Fine-tuning cell organelle dynamics during mitosis by small GTPases
Zijian Zhang1, Wei Zhang2, Quentin Liu1,3()
1. Sun Yat-sen University Cancer Center; State Key Laboratory of Oncology in South China; Collaborative Innovation Center for Cancer Medicine, Guangzhou 510060, China 2. Department of Clinical Immunology, The Third Affiliated Hospital, Sun Yat-sen University, Guangzhou 510630, China 3. Institute of Cancer Stem Cell, Dalian Medical University, Dalian 116044, China
During mitosis, the allocation of genetic material concurs with organelle transformation and distribution. The coordination of genetic material inheritance with organelle dynamics directs accurate mitotic progression, cell fate determination, and organismal homeostasis. Small GTPases belonging to the Ras superfamily regulate various cell organelles during division. Being the key regulators of membrane dynamics, the dysregulation of small GTPases is widely associated with cell organelle disruption in neoplastic and non-neoplastic diseases, such as cancer and Alzheimer’s disease. Recent discoveries shed light on the molecular properties of small GTPases as sophisticated modulators of a remarkably complex and perfect adaptors for rapid structure reformation. This review collects current knowledge on small GTPases in the regulation of cell organelles during mitosis and highlights the mediator role of small GTPase in transducing cell cycle signaling to organelle dynamics during mitosis.
RanGTP recruits essential centrosome and kinetochore components and releases and activates spindle assembly factors to nucleate, bind, and organize nascent spindle microtubules
[13,36–41]
Cdc42
Bi-orientation and stabilization of spindle microtubule attachment to kinetochores, spindle assembly, and spindle orientation
[42,43]
RhoA
Maintenance of spindle orientation
[42]
Rab5
Regulation of the astral microtubule size and spindle alignment
[45]
Rab11
Bringing microtubule-nucleating factors and spindle pole proteins to spindle poles
[44,46,47]
Arl8A, Arl8B
Centrosome maturation and chromosome segregation
[48,49]
RalA
Regulation of the kinetochore–microtubule interaction in early mitosis
[50]
Plasma membrane
Rap1
Focal adhesion assembly–disassembly
[25,71,72]
RhoA
Actomyosin cortex organization beneath the plasma membrane during mitosis
[73,76,77]
Ran
Polar cortex relaxation and ingression furrow position
Rac1
Repolarization of the actomyosin cortex
[69,80]
ER & nuclear envelope
Rab5
ER membrane remodeling and NEBD. Rab5 depletion inhibits nuclear envelope disassembly
[108]
Ran
Ran activities regulate microtubule dynamics and the mechanical rupture of nuclear envelope during NEBD. After division, Ran promotes the assembly of NPCs and vesicle fusion
[114,118–123]
Cd42
Nuclear envelope sealing and ER remodeling
[126]
Golgi apparatus
Arf1
Participation in the Golgi cycle through the regulation of vesicle transportation
[96,133,134]
Sar1
Participation in the Golgi cycle through the regulation of vesicle transportation
Promotion of mitochondrial fission during mitotic entry
[21]
Arf1
Recruitment of PI(4)P-containing vesicles at ER-mitochondria contact site and promotion of mitochondrial fission
[152]
Miro
Miro1 and Miro2 bind CENP-F and associate with microtubule-growing tips. Miro loss decreases the spreading of the mitochondrial network and causes cytokinesis-specific defects
[154]
Midbody
RhoA
Position of ingression furrow and membrane ingression and abscission
[161,169–172,175,176]
Rac1
Membrane ingression. The overexpression of constitutively active Rac1 causes multinucleation and cytokinesis failure
[42,187,192]
Rab1
Rab1 facilitates new membrane supplementation along the ingressing cleavage furrow
[191]
Rab11
Through en dosome transport to facilitate furrow ingression and F-actin elimination for final abscission
[192,194,198,200,201]
Rab35
Through endosome transport to facilitate F-actin elimination for final abscission
[194,200–202]
Arf1
Golgi organization and Golgi output for ingression furrow function
[193]
Arf6
Bridge stability and abscission
[65,204]
RalA & RalB
RalA and RalB control the exocyst localization at the furrow and midbody, respectively. Their collaboration is required for abscission completion
[205,206]
Autophagosome
Rabs & Sec4
Autophagosome formation. Role in mitosis is unknown
[212–215]
Rab7, Rab8B & Rab24
Autophagosome maturation. Role in mitosis is unknown
[213,214,216–219]
Arfs & Sar1
Autophagosome biogenesis and cellular localization. Role in mitosis is unknown
[213,220]
Peroxisomes
Rho, Rab, Arf & Miro
In the interphase, small GTPases regulate peroxisome distribution and biogenesis. The disruption of spindle pole localization of peroxisomes impairs spindle orientation. The direct role in mitosis is unclear
S Song, W Cong, S Zhou, Y Shi, W Dai, H Zhang, X Wang, B He, Q Zhang. Small GTPases: structure, biological function and its interaction with nanoparticles. Asian J Pharm Sci 2019; 14( 1): 30– 39 https://doi.org/10.1016/j.ajps.2018.06.004
5
IR Vetter. The structure of the G domain of the Ras superfamily. In: Wittinghofer A. Ras Superfamily Small G Proteins: Biology and Mechanisms 1. Springer Vienna, 2014: 25- 50 doi:10.1007/978-3-7091-1806-1_2
6
K Wennerberg, KL Rossman, CJ Der. The Ras superfamily at a glance. J Cell Sci 2005; 118( 5): 843– 846 https://doi.org/10.1242/jcs.01660
7
Hodge RG, Schaefer A, Howard SV, Der CJ. RAS and RHO family GTPase mutations in cancer: twin sons of different mothers? Crit Rev Biochem Mol Biol 2020; 55(4): 386–407
pmid: 32838579" target="_blank">32838579
8
AM Rojas, G Fuentes, A Rausell, A Valencia. The Ras protein superfamily: evolutionary tree and role of conserved amino acids. J Cell Biol. 2012; 196 : 189– 201 https://doi.org/10.1083/jcb.201103008
J Bos H Rehmann A Wittinghofer. GEFs and GAPs: critical elements in the control of small G proteins. Cell 2007; 129(5): 865–877 Erratum in: Cell 2007; 130(2): 385
pmid: 17540168
11
J Cherfils. GEFs and GAPs: mechanisms and structures. In: Wittinghofer A. Ras Superfamily Small G Proteins: Biology and Mechanisms 1. Springer Vienna; 2014: 51- 63
PR Clarke, C Zhang. Spatial and temporal coordination of mitosis by Ran GTPase. Nat Rev Mol Cell Biol 2008; 9( 6): 464– 477 https://doi.org/10.1038/nrm2410
14
CL Jackson, S Bouvet. Arfs at a glance. J Cell Sci 2014; 127( 19): 4103– 4109
