formation.

Wnt signaling has been found to regulate the formation and function of several blood-cell lineages and of hematopoietic progenitors. Indeed, Scheller et al have shown that constitutive activation of β-catenin in the hematopoietic system of the mouse blocked multilineage differentiation of HSCs resulting in severe anemia, thrombocytopenia, and a decrease in bone marrow cellularity.³⁶  Deletion of β-catenin in the hematopoietic system, by comparison, was shown to result in no defects, possibly because of compensation by other catenin family members.³⁷  Although the constitutive expression of β-catenin in HSCs inhibits the generation of all hematopoietic lineages, it is unclear what role the Wnt pathway plays in later stages of MK differentiation and proplatelet formation.

Through gene expression analyses of in vitro differentiated human MKs we identified the presence of key components of the canonical Wnt signaling pathway, as well as several components of the noncanonical pathway. Consistent with our observations in platelets,¹⁰  the transcript encoding the FZD6 receptor was expressed in MKs. Several additional FZD receptors were detected by either microarray or RT-PCR approaches, suggesting that MKs may be responsive to instruction from a variety of Wnt signals. Beyond the receptor, components of the axin/APC destruction complex were detected at the transcript level. Several transcripts encoding noncanonical Wnt signaling proteins, including NLK, DAAM1, VANGL2, and PRICKLE1, were found. Intriguingly, several of these latter transcripts were among the most MK-specific compared with purified populations of erythroblasts²²  or other blood cells.²¹  MKs also express the noncanonical Wnt11 and Wnt5b, and the transcript encoding canonical antagonist, DKK1. It is possible that these proteins may be secreted from MKs and function in an autocrine or paracrine manner, modulating MK development or influencing other cells within the hematopoietic niche.⁷ 

These observations support a potential role for Wnt signaling in MK development and platelet formation, in addition to platelet function. To explore this, we used the recombinant ligands Wnt3a, Wnt5a, and DKK1 to investigate Wnt signaling in MKs. First, we established time and dose-dependent canonical Wnt signaling in MKs, using the human cell line CHRF288-11. This cell line is a model for studies of MK differentiation and gene expression patterns,²⁹  and expresses Wnt signaling components at levels that are similar to that of MKs differentiated from CD34⁺ HPCs (supplemental Figure 1). Furthermore, in this model Wnt3a signaling was inhibited by Wnt5a, which acts as an antagonist of canonical Wnt signaling in human embryonic kidney 293 cells³⁸  and HSCs.³⁹  Similarly Wnt3a and Wnt5a have antagonistic roles in the development of HSCs into early lymphoid cells.⁴ 

Whole genome microarray analysis was used to further explore the role of Wnt signaling in the regulation of MKs, and the functional interaction between Wnt3a and Wnt5a signaling pathways. The canonical and noncanonical Wnt signaling pathways appear to play overlapping, diverse, and antagonistic roles in the regulation of gene expression in megakaryocytic cells, which may contribute to MK differentiation and maturation. Indeed, many of the “Wnt responsive” genes have known roles in hematopoiesis and megakaryopoiesis, suggesting that Wnt ligands and signaling pathways may modulate MK differentiation or commitment in vivo.

Several known Wnt3a responsive genes including EPAS1³⁰  showed increased expression after Wnt3a treatment. EPAS1, also known as hypoxia inducible factor 2α (HIF2α), is essential for normal blood development in mice, with EPAS1 deficient mice displaying pancytopenia.⁴⁰  As with the antagonism between Wnt3a and Wnt5a observed at the level of β-catenin stabilization, the increase in expression of EPAS1 induced by Wnt3a was abrogated in the presence of Wnt5a. In contrast, the Wnt3a induction of the transcript encoding the recently identified platelet receptor LRRC32 (GARP)²²  was not inhibited by Wnt5a coincubation. By Western blotting however, a modest increase in LRRC32 expression was detected with Wnt3a, whereas a substantial decrease in expression was observed with Wnt5a. Thus, LRRC32 may be regulated at multiple levels by Wnt5a and Wnt3a independently. (This leucine-rich repeat receptor is important for the development of regulatory T-cells,⁴¹  and as demonstrated in a recent zebrafish morpholino knockdown model, has a role in thrombocyte adhesion and thrombus formation.³⁴  LRRC32 is also engaged in tethering TGF-β at the cell surface⁴²  and may in part explain known interactions between the WNT and TGF signaling pathways⁴³ ).

