Current Opinion in Hematology:
ERYTHROID SYSTEM AND ITS DISEASES: Edited by Narla Mohandas
Rho GTPases in erythroid maturation
Kalfa, Theodosia A.; Zheng, Yi
Cancer and Blood Diseases Institute, Cincinnati Children's Hospital Medical Center, University of Cincinnati College of Medicine, Cincinnati, Ohio, USA
Correspondence to Theodosia A. Kalfa, MD, PhD, Division of Hematology/Oncology, Cincinnati Children's Hospital Medical Center, 3333 Burnet Avenue, MLC 7015, Cincinnati, OH 45229-3039, USA. Tel: +1 513 636 0989; fax: +1 513 636 3549; e-mail: email@example.com
Purpose of review
This review summarizes our current understanding of the roles of Rho GTPases in early erythropoiesis, downstream of cytokine signaling, and in terminal erythroblast maturation and enucleation, as master regulators of the cytoskeleton and cytokinesis.
Similarities of structural and signaling requirements of erythroblast enucleation with the cytokinesis process have been confirmed and expanded in the last year, suggesting that enucleation is a form of asymmetric cell division. Myosin, the classic actin partner in cytokinesis, was shown to play an essential role in enucleation. Studies with multispectral high-speed cell imaging in flow demonstrated a sequential process requiring establishment of polarity through a unipolar microtubule spindle in orthochromatic erythroblasts, followed by Rac-directed formation of a contractile actomyosin ring and coalescence of lipid rafts between reticulocyte and pyrenocyte, steps which reiterate the choreography of cytokinesis. mDia2, a Rho effector known to play a role in enucleation, was also found essential for erythroblast cytokinesis as its deficiency in mice caused failure of primitive erythropoiesis and embryonic death.
Further elucidation of the role of Rho GTPases in the erythroid lineage development may reveal potential targets for improving red blood cell production in vivo and in vitro.
Rho (Ras homology) GTPases belong to the Ras superfamily of small G proteins. They are found in all eukaryotic organisms and regulate a wide spectrum of cellular functions including actin cytoskeleton, cell polarity and motility, microtubule dynamics, and vesicular transport pathways, as well as survival and cell cycle [1–4,5▪]. The classical Rho GTPases, comprising the subfamilies Rho (RhoA, RhoB, and RhoC), Rac (Rac1, Rac2, Rac3, and RhoG), Cdc42 (Cdc42, TC10 or RhoQ, and TCL or RhoJ), RhoF and RhoD, switch between the inactive GDP-bound form and the active GTP-bound form in response to a variety of cell signals. Upon activation, they interact with multiple downstream effector proteins in a spatially and temporally controlled manner . Rho GTPases are typically modified posttranslationally by lipid moieties, so they can localize to specific cell membranes, where they modulate membrane dynamics and mediate signaling . For example, palmitoylation of Rac1 at the C-terminus, following its geranylgeranylation, leads to its translocation to the cholesterol-rich, detergent-resistant subdomains in the plasma membrane known as lipid rafts upon stimulation by cytokines or adhesion interactions .
Initial studies on the role of Rho GTPases in hematopoiesis utilized overexpression of constitutively active or dominant-negative mutants, which suffer from limited specificity, variable dosage, and uncontrolled special and temporal distribution in cells. Recent gene targeting of individual Rho GTPases in mice has allowed studies of their role in primary cells under more physiological conditions . Pharmacological inhibitors are also available in assisting the study of the role of Rho GTPases during a specific stage of a hematopoietic lineage progression [10,11]. A network of cross-talking and collaborating Rho GTPases are found involved in mediating complex signaling events in the dynamic settings of hematopoiesis .