15
SL Schwartz, C Cao, O Pylypenko, A Rak, A Wandinger-Ness. Rab GTPases at a glance. J Cell Sci 2007; 120( 22): 3905– 3910 https://doi.org/10.1242/jcs.015909
16
C D’Souza-Schorey, P Chavrier. ARF proteins: roles in membrane traffic and beyond. Nat Rev Mol Cell Biol 2006; 7( 5): 347– 358 https://doi.org/10.1038/nrm1910
17
I Kjos, K Vestre, NA Guadagno, M Borg Distefano, C Progida. Rab and Arf proteins at the crossroad between membrane transport and cytoskeleton dynamics. Biochim Biophys Acta Mol Cell Res 2018; 1865( 10): 1397– 1409 https://doi.org/10.1016/j.bbamcr.2018.07.009
18
SI Bannykh, H Plutner, J Matteson, WE Balch. The role of ARF1 and rab GTPases in polarization of the Golgi stack. Traffic 2005; 6( 9): 803– 819 https://doi.org/10.1111/j.1600-0854.2005.00319.x
19
N Yahara, T Ueda, K Sato, A Nakano. Multiple roles of Arf1 GTPase in the yeast exocytic and endocytic pathways. Mol Biol Cell 2001; 12( 1): 221– 238 https://doi.org/10.1091/mbc.12.1.221
RG Hodge, AJ Ridley. Regulating Rho GTPases and their regulators. Nat Rev Mol Cell Biol 2016; 17( 8): 496– 510 https://doi.org/10.1038/nrm.2016.67
24
EA Nigg. Mitotic kinases as regulators of cell division and its checkpoints. Nat Rev Mol Cell Biol 2001; 2( 1): 21– 32 https://doi.org/10.1038/35048096
25
VT Dao, AG Dupuy, O Gavet, E Caron, J de Gunzburg. Dynamic changes in Rap1 activity are required for cell retraction and spreading during mitosis. J Cell Sci 2009; 122( 16): 2996– 3004 https://doi.org/10.1242/jcs.041301
26
M Glotzer, AW Murray, MW Kirschner. Cyclin is degraded by the ubiquitin pathway. Nature 1991; 349( 6305): 132– 138 https://doi.org/10.1038/349132a0
27
Z Lei, J Wang, L Zhang, CH Liu. Ubiquitination-dependent regulation of small GTPases in membrane trafficking: from cell biology to human diseases. Front Cell Dev Biol 2021; 9 : 688352 https://doi.org/10.3389/fcell.2021.688352
28
M de la Vega, JF Burrows, JA Johnston. Ubiquitination: added complexity in Ras and Rho family GTPase function. Small GTPases 2011; 2( 4): 192– 201 https://doi.org/10.4161/sgtp.2.4.16707
P Song, K Trajkovic, T Tsunemi, D Krainc. Parkin modulates endosomal organization and function of the endo-lysosomal pathway. J Neurosci 2016; 36( 8): 2425– 2437 https://doi.org/10.1523/JNEUROSCI.2569-15.2016
31
H-R Wang, Y Zhang, B Ozdamar, AA Ogunjimi, E Alexandrova, GH Thomsen, JL Wrana. Regulation of cell polarity and protrusion formation by targeting RhoA for degradation. Science 2003; 302( 5651): 1775– 1779 https://doi.org/10.1126/science.1090772
32
MC Seabra, JL Goldstein, TC Südhof, MS Brown. Rab geranylgeranyl transferase. A multisubunit enzyme that prenylates GTP-binding proteins terminating in Cys-X-Cys or Cys-Cys. J Biol Chem 1992; 267( 20): 14497– 14503 https://doi.org/10.1016/S0021-9258(19)49740-8
33
KF Leung, R Baron, BR Ali, AI Magee, MC Seabra. Rab GTPases containing a CAAX motif are processed post-geranylgeranylation by proteolysis and methylation. J Biol Chem 2007; 282( 2): 1487– 1497 https://doi.org/10.1074/jbc.M605557200
34
R Heald, A Khodjakov. Thirty years of search and capture: the complex simplicity of mitotic spindle assembly. J Cell Biol 2015; 211( 6): 1103– 1111 https://doi.org/10.1083/jcb.201510015
35
CB O’Connell, AL Khodjakov. Cooperative mechanisms of mitotic spindle formation. J Cell Sci 2007; 120( 10): 1717– 1722 https://doi.org/10.1242/jcs.03442
Y Feng, JH Yuan, SC Maloid, R Fisher, TD Copeland, DL Longo, TP Conrads, TD Veenstra, A Ferris, S Hughes, DS Dimitrov, DK Ferris. Polo-like kinase 1-mediated phosphorylation of the GTP-binding protein Ran is important for bipolar spindle formation. Biochem Biophys Res Commun 2006; 349( 1): 144– 152 https://doi.org/10.1016/j.bbrc.2006.08.028
38
G Bompard, G Rabeharivelo, M Frank, J Cau, C Delsert, N Morin. Subgroup II PAK-mediated phosphorylation regulates Ran activity during mitosis. J Cell Biol 2010; 190( 5): 807– 822 https://doi.org/10.1083/jcb.200912056
39
A Tedeschi, M Ciciarello, R Mangiacasale, E Roscioli, WM Rensen, P Lavia. RANBP1 localizes a subset of mitotic regulatory factors on spindle microtubules and regulates chromosome segregation in human cells. J Cell Sci 2007; 120( 21): 3748– 3761 https://doi.org/10.1242/jcs.009308
40
ST Sit, E Manser. Rho GTPases and their role in organizing the actin cytoskeleton. J Cell Sci 2011; 124( 5): 679– 683 https://doi.org/10.1242/jcs.064964
41
PM Müller, J Rademacher, RD Bagshaw, C Wortmann, C Barth, Unen J van, KM Alp, G Giudice, RL Eccles, LE Heinrich, P Pascual-Vargas, M Sanchez-Castro, L Brandenburg, G Mbamalu, M Tucholska, L Spatt, MT Czajkowski, RW Welke, S Zhang, V Nguyen, T Rrustemi, P Trnka, K Freitag, B Larsen, O Popp, P Mertins, AC Gingras, FP Roth, K Colwill, C Bakal, O Pertz, T Pawson, E Petsalaki, O Rocks. Systems analysis of RhoGEF and RhoGAP regulatory proteins reveals spatially organized RAC1 signalling from integrin adhesions. Nat Cell Biol 2020; 22( 4): 498– 511 https://doi.org/10.1038/s41556-020-0488-x
42
M Chircop. Rho GTPases as regulators of mitosis and cytokinesis in mammalian cells. Small GTPases 2014; 5( 2): e29770 https://doi.org/10.4161/sgtp.29770
43
S Yasuda, H Taniguchi, F Oceguera-Yanez, Y Ando, S Watanabe, J Monypenny, S Narumiya. An essential role of Cdc42-like GTPases in mitosis of HeLa cells. FEBS Lett 2006; 580( 14): 3375– 3380 https://doi.org/10.1016/j.febslet.2006.05.009
KC Hobdy-Henderson, CM Hales, LA Lapierre, RE Cheney, JR Goldenring. Dynamics of the apical plasma membrane recycling system during cell division. Traffic 2003; 4( 10): 681– 693 https://doi.org/10.1034/j.1600-0854.2003.00124.x
48
C Zhou, L Cunningham, AI Marcus, Y Li, RA Kahn. Arl2 and Arl3 regulate different microtubule-dependent processes. Mol Biol Cell 2006; 17( 5): 2476– 2487 https://doi.org/10.1091/mbc.e05-10-0929
49
T Okai, Y Araki, M Tada, T Tateno, K Kontani, T Katada. Novel small GTPase subfamily capable of associating with tubulin is required for chromosome segregation. J Cell Sci 2004; 117( 20): 4705– 4715 https://doi.org/10.1242/jcs.01347
50
D Papini, L Langemeyer, MA Abad, A Kerr, I Samejima, PA Eyers, AA Jeyaprakash, JMG Higgins, FA Barr, WC Earnshaw. TD-60 links RalA GTPase function to the CPC in mitosis. Nat Commun 2015; 6( 1): 7678 https://doi.org/10.1038/ncomms8678
51
