Abstract
It is generally believed that cytoskeletal activities drive random cell migration, whereas signal transduction events initiated by receptors regulate the cytoskeleton to guide cells. However, we find that the cytoskeletal network, involving SCAR/WAVE, Arp 2/3 and actin-binding proteins, is capable of generating only rapid oscillations and undulations of the cell boundary. The signal transduction network, comprising multiple pathways that include Ras GTPases, PI(3)K and Rac GTPases, is required to generate the sustained protrusions of migrating cells. The signal transduction network is excitable, exhibiting wave propagation, refractoriness and maximal response to suprathreshold stimuli, even in the absence of the cytoskeleton. We suggest that cell motility results from coupling of ‘pacemaker’ signal transduction and ‘idling motor’ cytoskeletal networks, and various guidance cues that modulate the threshold for triggering signal transduction events are integrated to control the mode and direction of migration.
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References
Ridley, A. J. et al. Cell migration: integrating signals from front to back. Science 302, 1704–1709 (2003).
Bosgraaf, L. & Van Haastert, P. J. The ordered extension of pseudopodia by amoeboid cells in the absence of external cues. PLoS ONE 4, e5253 (2009).
Tranquillo, R. T., Lauffenburger, D. A. & Zigmond, S. H. A stochastic model for leukocyte random motility and chemotaxis based on receptor binding fluctuations. J. Cell Biol. 106, 303–309 (1988).
Arrieumerlou, C. & Meyer, T. A local coupling model and compass parameter for eukaryotic chemotaxis. Dev. Cell 8, 215–227 (2005).
Welf, E. S. & Haugh, J. M. Signaling pathways that control cell migration: models and analysis. WIRes Syst. Biol. Med. 3, 231–240 (2011).
Pollard, T. D. & Borisy, G. G. Cellular motility driven by assembly and disassembly of actin filaments. Cell 112, 453–465 (2003).
Hall, A. Rho GTPases and the control of cell behaviour. Biochem. Soc. Trans. 33, 891–895 (2005).
Ridley, A. J. Rho GTPases and actin dynamics in membrane protrusions and vesicle trafficking. Trends Cell Biol. 16, 522–529 (2006).
Machacek, M. et al. Coordination of Rho GTPase activities during cell protrusion. Nature 461, 99–103 (2009).
Welch, C. M., Elliott, H., Danuser, G. & Hahn, K. M. Imaging the coordination of multiple signalling activities in living cells. Nat. Rev. Mol. Cell Biol. 12, 749–756 (2011).
Cain, R. J. & Ridley, A. J. Phosphoinositide 3-kinases in cell migration. Biol. Cell 101, 13–29 (2009).
Sasaki, A. T. et al. G protein-independent Ras/PI3K/F-actin circuit regulates basic cell motility. J. Cell Biol. 178, 185–191 (2007).
Inoue, T. & Meyer, T. Synthetic activation of endogenous PI3K and Racidentifies an AND-gate switch for cell polarization and migration. PLoS ONE 3, e3068 (2008).
Weiner, O. D. et al. A PtdInsP(3)- and Rho GTPase-mediated positive feedback loop regulates neutrophil polarity. Nat. Cell Biol. 4, 509–513 (2002).
Asano, Y., Nagasaki, A. & Uyeda, T. Q. Correlated waves of actin filaments and PIP3 in Dictyostelium cells. Cell Motil. Cytoskeleton 65, 923–934 (2008).
Bretschneider, T. et al. The three-dimensional dynamics of actin waves, a model of cytoskeletal self-organization. Biophys. J. 96, 2888–2900 (2009).
Case, L. B. & Waterman, C. M. Adhesive F-actin waves: a novel integrin-mediated adhesion complex coupled to ventral actin polymerization. PLoS ONE 6, e26631 (2011).
Gerisch, G. Self-organizing actin waves that simulate phagocytic cup structures. PMC Biophys. 3, 7 (2010).