Several genes were uniquely up-regulated in response to Wnt5a, including VASH1, an inhibitor of VEGF and hypoxia induced angiogenesis.⁴⁴  Wnt5a also reduced the expression of several transcription factors known to be involved in MK differentiation and/or hematopoiesis, including GFI1B and CEBPB. PTH2, up-regulated in response to both Wnt3a and Wnt5 independently, may be analogous to its homologue PTH, which is known to facilitate the interaction between HSCs and the osteoblastic niche.⁴⁵ 

To further investigate the role of Wnt signaling in megakaryopoiesis, we examined fetal liver cells from LRP6^−/− mice. LRP6^−/− embryos exhibit severe developmental defects consistent with a significant reduction in canonical Wnt signaling.²⁴  LRP6^−/− mice die at birth, prohibiting the analysis of adult hematopoiesis, although peripheral blood counts from adult heterozygous LRP6^+/− mice showed no hematopoietic defect (data not shown). Thus, we isolated embryonic fetal liver cells from the mice to investigate MK development ex vivo. The LRP6^−/− cells generated 5-fold fewer MKs than LRP6^+/+ cells. Of the few MKs which developed from the LRP6^−/−, significantly fewer reached higher levels of ploidy (16N, 32N). Although it is probable that total hematopoiesis, and not just megakaryopoiesis, is affected, these data confirm a defect in MK maturation in these mice. Proplatelet formation was observed in some of the LRP6^−/− MKs, although given the low frequency of MKs in these cultures, the effect of LRP6 knockout on the frequency of proplatelet formation was difficult to assess. Our results suggest that LRP6-dependent canonical Wnt signaling is required for MK proliferation and maturity, but is not essential per se for MK commitment. We note that a lower level of canonical Wnt signaling is still present via the LRP5 receptor, although its contribution alone is not sufficient for most embryonic developmental processes.

Wnt signaling was shown to be critical for the regulation of cell shape and polarity, specifically in the formation of protrusive structures from migrating cells, including neurite outgrowth.⁴⁶  Because the LRP6^−/− culture model did not allow accurate assessment of late MK differentiation and proplatelet formation, we used WT fetal liver cultures to assess the contribution of exogenous canonical and noncanonical Wnt signals to proplatelet formation. Strikingly, Wnt3a increased the number of mouse fetal liver primary MKs displaying proplatelets. This effect was completely inhibited by DKK1, consistent with a role for canonical Wnt signaling in proplatelet formation. Wnt5a showed no significant effect on proplatelet formation, suggesting that Wnt is mediating this effect solely through the canonical pathway. Although identification of the specific mechanisms underlying this process are beyond the scope of this paper, Wnt signaling regulates actin cytoskeleton and microtubule assembly and stabilization in different cell types,^47,48  which are key steps in the formation of proplatelets.^17,49,50  Furthermore, it has been demonstrated that constitutive activation of αIIbβ3–mediated outside-in signaling in human MKs negatively influences proplatelet formation.⁵⁰  As we have previously shown that Wnt3a functions in both human and mouse platelets to inhibit αIIbβ3–mediated outside-in signaling,¹⁰  we can hypothesize that Wnt3a may be driving proplatelet formation in MKs by inhibiting αIIbβ3–mediated outside-in signaling.

Although the exact function of Wnt signaling in hematopoiesis is complex and not yet fully understood, it is clear that during their differentiation hematopoietic cells are exposed and respond to a multitude of Wnt ligands.⁷  Here, we have demonstrated that Wnt signals specifically regulate the expression of known MK and hematopoietic genes in vitro, and modulate MK proliferation, maturation, and proplatelet formation ex vivo. Taken together, these data reveal a novel regulatory pathway in megakaryopoiesis, and offer the first insights into the exogenous regulation of platelet formation in the mature megakaryocyte.

This work was supported by grants and fellowships provided by the Science Foundation Ireland (P.B.M., 10/IN.1/B3012); the Irish Research Council for Science, Engineering, and Technology (I.C.M., PD/2008/33), the Program for Research in Third-Level Institutions, administered by the Higher Education Authority of Ireland (D.J.F. and P.B.M.), the National Institute for Health Research, United Kingdom (P.B. and N.A.W.), and National Institutes of Health (NIH) Grant HL68130 (J.E.I.) and GM74241 (X.H.). J.E.I. is an American Society of Hematology Junior Faculty Scholar. J.N.T. is an American Society of Hematology Scholar. M.R.T. is a Marie Curie Intra-European Fellow (237296).

National Institutes of Health

Contribution: I.C.M., J.N.T., M.R.T., B.T.M., X.H., D.J.F., J.E.I., and P.B.M. designed research; I.C.M., J.N.T., M.R.T., B.M.S., B.T.M., G.M., P.B., V.S., R.P.M., and C.B. performed experiments; I.C.M., J.N.T., M.R.T., B.T.M., B.M.S., G.M., A.R., R.P.M., N.A.W., J.E.I., and P.B.M. analyzed data; and I.C.M., J.N.T., J.E.I. and P.B.M. wrote the paper.

Conflict-of-interest disclosure: The authors declare no competing financial interests.

Correspondence: Patricia B. Maguire, School of Biomolecular and Biomedical Science, UCD Conway Institute, University College Dublin, Belfield, Dublin 4, Ireland; e-mail: patricia.maguire@ucd.ie.