S Boeynaems, S Alberti, NL Fawzi, T Mittag, M Polymenidou, F Rousseau, J Schymkowitz, J Shorter, B Wolozin, L Van Den Bosch, P Tompa, M Fuxreiter. Protein phase separation: a new phase in cell biology. Trends Cell Biol 2018; 28( 6): 420– 435 https://doi.org/10.1016/j.tcb.2018.02.004
TJ Nott, E Petsalaki, P Farber, D Jervis, E Fussner, A Plochowietz, TD Craggs, DP Bazett-Jones, T Pawson, JD Forman-Kay, AJ Baldwin. Phase transition of a disordered nuage protein generates environmentally responsive membraneless organelles. Mol Cell 2015; 57( 5): 936– 947 https://doi.org/10.1016/j.molcel.2015.01.013
AK Rai, JXX Chen, M Selbach, L Pelkmans. Kinase-controlled phase transition of membraneless organelles in mitosis. Nature 2018; 559( 7713): 211– 216 https://doi.org/10.1038/s41586-018-0279-8
56
H Jiang, S Wang, Y Huang, X He, H Cui, X Zhu, Y Zheng. Phase transition of spindle-associated protein regulate spindle apparatus assembly. Cell 2015; 163( 1): 108– 122 https://doi.org/10.1016/j.cell.2015.08.010
57
JB Woodruff, B Ferreira Gomes, PO Widlund, J Mahamid, A Honigmann, AA Hyman. The centrosome is a selective condensate that nucleates microtubules by concentrating tubulin. Cell 2017; 169( 6): 1066– 1077.e10 https://doi.org/10.1016/j.cell.2017.05.028
58
G Keryer, O Witczak, A Delouvée, WA Kemmner, D Rouillard, K Taskén, M Bornens. Dissociating the centrosomal matrix protein AKAP450 from centrioles impairs centriole duplication and cell cycle progression. Mol Biol Cell 2003; 14( 6): 2436– 2446 https://doi.org/10.1091/mbc.e02-09-0614
59
G Keryer, Fiore B Di, C Celati, KF Lechtreck, M Mogensen, A Delouvée, P Lavia, M Bornens, AM Tassin. Part of Ran is associated with AKAP450 at the centrosome: involvement in microtubule-organizing activity. Mol Biol Cell 2003; 14( 10): 4260– 4271 https://doi.org/10.1091/mbc.e02-11-0773
60
G Bompard, G Rabeharivelo, J Cau, A Abrieu, C Delsert, N Morin. P21-activated kinase 4 (PAK4) is required for metaphase spindle positioning and anchoring. Oncogene 2013; 32( 7): 910– 919 https://doi.org/10.1038/onc.2012.98
61
C Kilchert, J Weidner, C Prescianotto-Baschong, A Spang. Defects in the secretory pathway and high Ca2+ induce multiple P-bodies. Mol Biol Cell 2010; 21( 15): 2624– 2638 https://doi.org/10.1091/mbc.e10-02-0099
62
G Serio, V Margaria, S Jensen, A Oldani, J Bartek, F Bussolino, L Lanzetti. Small GTPase Rab5 participates in chromosome congression and regulates localization of the centromere-associated protein CENP-F to kinetochores. Proc Natl Acad Sci USA 2011; 108( 42): 17337– 17342 https://doi.org/10.1073/pnas.1103516108
63
X Zhang, J Hagen, VP Muniz, T Smith, GS Coombs, CM Eischen, DI Mackie, DL Roman, R Van Rheeden, B Darbro, VS Tompkins, DE Quelle. RABL6A, a novel RAB-like protein, controls centrosome amplification and chromosome instability in primary fibroblasts. PLoS One 2013; 8( 11): e80228 https://doi.org/10.1371/journal.pone.0080228
64
H Hehnly, CTT Chen, CM Powers, HLL Liu, S Doxsey. The centrosome regulates the Rab11-dependent recycling endosome pathway at appendages of the mother centriole. Curr Biol 2012; 22( 20): 1944– 1950 https://doi.org/10.1016/j.cub.2012.08.022
65
S Takahashi, T Takei, H Koga, H Takatsu, HW Shin, K Nakayama. Distinct roles of Rab11 and Arf6 in the regulation of Rab11-FIP3/arfophilin-1 localization in mitotic cells. Genes Cells 2011; 16( 9): 938– 950 https://doi.org/10.1111/j.1365-2443.2011.01538.x
N Ramkumar, B Baum. Coupling changes in cell shape to chromosome segregation. Nat Rev Mol Cell Biol 2016; 17( 8): 511– 521 https://doi.org/10.1038/nrm.2016.75
68
GE Atilla-Gokcumen, E Muro, J Relat-Goberna, S Sasse, A Bedigian, ML Coughlin, S Garcia-Manyes, US Eggert. Dividing cells regulate their lipid composition and localization. Cell 2014; 156( 3): 428– 439 https://doi.org/10.1016/j.cell.2013.12.015
HS Lee, CJ Lim, W Puzon-McLaughlin, SJ Shattil, MH Ginsberg. RIAM activates integrins by linking talin to ras GTPase membrane-targeting sequences. J Biol Chem 2009; 284( 8): 5119– 5127 https://doi.org/10.1074/jbc.M807117200
72
EM Lafuente, AAFL van Puijenbroek, M Krause, CV Carman, GJ Freeman, A Berezovskaya, E Constantine, TA Springer, FB Gertler, VA Boussiotis. RIAM, an Ena/VASP and Profilin ligand, interacts with Rap1-GTP and mediates Rap1-induced adhesion. Dev Cell 2004; 7( 4): 585– 595 https://doi.org/10.1016/j.devcel.2004.07.021
73
S Marchesi, F Montani, G Deflorian, R D’Antuono, A Cuomo, S Bologna, C Mazzoccoli, T Bonaldi, Fiore PP Di, F Nicassio. DEPDC1B coordinates de-adhesion events and cell-cycle progression at mitosis. Dev Cell 2014; 31( 4): 420– 433 https://doi.org/10.1016/j.devcel.2014.09.009
74
OM Lancaster, M Le Berre, A Dimitracopoulos, D Bonazzi, E Zlotek-Zlotkiewicz, R Picone, T Duke, M Piel, B Baum. Mitotic rounding alters cell geometry to ensure efficient bipolar spindle formation. Dev Cell 2013; 25( 3): 270– 283 https://doi.org/10.1016/j.devcel.2013.03.014
TR Arnold, RE Stephenson, AL Miller. Rho GTPases and actomyosin: partners in regulating epithelial cell-cell junction structure and function. Exp Cell Res 2017; 358( 1): 20– 30 https://doi.org/10.1016/j.yexcr.2017.03.053
77
A Rosa, E Vlassaks, F Pichaud, B Baum. Ect2/Pbl acts via Rho and polarity proteins to direct the assembly of an isotropic actomyosin cortex upon mitotic entry. Dev Cell 2015; 32( 5): 604– 616 https://doi.org/10.1016/j.devcel.2015.01.012
H Neto, LL Collins, GW Gould. Vesicle trafficking and membrane remodelling in cytokinesis. Biochem J 2011; 437( 1): 13– 24 https://doi.org/10.1042/BJ20110153
81
T Kiyomitsu, IM Cheeseman. Cortical dynein and asymmetric membrane elongation coordinately position the spindle in anaphase. Cell 2013; 154( 2): 391– 402 https://doi.org/10.1016/j.cell.2013.06.010
82
T Kiyomitsu, IM Cheeseman. Chromosome- and spindle-pole-derived signals generate an intrinsic code for spindle position and orientation. Nat Cell Biol 2012; 14( 3): 311– 317 https://doi.org/10.1038/ncb2440
83
SL Bird, R Heald, K Weis. RanGTP and CLASP1 cooperate to position the mitotic spindle. Mol Biol Cell 2013; 24( 16): 2506– 2514 https://doi.org/10.1091/mbc.e13-03-0150
O Baumann, B Walz. Endoplasmic reticulum of animal cells and its organization into structural and functional domains. Int Rev Cytol 2001; 205 : 149– 214 https://doi.org/10.1016/s0074-7696(01)05004-5
86