Gerisch, G. et al. Self-organizing actin waves as planar phagocytic cup structures. Cell Adhes. Migr. 3, 373–382 (2009).
Gerisch, G. et al. Mobile actin clusters and traveling waves in cells recovering from actin depolymerization. Biophys. J. 87, 3493–3503 (2004).
Vicker, M. G. F-actin assembly in Dictyostelium cell locomotion and shape oscillations propagates as a self-organized reaction-diffusion wave. FEBS Lett. 510, 5–9 (2002).
Vicker, M. G. Eukaryotic cell locomotion depends on the propagation of self-organized reaction-diffusion waves and oscillations of actin filament assembly. Exp. Cell Res. 275, 54–66 (2002).
Weiner, O. D., Marganski, W. A., Wu, L. F., Altschuler, S. J. & Kirschner, M. W. An actin-based wave generator organizes cell motility. PLoS Biol. 5, e221 (2007).
Xiong, Y., Huang, C. H., Iglesias, P. A. & Devreotes, P. N. Cells navigate with a local-excitation, global-inhibition-biased excitable network. Proc. Natl Acad. Sci. USA 107, 17079–17086 (2010).
Arai, Y. et al. Self-organization of the phosphatidylinositol lipids signaling system for random cell migration. Proc. Natl Acad. Sci. USA 107, 12399–12404 (2010).
Hecht, I., Kessler, D. A. & Levine, H. Transient localized patterns in noise-driven reaction-diffusion systems. Phys. Rev. Lett. 104, 158301 (2010).
Vicker, M. G. Reaction-diffusion waves of actin filament polymerization/depolymerization in Dictyostelium pseudopodium extension and cell locomotion. Biophys. Chem. 84, 87–98 (2000).
Meinhardt, H. Orientation of chemotactic cells and growth cones: models and mechanisms. J. Cell Sci. 112, 2867–2874 (1999).
Hecht, I. et al. Activated membrane patches guide chemotactic cell motility. PLoS Comput. Biol. 7, e1002044 (2011).
Bretschneider, T. et al. Dynamic actin patterns and Arp2/3 assembly at the substrate-attached surface of motile cells. Curr. Biol. 14, 1–10 (2004).
Kae, H., Lim, C. J., Spiegelman, G. B. & Weeks, G. Chemoattractant-induced Ras activation during Dictyostelium aggregation. EMBO Rep. 5, 602–606 (2004).
Parent, C. A., Blacklock, B. J., Froehlich, W. M., Murphy, D. B. & Devreotes, P. N. G protein signaling events are activated at the leading edge of chemotactic cells. Cell 95, 81–91 (1998).
Kabacoff, C. et al. Dynacortin facilitates polarization of chemotaxing cells. BMC Biol. 5, 53 (2007).
Veltman, D. M., King, J. S., Machesky, L. M. & Insall, R. H. SCAR knockouts in Dictyostelium: WASP assumes SCAR’s position and upstream regulators in pseudopods. J. Cell Biol. 198, 501–508 (2012).
Uetrecht, A. C. & Bear, J. E. Coronins: the return of the crown. Trends Cell Biol. 16, 421–426 (2006).
Sirotkin, V., Berro, J., Macmillan, K., Zhao, L. & Pollard, T. D. Quantitative analysis of the mechanism of endocytic actin patch assembly and disassembly in fission yeast. Mol. Biol. Cell 21, 2894–2904 (2010).
Uchida, K. S. & Yumura, S. Dynamics of novel feet of Dictyostelium cells during migration. J. Cell Sci. 117, 1443–1455 (2004).
Chen, L. et al. Two phases of actin polymerization display different dependencies on PI(3,4,5)P3 accumulation and have unique roles during chemotaxis. Mol. Biol. Cell 14, 5028–5037 (2003).
Postma, M. et al. Uniform cAMP stimulation of Dictyostelium cells induces localized patches of signal transduction and pseudopodia. Mol. Biol. Cell 14, 5019–5027 (2003).
