Abstract
RAF activation requires coordinated interactions with both RAS and membrane lipids, yet the molecular basis of this process remains unclear. Using a bottom-up reconstitution approach, we show how coordinated protein–protein and protein–lipid interactions regulate membrane binding dynamics of RAF to drive its multistep activation. Within membrane environments, the RAS-binding domain (RBD) and cysteine-rich domain (CRD) exhibit cooperativity, with CRD-mediated phosphatidylserine binding stabilizing the RBD:RAS complex. Importantly, RAF remains membrane-bound through lateral rebinding to RAS, where a weak CRD–lipid interaction plays an essential role. The lateral rebinding extends RAF’s membrane dwell time under high RAS density conditions. This prolonged membrane residence may facilitate completion of RAF’s multistep activation. Given the high abundance of weak multivalent membrane interactions, lateral rebinding may be a common mechanism for regulating the activity of signaling proteins through sustained membrane retention.
Data availability
The authors declare that the data supporting the findings of this study are available within the paper and its Supplementary Information files. The raw image data are available from the corresponding author upon request. These image data are not deposited in a public database because of their large file sizes. Source Data are provided with this paper. The structures of the CRAF/MEK1/14-3-3 complex in the autoinhibited conformation and the CRAF RBD-CRD/KRAS complex were obtained from the Protein Data Bank under accession codes 9MMP [https://doi.org/10.2210/pdb9mmp/pdb] and 6XI7 [https://doi.org/10.2210/pdb6xi7/pdb], respectively. Source data are provided with this paper.
Code availability
The custom MATLAB script used for TrackMate data processing, association kinetics, and step size distribution analysis is available on GitHub at https://github.com/youngkwanglee-mem/SPT_Kon_StepSize. The specific version of the code used for the analysis in this study has been deposited in Zenodo with the https://doi.org/10.5281/zenodo.1812651770.
References
Lavoie, H. & Therrien, M. Regulation of RAF protein kinases in ERK signalling. Nat. Rev. Mol. Cell Biol. 16, 281–298 (2015).
Spencer-Smith, R. et al. RASopathy mutations provide functional insight into the BRAF cysteine-rich domain and reveal the importance of autoinhibition in BRAF regulation. Mol. Cell 82, 4262–4276 (2022).
Davies, H. et al. Mutations of the BRAF gene in human cancer. Nature 417, 949–954 (2002).
Holderfield, M., Deuker, M. M., McCormick, F. & McMahon, M. Targeting RAF kinases for cancer therapy: BRAF-mutated melanoma and beyond. Nat. Rev. Cancer 14, 455–467 (2014).
Samatar, A. A. & Poulikakos, P. I. Targeting RAS-ERK signalling in cancer: promises and challenges. Nat. Rev. Drug. Discov. 13, 928–942 (2014).
Rajakulendran, T., Sahmi, M., Lefrançois, M., Sicheri, F. & Therrien, M. A dimerization-dependent mechanism drives RAF catalytic activation. Nature 461, 542–545 (2009).
Hatzivassiliou, G. et al. RAF inhibitors prime wild-type RAF to activate the MAPK pathway and enhance growth. Nature 464, 431–435 (2010).
Heidorn, S. J. et al. Kinase-dead BRAF and oncogenic RAS cooperate to drive tumor progression through CRAF. Cell 140, 209–221 (2010).
Poulikakos, P. I., Zhang, C., Bollag, G., Shokat, K. M. & Rosen, N. RAF inhibitors transactivate RAF dimers and ERK signalling in cells with wild-type BRAF. Nature 464, 427–430 (2010).
Freeman, A. K., Ritt, D. A. & Morrison, D. K. The importance of Raf dimerization in cell signaling. Small GTPases 4, 180–185 (2013).
Bugaj, L. et al. Cancer mutations and targeted drugs can disrupt dynamic signal encoding by the Ras-Erk pathway. Science 361, eaao3048 (2018).
Simanshu, D. K. & Morrison, D. K. A structure is worth a thousand words: new insights for RAS and RAF regulation. Cancer Discov. 12, 899–912 (2022).
Willumsen, B. M., Christensen, A., Hubbert, N. L., Papageorge, A. G. & Lowy, D. R. The p21 ras C-terminus is required for transformation and membrane association. Nature 310, 583–586 (1984).
Stokoe, D., Macdonald, S. G., Cadwallader, K., Symons, M. & Hancock, J. F. Activation of Raf as a result of recruitment to the plasma membrane. Science 264, 1463–1467 (1994).
Zhang, X.-F. et al. Normal and oncogenic p21ras proteins bind to the amino-terminal regulatory domain of c-Raf-1. Nature 364, 308–313 (1993).
Fang, Z. et al. Multivalent assembly of KRAS with the RAS-binding and cysteine-rich domains of CRAF on the membrane. Proc. Natl. Acad. Sci. U.S.A. 117, 12101–12108 (2020).
Williams, J. et al. Elucidation of binding determinants and functional consequences of Ras/Raf-cysteine-rich domain interactions. J. Biol. Chem. 275, 22172–22179 (2000).
Ghosh, S. et al. The cysteine-rich region of raf-1 kinase contains zinc, translocates to liposomes, and is adjacent to a segment that binds GTP-ras. J. Biol. Chem. 269, 10000–10007 (1994).
Winkler, D. G. et al. Identification of residues in the cysteine-rich domain of Raf-1 that control Ras binding and Raf-1 activity. J. Biol. Chem. 273, 21578–21584 (1998).