ERYTHROID COMMITMENT AND EARLY ERYTHROPOIESIS
In the erythroid lineage, the earliest committed progenitors in the mouse bone marrow are the megakaryocyte-erythroid progenitors (MEPs). This population consists of cells with burst forming unit-erythroid (BFU-E), colony forming unit-erythroid (CFU-E), and CFU-megakaryocytic (CFU-Meg) potential [13,14]. The process of erythropoiesis is under tight regulation by cytokines including stem cell factor (SCF), interleukin-3 (IL3), and erythropoietin (Epo), other growth factors including steroids, and the microenvironment, which may vary depending on the developmental stage and the red blood cell (RBC) production needs [15–17]. Rho GTPases such as Rac (Rac1, Rac2, and Rac3), Cdc42, and RhoA have been implicated in signaling at the erythroid progenitor commitment and proliferation stages, downstream of cytokines and upstream of transcription factor network.
Rac GTPases are essential for normal erythropoiesis in the bone marrow but dispensable for stress erythropoiesis in the spleen
Among the three Rac GTPases, Rac1 and Rac3 are ubiquitously expressed, whereas Rac2 is expressed only in hematopoietic cells [18–20]. Rac1 and Rac2 GTPases were the first Rho GTPases shown to play vital distinct as well as overlapping roles in hematopoietic stem cells/progenitors (HSC/Ps) and mature blood cells. Both Rac isoforms regulate homing, engraftment, actin cytoskeleton, cell survival, and proliferation of HSC/Ps [21,22]. In neutrophils, Rac1 controls cell spreading and adhesion, whereas Rac2 regulates directed migration and superoxide production [21,23].
Rac1 is indispensable for embryonic development , therefore combined deficiency of Rac1 and Rac2 in hematopoietic cells can be attained in gene-targeted mice with germline deletion of Rac2 gene and conditional Rac1flox/flox alleles with a Cre transgene driven by the Mx1 promoter. Cre recombinase is expressed in the hematopoietic cells after intraperitoneal injections of polyinosinic-polycytidylic acid (pI-pC) leading to Rac1 deletion and the development of Mx1-CreTg/+;Rac1Δ/Δ;Rac2−/− hematopoietic cells, including Rac1/Rac2-deficient erythroid progenitors and precursors [25,26]. Deletion of either Rac1 or Rac2 in hematopoietic lineages led to no significant abnormalities in erythropoiesis or the mature RBCs, suggesting a redundancy for these two GTPases in the erythroid lineage.
The number of cells with BFU-E activity in Rac1Δ/Δ;Rac2−/− mouse bone marrow is slightly decreased, but most notably affected is the morphology of the Rac-deficient colonies which are small, round, and condensed. In erythroid differentiation sequence, CFU-E and erythroblasts are significantly decreased in Rac1Δ/Δ;Rac2−/− bone marrow. MEPs of the bone marrow (including BFU-E, CFU-E, and CFU-Meg) are significantly reduced with decreased proliferation, whereas, in contrast, they are significantly increased in the spleen, particularly the subset population of CFU-E mounting stress erythropoiesis . Similarly with the Rac1/Rac2-deficient HSC/Ps , MEPs demonstrate increased homing in the spleen as well as increased proliferation and decreased apoptosis . Rac1 and Rac2 GTPases have been shown in HSC/Ps to be downstream of the c-kit receptor, promoting proliferation and survival upon SCF stimulation . Similarly, Rac1/Rac2 deficiency compromises baseline erythropoiesis in the early stages mediated by SCF (Fig. 1). However, within the splenic microenvironment or under the influence of unique cytokines acting in the spleen during stress erythropoiesis, such as bone morphogenetic protein 4 (BMP4) , Rac1/Rac2 appear to be dispensable for erythroid progenitor proliferation and differentiation .