JR Friedman, GK Voeltz. The ER in 3D: a multifunctional dynamic membrane network. Trends Cell Biol 2011; 21( 12): 709– 717 https://doi.org/10.1016/j.tcb.2011.07.004
DS Schwarz, MD Blower. The endoplasmic reticulum: structure, function and response to cellular signaling. Cell Mol Life Sci 2016; 73( 1): 79– 94 https://doi.org/10.1007/s00018-015-2052-6
89
AR English, GK Voeltz. Endoplasmic reticulum structure and interconnections with other organelles. Cold Spring Harb Perspect Biol 2013; 5( 4): a013227 https://doi.org/10.1101/cshperspect.a013227
90
H Merta, Rodríguez JW Carrasquillo, MI Anjur-Dietrich, T Vitale, ME Granade, TE Harris, DJ Needleman, S Bahmanyar. Cell cycle regulation of ER membrane biogenesis protects against chromosome missegregation. Dev Cell 2021; 56( 24): 3364– 3379.e10 https://doi.org/10.1016/j.devcel.2021.11.009
91
T Oertle, M Klinger, CAO Stuermer, ME Schwab. A reticular rhapsody: phylogenic evolution and nomenclature of the RTN/Nogo gene family. FASEB J 2003; 17( 10): 1238– 1247 https://doi.org/10.1096/fj.02-1166hyp
92
F Di Sano, P Bernardoni, M Piacentini. The reticulons: guardians of the structure and function of the endoplasmic reticulum. Exp Cell Res 2012; 318( 11): 1201– 1207 https://doi.org/10.1016/j.yexcr.2012.03.002
93
GK Voeltz, WA Prinz, Y Shibata, JM Rist, TA Rapoport. A class of membrane proteins shaping the tubular endoplasmic reticulum. Cell 2006; 124( 3): 573– 586 https://doi.org/10.1016/j.cell.2005.11.047
94
A Gerondopoulos, RN Bastos, S Yoshimura, R Anderson, S Carpanini, I Aligianis, MT Handley, FA Barr. Rab18 and a Rab18 GEF complex are required for normal ER structure. J Cell Biol 2014; 205( 5): 707– 720 https://doi.org/10.1083/jcb.201403026
95
AR English, GK Voeltz. Rab10 GTPase regulates ER dynamics and morphology. Nat Cell Biol 2013; 15( 2): 169– 178 https://doi.org/10.1038/ncb2647
96
Y Morohashi, Z Balklava, M Ball, H Hughes, M Lowe. Phosphorylation and membrane dissociation of the ARF exchange factor GBF1 in mitosis. Biochem J 2010; 427( 3): 401– 412 https://doi.org/10.1042/BJ20091681
97
D Kumar, B Golchoubian, I Belevich, E Jokitalo, ALL Schlaitz. REEP3 and REEP4 determine the tubular morphology of the endoplasmic reticulum during mitosis. Mol Biol Cell 2019; 30( 12): 1377– 1389 https://doi.org/10.1091/mbc.E18-11-0698
98
AL Schlaitz, J Thompson, CCLL Wong, JR 3rd Yates, R Heald. REEP3/4 ensure endoplasmic reticulum clearance from metaphase chromatin and proper nuclear envelope architecture. Dev Cell 2013; 26( 3): 315– 323 https://doi.org/10.1016/j.devcel.2013.06.016
99
JT Arnone, AD Walters, O Cohen-Fix. The dynamic nature of the nuclear envelope: lessons from closed mitosis. Nucleus 2013; 4( 4): 261– 266 https://doi.org/10.4161/nucl.25341
M Peter, J Nakagawa, M Dorée, JC Labbé, EA Nigg. Identification of major nucleolar proteins as candidate mitotic substrates of cdc2 kinase. Cell 1990; 60( 5): 791– 801 https://doi.org/10.1016/0092-8674(90)90093-T
105
R Heald, F McKeon. Mutations of phosphorylation sites in lamin A that prevent nuclear lamina disassembly in mitosis. Cell 1990; 61( 4): 579– 589 https://doi.org/10.1016/0092-8674(90)90470-Y
106
E Torvaldson, V Kochin, JE Eriksson. Phosphorylation of lamins determine their structural properties and signaling functions. Nucleus 2015; 6( 3): 166– 171 https://doi.org/10.1080/19491034.2015.1017167
107
O Martinez de Ilarduya, J Vicente-Carbajosa, P Sanchez de la Hoz, P Carbonero. Sucrose synthase genes in barley. cDNA cloning of the Ss2 type and tissue-specific expression of Ss1 and Ss2. FEBS Lett 1993; 320( 2): 177– 181 https://doi.org/10.1016/0014-5793(93)80087-B
108
A Audhya, A Desai, K Oegema. A role for Rab5 in structuring the endoplasmic reticulum. J Cell Biol 2007; 178( 1): 43– 56 https://doi.org/10.1083/jcb.200701139
109
E Nielsen, F Severin, JM Backer, AA Hyman, M Zerial. Rab5 regulates motility of early endosomes on microtubules. Nat Cell Biol 1999; 1( 6): 376– 382 https://doi.org/10.1038/14075
110
C Bucci, RG Parton, IH Mather, H Stunnenberg, K Simons, B Hoflack, M Zerial. The small GTPase rab5 functions as a regulatory factor in the early endocytic pathway. Cell 1992; 70( 5): 715– 728 https://doi.org/10.1016/0092-8674(92)90306-W
111
T Cavazza, I Vernos. The RanGTP pathway: from nucleo-cytoplasmic transport to spindle assembly and beyond. Front Cell Dev Biol 2016; 3 : 82 https://doi.org/10.3389/fcell.2015.00082
112
N Wesolowska, I Avilov, P Machado, C Geiss, H Kondo, M Mori, P Lénárt. Actin assembly ruptures the nuclear envelope by prying the lamina away from nuclear pores and nuclear membranes in starfish oocytes. eLife 2020; 9 : e49774 https://doi.org/10.7554/eLife.49774
113
L Penfield, B Wysolmerski, M Mauro, R Farhadifar, MA Martinez, R Biggs, HY Wu, C Broberg, D Needleman, S Bahmanyar. Dynein pulling forces counteract lamin-mediated nuclear stability during nuclear envelope repair. Mol Biol Cell 2018; 29( 7): 852– 868 https://doi.org/10.1091/mbc.E17-06-0374
114
P Mühlhäusser, U Kutay. An in vitro nuclear disassembly system reveals a role for the RanGTPase system and microtubule-dependent steps in nuclear envelope breakdown. J Cell Biol 2007; 178( 4): 595– 610 https://doi.org/10.1083/jcb.200703002
115
J Beaudouin, D Gerlich, N Daigle, R Eils, J Ellenberg. Nuclear envelope breakdown proceeds by microtubule-induced tearing of the lamina. Cell 2002; 108( 1): 83– 96 https://doi.org/10.1016/S0092-8674(01)00627-4
116
D Salina, K Bodoor, DMM Eckley, TA Schroer, JBB Rattner, B Burke. Cytoplasmic dynein as a facilitator of nuclear envelope breakdown. Cell 2002; 108( 1): 97– 107 https://doi.org/10.1016/S0092-8674(01)00628-6
117
M Sullivan, DO Morgan. Finishing mitosis, one step at a time. Nat Rev Mol Cell Biol 2007; 8( 11): 894– 903 https://doi.org/10.1038/nrm2276
118
C Zhang, PR Clarke. Chromatin-independent nuclear envelope assembly induced by Ran GTPase in Xenopus egg extracts. Science 2000; 288( 5470): 1429– 1432 https://doi.org/10.1126/science.288.5470.1429
119
M Hetzer, OJ Gruss, IW Mattaj. The Ran GTPase as a marker of chromosome position in spindle formation and nuclear envelope assembly. Nat Cell Biol 2002; 4( 7): E177– E184 https://doi.org/10.1038/ncb0702-e177
120
C Bamba, Y Bobinnec, M Fukuda, E Nishida. The GTPase Ran regulates chromosome positioning and nuclear envelope assembly in vivo. Curr Biol 2002; 12( 6): 503– 507 https://doi.org/10.1016/S0960-9822(02)00741-8