Ridley, A. J., Paterson, H. F., Johnston, C. L., Diekmann, D. & Hall, A. The small GTP-binding protein rac regulates growth factor-induced membrane ruffling. Cell 70, 401–410 (1992).
Jaffe, A. B. & Hall, A. Rho GTPases: biochemistry and biology. Annu. Rev. Cell Dev. Biol. 21, 247–269 (2005).
Filic, V., Marinovic, M., Faix, J. & Weber, I. A dual role for Rac1 GTPases in the regulation of cell motility. J. Cell Sci. 125, 387–398 (2012).
Dumontier, M., Hocht, P., Mintert, U. & Faix, J. Rac1 GTPases control filopodia formation, cell motility, endocytosis, cytokinesis and development in Dictyostelium. J. Cell Sci. 113, 2253–2265 (2000).
Eden, S., Rohatgi, R., Podtelejnikov, A. V., Mann, M. & Kirschner, M. W. Mechanism of regulation of WAVE1-induced actin nucleation by Rac1 and Nck. Nature 418, 790–793 (2002).
Kitamura, Y. et al. Interaction of Nck-associated protein 1 with activated GTP-binding protein Rac. Biochem. J. 322, 873–878 (1997).
Taniguchi, D. et al. Phase geometries of two-dimensional excitable waves govern self-organized morphodynamics of amoeboid cells. Proc. Natl Acad. Sci. USA 110, 5016–5021 (2013).
Iglesias, P. A. & Devreotes, P. N. Biased excitable networks: how cells direct motion in response to gradients. Curr. Opin. Cell Biol. 24, 245–253 (2012).
Hoeller, O. & Kay, R. R. Chemotaxis in the absence of PIP3 gradients. Curr. Biol. 17, 813–817 (2007).
Cai, H. et al. Ras-mediated activation of the TORC2-PKB pathway is critical for chemotaxis. J. Cell Biol. 190, 233–245 (2010).
Zhang, S., Charest, P. G. & Firtel, R. A. Spatiotemporal regulation of Ras activity provides directional sensing. Curr. Biol. 18, 1587–1593 (2008).
Srinivasan, S. et al. Rac and Cdc42 play distinct roles in regulating PI(3,4,5)P3 and polarity during neutrophil chemotaxis. J. Cell Biol. 160, 375–385 (2003).
Yoo, S. K. et al. Differential regulation of protrusion and polarity by PI3K during neutrophil motility in live zebrafish. Dev. Cell 18, 226–236 (2010).
Decave, E. et al. Shear flow-induced motility of Dictyostelium discoideum cells on solid substrate. J. Cell Sci. 116, 4331–4343 (2003).
Zhao, M. et al. Electrical signals control wound healing through phosphatidylinositol-3-OH kinase-gamma and PTEN. Nature 442, 457–460 (2006).
Welf, E. S., Ahmed, S., Johnson, H. E., Melvin, A. T. & Haugh, J. M. Migrating fibroblasts reorient directionality by a metastable, PI3K-dependent mechanism. J. Cell Biol. 197, 105–114 (2012).
Westendorf, C. et al. Actin cytoskeleton of chemotactic amoebae operates close to the onset of oscillations. Proc. Natl Acad. Sci. USA 110, 3853–3858 (2013).
Lee, S., Shen, Z., Robinson, D. N., Briggs, S. & Firtel, R. A. Involvement of the cytoskeleton in controlling leading-edge function during chemotaxis. Mol. Biol. Cell 21, 1810–1824 (2010).
Charest, P. G. et al. A Ras signaling complex controls the RasC-TORC2 pathway and directed cell migration. Dev. Cell 18, 737–749 (2010).
Wu, L., Valkema, R., Van Haastert, P.J. & Devreotes, P. N. The G protein beta subunit is essential for multiple responses to chemoattractants in Dictyostelium. J. Cell Biol. 129, 1667–1675 (1995).