Cdc42 regulates the balance between myelopoiesis and erythropoiesis
The role of Cdc42 in erythropoiesis has been studied in mice with either deletion of a negative regulator, Cdc42GAP, or an inducible deletion of Cdc42 in hematopoietic lineages [29,30]. Homozygous deletion of Cdc42GAP, the GTPase-activating protein of Cdc42 that downregulates Cdc42 activity by promoting the hydrolysis of GTP to GDP, results in a three-fold increase in Cdc42 activity in mouse fetal liver and bone marrow cells. These mice suffer massive neonatal mortality (up to 93% within 1 week of birth), with the surviving ones displaying significant anemia and decreased fetal liver and bone marrow cellularity, along with a reduction of cells with BFU-E and CFU-E activity, as well as CFU-GEMM (granulocyte, erythroid, macrophage, and megakaryocyte potential), but normal CFU-GM . This decrease in both erythroid and myeloid progenitors correlates with increased apoptosis associated with increased JNK phosphorylation and reduction of the survival factor BID . Although such increased Cdc42 activity affects erythropoiesis by inducing apoptosis, decreased Cdc42 also negatively impacts on erythropoiesis by altering a key transcription factor program. Deletion of Cdc42 from HSC/Ps leads to the development of a fatal myeloproliferative disorder along with a fast decline of erythropoiesis, caused by a significant decrease in the MEP population, as well as in BFU-E and CFU-E activities, leading to profound anemia. These effects appear to be mediated by downregulation of the proerythroid transcription factor GATA2 and upregulation of the promyeloid transcription factors PU.1, C/EBPα, and Gfi-1 .
RhoA is essential for progenitor commitment and proliferation
The role of RhoA in hematopoiesis is less studied compared with that of Rac1, Rac2, and Cdc42. Hematopoietic-specific deletion of RhoA in MxCreTg/+;RhoAflox/flox mice leads to the development of fatal aplastic anemia as RhoA−/− HSCs retain long-term engraftment potential but fail to produce multipotent progenitors and lineage-defined blood cells , limiting the ability to derive the effect of RhoA in the erythroid lineage in this model. It will be an interesting area to pursue using an erythroid lineage-specific genetic mouse model in the future, as RhoA has been shown to be regulated by SCF in human erythroid progenitors .
TERMINAL ERYTHROID MATURATION AND ENUCLEATION
CFU-E subpopulation cells give rise to the morphologically recognizable proerythroblasts, which differentiate through four to five successive divisions into orthochromatic erythroblasts that enucleate to produce reticulocytes . The signaling role of Rho GTPases in regulating the terminal erythroid maturation and enucleation is beginning to be appreciated.
Evolving understanding of the role of RhoA in erythroid maturation
After downregulation of the cKIT receptor at the proerythroblast stage, RhoA activity is no further stimulated by SCF . Moreover, the Rho-associated kinase (ROCK-1), a major RhoA effector, was found to be activated at the erythroblast stage in culture by caspase-3-mediated cleavage, independently of Rho signaling, and to promote phosphorylation of the light chain of myosin II . Inhibition of ROCK by the small-molecule inhibitor Y27632 or by shRNA causes a decrease of erythroblast maturation in vitro. In contrast, deletion of ROCK1 in mice enhances the response to stress erythropoiesis after phenylhydrazine-induced hemolysis. Constitutional ROCK1 deficiency decreased the level of reactive oxygen species (ROS) production in the bone marrow and spleen erythroid cells, reduced the expression and phosphorylation of p53, and reduced caspase-3 cleavage promoting erythroblast survival, implicating ROCK1 as a negative regulator of stress erythropoiesis .
Mice with constitutive gene deletion of mDia2, a formin isoform and Rho effector that typically nucleates unbranched actin filaments, were recently described [36▪]. This mouse model is embryonic lethal, survives up to embryonic day 11.5 (E11.5) and exhibits severe anemia with multinucleated primitive RBCs. BFU-E and CFU-E colonies can be produced by mDia2-deficient fetal liver cells at E11.5, although the colony numbers are significantly decreased. Erythroblast cytokinesis fails with increasing rate as the size of the erythroblasts declines along with the progression of erythroid maturation. mDia2-deficient erythroblasts are able to enucleate, although with decreased frequency. Cytochalasin-D or NSC23766 , inhibiting filamentous (F)-actin polymerization or Rac GTPases respectively, block nucleus protrusion completely when directly applied to an erythroblast under microscopic observation [36▪]. However, when the same inhibitors are applied to erythropoiesis cultures in vitro and the whole population is examined, the block of enucleation is not complete either [37,38▪▪]. Downregulation of mDia2 by small interfering RNA (siRNA) in fetal liver cell culture similarly decreases erythroblast enucleation, whereas overexpression of a constitutively active mutant of mDia2 rescues the enucleation defect induced by inhibition of Rac GTPases , placing mDia2 downstream of Rac in this process. The conclusion that mDia2 may be more essential for the erythroblast maturation rather than for enucleation, therefore, needs to be cautioned.