121
M Hetzer, D Bilbao-Cortés, TC Walther, OJ Gruss, IW Mattaj. GTP hydrolysis by Ran is required for nuclear envelope assembly. Mol Cell 2000; 5( 6): 1013– 1024 https://doi.org/10.1016/S1097-2765(00)80266-X
122
AK Schellhaus P De Magistris W Antonin. Nuclear reformation at the end of mitosis. J Mol Biol 2016; 428(10Pt A): 1962–1985 doi:10.1016/j.jmb.2015.09.016
pmid: 26423234
123
KB Matchett, S McFarlane, SE Hamilton, YSA Eltuhamy, MA Davidson, JT Murray, AM Faheem, M El-Tanani. Ran GTPase in Nuclear Envelope Formation and Cancer Metastasis. Adv Exp Med Biol 2014; 773 : 323– 351 https://doi.org/10.1007/978-1-4899-8032-8_15
124
AK Townley, Y Feng, K Schmidt, DA Carter, R Porter, P Verkade, DJ Stephens. Efficient coupling of Sec23-Sec24 to Sec13-Sec31 drives COPII-dependent collagen secretion and is essential for normal craniofacial development. J Cell Sci 2008; 121( 18): 3025– 3034 https://doi.org/10.1242/jcs.031070
125
S Siniossoglou, M Lutzmann, H Santos-Rosa, K Leonard, S Mueller, U Aebi, E Hurt. Structure and assembly of the Nup84p complex. J Cell Biol 2000; 149( 1): 41– 54 https://doi.org/10.1083/jcb.149.1.41
126
MS Lu, DG Drubin. Cdc42 GTPase regulates ESCRTs in nuclear envelope sealing and ER remodeling. J Cell Biol 2020; 219( 8): e201910119 https://doi.org/10.1083/jcb.201910119
127
X Chen, ES Simon, Y Xiang, M Kachman, PC Andrews, Y Wang. Quantitative proteomics analysis of cell cycle-regulated Golgi disassembly and reassembly. J Biol Chem 2010; 285( 10): 7197– 7207 https://doi.org/10.1074/jbc.M109.047084
Y Xiang, Y Wang. GRASP55 and GRASP65 play complementary and essential roles in Golgi cisternal stacking. J Cell Biol 2010; 188( 2): 237– 251 https://doi.org/10.1083/jcb.200907132
C Valente, A Colanzi. Mechanisms and regulation of the mitotic inheritance of the Golgi complex. Front Cell Dev Biol 2015; 3 : 79 https://doi.org/10.3389/fcell.2015.00079
133
L Mao N Li Y Guo X Xu L Gao Y Xu L Zhou W Liu. AMPK phosphorylates GBF1 for mitotic Golgi disassembly. J Cell Sci 2013; 126(Pt 6): 1498–1505 doi:10.1242/jcs.121954
pmid: 23418352
134
S Yadav, MA Puthenveedu, AD Linstedt. Golgin160 recruits the dynein motor to position the Golgi apparatus. Dev Cell 2012; 23( 1): 153– 165 https://doi.org/10.1016/j.devcel.2012.05.023
135
F Kano, AR Tanaka, S Yamauchi, H Kondo, M Murata. Cdc2 kinase-dependent disassembly of endoplasmic reticulum (ER) exit sites inhibits ER-to-Golgi vesicular transport during mitosis. Mol Biol Cell 2004; 15( 9): 4289– 4298 https://doi.org/10.1091/mbc.e03-11-0822
136
AR Prescott, T Farmaki, C Thomson, J James, JP Paccaud, BL Tang, W Hong, M Quinn, S Ponnambalam, J Lucocq. Evidence for prebudding arrest of ER export in animal cell mitosis and its role in generating Golgi partitioning intermediates. Traffic 2001; 2( 5): 321– 335 https://doi.org/10.1034/j.1600-0854.2001.002005321.x
137
WJ Stroud, S Jiang, G Jack, B Storrie. Persistence of Golgi matrix distribution exhibits the same dependence on Sar1p activity as a Golgi glycosyltransferase. Traffic 2003; 4( 9): 631– 641 https://doi.org/10.1034/j.1600-0854.2003.00122.x
138
TH Ward, RS Polishchuk, S Caplan, K Hirschberg, J Lippincott-Schwartz. Maintenance of Golgi structure and function depends on the integrity of ER export. J Cell Biol 2001; 155( 4): 557– 570 https://doi.org/10.1083/jcb.200107045
139
S Miles, H McManus, KE Forsten, B Storrie. Evidence that the entire Golgi apparatus cycles in interphase HeLa cells: sensitivity of Golgi matrix proteins to an ER exit block. J Cell Biol 2001; 155( 4): 543– 556 https://doi.org/10.1083/jcb.200103104
140
D Corda, ML Barretta, RI Cervigni, A Colanzi. Golgi complex fragmentation in G2/M transition: an organelle-based cell-cycle checkpoint. IUBMB Life 2012; 64( 8): 661– 670 https://doi.org/10.1002/iub.1054
141
A Persico, RI Cervigni, ML Barretta, D Corda, A Colanzi. Golgi partitioning controls mitotic entry through Aurora-A kinase. Mol Biol Cell 2010; 21( 21): 3708– 3721 https://doi.org/10.1091/mbc.e10-03-0243
142
N Altan-Bonnet, R Sougrat, J Lippincott-Schwartz. Molecular basis for Golgi maintenance and biogenesis. Curr Opin Cell Biol 2004; 16( 4): 364– 372 https://doi.org/10.1016/j.ceb.2004.06.011
143
N Altan-Bonnet, R Sougrat, W Liu, EL Snapp, T Ward, J Lippincott-Schwartz. Golgi inheritance in mammalian cells is mediated through endoplasmic reticulum export activities. Mol Biol Cell 2006; 17( 2): 990– 1005 https://doi.org/10.1091/mbc.e05-02-0155
144
R Magliozzi, ZI Carrero, TY Low, L Yuniati, C Valdes-Quezada, F Kruiswijk, K van Wijk, AJR Heck, CL Jackson, D Guardavaccaro. Inheritance of the Golgi apparatus and cytokinesis are controlled by degradation of GBF1. Cell Rep 2018; 23( 11): 3381– 3391.e4 https://doi.org/10.1016/j.celrep.2018.05.031
145
S Miserey-Lenkei, A Couëdel-Courteille, Nery E Del, S Bardin, M Piel, V Racine, JB Sibarita, F Perez, M Bornens, B Goud. A role for the Rab6A′ GTPase in the inactivation of the Mad2-spindle checkpoint. EMBO J 2006; 25( 2): 278– 289 https://doi.org/10.1038/sj.emboj.7600929
146
P Mishra, DC Chan. Mitochondrial dynamics and inheritance during cell division, development and disease. Nat Rev Mol Cell Biol 2014; 15( 10): 634– 646 https://doi.org/10.1038/nrm3877
147
M Giacomello, A Pyakurel, C Glytsou, L Scorrano. The cell biology of mitochondrial membrane dynamics. Nat Rev Mol Cell Biol 2020; 21( 4): 204– 224 https://doi.org/10.1038/s41580-020-0210-7
148
DF Kashatus, KH Lim, DC Brady, NLK Pershing, AD Cox, CM Counter. RALA and RALBP1 regulate mitochondrial fission at mitosis. Nat Cell Biol 2011; 13( 9): 1108– 1115 https://doi.org/10.1038/ncb2310
149
G Kanfer, B Kornmann. Dynamics of the mitochondrial network during mitosis. Biochem Soc Trans 2016; 44( 2): 510– 516 https://doi.org/10.1042/BST20150274
150
G Benard, N Bellance, D James, P Parrone, H Fernandez, T Letellier, R Rossignol. Mitochondrial bioenergetics and structural network organization. J Cell Sci 2007; 120( 5): 838– 848 https://doi.org/10.1242/jcs.03381
151
PA Parone, S Da Cruz, D Tondera, Y Mattenberger, DI James, P Maechler, F Barja, JC Martinou. Preventing mitochondrial fission impairs mitochondrial function and leads to loss of mitochondrial DNA. PLoS One 2008; 3( 9): e3257 https://doi.org/10.1371/journal.pone.0003257
152
