Phc2 controls hematopoietic stem and progenitor cell mobilization from bone marrow by repressing Vcam1 expression

Bae, Joonbeom; Choi, Sang-Pil; Isono, Kyoichi; Lee, Ji Yoon; Park, Si-Won; Choi, Chang-Yong; Han, Jihye; Kim, Sang-Hoon; Lee, Han-Hyoung; Park, Kyungmin; Jin, Hyun Yong; Lee, Suk Jun; Park, Chung-Gyu; Koseki, Haruhiko; Lee, Young Sik; Chun, Taehoon

doi:10.1038/s41467-019-11386-4

Download PDF

Article
Open access
Published: 02 August 2019

Phc2 controls hematopoietic stem and progenitor cell mobilization from bone marrow by repressing Vcam1 expression

Joonbeom Bae¹^na1,
Sang-Pil Choi¹^na1,
Kyoichi Isono²,
Ji Yoon Lee³,
Si-Won Park¹,
Chang-Yong Choi¹,
Jihye Han¹,
Sang-Hoon Kim¹,
Han-Hyoung Lee¹,
Kyungmin Park¹,
Hyun Yong Jin⁴,
Suk Jun Lee⁵,
Chung-Gyu Park ORCID: orcid.org/0000-0003-4083-8791⁶,
Haruhiko Koseki⁷,
Young Sik Lee ORCID: orcid.org/0000-0002-6709-3809¹ &
…
Taehoon Chun ORCID: orcid.org/0000-0002-5940-8620¹

Nature Communications volume 10, Article number: 3496 (2019) Cite this article

4582 Accesses
10 Citations
1 Altmetric
Metrics details

Subjects

Abstract

The timely mobilization of hematopoietic stem and progenitor cells (HSPCs) is essential for maintaining hematopoietic and tissue leukocyte homeostasis. Understanding how HSPCs migrate between bone marrow (BM) and peripheral tissues is of great significance in the clinical setting, where therapeutic strategies for modulating their migration capacity determine the clinical outcome. Here, we identify an epigenetic regulator, Phc2, as a critical modulator of HSPC trafficking. The genetic ablation of Phc2 in mice causes a severe defect in HSPC mobilization through the derepression of Vcam1 in bone marrow stromal cells (BMSCs), ultimately leading to a systemic immunodeficiency. Moreover, the pharmacological inhibition of VCAM-1 in Phc2-deficient mice reverses the symptoms. We further determine that Phc2-dependent Vcam1 repression in BMSCs is mediated by the epigenetic regulation of H3K27me3 and H2AK119ub. Together, our data demonstrate a cell-extrinsic role for Phc2 in controlling the mobilization of HSPCs by finely tuning their bone marrow niche.

FOXO1 enhances CAR T cell stemness, metabolic fitness and efficacy

Article Open access 10 April 2024

Jack D. Chan, Christina M. Scheffler, … Phillip K. Darcy

Depleting myeloid-biased haematopoietic stem cells rejuvenates aged immunity

Article 27 March 2024

Jason B. Ross, Lara M. Myers, … Irving L. Weissman

An immunophenotype-coupled transcriptomic atlas of human hematopoietic progenitors

Article Open access 21 March 2024

Xuan Zhang, Baobao Song, … H. Leighton Grimes

Introduction

Hematopoietic stem and progenitor cells (HSPCs) are rare populations of cells that can sustain the hematopoietic system by continuously replenishing blood cells^1,2. Postnatally, most HSPCs engraft and reside in the BM niche, but a small fraction of these cells is mobilized and migrate into the peripheral blood (PB) to reconstitute the hematopoietic system under specific signaling cues^1,3,4. Therefore, identifying key regulators that critically control HSPC mobilization and understanding their underlying mechanisms have been of significant interest to facilitate BM transplantation efficiency and to therapeutically inhibit the malignant migration of the transformed hematopoietic cells into peripheral tissues⁵. Indeed, several BM niche proteins, including stem cell factor (kit ligand), CXCL12 (SDF-1α), and β1 integrin have been identified as key signaling components to control the maturation of HSPCs, their migration into the circulation and their homing to the BM by mediating the interaction between HSPCs and bone marrow stromal cells (BMSCs)^2,5,6,7. However, the molecular pathways that regulate the expression of these BM niche proteins remain unclear.

Polycomb group (PcG) proteins function as transcriptional repressors of target genes by mainly modulating histone methylation⁸. These PcG proteins can be divided into two functionally distinct complexes: polycomb repressor complex 1 (PRC1) and polycomb repressor complex 2 (PRC2). PRC2 induces the formation of trimethylated histone H3 at lysine 27 (H3K27me3) through methyltransferase activity of Ezh proteins which are component proteins in PRC2 complex⁹. The canonical PRC1 then recognizes and binds to H3K27me3 to sustain the transcriptional repression of a target gene^8,10,11. Both canonical and noncanonical PRC1 complexes can cause additional transcriptional silencing as E3 ubiquitin ligases by forming monoubiquitylated histone H2A at lysine 119 (H2AK119ub)^8,12,13.

In this study, we demonstrate that Phc2, a component of the canonical PRC1, regulates HSPC mobilization through the repression of Vcam1 expression by enhancing both H3K27me3 and H2AK119ub in BMSCs. Therefore, Phc2 deficiency causes a severe HSPC mobilization defect via the derepression of Vcam1 in BMSCs, and the pharmacological inhibition of VCAM-1 in BMSCs significantly reverses the symptoms of Phc2-deficient mice. These data demonstrate the critical cell-extrinsic role of Phc2 in controlling HSPC mobilization and provide the first evidence of epigenetic control over HSPC mobilization.

Results

Phc2 deficiency leads to a defect in HSPC mobilization

As an initial step to elucidate the functional role of Phc2 during hematopoiesis, we characterized immune phenotypes of Phc2^−/− (KO) mice¹⁴ compared to those of Phc2^+/+ (wild-type, WT) mice. We observed macroscopic abnormalities in the thymus and peripheral lymphoid organs of KO mice compared to those of WT mice. Both the thymus and spleen of the KO mice maintained normal architecture, but these organs were smaller than those of the WT mice (Fig. 1a, b). Consistent with this observation, the absolute numbers of immune cells and their precursors in the PB, thymus, spleen, and liver of the KO mice were significantly reduced compared to those of the WT mice (Tables 1 and 2, Fig. 1c). Notably, the absolute number of early T-cell precursors (ETPs) in the thymus or immature B cells in the spleen was significantly lower in the KO mice relative to the WT mice (Table 1).

Table 1 Absolute numbers of immune cells and their precursors in Phc2^+/+ and Phc2^−/− mice^a

Full size table

Table 2 Complete blood counts in Phc2^+/+ and Phc2^−/− mice^a

Full size table

Unexpectedly, the absolute numbers and relative ratios of HSPCs, early progenitor cells, and immune cells in the BM were similar among all examined mice (Table 1 and Fig. 1c, d). Additionally, the loss of Phc2 did not influence the cell cycle progression or apoptosis of HSPCs (Fig. 1e, f), and both the WT and KO BM-resident HSPCs exhibited no difference in terms of their ability to generate multipotential or myeloid progenitor cells (Fig. 1g). The absolute numbers of WT and KO B cells in the BM at each developmental stage were not significantly different either (Fig. 1h). Given that no functional defect was evident in the HSPCs of the BM but that there was a shortage of ETPs and immature B cells from the BM, we postulated that a Phc2 deficiency could lead to a systemic immunodeficiency due to a defect in HSPC migration into the circulation.

To test this hypothesis, we examined the numbers of circulating HSPCs from WT and KO mice using a colony-forming unit (CFU) assay. The absolute numbers of clonogenic progenitors in the PB and spleen were decreased by approximately half in the KO mice compared to the WT mice, whereas the absolute numbers of clonogenic progenitors in the BM were comparable between the WT and KO mice (Supplementary Fig. 1). To confirm this result, we performed in vivo HSPC mobilization assays using two commonly used mobilization regimens for therapy, granulocyte colony-stimulating factor (G-CSF) and AMD3100 (CXCR4 antagonist)^15,16,17,18. Five days after G-CSF treatment, the absolute numbers of white blood cells (WBCs) and splenocytes from the KO mice remained significantly lower than those from the WT mice (Fig. 2a, b). The spleen size of the KO mice also remained much smaller than that of the WT mice after G-CSF treatment (Fig. 2b). Consistent with these results, both the frequencies and absolute numbers of Lin⁻Sca-1⁺c-kit⁺ cells (LSK cells) in the PB and spleen were significantly lower in the KO mice than in the WT mice (Supplementary Fig. 2). Likewise, the absolute numbers of clonogenic progenitors in the PB and spleen of the KO mice were significantly reduced compared to those of the WT mice (Fig. 2c). However, the frequencies and absolute numbers of LSK cells in the BM were comparable between the WT and KO mice (Supplementary Fig. 2). Moreover, the absolute numbers of clonogenic progenitors in the BM were not significantly different between the WT and KO mice (Fig. 2c). When we used an AMD3100 as a mobilizing agent of LSK, we still observed that the migration of KO LSK into the periphery is statistically decreased compared with that of WT LSK (Fig. 2d, e). However, the defective migration of KO LSK after treatment of AMD3100 is relatively modest when we compared with results from G-CSF treatment (Fig. 2d, e).