The human homolog of mDia1 (DIAPH1 gene) localizes in the human chromosome 5q31.3 and its loss may contribute to the development of myelodysplastic syndrome (MDS) with interstitial deletion of 5q (5q− MDS), which carries high risk for leukemia . Mice with targeted deletion of the murine DIAPH1 homolog Drf1 develop splenomegaly, fibrotic and hypercellular bone marrow, and extramedullary hematopoiesis in both spleen and liver, including expansion of erythroid precursors . Additional deletion of RhoB, one of the upstream GTPases for mDia1, accelerates MDS development and is associated with increased RBC dysplasia .
Rac GTPases promote erythroblast enucleation
Cultured mouse fetal liver erythroblasts infected with retrovirus overexpressing constitutively active or dominant negative Rac1 or Rac2 mutant have significantly decreased enucleation, indicating that excessive activation or inhibition of Rac GTPases in vitro inhibits enucleation . Pharmacologic inhibition of Rac GTPases by NSC23766, an inhibitor for all Rac GTPases , also inhibits enucleation [37,38▪▪,41]. However, enucleation is not compromised in Rac1Δ/Δ;Rac2−/− erythroblasts, where Rac3 is upregulated and may compensate for Rac1 and Rac2 deficiency [38▪▪,41]. Erythroblast enucleation is a process vital for mammalian life; therefore, such redundancy may have been built into the signaling mechanism, supporting this process in vivo.
Molecules that are involved in cytokinesis were noted to participate in erythroblast enucleation over 25 years ago. F-actin bundles were observed to concentrate between the extruding nucleus and nascent reticulocyte , whereas microtubules were also found to be essential for the nuclear extrusion process by detailed in-vivo and in-vitro studies of rat erythroblasts after treatment with colchicine . Nonmuscle myosin IIB was shown recently to play an essential role in erythroblast enucleation, interacting with F-actin at the cleavage furrow between reticulocyte and nucleus and contributing to a contractile actomyosin ring [44▪▪]. Microtubules, F-actin, and myosin are classic collaborators in cytokinesis: microtubules are organized in the astral spindles around centrosomes at the poles; during anaphase, the pole–pole spacing increases by further microtubule polymerization and a scaffold organized by RhoA and anillin at the spindle mid-zone determines the position of the division plane . This formation of a highly localized zone of RhoA activity happens before contractile ring formation and even in the absence of actin accumulation . In sequence, detergent-resistant membrane domains (lipid rafts) concentrate in the furrow , which ingresses during telophase, developing a barrier between the daughter cells and constricting the spindle mid-zone (the array of interpolar microtubules lying between separated chromatids) into a structure called the midbody. During abscission, the furrow ‘seals’ by vesicular trafficking of endosomes, which fuse to create new membranes that separate the daughter cells [48,49].