Iijima, M. & Devreotes, P. Tumor suppressor PTEN mediates sensing of chemoattractant gradients. Cell 109, 599–610 (2002).
Chen, L. et al. PLA2 and PI3K/PTEN pathways act in parallel to mediate chemotaxis. Dev. Cell 12, 603–614 (2007).
Fitzhugh, R. Impulses and physiological states in theoretical models of nerve membrane. Biophys. J. 1, 445–466 (1961).
Kim, J., Heslop-Harrison, P., Postlethwaite, I. & Bates, D. G. Stochastic noise and synchronisation during Dictyostelium aggregation make cAMP oscillations robust. PLoS Comput. Biol. 3, e218 (2007).
Vilar, J. M., Sole, R. V. & Rubi, J. M. Noise and periodic modulations in neural excitable media. Phys. Rev. E 59, 5920–5927 (1999).
Weinberger, L. S., Burnett, J. C., Toettcher, J. E., Arkin, A. P. & Schaffer, D. V. Stochastic gene expression in a lentiviral positive-feedback loop: HIV-1 Tat fluctuations drive phenotypic diversity. Cell 122, 169–182 (2005).
Yang, L. et al. Modeling cellular deformations using the level set formalism. BMC Syst. Biol. 2, 68 (2008).
Poirier, C. C., Ng, W. P., Robinson, D. N. & Iglesias, P. A. Deconvolution of the cellular force-generating subsystems that govern cytokinesis furrow ingression. PLoS Comput. Biol. 8, e1002467 (2012).
Mitchell, I. M. The flexible, extensible and efficient toolbox of level set methods. J. Sci. Comput. 35, 300–329 (2008).
Acknowledgements
The authors would like to thank M. Amzel, D. Montell, M. Iijima, T. Inoue and members of the Devreotes and Iglesias laboratories for helpful suggestions, B. Diplas for generating cell centroid tracks, P. Van Haastert for the RBD–GFP construct, R. Insall (The Beatson Institute, UK) for the HSPC300–GFP construct, G. Gerisch (Max Planck Institute for Biochemistry, Germany) for the LimE–RFP construct, and D. Robinson (Johns Hopkins University, USA) for coronin–GFP and the original video of dynacortin-expressing cells. We are grateful to V. Filic and I. Weber (Ruder Boskovic Institute, Croatia) for sharing the PAK(GBD)–YFP biosensor for Rac activity. This work was supported in part by grants from the National Institutes of Health, GM28007 (to P.N.D.), GM34933 (to P.N.D.) and GM71920 (to P.A.I.), and a H. L. Plotnick Fellowship from the Damon Runyon Cancer Research Foundation, DRG2019-09 (to C.H.H.).
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C-H.H. and M.T. performed the experiments. C.S. and P.A.I. carried out computer simulations. All authors analysed the data and wrote the manuscript. P.N.D. supervised the study.
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Integrated supplementary information
Supplementary Figure 1 Cytoskeletal network.
(a) Illustration of the t-stack technique. The frames of a TIRF video (left) are stacked to produce the t-stack (right). The position and orientation of frames t1, t2, and t3 in the t-stack is shown (middle). The immobile red oval generates the red cylinder in the t-stack, while the expansion of the green region over time creates the oblique cone-like appendage. (b-d) T-stacks derived from published TIRF time-lapse videos of a wild-type cell expressing GFP-dynacortin (b) 1, a wild-type cell expressing GFP-Arp3 (c) 2, and a SCAR- cell expressing GFP-WASP (d) 3 showing fast oscillations of cytoskeletal proteins. The red arrowhead indicates a pseudopodium preceding oscillations of dynacortin (green arrowheads). (e) T-stacks from a cell co-expressing HSPC300-GFP and cAR1-RFP. (f-h) T-stacks of LimE expressed in gβ- cells (f), pten- cells (g), and LY294002-treated wild-type cells (h). (i) Cytoskeletal oscillations in cells expressing constitutively active Ras. LimE-RFP in rasC- cells expressing Flag-RasC (left) or Flag-RasCQ62L (right). The videos used for these t-stacks were published earlier4. (j) TIRF image(top) and t-stack (bottom) of a latrunculin-treated cell expressing HSPC300-GFP, showing foci of fluorescence that did not oscillate.