To remove circulating HSPCs and visualize neo-HSPC mobilization from BM, we further treated WT and KO mice with 5-fluorouracil (5-FU), a chemotherapeutic agent that depletes circulating HSPCs and promotes HSPC release from BM during hematopoietic repopulation^19,20. The absolute numbers of WBCs and splenocytes recovered from KO mice were lower than those recovered from WT mice starting on day 8 after 5-FU treatment (Fig. 2f, g). The most prominent differences in the absolute numbers of WBCs and splenocytes or the size of the spleen between WT and KO mice was observed on day 16 after 5-FU treatment (Fig. 2f, g). On day 16 after 5-FU treatment, the frequency and the absolute number of recovered LSK cells and the absolute number of recovered clonogenic progenitors in the PB and spleen were significantly lower in KO mice than in WT mice, whereas those in the BM were comparable between the WT and KO mice (Fig. 2h, Supplementary Fig. 3). Taken together, these results indicate that Phc2 deficiency causes a defect in HSPC mobilization from the BM into the periphery.

Phc2 ^−/− BMSCs cause a defect in HSPC mobilization

To identify which cell type in the BM niche contributed to the defect in HSPC release into the circulation of KO mice, we adoptively transferred LSK cells isolated from WT CD45.1 mice into irradiated WT or KO CD45.2 recipient mice (Fig. 3a). KO recipients showed impaired repopulation of donor-derived immune cells in the thymus and spleen (Fig. 3b, c). However, the absolute numbers of LSK cells and lineage-committed progenitors (Lin⁻c-kit⁺ cells; LK cells) in the BM of KO recipients were comparable to those in the WT recipients (Fig. 3b–d). To confirm these observations, irradiated WT CD45.1 mice were reconstituted with LSK cells isolated from WT or KO CD45.2 mice (Fig. 3e). The origin of the donor LSK cells did not affect the repopulation of leukocytes in WT recipients (Fig. 3f, g). The origin of the donor LSK cells did not affect the absolute number of LSK cells or LK cells in the BM of WT recipients either (Fig. 3h). We also performed a serial competitive BM repopulation assay to further determine whether KO HSPCs had an intrinsic defect. We found that KO HSPCs had the same ability to reconstitute immune cells as WT HSPCs (Supplementary Fig. 4). This strongly suggests that the defect in HSPC release into the circulation in KO mice is caused by an extrinsic factor from BMSCs within BM niches.

To confirm this result, we performed an in vivo homing assay with CFSE-labeled WT and KO LSK cells. The number of CFSE⁺ LSK cells homing to the BM was higher among the KO recipients than among the WT recipients (Fig. 4a). Such an increase in the short-term migration of CFSE⁺ LSK cells into the BM of KO recipients led to fewer CFSE⁺ LSK cells homing to the PB and spleen of the KO recipients (Fig. 4a). Accordingly, the frequency of clonogenic progenitors in the BM of the KO recipients was increased, whereas the frequencies of clonogenic progenitors in the PB and spleen of the KO recipients were decreased compared to those of the WT recipients (Fig. 4b, Supplementary Fig. 5). We next measured the capacity of WT and KO LSK cells to transmigrate across their BMSCs using a trans-stromal migration assay. The number of LSK cells transmigrating across KO BMSCs was smaller than the number of LSK cells transmigrating across WT BMSCs (Fig. 4c, Supplementary Fig. 6). In contrast, the number of LSK cells adhering to KO BMSCs was greater than the number of LSK cells adhering to WT BMSCs (Fig. 4d, Supplementary Fig. 6). Collectively, these data demonstrate that an extrinsic factor from BMSCs causes HSPCs to adhere more strongly to BMSCs, ultimately leading to the defective mobilization of HSPCs from the BM into the periphery in KO mice.

PcG proteins repress Vcam1 gene expression in BMSCs

To understand the molecular mechanisms through which PcG strengthens the adhesion properties of HSPCs to BMSCs, we first investigated the compositions and architectures of BM niches in WT and KO mice and measured the expression levels of candidate genes that are known to be involved in these processes. Endothelial cells, mesenchymal stem cells, and osteoblasts are major BMSCs found in BM niches^21,22,23. Importantly, neither a change in BMSC composition nor an abnormal architecture was found in the KO BM niches (Supplementary Figs. 7 and 8). Next, we examined the expression patterns of soluble factors and cell surface molecules that might regulate HSPC mobilization in WT and KO BMSCs^2,7 (Fig. 5a, Supplementary Fig. 9). Intriguingly, both the mRNA and protein levels of VCAM-1 were significantly increased in KO BMSCs compared to WT BMSCs (Fig. 5a, b). Flow cytometry analysis further confirmed that the expression of VCAM-1 was significantly higher in KO BMSCs than in WT BMSCs (Fig. 5c). Consistent with this observation, Vcam1 mRNA levels were significantly elevated in activated KO peritoneal macrophages compared to those of WT (Supplementary Fig. 10).

Taken together, these results indicate that Phc2 may repress Vcam1 expression in BMSCs. To further examine Phc2-dependent Vcam1 repression, we knocked down Phc2 expression in BMSCs (OP9 cells) and concurrently monitored Vcam1 expression levels under treatment with TNF-α, a well-known inducer of Vcam1 transcription²⁴ (Fig. 5d). As expected, TNF-α treatment induced the expression of Vcam1 at 3 h post-treatment. However, this was significantly exacerbated when Phc2 was depleted, and thus, the VCAM-1 level was not dampened up to 12 h post-TNF-α treatment (Fig. 5e, f). Overall, these results suggest that Phc2 represses the expression of Vcam1 in BMSCs at the transcriptional level.

To demonstrate a role for Phc2 in the transcriptional repression of Vcam1, we performed a chromatin immunoprecipitation (ChIP) assay with seven primer pairs covering the putative Phc2 binding sites located in the Vcam1 gene (Fig. 6a). This analysis revealed the strong binding of Phc2 to the promoter region of the Vcam1 locus (Fig. 6b, primers #2 and #3). Interestingly, direct binding by other members of the canonical PRC1 family, such as Bmi1, Ring1b, and Cbx7, was also found around the same region covered by primers #2 and #3 (Fig. 6c). Consistent with this, Bmi1, Ring1b, and Cbx7 binding to these regions were significantly decreased in the absence of Phc2 (Fig. 6c). The acetylation of histone H3 at lysine 9/14 (H3K9ac), trimethylation of histone H3 at lysine 4 (H3K4me3), H3K27me3, and H2AK119ub were observed around the same region covered by primers #2 and #3 (Fig. 6c). H3K9ac and H3K4me3 were increased, whereas H3K27me3 and H2AK119ub were decreased in KO BM cells compared to WT BM cells (Fig. 6c). Furthermore, the treatment of BMSCs (OP9 cells) with GSK126, an Ezh2 inhibitor²⁵, led to the upregulation of Vcam1 expression in a dose-dependent manner (Fig. 6d, e and Supplementary Fig. 11). Consistent with these observations, the binding of Phc2, Bmi1, and Ring1b to the regions covered by primers #2 and #3 was decreased in GSK126-treated BMSCs (OP9 cells) (Fig. 6f).

Next, we then asked whether GSK126 treatment could mimic Phc2 deficiency in vivo. Different dose of GSK126 was administered intraperitoneally into WT mice. Sixteen hours after GSK injection, BMSCs were isolated and analyzed for VCAM-1 expression. We also measured the capacity of WT LSK cells to transmigrate across their GSK126-treated BMSCs using a trans-stromal migration assay. Results clearly showed that GSK126 treatment increased both VCAM-1 expression in BMSCs and adherence of LSKs onto BMSCs in a dose-dependent manner (Supplementary Fig. 12). Therefore, the canonical PRC1 containing Phc2 can repress Vcam1 expression through histone modifications, such as by enhancing H3K27me3 and H2AK119ub, in BMSCs.