In agreement with the analogies noted above between erythroblast enucleation and cytokinesis, immunofluorescence staining of enucleating erythroblasts and analysis by multiparameter high-speed cell imaging in flow revealed a unipolar spindle of microtubules in the polarized orthochromatic erythroblasts preparing for enucleation (Fig. 2). F-actin and myosin, labeled at phosphorylated myosin regulatory light chain (pMRLC), assemble into an actomyosin ring between nascent reticulocyte and nucleus in the population of enucleating erythroblasts, and the lipid raft marker GM1 ganglioside concentrates in the furrow [38▪▪]. Erythroblasts treated with NSC23766 to inhibit Rac activity, cytochalasin-D or colchicine to inhibit actin or tubulin polymerization, respectively, ML7 to inhibit MRLC phosphorylation, or filipin to cause cholesterol depletion and inhibit lipid raft assembly exhibited decreased enucleation efficiency. As assessed by multiparameter high-speed cell imaging in flow, colchicine inhibited erythroblast polarization, implicating microtubules during the preparatory stage of enucleation, whereas NSC23766 led to the absence of lipid raft assembly in the reticulocyte–pyrenocyte border [38▪▪]. These results support the notion that enucleation is a form of asymmetric cytokinesis, requiring establishment of cell polarity through microtubule function, followed by the formation of a contractile actomyosin ring and coalescence of lipid rafts between reticulocyte and pyrenocyte [50▪▪,51▪▪].
An accumulation of vacuoles in the cytoplasm proximal to the extruding nucleus has been observed during erythroblast enucleation, indicating that vesicle trafficking contributes to the creation of new membranes necessary for separating reticulocyte from pyrenocyte [52,53]. Chemical inhibitors of vesicle trafficking or knockdown of clathrin that blocks endocytosis inhibit erythroblast enucleation , pointing to another similarity with cytokinesis, in which endosomes fuse to create new membrane that completely separates the daughter cells [48,49]. Vesicle trafficking is typically regulated by Rho GTPases ; more work is needed to identify the GTPase(s)-mediated mechanism orchestrating this final event in enucleation.
Signaling of Rho GTPases in mature red blood cells
Mice deficient of Rac1 and Rac2 GTPases in their hematopoietic cells exhibit hemolytic anemia because of disturbed actin oligomerization in the erythrocyte cytoskeleton, resulting in decreased deformability and increased fragility of the RBCs under shear stress in the circulation . Adducin, the capping protein for the actin oligomer at the fast-growing barbed end, shows increased phosphorylation at Ser724, a protein kinase C (PKC) target, in the Rac1−/−;Rac2−/− RBCs; this likely facilitates uncapping, promotion of actin polymerization, and actin dissociation from spectrin [25,54,55]. The ensuing abnormal cytoskeleton may be the result of an abnormal assembly during erythroblast maturation; however, one cannot exclude the possibility that there is also dynamic regulation of the actin oligomers by Rac GTPases within the mature RBCs in the circulation.
Rac GTPases contribute to the generation of ROS in human mature RBCs via NADPH oxidase, downstream of intracellular Ca2+ and PKC signaling [56▪]. Rac-GTP is known to participate as a functional subunit of the NOX1 and NOX2 isoforms of NADPH oxidase . This enzymatically mediated production of ROS is higher in the erythrocytes of patients with sickle cell disease (SCD), being stimulated by increased inflammatory cytokines in the plasma, such as TGFβ1 and ET-1, via their receptors on the RBC membrane, raising the possibility for targeted therapy in SCD.
Rho GTPases play important regulatory roles in all stages of erythropoiesis and are vital for the process of erythroblast enucleation. Recent mouse genetic studies have placed them in a signaling network of primitive and definitive erythropoiesis as well as stress erythropoiesis. Further elucidation of the pathways involving various members of Rho GTPases in erythroid biology may offer insights and therapeutic principles for the management of diseases characterized by defective erythropoiesis and hemolysis such as SCD, as well as for advancing the efficiency of red blood cell production in vitro.
This work was supported in part by the NIH grants R01HL116352 and P30DK090971.
Conflicts of interest
There are no conflicts of interest.