S Nagashima, LC Tábara, L Tilokani, V Paupe, H Anand, JH Pogson, R Zunino, HM McBride, J Prudent. Golgi-derived PI(4)P-containing vesicles drive late steps of mitochondrial division. Science 2020; 367( 6484): 1366– 1371 https://doi.org/10.1126/science.aax6089
G Kanfer, T Courthéoux, M Peterka, S Meier, M Soste, A Melnik, K Reis, P Aspenström, M Peter, P Picotti, B Kornmann. Mitotic redistribution of the mitochondrial network by Miro and Cenp-F. Nat Commun 2015; 6( 1): 8015 https://doi.org/10.1038/ncomms9015
155
L Walch, E Pellier, W Leng, G Lakisic, A Gautreau, V Contremoulins, JM Verbavatz, CL Jackson. GBF1 and Arf1 interact with Miro and regulate mitochondrial positioning within cells. Sci Rep 2018; 8( 1): 17121 https://doi.org/10.1038/s41598-018-35190-0
AN Kettenbach, DK Schweppe, BK Faherty, D Pechenick, AA Pletnev, SA Gerber. Quantitative phosphoproteomics identifies substrates and functional modules of Aurora and Polo-like kinase activities in mitotic cells. Sci Signal 2011; 4( 179): rs5 https://doi.org/10.1126/scisignal.2001497
158
N Dephoure, C Zhou, J Villén, SA Beausoleil, CE Bakalarski, SJ Elledge, SP Gygi. A quantitative atlas of mitotic phosphorylation. Proc Natl Acad Sci USA 2008; 105( 31): 10762– 10767 https://doi.org/10.1073/pnas.0805139105
159
R Malik, R Lenobel, A Santamaria, A Ries, EA Nigg, R Körner. Quantitative analysis of the human spindle phosphoproteome at distinct mitotic stages. J Proteome Res 2009; 8( 10): 4553– 4563 https://doi.org/10.1021/pr9003773
A Kechad, S Jananji, Y Ruella, GRX Hickson. Anillin acts as a bifunctional linker coordinating midbody ring biogenesis during cytokinesis. Curr Biol 2012; 22( 3): 197– 203 https://doi.org/10.1016/j.cub.2011.11.062
162
P Steigemann, DW Gerlich. Cytokinetic abscission: cellular dynamics at the midbody. Trends Cell Biol 2009; 19( 11): 606– 616 https://doi.org/10.1016/j.tcb.2009.07.008
163
CK Hu, M Coughlin, TJ Mitchison. Midbody assembly and its regulation during cytokinesis. Mol Biol Cell 2012; 23( 6): 1024– 1034 https://doi.org/10.1091/mbc.e11-08-0721
SN Jordan, JC Canman. Rho GTPases in animal cell cytokinesis: an occupation by the one percent. Cytoskeleton (Hoboken) 2012; 69( 11): 919– 930 https://doi.org/10.1002/cm.21071
WM Bement, HAHA Benink, G von Dassow. A microtubule-dependent zone of active RhoA during cleavage plane specification. J Cell Biol 2005; 170( 1): 91– 101 https://doi.org/10.1083/jcb.200501131
170
O Yüce, A Piekny, M Glotzer. An ECT2-centralspindlin complex regulates the localization and function of RhoA. J Cell Biol 2005; 170( 4): 571– 582 https://doi.org/10.1083/jcb.200501097
171
H Yoshizaki, Y Ohba, K Kurokawa, RE Itoh, T Nakamura, N Mochizuki, K Nagashima, M Matsuda. Activity of Rho-family GTPases during cell division as visualized with FRET-based probes. J Cell Biol 2003; 162( 2): 223– 232 https://doi.org/10.1083/jcb.200212049
172
K Kotýnková, KC Su, SC West, M Petronczki. Plasma membrane association but not midzone recruitment of RhoGEF ECT2 is essential for cytokinesis. Cell Rep 2016; 17( 10): 2672– 2686 https://doi.org/10.1016/j.celrep.2016.11.029
173
TE Schroeder. The contractile ring. I. Fine structure of dividing mammalian (HeLa) cells and the effects of cytochalasin B. Z Zellforsch Mikrosk Anat 1970; 109( 4): 431– 449 https://doi.org/10.1007/BF00343960
174
TE Schroeder. Actin in dividing cells: contractile ring filaments bind heavy meromyosin. Proc Natl Acad Sci USA 1973; 70( 6): 1688– 1692 https://doi.org/10.1073/pnas.70.6.1688
175
T Otomo, C Otomo, DR Tomchick, M Machius, MK Rosen. Structural basis of Rho GTPase-mediated activation of the formin mDia1. Mol Cell 2005; 18( 3): 273– 281 https://doi.org/10.1016/j.molcel.2005.04.002
176
R Rose, M Weyand, M Lammers, T Ishizaki, MR Ahmadian, A Wittinghofer. Structural and mechanistic insights into the interaction between Rho and mammalian Dia. Nature 2005; 435( 7041): 513– 518 https://doi.org/10.1038/nature03604
177
DH Castrillon, SA Wasserman. Diaphanous is required for cytokinesis in Drosophila and shares domains of similarity with the products of the limb deformity gene. Development 1994; 120( 12): 3367– 3377 https://doi.org/10.1242/dev.120.12.3367
178
M Evangelista, D Pruyne, DC Amberg, C Boone, A Bretscher. Formins direct Arp2/3-independent actin filament assembly to polarize cell growth in yeast. Nat Cell Biol 2002; 4( 3): 260– 269 https://doi.org/10.1038/ncb770
179
I Sagot, AA Rodal, J Moseley, BL Goode, D Pellman. An actin nucleation mechanism mediated by Bni1 and profilin. Nat Cell Biol 2002; 4( 8): 626– 631 https://doi.org/10.1038/ncb834
180
N Watanabe, P Madaule, T Reid, T Ishizaki, G Watanabe, A Kakizuka, Y Saito, K Nakao, BM Jockusch, S Narumiya. p140mDia, a mammalian homolog of Drosophila diaphanous, is a target protein for Rho small GTPase and is a ligand for profilin. EMBO J 1997; 16( 11): 3044– 3056 https://doi.org/10.1093/emboj/16.11.3044
181
Y Kawano, Y Fukata, N Oshiro, M Amano, T Nakamura, M Ito, F Matsumura, M Inagaki, K Kaibuchi. Phosphorylation of myosin-binding subunit (MBS) of myosin phosphatase by Rho-kinase in vivo. J Cell Biol 1999; 147( 5): 1023– 1038 https://doi.org/10.1083/jcb.147.5.1023
182
H Kosako, T Yoshida, F Matsumura, T Ishizaki, S Narumiya, M Inagaki. Rho-kinase/ROCK is involved in cytokinesis through the phosphorylation of myosin light chain and not ezrin/radixin/moesin proteins at the cleavage furrow. Oncogene 2000; 19( 52): 6059– 6064 https://doi.org/10.1038/sj.onc.1203987
183
T Yokoyama, H Goto, I Izawa, H Mizutani, M Inagaki. Aurora-B and Rho-kinase/ROCK, the two cleavage furrow kinases, independently regulate the progression of cytokinesis: possible existence of a novel cleavage furrow kinase phosphorylates ezrin/radixin/moesin (ERM). Genes Cells 2005; 10( 2): 127– 137 https://doi.org/10.1111/j.1365-2443.2005.00824.x
184
M Khasnis, A Nakatomi, K Gumpper, M Eto. Reconstituted human myosin light chain phosphatase reveals distinct roles of two inhibitory phosphorylation sites of the regulatory subunit, MYPT1. Biochemistry 2014; 53( 16): 2701– 2709 https://doi.org/10.1021/bi5001728
185
M Gai, P Camera, A Dema, F Bianchi, G Berto, E Scarpa, G Germena, F Di Cunto. Citron kinase controls abscission through RhoA and anillin. Mol Biol Cell 2011; 22( 20): 3768– 3778 https://doi.org/10.1091/mbc.e10-12-0952
186
PP D’Avino. Citron kinase—renaissance of a neglected mitotic kinase. J Cell Sci 2017; 130( 10): 1701– 1708 https://doi.org/10.1242/jcs.200253