Anti-VCAM-1 Ab treatment restores Phc2 ^−/− HSPC mobilization

Next, we examined whether blocking the interaction between VCAM-1 and VLA-4 could restore HSPC mobilization in KO mice. We first attempted to measure the mobilization capacity of WT LSK cells across KO BMSCs after treatment with neutralizing antibodies (Abs) against VCAM-1 and/or VLA-4. Treatment with either Ab restored the trans-stromal migration activity of LSK cells across KO BMSCs to a level similar to that of LSK cells across WT BMSCs (Fig. 7a). Additionally, there was no significant difference in the relative ratio of LSK cell adhesion to KO or WT BMSCs after treatment with the neutralizing Abs (Fig. 7b). The in vivo homing assay further confirmed that blocking the interaction between VCAM-1 and VLA-4 could restore LSK cell mobilization from the KO BM into the PB and spleen (Fig. 7c, d and Supplementary Fig. 13). We then tested whether treatment of the neutralizing VCAM-1 Ab could rescue steady-state HSPC mobilization in KO mice. Results clearly demonstrated that the administration of the neutralizing VCAM-1 Ab in KO mice successfully reconstitutes HSPC mobilization from BM into periphery (Fig. 7e–g).

We also performed a G-CSF-, AMD3100-, or 5-FU-induced LSK cell mobilization assay using WT and KO mice treated with the neutralizing VCAM-1 Ab. There were no significant differences in the absolute numbers of WBCs and splenocytes between the WT and KO mice treated with anti-VCAM-1 on day 5 after the G-CSF treatment and on day 16 following the 5-FU challenge (Fig. 8a, b, f, g). Similarly, the absolute number of LSK cells and the clonogenic progenitor frequency in the BM, PB, and spleen were comparable between WT and KO recipients treated with the neutralizing Ab on day 5 after the G-CSF treatment and on day 16 following the 5-FU challenge (Fig. 8c, h, Supplementary Figs. 14 and 15). Consistent with these results, the defective HSPC migration into the PB of the KO mice was reversed by treating the mice with anti-VCAM-1, as observed in the HSPC mobilization assay using AMD3100 alone or in combination with G-CSF (Fig. 8d, e and Supplementary Fig. 16).

To further reinforce these observations, we assessed the significance of VCAM-1 blockage when the migration defect of HSPCs are driven by extrinsic microenvironment which mimics the phenotype associated with Phc2 KO mice. First, we adoptively transferred LSK cells isolated from WT CD45.1 mice into irradiated WT or KO CD45.2 recipient mice and then performed the same G-CSF-induced LSK cell mobilization assay using recipient mice treated with the neutralizing VCAM-1 Ab (Supplementary Fig. 17). Consistent to the HSPC mobilization assay in KO mice, WT cells reconstituted in irradiated KO recipient cells were only partially rescued the mobilization defects when the single G-CSF agent was treated (Supplementary Fig. 17). However, the administration of the neutralizing VCAM-1 Ab in combination with G-CSF in KO recipient mice completely reconstituted WT donor HSPC mobilization from BM into periphery, the same degree to WT recipient mice (Supplementary Fig. 17). Taken together, these results demonstrate that blocking the interaction between VCAM-1 and VLA-4 can restore HSPC migration from the BM into the periphery of KO mice.

Discussion

In this study, we demonstrated that Phc2 binds to the Vcam1 locus to repress its transcription by enhancing H3K27me3 and H2AK119ub in BMSCs. In the absence of Phc2, the increased Vcam1 expression in BMSCs strengthened the interaction between HSPCs and BMSCs, compromising timely HSPC mobilization from the BM into the periphery, which in turn led to a systemic immunodeficiency. Consistent with these observations, treatment with a neutralizing Ab against VCAM-1 in Phc2-deficient mice restored HSPC mobilization from the BM into the periphery. These data firmly establish a causative role for the epigenetic regulation of VCAM-1 in regulating HSPC mobilization, as a key downstream mediator of Phc2 functions.

Recent genetic evidence from conditional VCAM-1- or VLA-4-deficient mice further supports our model of the VLA-4/VCAM-1 pathway as downstream of Phc2 function, and as expected from our results with Phc2-deficient mice overexpressing VCAM-1, VCAM-1- or VLA-4 deficient mice exhibit increased circulating progenitors and immature B cells, and impaired HSPC homing to BM^{26,27,28,29,30}. The BM homing defect of HSPCs in these mice became obvious when the mice were treated with 5-FU or G-CSF^26,27. However, the Phc2-deficient mice still displayed the migration defect of HSPCs from the BM into the periphery after treatment with these mobilization agents.

The identification of a single key mediator of Phc2 function may have important clinical implications. Similar to previous observations with conditional VCAM-1- or VLA-4-deficient mice^{26,27,28,29,30}, we found an abnormality of only steady-state HSPC mobilization in Phc2-deficient mice. Additionally, treatment with the anti-VCAM-1 Ab or anti-VLA-4 Ab in primates or mice does not cause any other physiological change^31,32. Combined evidence may suggest a dominant role for VCAM-1 in steady-state HSPC migration due to the VCAM-1 expression pattern. In steady-state conditions, the BMSC is the only cell type that constitutively expresses VCAM-1 at physiological levels, although vascular endothelial cells and other immune cell populations express minimally detectable levels of VCAM-1^{33,34,35,36,37,38}. Furthermore, with a proof-of-concept experiment, we successfully demonstrated that blocking VCAM-1 in BM niches critically reverses the HSPC mobilization defect in Phc2-deficient mice. Therefore, along with other recent data^{39,40,41,42,43}, our results suggest that modulating the interaction between VCAM-1 and VLA-4 in BM niches provides potential strategies to develop HSPC mobilizing agents or anti-leukemia drugs. Therefore, it will be interesting to observe whether a specific inhibitor that blocks Phc2 function is useful for keeping malignant cells from hematopoietic lineages within the BM.

To our knowledge, we are the first to provide evidence that a systemic immunodeficiency can be caused by a defect in a particular epigenetic regulator that represses the expression of a certain cell adhesion molecule in BMSCs. Our study also demonstrates the molecular mechanism through which the epigenetic regulation of extrinsic factors can help finely tune the interaction between HSPCs and BMSCs within BM niches during HSPC mobilization. Although several genes that are involved in hematopoiesis have been identified as targets for epigenetic regulation, the epigenetic effect on HSPC mobilization has not been elucidated. Notably, the vast majority of previously identified genes play important roles in defining the intrinsic property of HSCs and the development of leukemia^8,44,45.

Like deficiencies in other epigenetic regulators, a single PcG gene deficiency in mice mostly causes early embryonic lethality or a limited life span with severe developmental defects, including an intrinsic defect in HSCs^8,46,47. This characteristic hinders the search for additional roles of polycomb proteins in the regulation of immune phenomena aside from their known functions in HSC differentiation. Similar to other members of the PcG protein family, Phc2 is expressed in various tissues and cells and regulates the transcription of Cdkn2a (p16^INK4a and p19^ARF) and hox genes through direct associations with chromatin^8,14. However, Phc2-deficient mice are fertile and exhibit less severe defects associated with the abnormal axial skeleton and Peyer’s patch^14,48. Moreover, the systemic immunodeficiency observed in Phc2-deficient mice is not caused by an intrinsic defect in HSC function, but instead, the Phc2 deficiency causes a defect in HSPC mobilization by enhancing the expression of VCAM-1 in BMSCs. This may suggest that most of the Phc2 functions in mammals are dispensable or can be replaced by other components of the canonical PRC1 due to a structural heterogeneity of PRC1 or functional redundancy of PcG proteins. In fact, each of the mammalian PRC2 or PRC1 subunits has several paralogs^{8,9,10,11,12,13}. For example, Phc2 has two paralogs, Phc1 and Phc3^{8,9,10,11,12,13}. Previous observation revealed that Phc1 deficiency causes a defect in HSC’s self-renewal activity^49,50. Therefore, Phc1, but not phc2, might be critical for HSC maintenance and function. Consistent with this idea, the expression and epigenetic pattern of Cdkn2a (p16^INK4a and p19^ARF) in KO BM cells showed no significant differences compared to those in WT BM cells (Supplementary Fig. 18). Another example of nonredundant function by each paralog within PRC2 or PRC1 components might be found in Ezh proteins or Cbx proteins, respectively^{51,52,53,54,55}. Among Ezh proteins, Ezh1 is critical for self-renewal activity of HSCs, whereas Ezh2 is dispensable for proper HSC function^51,52. Also, Cbx7 is the only paralog which is necessary for self-renewal activity of HSC among Cbx proteins^53,54.