REFERENCES AND RECOMMENDED READING
Papers of particular interest, published within the annual period of review, have been highlighted as:
- ▪ of special interest
- ▪▪ of outstanding interest
1. Hall A. Rho GTPases and the actin cytoskeleton. Science. 1998; 279:509–514.
2. Schwartz M. Rho signalling at a glance. J Cell Sci. 2004; 117:5457–5458.
3. Burridge K, Wennerberg K. Rho and Rac take center stage. Cell. 2004; 116:167–179.
4. Etienne-Manneville S, Hall A. Rho GTPases in cell biology. Nature. 2002; 420:629–635.
5▪. Jordan SN, Canman JC. Rho GTPases in animal cell cytokinesis: an occupation by the one percentage. Cytoskeleton (Hoboken). 2012; 69:919–930.
This is a comprehensive review about the function and regulation of Rho GTPases during cytokinesis in animal cells.
6. Heasman SJ, Ridley AJ. Mammalian Rho GTPases: new insights into their functions from in vivo studies. Nat Rev Mol Cell Biol. 2008; 9:690–701.
7. Ridley AJ. Rho GTPases and actin dynamics in membrane protrusions and vesicle trafficking. Trends Cell Biol. 2006; 16:522–529.
8. Navarro-Lerida I, Sanchez-Perales S, Calvo M, et al. A palmitoylation switch mechanism regulates Rac1 function and membrane organization. EMBO J. 2012; 31:534–551.
9. Wang L, Zheng Y. Cell type-specific functions of Rho GTPases revealed by gene targeting in mice. Trends Cell Biol. 2007; 17:58–64.
10. Gao Y, Dickerson JB, Guo F, et al. Rational design and characterization of a Rac GTPase-specific small molecule inhibitor. Proc Natl Acad Sci USA. 2004; 101:7618–7623.
11. Shang X, Marchioni F, Sipes N, et al. Rational design of small molecule inhibitors targeting RhoA subfamily Rho GTPases. Chem Biol. 2012; 19:699–710.
12. Yang FC, Atkinson SJ, Gu Y, et al. Rac and Cdc42 GTPases control hematopoietic stem cell shape, adhesion, migration, and mobilization. Proc Natl Acad Sci USA. 2001; 98:5614–5618.
13. Akashi K, Traver D, Miyamoto T, Weissman IL. A clonogenic common myeloid progenitor that gives rise to all myeloid lineages. Nature. 2000; 404:193–197.
14. Iscove NN, Sieber F, Winterhalter KH. Erythroid colony formation in cultures of mouse and human bone marrow: analysis of the requirement for erythropoietin by gel filtration and affinity chromatography on agarose-concanavalin A. J Cell Physiol. 1974; 83:309–320.
15. Pronk CJ, Rossi DJ, Mansson R, et al. Elucidation of the phenotypic, functional, and molecular topography of a myeloerythroid progenitor cell hierarchy. Cell Stem Cell. 2007; 1:428–442.
16. Hattangadi SM, Wong P, Zhang L, et al. From stem cell to red cell: regulation of erythropoiesis at multiple levels by multiple proteins, RNAs, and chromatin modifications. Blood. 2011; 118:6258–6268.
17. Cantor AB, Orkin SH. Transcriptional regulation of erythropoiesis: an affair involving multiple partners. Oncogene. 2002; 21:3368–3376.
18. Moll J, Sansig G, Fattori E, van der Putten H. The murine rac1 gene: cDNA cloning, tissue distribution and regulated expression of rac1 mRNA by disassembly of actin microfilaments. Oncogene. 1991; 6:863–866.
19. Shirsat NV, Pignolo RJ, Kreider BL, Rovera G. A member of the ras gene superfamily is expressed specifically in T, B and myeloid hemopoietic cells. Oncogene. 1990; 5:769–772.
20. Bolis A, Corbetta S, Cioce A, de Curtis I. Differential distribution of Rac1 and Rac3 GTPases in the developing mouse brain: implications for a role of Rac3 in Purkinje cell differentiation. Eur J Neurosci. 2003; 18:2417–2424.
21. Gu Y, Filippi MD, Cancelas JA, et al. Hematopoietic cell regulation by Rac1 and Rac2 guanosine triphosphatases. Science. 2003; 302:445–449.