187
JC Canman, L Lewellyn, K Laband, SJ Smerdon, A Desai, B Bowerman, K Oegema. Inhibition of Rac by the GAP activity of centralspindlin is essential for cytokinesis. Science 2008; 322( 5907): 1543– 1546 https://doi.org/10.1126/science.1163086
188
E Boucrot, T Kirchhausen. Endosomal recycling controls plasma membrane area during mitosis. Proc Natl Acad Sci USA 2007; 104( 19): 7939– 7944 https://doi.org/10.1073/pnas.0702511104
S Sechi, A Frappaolo, R Fraschini, L Capalbo, M Gottardo, G Belloni, DM Glover, A Wainman, MG Giansanti. Rab1 interacts with GOLPH3 and controls Golgi structure and contractile ring constriction during cytokinesis in Drosophila melanogaster. Open Biol 2017; 7( 1): 160257 https://doi.org/10.1098/rsob.160257
192
J Cao, R Albertson, B Riggs, CM Field, W Sullivan. Nuf, a Rab11 effector, maintains cytokinetic furrow integrity by promoting local actin polymerization. J Cell Biol 2008; 182( 2): 301– 313 https://doi.org/10.1083/jcb.200712036
193
FF Rodrigues, W Shao, TJC Harris. The Arf GAP Asap promotes Arf1 function at the Golgi for cleavage furrow biosynthesis in Drosophila. Mol Biol Cell 2016; 27( 20): 3143– 3155 https://doi.org/10.1091/mbc.e16-05-0272
R Albertson, B Riggs, W Sullivan. Membrane traffic: a driving force in cytokinesis. Trends Cell Biol 2005; 15( 2): 92– 101 https://doi.org/10.1016/j.tcb.2004.12.008
196
G Montagnac, A Echard, P Chavrier. Endocytic traffic in animal cell cytokinesis. Curr Opin Cell Biol 2008; 20( 4): 454– 461 https://doi.org/10.1016/j.ceb.2008.03.011
197
JA Schiel, C Childs, R Prekeris. Endocytic transport and cytokinesis: from regulation of the cytoskeleton to midbody inheritance. Trends Cell Biol 2013; 23( 7): 319– 327 https://doi.org/10.1016/j.tcb.2013.02.003
198
JA Schiel, GC Simon, C Zaharris, J Weisz, D Castle, CC Wu, R Prekeris. FIP3-endosome-dependent formation of the secondary ingression mediates ESCRT-III recruitment during cytokinesis. Nat Cell Biol 2012; 14( 10): 1068– 1078 https://doi.org/10.1038/ncb2577
199
Y Minoshima, T Kawashima, K Hirose, Y Tonozuka, A Kawajiri, YC Bao, X Deng, M Tatsuka, S Narumiya, WS Jr May, T Nosaka, K Semba, T Inoue, T Satoh, M Inagaki, T Kitamura. Phosphorylation by aurora B converts MgcRacGAP to a RhoGAP during cytokinesis. Dev Cell 2003; 4( 4): 549– 560 https://doi.org/10.1016/S1534-5807(03)00089-3
A Hanai, M Ohgi, C Yagi, T Ueda, HW Shin, K Nakayama. Class I Arfs (Arf1 and Arf3) and Arf6 are localized to the Flemming body and play important roles in cytokinesis. J Biochem 2016; 159( 2): 201– 208 https://doi.org/10.1093/jb/mvv088
202
D Dambournet, M Machicoane, L Chesneau, M Sachse, M Rocancourt, A El Marjou, E Formstecher, R Salomon, B Goud, A Echard. Rab35 GTPase and OCRL phosphatase remodel lipids and F-actin for successful cytokinesis. Nat Cell Biol 2011; 13( 8): 981– 988 https://doi.org/10.1038/ncb2279
203
S Frémont, H Hammich, J Bai, H Wioland, K Klinkert, M Rocancourt, C Kikuti, D Stroebel, G Romet-Lemonne, O Pylypenko, A Houdusse, A Echard. Oxidation of F-actin controls the terminal steps of cytokinesis. Nat Commun 2017; 8( 1): 14528 https://doi.org/10.1038/ncomms14528
204
G Montagnac, JB Sibarita, S Loubéry, L Daviet, M Romao, G Raposo, P Chavrier. ARF6 interacts with JIP4 to control a motor switch mechanism regulating endosome traffic in cytokinesis. Curr Biol 2009; 19( 3): 184– 195 https://doi.org/10.1016/j.cub.2008.12.043
205
I Cascone, R Selimoglu, C Ozdemir, E Del Nery, C Yeaman, M White, J Camonis. Distinct roles of RalA and RalB in the progression of cytokinesis are supported by distinct RalGEFs. EMBO J 2008; 27( 18): 2375– 2387 https://doi.org/10.1038/emboj.2008.166
206
XW Chen, M Inoue, SC Hsu, AR Saltiel. RalA-exocyst-dependent recycling endosome trafficking is required for the completion of cytokinesis. J Biol Chem 2006; 281( 50): 38609– 38616 https://doi.org/10.1074/jbc.M512847200
207
B Neumann, T Walter, JKK Hériché, J Bulkescher, H Erfle, C Conrad, P Rogers, I Poser, M Held, U Liebel, C Cetin, F Sieckmann, G Pau, R Kabbe, A Wünsche, V Satagopam, MH Schmitz, C Chapuis, DW Gerlich, R Schneider, R Eils, W Huber, JM Peters, AA Hyman, R Durbin, R Pepperkok, J Ellenberg. Phenotypic profiling of the human genome by time-lapse microscopy reveals cell division genes. Nature 2010; 464( 7289): 721– 727 https://doi.org/10.1038/nature08869
El Kadhi K Ben, C Roubinet, S Solinet, G Emery, S Carréno. The inositol 5-phosphatase dOCRL controls PI(4,5)P2 homeostasis and is necessary for cytokinesis. Curr Biol 2011; 21( 12): 1074– 1079 https://doi.org/10.1016/j.cub.2011.05.030
211
SJ Field, N Madson, ML Kerr, KAA Galbraith, CE Kennedy, M Tahiliani, A Wilkins, LC Cantley. PtdIns(4,5)P2 functions at the cleavage furrow during cytokinesis. Curr Biol 2005; 15( 15): 1407– 1412 https://doi.org/10.1016/j.cub.2005.06.059
212
FCM Zoppino, RD Militello, I Slavin, C Álvarez, MI Colombo. Autophagosome formation depends on the small GTPase Rab1 and functional ER exit sites. Traffic 2010; 11( 9): 1246– 1261 https://doi.org/10.1111/j.1600-0854.2010.01086.x
213
X Ao, L Zou, Y Wu. Regulation of autophagy by the Rab GTPase network. Cell Death Differ 2014; 21( 3): 348– 358 https://doi.org/10.1038/cdd.2013.187
214
CEL Chua, BQ Gan, BL Tang. Involvement of members of the Rab family and related small GTPases in autophagosome formation and maturation. Cell Mol Life Sci 2011; 68( 20): 3349– 3358 https://doi.org/10.1007/s00018-011-0748-9
IG Ganley, PM Wong, N Gammoh, X Jiang. Distinct autophagosomal-lysosomal fusion mechanism revealed by thapsigargin-induced autophagy arrest. Mol Cell 2011; 42( 6): 731– 743 https://doi.org/10.1016/j.molcel.2011.04.024
217
M Pilli, J Arko-Mensah, M Ponpuak, E Roberts, S Master, MA Mandell, N Dupont, W Ornatowski, S Jiang, SB Bradfute, JA Bruun, TE Hansen, T Johansen, V Deretic. TBK-1 promotes autophagy-mediated antimicrobial defense by controlling autophagosome maturation. Immunity 2012; 37( 2): 223– 234 https://doi.org/10.1016/j.immuni.2012.04.015
218
DB Munafó, MI Colombo. Induction of autophagy causes dramatic changes in the subcellular distribution of GFP-Rab24. Traffic 2002; 3( 7): 472– 482 https://doi.org/10.1034/j.1600-0854.2002.30704.x
219