In our molecular model, PRC2 containing Ezh2 with methyltransferase activity initiates H3K27me3 on the Vcam1 locus in BMSCs because the Ezh2 inhibitor (GSK126) treatment of BMSCs increases the Vcam1 mRNA levels by negating the recognition of H3K27me3 by the canonical PRC1 complex containing Phc2 on the same locus. The canonical PRC1 then recognizes and binds to H3K27me3 to maintain Vcam1 gene suppression. The recognition of H3K27me3 on the Vcam1 locus by the canonical PRC1 is dependent on Phc2 expression. Consistently, we observed reductions in the binding of other canonical PRC1 components to the Vcam1 locus when Phc2 was not expressed. Our study also revealed that the H2AK119ub activity of the canonical PRC1 on the Vcam1 locus was dependent on Phc2 expression, which is consistent with a recent observation that the interaction between Bmi1 and Phc2 is critical for the H2AK119ub activity of the canonical PRC1⁵⁵.

In conclusion, the results of our study demonstrated Phc2-regulated HSPC mobilization through the direct repression of Vcam1 gene expression in BMSCs. These findings may offer a novel approach to manipulating the epigenetic patterns of genes involved in HSPC mobilization, leading to new therapeutic strategies for BM transplantation and leukemia treatment.

Methods

Experimental mice and phenotypic analysis

Phc2^+/− (Phc2 heterozygote) mice with a C57BL/6 background were used in this study¹⁴. C57BL/6 and B6 CD45.1 mice were obtained from The Jackson Laboratory. WT and KO mice were bred from Phc2^+/− mice. All animals received proper care in accordance with the National Institutes of Health Guide for the Care and Use of Laboratory Animals. The study protocol was approved by the Institutional Animal Care and Use Committee of Korea University (protocol numbers: KUIACUC-20110104-3, KUIACUC-20141002-4, and KUIACUC-20160927-3).

Cell culture

BMSCs were obtained and maintained from WT and KO mice⁵⁶. Briefly, bone marrow (BM) cells were isolated from the femurs and tibias of 8-week-old mice and cultured in Dulbecco’s modified Eagle medium (Welgene LM 001-05) supplemented with 10% fetal bovine serum (FBS; Welgene S 001–01), 10% horse serum (Welgene S 104–01), 2 mM L-glutamine (Welgene LS 002–01), 2 mM sodium pyruvate (Welgene LS 002–02), and 100 U ml⁻¹ penicillin/streptomycin (Welgene LS 202–02) at 37 °C and 5% CO₂. Non-adherent cells were removed by washing with PBS after overnight incubation. Adherent cells were cultured and fresh medium was added every 2 days. After 4 weeks of culture, cells were harvested by incubation with trypsin/EDTA (Welgene LS 015–01) for 2 min at 37 °C and plated onto culture dishes. At two weeks after the first passage, cells were harvested and cultured under the same conditions for subsequent passages (passages 2–7). OP9 BMSC line (ATCC CRL-2749) was maintained in alpha MEM (Welgene LM 008-02) supplemented with 20% FBS and 1% penicillin/streptomycin at 37 °C and 5% CO₂. For induction of VCAM-1, OP9 cells were treated with TNF-α (100 ng ml⁻¹; R&D Systems 410-MT) for the indicated time period. To inhibit Ezh activity, OP9 cells were treated with various concentrations of GSK126, an Ezh2 inhibitor (Xcessbio Biosciences M60071-2), for 48 h.

PB count, flow cytometry analysis, and cell sorting

PB samples from each mouse were collected by retro-orbital bleeding and analyzed using a Coulter LH 780 Hematology Analyzer (Beckman Coulter). For flow cytometry, single cell suspensions were prepared from the BM, PB, thymus, and spleen of each mouse. After removing red blood cells, cells were stained with MACS buffer at 4 °C in the presence of Fc Block Ab (BD Biosciences 553141, dilution 1:100). Abs purchased from BD Biosciences, Biolegend or Thermo Fisher Scientific were used to detect the following cell surface markers by flow cytometry: B220 (BD Biosciences 553090, dilution 1:100), CD3ε (Thermo Fisher Scientific 11-0031-63, dilution 1:100), CD4 (BD Biosciences 553729, dilution 1:100), CD8 (BD Biosciences 553030, dilution 1:100), CD11b (Thermo Fisher Scientific 11-0112-41, dilution 1:100), CD11c (BD Biosciences 553802, dilution 1:100), CD16:32 (Thermo Fisher Scientific 14-0161-81, dilution 1:100), CD25 (Thermo Fisher Scientific 17-0251-81, dilution 1:100), CD31 (BD Biosciences 561814, dilution 1:100), CD34 (BD Biosciences 560238, dilution 1:100), CD44 (BD Biosciences 561861, dilution 1:100), CD45 (BD Biosciences 550539, dilution 1:100), CD48 (Biolegend 103412, dilution 1:100), CD51 (BD Biosciences 551187, dilution 1:100), CD106 (BD Biosciences 553332, dilution 1:100), CD127 (Thermo Fisher Scientific 45-1271-80, dilution 1:100), CD150 (Biolegend 115922, dilution 1:100), c-kit (Thermo Fisher Scientific 17-1171-81, dilution 1:100), F4/80 (Thermo Fisher Scientific MF48004, dilution 1:100), Flt3 (Thermo Fisher Scientific 46-1351-80, dilution 1:100), IgD (BD Biosciences 562022, dilution 1:100), IgM (BD Biosciences 550676, dilution 1:100), NK1.1 (BD Biosciences 557391, dilution 1:100), and Sca-1 (BD Biosciences 558162, dilution 1:100). After washing several times with PBS, stained cells were resuspended in PBS and analyzed by flow cytometry using a FACSCalibur with CellQuest software (BD Biosciences). Analysis and sorting of HSPCs (Lin^–Sca-1⁺c-kit⁺ cells; LSK cells) and early progenitor cells were performed using MACS cell separation system and FACSAria Fusion Cell Sorter (BD Biosciences)⁵⁷. Depletion of specific lineage cells was achieved with a lineage-specific Ab cocktail and anti-biotin microbeads (Miltenyi Biotec 130-090-858, dilution 1:5). Gating strategy for LSK cell sorting⁵⁸ was depicted in Supplementary Fig. 19.

Histological analysis and immunoblotting

For histological analysis⁵⁹, tissue samples were fixed with 10% formalin (Sigma, HT5011) and embedded in paraffin. Then, sections measuring 5 μm were cut using a Leica CM1800 cryostat (Leica Microsystems), and air dried at room temperature. After dry, slides containing each tissue sample were stained with hematoxylin (Merck 1.05174.0500) and eosin (Merck 109844) per the manufacturer’s protocol.

For immunoblot analysis⁵⁹, cells were lysed with RIPA lysis buffer containing 50 mM Tris, pH 7.4, 150 mM NaCl, 1% NP-40 (Sigma, 74385), 0.5% sodium deoxycholate (Sigma, D6750), 0.1% SDS (Sigma, L4509) with 200 μg ml⁻¹ of phenylmethylsulfonyl fluoride (Sigma, P7626), phosphatase inhibitor cocktail (Sigma, P0044) and protease inhibitor cocktail (Millipore, 535140). The cell lysates were then resolved by 12% SDS-polyacrylamide gel electrophoresis, transferred onto Immobilon P membranes (Millipore, IPVH00010), and immunoblotted with anti-VCAM-1 Ab (Santa Cruz Biotechnology, Inc. sc-8304, dilution 1:1000), anti-H3K27me3 Ab (EMD Millipore 07-449, dilution 1:1000), or anti-histone H3 Ab (Cell Signaling Technology 9715, dilution 1:1000) coupled with goat anti-rabbit IgG-HRP (Santa Cruz Biotechnology, Inc. sc-2004, dilution 1:2500), and anti-Phc2 Ab (mouse IgG, dilution 1:200)¹⁴ or anti-β-actin Ab (Sigma-Aldrich A5441, dilution 1:25,000) coupled with goat anti-mouse IgG-HRP (Santa Cruz Biotechnology, Inc. sc-2005, dilution 1:2500). Immunoreactive bands were visualized using an ECL solution (Thermo Fisher Scientific 34080). To quantify the relative protein expression, immunoreactive bands were normalized to levels of β-actin. The relative band intensity of protein expression was quantified using ImageJ software (National Institutes of Health). Uncropped blots can be found in the Source Data.