Supplementary Figure 2 Signal transduction network.
(a) TIRF images of a cell co-expressing RBD-GFP and PH-RFP showing coordinated propagation of RBD and PH waves. Video rate was 3 spf (Supplementary Video S3). (b) The temporal profiles of RBD intensity at three spots marked 1, 2, 3 in (a). (c) The progression of contour lines for gray values 10, 20 and 30 along the yellow line in (a) was used to calculate the speed of the wave propagation. In the example, the speed of the wave between 15 sec and 48 sec was 12.8 μm/min by fitting the gray value 20 contour with a least square line. (d-h) Snapshots from TIRF videos of PH-GFP in cells treated with 4 μM latrunculin A (top, Supplementary Movies S4–S8) and the corresponding t-stacks (bottom). Panels (e) and (f) are the same cells at different times, (h) is the same cell as the left cell in (d), and (g) is a different cell. To visualize interior activities, a basal level of cellular fluorescence was subtracted from each video before the t-stacks were generated.
Supplementary Figure 3 Signaling and cytoskeletal activities on protrusions.
(a) T-stacks of two cells co-expressing RBD-GFP and LimE-RFP as well as the merged t-stack. The brackets in the cell on the left point to protrusions with high RBD and LimE. The cell on the right has very low level of RBD-GFP expression, but fast LimE oscillations are visible. Note that weak oscillations in the RBD t-stack (left cell) reflect changes in the boundary which delineates cytosolic RBD rather than RBD intensity on the cortex. Video rate was 2 spf. (b) Frames from a TIRF video of cells co-expressing RBD-GFP and LimE-RFP showing the distributions of RBD and LimE in protrusions. (c) Close-up views of a protrusion (yellow boxes in (a)) showing a smoother change of RBD intensity compared with that of LimE. (d) Frames from the TIRF video of a single large protrusion of a cell expressing HSPC300-GFP (Supplementary Movie S10). (e) t-stack of the video in (d). (f) Kymograph across the dashed line in (d). Arrowheads point to pauses in HSPC300 recruitment where cell boundary expansion stalled.
Supplementary Figure 4 Simulation of coupled systems.
(a) The slow excitable system is implemented as an activator (Xs)-inhibitor (Ys) system. (b) Phase plane plot of the slow excitable system. Red and green lines are nullclines for the activator and inhibitor components, respectively. The solid black circle represents the unique, stable equilibrium, found at the intersection of the two nullclines. The blue arrows represent the system evolution at different points in the phase plane. Two different trajectories are denoted by the black lines. The dotted black line represents a sub-threshold perturbation from which the system returns quickly to the equilibrium. The solid black line illustrates a super-threshold perturbation that causes the system to undergo a large excursion before returning to the equilibrium. (c) The Fast oscillatory system is also implemented using an activator (Xf)-inhibitor (Y f) system and also incorporates the influence of stochastic perturbations. (d) Phase plane plot of the fast oscillatory system. Red and green lines are nullclines for the activator and inhibitor components, respectively. In this case the system has three equilibria, at the points where the nullclines intersect. The solid black circles denote two stable equilibria, the open black circle the unique, unstable equilibrium. The blue arrows represent the evolution at different points in the phase plane. Trajectories are denoted by the black lines.
Supplementary Figure 5 Washout of LY294002 reversed the motility to plaA-/piaA- cells.