A Sakurai, F Maruyama, J Funao, T Nozawa, C Aikawa, N Okahashi, S Shintani, S Hamada, T Ooshima, I Nakagawa. Specific behavior of intracellular Streptococcus pyogenes that has undergone autophagic degradation is associated with bacterial streptolysin O and host small G proteins Rab5 and Rab7. J Biol Chem 2010; 285( 29): 22666– 22675 https://doi.org/10.1074/jbc.M109.100131
220
CF Bento, C Puri, K Moreau, DC Rubinsztein. The role of membrane-trafficking small GTPases in the regulation of autophagy. J Cell Sci 2013; 126( 5): 1059– 1069 https://doi.org/10.1242/jcs.123075
221
BO Bodemann, A Orvedahl, T Cheng, RR Ram, YH Ou, E Formstecher, M Maiti, CC Hazelett, EM Wauson, M Balakireva, JH Camonis, C Yeaman, B Levine, MA White. RalB and the exocyst mediate the cellular starvation response by direct activation of autophagosome assembly. Cell 2011; 144( 2): 253– 267 https://doi.org/10.1016/j.cell.2010.12.018
222
N Nakashima, E Noguchi, T Nishimoto. Saccharomyces cerevisiae putative G protein, Gtr1p, which forms complexes with itself and a novel protein designated as Gtr2p, negatively regulates the Ran/Gsp1p G protein cycle through Gtr2p. Genetics 1999; 152( 3): 853– 867 https://doi.org/10.1093/genetics/152.3.853
223
T Sekiguchi, E Hirose, N Nakashima, M Ii, T Nishimoto. Novel G proteins, Rag C and Rag D, interact with GTP-binding proteins, Rag A and Rag B. J Biol Chem 2001; 276( 10): 7246– 7257 https://doi.org/10.1074/jbc.M004389200
224
Y Sancak, L Bar-Peled, R Zoncu, AL Markhard, S Nada, DM Sabatini. Ragulator-Rag complex targets mTORC1 to the lysosomal surface and is necessary for its activation by amino acids. Cell 2010; 141( 2): 290– 303 https://doi.org/10.1016/j.cell.2010.02.024
225
Y Sancak, TR Peterson, YD Shaul, RA Lindquist, CC Thoreen, L Bar-Peled, DM Sabatini. The rag GTPases bind raptor and mediate amino acid signaling to mTORC1. Science 2008; 320( 5882): 1496– 1501 https://doi.org/10.1126/science.1157535
226
RI Odle, SA Walker, D Oxley, AM Kidger, K Balmanno, R Gilley, H Okkenhaug, O Florey, NT Ktistakis, SJ Cook. An mTORC1-to-CDK1 switch maintains autophagy suppression during mitosis. Mol Cell 2020; 77( 2): 228– 240.e7 https://doi.org/10.1016/j.molcel.2019.10.016
227
AR Thiam, RV Jr Farese, TC Walther. The biophysics and cell biology of lipid droplets. Nat Rev Mol Cell Biol 2013; 14( 12): 775– 786 https://doi.org/10.1038/nrm3699
ALS Cruz, N Carrossini, LK Teixeira, LF Ribeiro-Pinto, PT Bozza, JPB Viola. Cell cycle progression regulates biogenesis and cellular localization of lipid droplets. Mol Cell Biol 2019; 39( 9): e00374– 18 https://doi.org/10.1128/MCB.00374-18
232
R Tan, W Wang, S Wang, Z Wang, L Sun, W He, R Fan, Y Zhou, X Xu, W Hong, T Wang. Small GTPase Rab40c associates with lipid droplets and modulates the biogenesis of lipid droplets. PLoS One 2013; 8( 4): e63213 https://doi.org/10.1371/journal.pone.0063213
233
S Ozeki, J Cheng, K Tauchi-Sato, N Hatano, H Taniguchi, T Fujimoto. Rab18 localizes to lipid droplets and induces their close apposition to the endoplasmic reticulum-derived membrane. J Cell Sci 2005; 118( 12): 2601– 2611 https://doi.org/10.1242/jcs.02401
234
B Schroeder, RJ Schulze, SG Weller, AC Sletten, CA Casey, MA McNiven. The small GTPase Rab7 as a central regulator of hepatocellular lipophagy. Hepatology 2015; 61( 6): 1896– 1907 https://doi.org/10.1002/hep.27667
B Knoblach, RA Rachubinski. How peroxisomes partition between cells. A story of yeast, mammals and filamentous fungi. Curr Opin Cell Biol 2016; 41 : 73– 80 https://doi.org/10.1016/j.ceb.2016.04.004
237
T Nguyen, J Bjorkman, BC Paton, DI Crane. Failure of microtubule-mediated peroxisome division and trafficking in disorders with reduced peroxisome abundance. J Cell Sci 2006; 119( 4): 636– 645 https://doi.org/10.1242/jcs.02776
238
A Asare, J Levorse, E Fuchs. Coupling organelle inheritance with mitosis to balance growth and differentiation. Science 2017; 355( 6342): eaah4701 https://doi.org/10.1126/science.aah4701
239
SJ Heasman, AJ Ridley. Mammalian Rho GTPases: new insights into their functions from in vivo studies. Nat Rev Mol Cell Biol 2008; 9( 9): 690– 701 https://doi.org/10.1038/nrm2476
240
IG Castro, DM Richards, J Metz, JL Costello, JB Passmore, TA Schrader, A Gouveia, D Ribeiro, M Schrader. A role for mitochondrial Rho GTPase 1 (MIRO1) in motility and membrane dynamics of peroxisomes. Traffic 2018; 19( 3): 229– 242 https://doi.org/10.1111/tra.12549
241
L Schollenberger, T Gronemeyer, CM Huber, D Lay, S Wiese, HE Meyer, B Warscheid, R Saffrich, J Peränen, K Gorgas, WW Just. RhoA regulates peroxisome association to microtubules and the actin cytoskeleton. PLoS One 2010; 5( 11): e13886 https://doi.org/10.1371/journal.pone.0013886
T Gronemeyer, S Wiese, S Grinhagens, L Schollenberger, A Satyagraha, LA Huber, HE Meyer, B Warscheid, WW Just. Localization of Rab proteins to peroxisomes: a proteomics and immunofluorescence study. FEBS Lett 2013; 587( 4): 328– 338 https://doi.org/10.1016/j.febslet.2012.12.025
244
M Zerial, H McBride. Rab proteins as membrane organizers. Nat Rev Mol Cell Biol 2001; 2( 2): 107– 117 https://doi.org/10.1038/35052055
245
D Cussac, P Leblanc, A L’Heritier, J Bertoglio, P Lang, C Kordon, A Enjalbert, D Saltarelli. Rho proteins are localized with different membrane compartments involved in vesicular trafficking in anterior pituitary cells. Mol Cell Endocrinol 1996; 119( 2): 195– 206 https://doi.org/10.1016/0303-7207(96)03814-2
246
P Croisé, C Estay-Ahumada, S Gasman, S Ory. Rho GTPases, phosphoinositides, and actin: a tripartite framework for efficient vesicular trafficking. Small GTPases 2014; 5( 2): e29469 https://doi.org/10.4161/sgtp.29469
247
A Wittinghofer. Ras Superfamily Small G Proteins: Biology and Mechanisms 1: general features, signaling. Springer Vienna, 2014
248
B Zhou AD Cox. Posttranslational modifications of small G proteins. In: Wittinghofer A. Ras Superfamily Small G Proteins: Biology and Mechanisms 1. Springer Vienna, 2014: 99– 131
S Eathiraj, X Pan, C Ritacco, DG Lambright. Structural basis of family-wide Rab GTPase recognition by rabenosyn-5. Nature 2005; 436( 7049): 415– 419 https://doi.org/10.1038/nature03798
251
A Spang, JH Saw, SL Jørgensen, K Zaremba-Niedzwiedzka, J Martijn, AE Lind, Eijk R van, C Schleper, L Guy, TJG Ettema. Complex archaea that bridge the gap between prokaryotes and eukaryotes. Nature 2015; 521( 7551): 173– 179 https://doi.org/10.1038/nature14447