Cell cycle analysis and measurement of apoptosis

BM-resident LSK cells from 8-week-old mice were isolated and incubated in 70% ethanol overnight at 4 °C. After washing with PBS, cells were stained with propidium iodide (Sigma-Aldrich P4170) for cell cycle analysis. To measure apoptosis, LSK cells were stained with 7-AAD (BD Biosciences 559925, dilution 1:20) and Annexin V-FITC (BD Biosciences 556547, dilution 1:20). After washing with PBS, stained cells were analyzed by flow cytometry.

CFU assay

Mononuclear cells isolated from the BM, PB, and spleen were plated onto Methocult GF M3434 (StemCell Technologies 03444) in 35 mm cell culture dishes. Cells were then incubated at 37 °C and 5% CO₂. After 7 days of incubation, type and number of colonies were determined⁶⁰.

In vivo HSPC mobilization assays

For G-CSF-induced mobilization assays¹⁵, recombinant human G-CSF (Amgen Filgrastim Neupogen) was diluted in PBS with 0.1% BSA (GenDEPOT A0100-050). G-CSF or vehicle was administered by daily subcutaneous injection to 8-week-old mice at a dose of 250 μg kg⁻¹ day⁻¹ for 5 days. For AMD3100-induced mobilization assays¹⁷, AMD3100 (Sigma-Aldrich A5602) was diluted in PBS and administered subcutaneously to 8-week-old mice at 5 mg kg⁻¹. For G-CSF and AMD3100-induced mobilization assays⁶¹, G-CSF or vehicle was administered by daily subcutaneous injection to 8-week-old mice at a dose of 250 μg kg⁻¹ day⁻¹ for 5 days. One h before final G-CSF dose, AMD3100 administered subcutaneously to the same group of mice at 5 mg kg⁻¹. Three h after the final G-CSF or AMD3100 dose, mice were sacrificed to assess the absolute numbers of nucleated cells in the PB and spleen. The absolute numbers of LSK cells in the BM, PB, and spleen were determined by flow cytometry and CFU assays. To block the VLA-4 and VCAM-1 interaction, anti-VCAM-1 (BD Biosciences 553330) Ab or the respective isotype control (2 mg kg⁻¹ day⁻¹; BD Biosciences 553926) was administered intravenously every day.

For 5-FU-induced mobilization assays⁶², 5-FU (Sigma-Aldrich F6627) was administered intravenously to 8-week-old mice at 200 mg kg⁻¹. The absolute numbers of nucleated cells in the PB and spleen were counted on days 4, 8, 12, and 16 after 5-FU treatment. On day 16 after 5-FU administration, mice were sacrificed, and the absolute numbers of Lin⁻Sca-1⁺c-kit⁺ cells (LSK cells) in the BM, PB, and spleen were determined by flow cytometry and CFU assays. To block the VLA-4 and VCAM-1 interaction, mice were injected with anti-VCAM-1 Ab or the respective isotype control (2 mg kg⁻¹ day⁻¹) from day 8 to day 15 after 5-FU administration.

For anti-VCAM-1 Ab-induced mobilization assays⁶³, anti-VCAM-1 Ab or the respective isotype control administered by daily subcutaneous injection to 8-week-old mice at a dose of 2 mg kg⁻¹ day⁻¹ for 3 days. Eight hours after the final Ab dose, mice were sacrificed, and the absolute numbers of nucleated cells in the PB and spleen were counted. The absolute numbers of LSK cells in the BM, PB, and spleen were determined by CFU assays described above.

LSK transplantation

LSK cells (1 × 10⁵) isolated from 8-week-old donor mice were injected intravenously into lethally irradiated (10 Gy) 8-week-old recipient mice. Twelve weeks after the LSK transfer, recipient mice were sacrificed and analyzed for reconstitution of donor immune cells. Donor cells and recipient cells were discriminated by flow cytometry using anti-CD45.2 (104)-PerCP-Cy5.5 Ab (BD 552950, dilution 1:100) for congenic strain (CD45.1) discrimination. For serial competitive LSK repopulation assays⁵⁸, LSK cells (5 × 10⁴) isolated from WT or KO mice (CD45.2) were mixed with an equal number of LSK cells isolated from competitor mice (WT in CD45.1). The cell mixture was then intravenously injected into lethally irradiated (10 Gy) 8-week-old recipient mice (WT in CD45.1). Secondary transplantation was performed at 12 weeks after primary engraftment. LSK cells (1 × 10⁵) harvested from primary transplants were intravenously injected into lethally irradiated (10 Gy) 8-week-old recipient mice (WT in CD45.1). The ratio of CD45.1 to CD45.2 positive cells in the BM, PB, thymus, and spleen of recipient mice was measured by flow cytometry.

In vivo homing assay

For in vivo homing assay⁶⁴, recipient mice were lethally irradiated (10 Gy) 24 h before LSK transplantation. Freshly isolated LSK cells from 8-week-old mice were labeled with 1 μM CFSE (Thermo Fisher Scientific C34554) per the manufacturer’s instructions. CFSE-labeled LSK cells (2 × 10⁵) were then resuspended in PBS and intravenously injected into recipient mice. Sixteen hours after injection, mice were sacrificed, and the frequencies of CFSE⁺ cells in the BM, PB, and spleen were determined by flow cytometry. To determine the frequency of clonogenic progenitors, mononuclear cells from the BM, PB, and spleen were subjected to CFU assays as described above. To block the interaction between VLA-4 and VCAM-1, CFSE-labeled LSK cells were incubated with an anti-VCAM-1 Ab (2 mg kg⁻¹) or an isotype control, and the cells were intravenously injected into recipients 1 h before transplantation.

Trans-stromal migration and adhesion assay

For the trans-stromal migration assay⁶⁵, LSK cells (1 × 10⁵ cells chamber⁻¹) were loaded into the top chamber of a 24-well transwell plate containing a monolayer of BMSCs. Recombinant mouse CXCL12 (100 ng mL⁻¹; R&D Systems P40224) was loaded into the bottom chamber. The plate was then incubated at 37 °C in 5% CO₂ for 16 h. After incubation, the number of migrating LSK cells in the bottom chamber was calculated. To perform the adhesion assay, CFSE-labeled LSK cells (5 × 10⁴) were co-cultured with BMSCs (2 × 10⁵) in 24-well cell culture plates. Three h after co-culture, nonadherent LSK cells were removed via three gentle washes with PBS, and adherent LSK cells were harvested. The frequency of CFSE⁺ LSK cells was determined by flow cytometry. To block the VLA-4 and VCAM-1 interaction, LSK cells were preincubated with anti-VLA-4 (10 μg mL⁻¹; Merck CBL1304) Ab or an isotype control (10 μg ml⁻¹; BD Biosciences 559478) for 30 min, and BMSCs were preincubated with anti-VCAM-1 Ab (10 μg mL⁻¹) or an isotype control for 30 min.

mRNA-seq data analysis

Total RNAs from WT and KO BM cells were extracted using TRIzol (Thermo Fisher Scientific 15596026) according to the manufacturer’s protocol. Subsequently, 1 μg of total RNA was used to construct cDNA libraries using TruSeq RNA library kit (Illumina, RS-122-2001) according to the manufacturer’s protocol. The size distribution and quality of cDNA libraries were monitored by Agilent 2100 Bioanalyzer (Agilent Technologies) and quantitative PCR using Kapa Library Quantification Kit (Kapa Biosystems KK4824). After the quality check, cDNA libraries were sequenced using an Illumina HiSeq4000 sequencer (Illumina).

After removing low quality and adapter sequences, the raw reads were aligned to the reference genome Mus musculus (mm10) (genome assembly information access, GCF_000001635.20) using HISAT v2.0.5⁶⁶. After aligning reads to the genome, StringTie v1.3.3b was used to assemble transcripts and estimate their abundance measured in fragments per kilobase of exon per million fragments mapped (FPKM)^67,68. False discovery rate (FDR) was controlled by adjusting p-value cutoff of 0.05 using Benjamini–Hochberg algorithm⁶⁹. Subsequently, hierarchical clustering analysis was performed to analyze differentially expressed gene (DEG) set using complete linkage and Euclidean distance as a measure of similarity. Gene set enrichment analysis including functional annotation and pathway analyses were performed based on Gene Ontology (www.geneontology.org/) and KEGG pathway (http://www.genome.jp/kegg/pathway.html). An overview of the gene expression data was deposited at NCBI’s Gene Expression Omnibus (GEO). It is accessible through GEO series accession number of GSE128705.