22. Cancelas JA, Lee AW, Prabhakar R, et al. Rac GTPases differentially integrate signals regulating hematopoietic stem cell localization. Nat Med. 2005; 11:886–891.
23. Roberts AW, Kim C, Zhen L, et al. Deficiency of the hematopoietic cell-specific Rho family GTPase Rac2 is characterized by abnormalities in neutrophil function and host defense. Immunity. 1999; 10:183–196.
24. Sugihara K, Nakatsuji N, Nakamura K, et al. Rac1 is required for the formation of three germ layers during gastrulation. Oncogene. 1998; 17:3427–3433.
25. Kalfa TA, Pushkaran S, Mohandas N, et al. Rac GTPases regulate the morphology and deformability of the erythrocyte cytoskeleton. Blood. 2006; 108:3637–3645.
26. Kalfa TA, Pushkaran S, Zhang X, et al. Rac1 and Rac2 GTPases are necessary for early erythropoietic expansion in the bone marrow but not in the spleen. Haematologica. 2010; 95:27–35.
27. Lenox LE, Perry JM, Paulson RF. BMP4 and Madh5 regulate the erythroid response to acute anemia. Blood. 2005; 105:2741–2748.
28. Mulloy JC, Cancelas JA, Filippi MD, et al. Rho GTPases in hematopoiesis and hemopathies. Blood. 2010; 115:936–947.
29. Wang L, Yang L, Filippi MD, et al. Genetic deletion of Cdc42GAP reveals a role of Cdc42 in erythropoiesis and hematopoietic stem/progenitor cell survival, adhesion, and engraftment. Blood. 2006; 107:98–105.
30. Yang L, Wang L, Kalfa T, et al. Cdc42 critically regulates the balance between myelopoiesis and erythropoiesis. Blood. 2007; 110:3853–3861.
31. Zhou X, Florian MC, Arumugam P, et al. RhoA GTPase controls cytokinesis and programmed necrosis of hematopoietic progenitors. J Exp Med. 2013; 210:2371–2385.
32. Gabet AS, Coulon S, Fricot A, et al. Caspase-activated ROCK-1 allows erythroblast terminal maturation independently of cytokine-induced Rho signaling. Cell Death Differ. 2011; 18:678–689.
33. Bessis M, Mize C, Prenant M. Erythropoiesis: comparison of in vivo and in vitro amplification. Blood Cells. 1978; 4:155–174.
34. Sebbagh M, Renvoize C, Hamelin J, et al. Caspase-3-mediated cleavage of ROCK I induces MLC phosphorylation and apoptotic membrane blebbing. Nat Cell Biol. 2001; 3:346–352.
35. Vemula S, Shi J, Mali RS, et al. ROCK1 functions as a critical regulator of stress erythropoiesis and survival by regulating p53. Blood. 2012; 120:2868–2878.
36▪. Watanabe S, De Zan T, Ishizaki T, et al. Loss of a Rho-regulated actin nucleator, mDia2, impairs cytokinesis during mouse fetal erythropoiesis. Cell Rep. 2013; 5:926–932.
This is the first study of the role of mDia2 in erythropoiesis in a gene-targeted mouse model, demonstrating the defects in erythroblast cytokinesis.
37. Ji P, Jayapal SR, Lodish HF. Enucleation of cultured mouse fetal erythroblasts requires Rac GTPases and mDia2. Nat Cell Biol. 2008; 10:314–321.
38▪▪. Konstantinidis DG, Pushkaran S, Johnson JF, et al. Signaling and cytoskeletal requirements in erythroblast enucleation. Blood. 2012; 119:6118–6127.
This study presents a new assay utilizing multispectral high-speed cell imaging in flow in order to visualize cytoskeletal and signaling components in a population enriched in enucleating erythroblasts.
39. DeWard AD, Leali K, West RA, et al. Loss of RhoB expression enhances the myelodysplastic phenotype of mammalian diaphanous-related Formin mDia1 knockout mice. PLoS ONE. 2009; 4:e7102
40. Peng J, Kitchen SM, West RA, et al. Myeloproliferative defects following targeting of the Drf1 gene encoding the mammalian diaphanous related formin mDia1. Cancer Res. 2007; 67:7565–7571.