(a) Trajectories of cell migration. Random migration of cells were recorded and quantified as in Figure 6. For the LY washout experiment, cells were changed to buffer without LY294002, and allowed to settle for 40 min before recording was started. Duration of tracks is 60 min. (b) Quantification of net speed, motility speed, and persistence (mean ± s.d. from n = 4, 3, 3 experiments for plaA-/piaA- with DMSO, plaA-/piaA- with LY294002, and wash off, respectively. The source data is provided in Supplementary Table 3.)
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HSPC300-GFP.
Time-lapse TIRF video of a Dictyostelium cell expressing HSPC300-GFP with a rate of 1 spf. The video is shown at 15 frames/s and corresponds to Fig. 1a,b (MOV 1052 kb)
T-stack of HSPC300-GFP.
Rotation of the t-stack along its t(time)-axis. The speed of the rotation is shown at 40 degrees/s. The t-stack was generated from Movie S1and corresponds to Fig. 1b. (MOV 477 kb)
RBD-GFP and PH-RFP.
Time-lapse TIRF video of a Dictyostelium cell expressing RBD-GFP and PH-RFP with a rate of 3 spf. The video is shown at 15 frames/s and corresponds to Supplementary Fig. 2a. (MOV 90 kb)
PH-GFP in latrunculin-treated cell.
Time-lapse TIRF video of latrunculin-treated Dictyostelium cells expressing PH-GFP with a rate of 5 spf. The video is shown at 15 frames/s and corresponds to Supplementary Fig. 2d. (MOV 135 kb)
PH-GFP in latrunculin-treated cell.
Time-lapse TIRF video of latrunculin-treated Dictyostelium cells expressing PH-GFP with a rate of 5 spf. The video is shown at 15 frames/s and corresponds to Supplementary Fig. 2e. (MOV 87 kb)
PH-GFP in latrunculin-treated cell.
Time-lapse TIRF video of latrunculin-treated Dictyostelium cells expressing PH-GFP with a rate of 10 spf. The video is shown at 15 frames/s and corresponds to Supplementary Fig. 2f. (MOV 73 kb)
PH-GFP in latrunculin-treated cell.
Time-lapse TIRF video of a latrunculin-treated Dictyostelium cell expressing PH-GFP with a rate of 10 spf. The video is shown at 15 frames/s and corresponds to Supplementary Fig. 2g. (MOV 69 kb)
PH-GFP in latrunculin-treated cell.
Time-lapse TIRF video of latrunculin-treated Dictyostelium cells expressing PH-GFP with a rate of 10 spf. The video is shown at 15 frames/s and corresponds to Supplementary Fig. 2h. (MOV 56 kb)
RBD-GFP and LimE-RFP in undulations and protrusions.
Time-lapse TIRF video of a Dictyostelium cell co-expressing RBD-GFP and LimE-RFP with a rate of 2 spf. Cytoplasmic fluorescence of RBD-GFP and LimE-RFP was subtracted to highlight areas of increased intensity. Cell boundary (in gray) was derived from the cytoplasmic fluorescence of RBD-GFP. The video is shown at 7 frames/s and corresponds to Fig. 4b. (MOV 259 kb)
HSPC300-GFP in protrusion.
Time-lapse TIRF video of a Dictyostelium cell expressing HSPC300-GFP with a rate of 1 spf. The video is shown at 15 frames/s and corresponds to Supplementary Fig. 4d–f. (MOV 368 kb)
Computer simulation of the STEN-CON coupling model.
Level set simulation of cell movement along with the activities of the slow (Ys, in green) and fast (Yf, in red) systems as well as the merged activities. Cell membrane is driven by the signal of Yf (see Extended Experimental Procedures for simulation details). The video is shown at 20 frames/s. (MOV 1891 kb)
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Huang, CH., Tang, M., Shi, C. et al. An excitable signal integrator couples to an idling cytoskeletal oscillator to drive cell migration. Nat Cell Biol 15, 1307–1316 (2013). https://doi.org/10.1038/ncb2859
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DOI: https://doi.org/10.1038/ncb2859
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