Real-time quantitative RT-PCR analysis

Total RNA was purified from BMSCs using Trizol reagent (Thermo Fisher Scientific 15596026) according to the manufacturer’s instructions; it was then reverse transcribed into cDNA using a RevertAid First Strand cDNA Synthesis Kit (Thermo Fisher Scientific K1621). After cDNA synthesis, quantitative PCR (qPCR) was conducted to measure mRNA levels of mouse Alcam, Angpt1, Cdh2, Ctsk, Cxcl12, Fn1, Kitl, Icam1, p16^INK4a, p19^ARF, Selp, Vcam1, and Gapdh using a 7500 Real-time PCR system (Thermo Fisher Scientific). Gapdh was used as an internal control to quantify the levels of other mRNA transcripts. The primer pairs used for qRT-PCR are listed in Supplementary Table 1.

Inhibition of Phc2 expression by shRNA

Lentiviral plasmids expressing shRNAs directed against several distinct regions of Phc2 (SHCLNG-NM_018774) and control shRNA plasmids (SHC001) were purchased from Sigma-Aldrich. OP9 cells (mouse BMSC line, ATCC CRL-2749) were transfected with each shRNA-containing plasmid using Lipofectamine 2000 transfection reagent (Thermo Fisher Scientific 11668019) according to the manufacturer’s instructions. After transfection, inhibition of Phc2 expression was determined by qRT-PCR and immunoblotting. Primer sequences for Phc2 for qRT-PCR are listed in Supplementary Table 1.

ChIP assay

The lysates of BM cells (2 × 10⁶) from 8-week-old mice were prepared for the ChIP assay⁷⁰. BM cell lysates were sonicated and immunoprecipitated with the anti-Bmi1 (Santa Cruz Biotechnology, Inc. sc-10745, 2 μg sample⁻¹), anti-Cbx7 (Santa Cruz Biotechnology, Inc. sc-70232, 2 μg sample⁻¹), anti-H2AK119ub (Cell Signaling Technology 8240, 2 μg sample⁻¹), anti-H3K9ac (Merck 06-942, 2 μg sample⁻¹), anti-H3K4me3 (Abcam ab12209, 2 μg sample⁻¹), anti-H3K27me3 (Merck 07-449, 2 μg sample⁻¹), anti-Phc2 (Santa Cruz Biotechnology, Inc. sc-160664, 2 μg sample⁻¹), and anti-Ring1b (Cell Signaling Technology 5694, 2 μg sample⁻¹) Abs. Additionally, GSK126-treated OP9 cell lysates were sonicated and immunoprecipitated with the anti-Bmi1, anti-Phc2, and anti-Ring1b Abs. After immunoprecipitation, immune complexes were collected with protein A agarose (Merck GE17-0963-03) and extracted with an extraction buffer (1% SDS, 0.1 M NaHCO₂). DNA cross-links were reversed by heating to 65 °C for 8 h. DNA was extracted with phenol/chloroform and precipitated with ethanol. DNA isolated from an aliquot of total nuclear extract was used as the loading control for PCR (input control). qPCR was performed as described above. Data are presented after normalizing each immunoprecipitated DNA Ct value to 10% of the input DNA Ct value.

In vivo administration of GSK126

WT mice were intraperitoneally injected with 50 or 100 mg kg⁻¹ of DMSO-dissolved GSK126. Mice were sacrificed at 16 h after GSK126 injection and the expression of VCAM-1 from BMSCs of sacrificed mice were analyzed by immunoblotting and flow cytometry. In addition, trans-stromal migration and adhesion assays using LSK cells and BMSCs of sacrificed mice were performed as described above.

Statistical analysis

Mean values among more than three experimental groups were compared by one-way ANOVA with Tukey HSD analysis and comparison between two groups was analyzed by two-tailed Student’s t-test using SPSS statistics software, ver. 24.0 (SPSS Inc). All data are presented as the mean ± standard error of mean (SEM). In each graph, significant differences as determined by p-values less than 0.05 and 0.01 are indicated by asterisks (* and **, respectively).

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

The raw mRNA-seq data were deposited into the Sequence Read Archive (SRA) of National Center for Biotechnology Information (NCBI) with the following accession numbers: GSM3683312, GSM3683313, GSM3683314, GSM3683315, GSM3683316, and GSM3683317. An overview of the gene expression data was deposited at NCBI’s Gene Expression Omnibus (GEO). It is accessible through GEO series accession number of GSE128705. Source data underlying Figs. 1–8, Tables 1–2, Supplementary Figs. 1–7, and Supplementary Figs. 10–18 are provided as a Source Data file. All other data that support the findings of this study are available from the corresponding author upon reasonable request.