41. Kalfa TA, Pushkaran S, Cancelas JA, et al. Deficiency of Rac1 and Rac2 GTPases perturbs erythroid proliferation and differentiation but not enucleation. Blood. 2006; 108:142a
42. Koury ST, Koury MJ, Bondurant MC. Cytoskeletal distribution and function during the maturation and enucleation of mammalian erythroblasts. J Cell Biol. 1989; 109:3005–3013.
43. Chasis JA, Prenant M, Leung A, Mohandas N. Membrane assembly and remodeling during reticulocyte maturation. Blood. 1989; 74:1112–1120.
44▪▪. Ubukawa K, Guo YM, Takahashi M, et al. Enucleation of human erythroblasts involves nonmuscle myosin IIB. Blood. 2012; 119:1036–1044.
This is the first study establishing a previously undefined role for myosin in enucleation.
45. Scholey JM, Brust-Mascher I, Mogilner A. Cell division. Nature. 2003; 422:746–752.
46. Bement WM, Benink HA, von Dassow G. A microtubule-dependent zone of active RhoA during cleavage plane specification. J Cell Biol. 2005; 170:91–101.
47. Ng MM, Chang F, Burgess DR. Movement of membrane domains and requirement of membrane signaling molecules for cytokinesis. Dev Cell. 2005; 9:781–790.
48. Baluska F, Menzel D, Barlow PW. Cytokinesis in plant and animal cells: endosomes ‘shut the door’. Dev Biol. 2006; 294:1–10.
49. Boucrot E, Kirchhausen T. Endosomal recycling controls plasma membrane area during mitosis. Proc Natl Acad Sci USA. 2007; 104:7939–7944.
50▪▪. Li R. The art of choreographing asymmetric cell division. Dev Cell. 2013; 25:439–450.
This is a well written review examining the divergent mechanisms of asymmetric cell division from prokaryotes to unicellular eukaryotes and multicellular species with diverse cell types.
51▪▪. Mohandas N. Exit strategy: one that works. Blood. 2012; 119:906–907.
A comprehensive and succinct editorial on the investigations of the mechanism of erythroblast enucleation.
52. Simpson CF, Kling JM. The mechanism of denucleation in circulating erythroblasts. J Cell Biol. 1967; 35:237–245.
53. Keerthivasan G, Small S, Liu H, et al. Vesicle trafficking plays a novel role in erythroblast enucleation. Blood. 2010; 116:3331–3340.
54. Ling E, Gardner K, Bennett V. Protein kinase C phosphorylates a recently identified membrane skeleton-associated calmodulin-binding protein in human erythrocytes. J Biol Chem. 1986; 261:13875–13878.
55. Matsuoka Y, Li X, Bennett V. Adducin is an in vivo substrate for protein kinase C: phosphorylation in the MARCKS-related domain inhibits activity in promoting spectrin–actin complexes and occurs in many cells, including dendritic spines of neurons. J Cell Biol. 1998; 142:485–497.
56▪. George A, Pushkaran S, Konstantinidis DG, et al. Erythrocyte NADPH oxidase activity modulated by Rac GTPases, PKC, and plasma cytokines contributes to oxidative stress in sickle cell disease. Blood. 2013; 121:2099–2107.
This is the first study demonstrating that production of reactive oxygen species in sickle RBCs is at a large part enzymatically mediated by Rac-controlled NADPH oxidase, stimulated by inflammatory cytokines.
57. Bedard K, Krause KH. The NOX family of ROS-generating NADPH oxidases: physiology and pathophysiology. Physiol Rev. 2007; 87:245–313.
Cdc42; erythroblast enucleation; erythropoiesis; Rac; Rho GTPases; RhoA
© 2014 Wolters Kluwer Health | Lippincott Williams & Wilkins
Highlight selected keywords in the article text.