References

Wright, D. E., Wagers, A. J., Gulati, A. P., Johnson, F. L. & Weissman, I. L. Physiological migration of hematopoietic stem and progenitor cells. Science 294, 1933–1936 (2001).
Article ADS CAS Google Scholar
Laird, D. J., von Andrian, U. H. & Wagers, A. J. Stem cell trafficking in tissue development, growth, and disease. Cell 132, 612–630 (2008).
Article CAS Google Scholar
Bhattacharya, D., Rossi, D. J., Bryder, D. & Weissman, I. L. Purified hematopoietic stem cell engraftment of rare niches corrects severe lymphoid deficiencies without host conditioning. J. Exp. Med. 203, 73–85 (2006).
Article CAS Google Scholar
Morrison, S. J. & Spradling, A. C. Stem cells and niches: mechanisms that promote stem cell maintenance throughout life. Cell 132, 598–611 (2008).
Article CAS Google Scholar
Mazo, I. B., Massberg, S. & von Andrian, U. H. Hematopoietic stem and progenitor cell trafficking. Trends Immunol. 32, 493–503 (2011).
Article CAS Google Scholar
Wilson, A. & Trumpp, A. Bone-marrow haematopoietic-stem-cell niches. Nat. Rev. Immunol. 6, 93–106 (2006).
Article CAS Google Scholar
Mercier, F. E., Ragu, C. & Scadden, D. T. The bone marrow at the crossroads of blood and immunity. Nat. Rev. Immunol. 12, 49–60 (2012).
Article CAS Google Scholar
Piunti, A. & Shilatifard, A. Epigenetic balance of gene expression by Polycomb and COMPASS families. Science 352, aad9780 (2016).
Article Google Scholar
Cao, R. et al. Role of histone H3 lysine 27 methylation in Polycomb-group silencing. Science 298, 1039–1043 (2002).
Article ADS CAS Google Scholar
Gao, Z. et al. PCGF homologs, CBX proteins, and RYBP define functionally distinct PRC1 family complexes. Mol. Cell. 45, 344–356 (2012).
Article CAS Google Scholar
Morey, L., Aloia, L., Cozzuto, L., Benitah, S. A. & Di Croce, L. RYBP and Cbx7 define specific biological functions of polycomb complexes in mouse embryonic stem cells. Cell Rep. 3, 60–69 (2013).
Article CAS Google Scholar
Wang, H. et al. Role of histone H2A ubiquitination in Polycomb silencing. Nature 431, 873–878 (2004).
Article ADS CAS Google Scholar
Tavares, L. et al. RYBP-PRC1 complexes mediate H2A ubiquitylation at polycomb target sites independently of PRC2 and H3K27me3. Cell 148, 664–678 (2012).
Article CAS Google Scholar
Isono, K. et al. Mammalian polyhomeotic homologues Phc2 and Phc1 act in synergy to mediate polycomb repression of Hox genes. Mol. Cell. Biol. 25, 6694–6706 (2005).
Article CAS Google Scholar
Petit, I. et al. G-CSF induces stem cell mobilization by decreasing bone marrow SDF-1 and up-regulating CXCR4. Nat. Immunol. 3, 687–694 (2002).
Article CAS Google Scholar
Bendall, L. J. & Bradstock, K. F. G-CSF: from granulopoietic stimulant to bone marrow stem cell mobilizing agent. Cytokine Growth Factor Rev. 25, 355–367 (2014).
Article CAS Google Scholar
Broxmeyer, H. E. et al. Rapid mobilization of murine and human hematopoietic stem and progenitor cells with AMD3100, a CXCR4 antagonist. J. Exp. Med. 201, 1307–1318 (2005).
Article CAS Google Scholar
Devine, S. M. et al. Rapid mobilization of functional donor hematopoietic cells without G-CSF using AMD3100, an antagonist of the CXCR4/SDF-1 interaction. Blood 112, 990–998 (2008).
Article CAS Google Scholar
Heissig, B. et al. Recruitment of stem and progenitor cells from the bone marrow niche requires MMP-9 mediated release of kit-ligand. Cell 109, 625–637 (2002).
Article CAS Google Scholar
Aicher, A. et al. Essential role of endothelial nitric oxide synthase for mobilization of stem and progenitor cells. Nat. Med. 9, 1370–1376 (2003).
Article CAS Google Scholar
Calvi, L. et al. Osteoblastic cells regulate the haematopoietic stem cell niche. Nature 425, 841–846 (2003).
Article ADS CAS Google Scholar
Kiel, M. J. et al. SLAM family receptors distinguish hematopoietic stem and progenitor cells and reveal endothelial niches for stem cells. Cell 121, 1109–1121 (2005).
Article CAS Google Scholar
Méndez-Ferrer, S. et al. Mesenchymal and haematopoietic stem cells form a unique bone marrow niche. Nature 466, 829–834 (2010).
Article ADS Google Scholar
Iademarco, M. F., Barks, J. L. & Dean, D. C. Regulation of vascular cell adhesion molecule-1 expression by IL-4 and TNF-alpha in cultured endothelial cells. J. Clin. Invest. 95, 264–271 (1995).
Article CAS Google Scholar
McCabe, M. T. et al. EZH2 inhibition as a therapeutic strategy for lymphoma with EZH2-activating mutations. Nature 492, 108–112 (2012).
Article ADS CAS Google Scholar
Koni, P. A. et al. Conditional vascular cell adhesion molecule 1 deletion in mice: impaired lymphocyte migration to bone marrow. J. Exp. Med. 193, 741–754 (2001).
Article CAS Google Scholar
Ulyanova, T. et al. VCAM-1 expression in adult hematopoietic and nonhematopoietic cells is controlled by tissue-inductive signals and reflects their developmental origin. Blood 106, 86–94 (2005).
Article CAS Google Scholar
Scott, L. M., Priestley, G. V. & Papayannopoulou, T. Deletion of α4 integrins from adult hematopoietic cells reveals roles in homeostasis, regeneration, and homing. Mol. Cell. Biol. 23, 9349–9360 (2003).
Article CAS Google Scholar
Priestley, G. V., Ulyanova, T. & Papayannopoulou, T. Sustained alterations in biodistribution of stem/progenitor cells in Tie2Cre+ α4f/f mice are hematopoietic cell autonomous. Blood 109, 109–111 (2007).
Article CAS Google Scholar
Papayannopoulou, T., Priestley, G. V., Nakamoto, B., Zafiropoulos, V. & Scott, L. M. Molecular pathways in bone marrow homing: dominant role of α4β1 over β2-integrins and selectins. Blood 98, 2403–2411 (2001).
Article CAS Google Scholar
Papayannopoulou, T. & Nakamoto, B. Peripheralization of hemopoietic progenitors in primates treated with anti-VLA4 integrin. Proc. Natl Acad. Sci. USA 90, 9374–9378 (1993).
Article ADS CAS Google Scholar
Kavanagh, D. P. et al. Haematopoietic stem cell recruitment to injured murine liver sinusoids depends on α4β1 integrin/VCAM-1 interactions. Gut 59, 79–87 (2010).
Article CAS Google Scholar
Osborn, L. et al. Direct expression cloning of vascular cell adhesion molecule 1, a cytokine-induced endothelial protein that binds to lymphocytes. Cell 59, 1203–1211 (1989).
Article CAS Google Scholar
Miyake, K. et al. A VCAM-like adhesion molecule on murine bone marrow stromal cells mediates binding of lymphocyte precursors in culture. J. Cell Biol. 114, 557–565 (1991).
Article CAS Google Scholar
Jacobsen, K., Kravitz, J., Kincade, P. & Osmond, D. Adhesion receptors on bone marrow stromal cells: in vivo expression of vascular cell adhesion molecule-1 by reticular cells and sinusoidal endothelium in normal and gamma-irradiated mice. Blood 87, 73–82 (1996).
CAS PubMed Google Scholar
Schweitzer, K. M. et al. Constitutive expression of E-selectin and vascular cell adhesion molecule-1 on endothelial cells of hematopoietic tissues. Am. J. Pathol. 148, 165–175 (1996).
CAS PubMed PubMed Central Google Scholar
Freedman, A. S. et al. Adhesion of human B cells to germinal centers in vitro involves VLA-4 and INCAM-110. Science 249, 1030–1033 (1990).
Article ADS CAS Google Scholar
Schlesinger, M. & Bendas, G. Vascular cell adhesion molecule‐1 (VCAM‐1)—an increasing insight into its role in tumorigenicity and metastasis. Int. J. Cancer 136, 2504–2514 (2015).
Article CAS Google Scholar
Bradstock, K. F. & Gottlieb, D. J. Interaction of acute leukemia cells with the bone marrow microenvironment: implications for control of minimal residual disease. Leuk. Lymphoma 18, 1–16 (1995).
Article CAS Google Scholar
Winter, S. S. et al. Enhanced T‐lineage acute lymphoblastic leukaemia cell survival on bone marrow stroma requires involvement of LFA‐1 and ICAM‐1. Br. J. Haematol. 115, 862–871 (2001).
Article CAS Google Scholar
Damiano, J. S., Cress, A. E., Hazlehurst, L. A., Shtil, A. A. & Dalton, W. S. Cell adhesion mediated drug resistance (CAM-DR): role of integrins and resistance to apoptosis in human myeloma cell lines. Blood 93, 1658–1667 (1999).
CAS PubMed PubMed Central Google Scholar
Tabe, Y. et al. Activation of integrin-linked kinase is a critical prosurvival pathway induced in leukemic cells by bone marrow-derived stromal cells. Cancer Res. 67, 684–694 (2007).
Article CAS Google Scholar
Jacamo, R. et al. Reciprocal leukemia-stroma VCAM-1/VLA-4-dependent activation of NF-κB mediates chemoresistance. Blood 123, 2691–2702 (2014).
Article CAS Google Scholar
Cullen, S. M., Mayle, A., Rossi, L. & Goodell, M. A. Hematopoietic stem cell development: an epigenetic journey. Curr. Top. Dev. Biol. 107, 39–75 (2014).
Article CAS Google Scholar
Hu, D. & Shilatifard, A. Epigenetics of hematopoiesis and hematological malignancies. Genes Dev. 30, 2021–2041 (2016).
Article CAS Google Scholar
Takamatsu-Ichihara, E. & Kitabayashi, I. The roles of Polycomb group proteins in hematopoietic stem cells and hematological malignancies. Int. J. Hematol. 103, 634–642 (2016).
Article CAS Google Scholar
Vidal, M. & Starowicz, K. Polycomb complexes PRC1 and their function in hematopoiesis. Exp. Hematol. 48, 12–31 (2017).
Article CAS Google Scholar
Sato, T. et al. Mammalian Polycomb complexes are required for Peyer’s patch development by regulating lymphoid cell proliferation. Gene 379, 166–174 (2006).
Article CAS Google Scholar
Ohta, H. et al. Polycomb group gene rae28 is required for sustaining activity of hematopoietic stem cells. J. Exp. Med. 195, 759–770 (2002).
Article CAS Google Scholar
Kim, J. Y. et al. Defective long-term repopulating ability in hematopoietic stem cells lacking the polycomb-group gene rae28. Eur. J. Haematol. 73, 75–84 (2004).
Article CAS Google Scholar
Hidalgo, I. et al. Ezh1 is required for hematopoietic stem cell maintenance and prevents senescence-like cell cycle arrest. Cell Stem Cell 11, 649–662 (2012).
Article CAS Google Scholar
Xie, H. et al. Polycomb repressive complex 2 regulates normal hematopoietic stem cell function in a developmental-stage-specific manner. Cell Stem Cell 14, 68–80 (2014).
Article CAS Google Scholar
van Den Boom, V. et al. Nonredundant and locus-specific gene repression functions of PRC1 paralog family members in human hematopoietic stem/progeitor cells. Blood 121, 2452–2461 (2013).
Article Google Scholar
Klauke, K. et al. Polycomb Cbx family members mediate the balance between haematopoietic stem cell self-renewal and differentiation. Nat. Cell Biol. 15, 353–362 (2013).
Article CAS Google Scholar
Gray, F. et al. BMI1 regulates PRC1 architecture and activity through homo-and hetero-oligomerization. Nat. Commun. 7, 13343 (2016).
Article ADS CAS Google Scholar
Peister, A. et al. Adult stem cells from bone marrow (MSCs) isolated from different strains of inbred mice vary in surface epitopes, rates of proliferation, and differentiation potential. Blood 103, 1662–1668 (2004).
Article CAS Google Scholar
Broske, A. M. et al. DNA methylation protects hematopoietic stem cell multipotency from myeloerythroid restriction. Nat. Genet. 41, 1207–1215 (2009).
Article Google Scholar
Vukovic, M. et al. Adult hematopoietic stem cells lacking Hif-1α self-renew normally. Blood 127, 2841–2846 (2016).
Article CAS Google Scholar
Han, J. et al. Autophagy induced by AXL receptor tyrosine kinase alleviates acute liver injury via inhibition of NLRP3 inflammasome activation in mice. Autophagy 12, 2326–2343 (2016).
Article CAS Google Scholar
Goldman, D. C. et al. BMP4 regulates the hematopoietic stem cell niche. Blood 114, 4393–4401 (2009).
Article CAS Google Scholar
Ramirez, P. et al. BIO5192, a small molecule inhibitor of VLA-4, mobilizes hematopoietic stem and progenitor cells. Blood 114, 1340–1343 (2009).
Article CAS Google Scholar
Chen., Z. et al. Wip1 deficiency impairs haematopoietic stem cell function via p53 and mTORC1 pathways. Nat. Commun. 6, 6808 (2015).
Article ADS CAS Google Scholar
Papayannopoulou, T., Priestley, G. V. & Nakamoto, B. Anti-VLA4/VCAM-1-induced mobilization requires cooperative signaling through the kit/mkit ligand pathway. Blood 91, 2231–2239 (1998).
CAS PubMed Google Scholar
Foudi, A. et al. Reduced retention of radioprotective hematopoietic cells within the bone marrow microenvironment in CXCR4 ^–/– chimeric mice. Blood 107, 2243–2251 (2006).
Article CAS Google Scholar
Gonzalez-Nieto, D. et al. Connexin-43 in the osteogenic BM niche regulates its cellular composition and the bidirectional traffic of hematopoietic stem cells and progenitors. Blood 119, 5144–5154 (2012).
Article CAS Google Scholar
Kim, D., Langmead, B. & Salzberg, S. L. HISAT: a fast spliced aligner with low memory requirements. Nat. Methods 12, 357–360 (2015).
Article CAS Google Scholar
Pertea, M. et al. StringTie enables improved reconstruction of a transcriptome from RNA-seq reads. Nat. Biotechnol. 33, 290–295 (2015).
Article CAS Google Scholar
Pertea, M., Kim, D., Pertea, G. M., Leek, J. T. & Salzberg, S. L. Transcript-level expression analysis of RNA-seq experiments with HISAT, StringTie and Ballgown. Nat. Protoc. 11, 1650–1667 (2016).
Article CAS Google Scholar
Benjamini, Y. & Hochberg, Y. Controlling the false discovery rate: a practical and powerful approach to multiple testing. J. R. Soc. Ser. B Stat. Methodol. 57, 289–300 (1995).
MathSciNet MATH Google Scholar
Cho, K. W., Bae, J., Lee, S. J. & Chun, T. Expression pattern and functional role of Phc2 during activation of helper T cells after antigenic stimulation. In Vitro Cell Dev. Biol. Anim 49, 360–370 (2013).
Article CAS Google Scholar

Download references

Acknowledgements

We thank Amgen Inc. (Thousand Oaks, CA, USA) for providing G-CSF. We also thank Eun-Kyeong Jo (Chungnam National University School of Medicine), Kyung-Mi Lee (Korea University College of Medicine), Seungkwon You (Korea University School of Life Sciences and Biotechnology), and Seok-Ho Hong (Kangwon National University College of Medicine) for their critical reading of our manuscript or helpful suggestions. This research was supported by the Bio & Medical Technology Development Program of the National Research Foundation (NRF) funded by the Ministry of Science & ICT (2017M3A9C8060392), and an intramural research program funded by Korea University grant (2016).

Author information

These authors contributed equally: Joonbeom Bae, Sang-Pil Choi.

Authors and Affiliations

Department of Biotechnology, College of Life Sciences and Biotechnology, Korea University, Seoul, 02841, Republic of Korea
Joonbeom Bae, Sang-Pil Choi, Si-Won Park, Chang-Yong Choi, Jihye Han, Sang-Hoon Kim, Han-Hyoung Lee, Kyungmin Park, Young Sik Lee & Taehoon Chun
Laboratory Animal Center, Wakayama Medical University, Wakayama, 641-8509, Japan
Kyoichi Isono
Department of Biomedical Science, CHA University, Seongnam, Gyounggi-do, 13488, Republic of Korea
Ji Yoon Lee
Department of Urology, School of Medicine, University of California, San Francisco, San Francisco, CA, 94158, USA
Hyun Yong Jin
Department of Biomedical Laboratory Science, College of Health Science, Cheongju University, Cheongju-si, 28503, Republic of Korea
Suk Jun Lee
Department of Microbiology and Immunology, Cancer Research Institute and Xenotransplantation Research Center, Seoul National University College of Medicine, Seoul, 03087, Republic of Korea
Chung-Gyu Park
Laboratory for Developmental Genetics, RIKEN Center for Integrative Medical Sciences, Yokohama, 230-0045, Japan
Haruhiko Koseki

Authors

Joonbeom Bae
View author publications
You can also search for this author in PubMed Google Scholar
Sang-Pil Choi
View author publications
You can also search for this author in PubMed Google Scholar
Kyoichi Isono
View author publications
You can also search for this author in PubMed Google Scholar
Ji Yoon Lee
View author publications
You can also search for this author in PubMed Google Scholar
Si-Won Park
View author publications
You can also search for this author in PubMed Google Scholar
Chang-Yong Choi
View author publications
You can also search for this author in PubMed Google Scholar
Jihye Han
View author publications
You can also search for this author in PubMed Google Scholar
Sang-Hoon Kim
View author publications
You can also search for this author in PubMed Google Scholar
Han-Hyoung Lee
View author publications
You can also search for this author in PubMed Google Scholar
Kyungmin Park
View author publications
You can also search for this author in PubMed Google Scholar
Hyun Yong Jin
View author publications
You can also search for this author in PubMed Google Scholar
Suk Jun Lee
View author publications
You can also search for this author in PubMed Google Scholar
Chung-Gyu Park
View author publications
You can also search for this author in PubMed Google Scholar
Haruhiko Koseki
View author publications
You can also search for this author in PubMed Google Scholar
Young Sik Lee
View author publications
You can also search for this author in PubMed Google Scholar
Taehoon Chun
View author publications
You can also search for this author in PubMed Google Scholar

Contributions

T.C. conceived, designed, and supervised this study. J.B., S.-P.C., K.I., J.Y.L., S.-W.P., C.-Y.C., J.H., S.-H.K., H.-H.L., K.P. and S.J.L. performed experiments. J.B., S.-P.C., C.-Y.C., C.-G.P. and T.C. analyzed and interpreted data. J.B., S.-P.C., H.Y.J., C.-G.P., H.K., Y.S.L. and T.C. discussed, wrote and edited the manuscript. All authors reviewed and approved the manuscript.

Corresponding author

Correspondence to Taehoon Chun.

Ethics declarations

Competing interests

The authors declare no competing interests.

Additional information

Peer review information: Nature Communications thanks Hal Broxmeyer and other anonymous reviewer(s) for their contribution to the peer review of this work. Peer reviewer reports are available.

Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Supplementary Information

Peer Review File

Reporting Summary

Source Data

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.

Reprints and permissions

About this article

Cite this article

Bae, J., Choi, SP., Isono, K. et al. Phc2 controls hematopoietic stem and progenitor cell mobilization from bone marrow by repressing Vcam1 expression. Nat Commun 10, 3496 (2019). https://doi.org/10.1038/s41467-019-11386-4

Download citation

Received: 18 April 2018
Accepted: 12 July 2019
Published: 02 August 2019
DOI: https://doi.org/10.1038/s41467-019-11386-4

This article is cited by

IL-2 delivery by engineered mesenchymal stem cells re-invigorates CD8+ T cells to overcome immunotherapy resistance in cancer
- Joonbeom Bae
- Longchao Liu
- Yang-Xin Fu
Nature Cell Biology (2022)
Construction of a circRNA-miRNA-mRNA network based on competitive endogenous RNA reveals the function of circRNAs in osteosarcoma
- Yu Qiu
- Chao Pu
- Baochuang Qi
Cancer Cell International (2020)

Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.