Hu, J. et al. Allosteric activation of functionally asymmetric RAF kinase dimers. Cell 154, 1036–1046 (2013).
Liau, N. P. D. et al. Structural basis for SHOC2 modulation of RAS signalling. Nature 609, 400–407 (2022).
Kwon, J. J. et al. Structure–function analysis of the SHOC2–MRAS–PP1C holophosphatase complex. Nature 609, 408–415 (2022).
Hauseman, Z. J. et al. Structure of the MRAS–SHOC2–PP1C phosphatase complex. Nature 609, 416–423 (2022).
Bonsor, D. A. et al. Structure of the SHOC2–MRAS–PP1C complex provides insights into RAF activation and Noonan syndrome. Nat. Struct. Mol. Biol. 29, 966–977 (2022).
Liau, N. P. D. et al. Dimerization induced by C-terminal 14-3-3 binding is sufficient for BRAF kinase activation. Biochemistry 59, 3982–3992 (2020).
Liau, N. P. D. et al. Negative regulation of RAF kinase activity by ATP is overcome by 14-3-3-induced dimerization. Nat. Struct. Mol. Biol. 27, 134–141 (2020).
Park, E. et al. Architecture of autoinhibited and active BRAF–MEK1–14-3-3 complexes. Nature 575, 545–550 (2019).
Martinez Fiesco, J. A., Durrant, D. E., Morrison, D. K. & Zhang, P. Structural insights into the BRAF monomer-to-dimer transition mediated by RAS binding. Nat. Commun. 13, 486 (2022).
Park, E. et al. Cryo-EM structure of a RAS/RAF recruitment complex. Nat. Commun. 14, 4580 (2023).
Jang, D. M. et al. Cryo-EM structures of CRAF/MEK1/14-3-3 complexes in autoinhibited and open-monomer states reveal features of RAF regulation. Nat. Commun. 16, 8150 (2025).
Ritt, D. A. et al. An in vitro BRAF activation assay elucidates molecular mechanisms driving disassembly of the autoinhibited BRAF state. Proc. Natl. Acad. Sci. USA 122, 38 (2025).
Tian, T. et al. Plasma membrane nanoswitches generate high-fidelity Ras signal transduction. Nat. Cell Biol. 9, 905–914 (2007).
Zhou, Y. & Hancock, J. F. Lipid profiles of RAS nanoclusters regulate RAS function. Biomolecules 11, 1439 (2021).
Cookis, T. & Mattos, C. Crystal structure reveals the full Ras–Raf interface and advances mechanistic understanding of Raf activation. Biomolecules 11, 996 (2021).
Tran, T. H. et al. KRAS interaction with RAF1 RAS-binding domain and cysteine-rich domain provides insights into RAS-mediated RAF activation. Nat. Commun. 12, 1176 (2021).
Lee S. H. et al. Systems-level consequences of low RAF abundance for EGFR-ERK signaling. Biophys. J. 125, 881–900 (2026).
Surve, S. V. et al. Localization dynamics of endogenous fluorescently labeled RAF1 in EGF-stimulated cells. Mol. Biol. Cell 30, 506–523 (2018).
Gill, T. E. et al. Oncogenic mutant RAS signaling activity is rescaled by the ERK/MAPK pathway. Mol. Syst. Biol. 16, 9518 (2020).
Lorent, J. H. et al. Plasma membranes are asymmetric in lipid unsaturation, packing and protein shape. Nat. Chem. Biol. 16, 644–652 (2020).
Mazhab-Jafari, M. T. et al. Oncogenic and RASopathy-associated K-RAS mutations relieve membrane-dependent occlusion of the effector-binding site. Proc. Natl. Acad. Sci. U.S.A. 112, 6625–6630 (2015).
Lee, Y. K. et al. Mechanism of SOS PR-domain autoinhibition revealed by single-molecule assays on native protein from lysate. Nat. Commun. 8, 15061 (2017).
Iversen, L. et al. Molecular kinetics. Ras activation by SOS: allosteric regulation by altered fluctuation dynamics. Science 345, 50–54 (2014).
Rudack, T. et al. The Ras dimer structure. Chem. Sci. 12, 8178–8189 (2021).
Liu, N. F., Enomoto, M., Marshall, C. B. & Ikura, M. Reconstitution and characterization of BRAF in complex with 14-3-3 and KRAS4B on nanodiscs. Protein Sci. 33, e5016 (2024).
Buckles, T. C., Ziemba, B. P., Masson, G. R., Williams, R. L. & Falke, J. J. Single-molecule study reveals how receptor and Ras synergistically activate PI3Kα and PIP₃ signaling. Biophys. J. 113, 2396–2405 (2017).
McCombs, A. M., Armendariz, J. R. & Falke, J. J. Ras signaling mechanisms: new insights from single-molecule biophysics. Biophys. J. 123, 3277–3280 (2024).
Buckles, T. C. et al. The G-Protein Rab5A activates VPS34 Complex II, a Class III PI3K, by a dual regulatory mechanism. Biophys. J. 119, 2205–2218 (2020).
Werkmüller, A., Triola, G., Waldmann, H. & Winter, R. Rotational and translational dynamics of Ras proteins upon binding to model membrane systems. ChemPhysChem 14, 3698–3705 (2013).
Van, Q. N. et al. Uncovering a membrane-distal conformation of KRAS available to recruit RAF to the plasma membrane. Proc. Natl. Acad. Sci. U.S.A. 117, 24258–24268 (2020).
Chung, J. K. et al. K-Ras4B remains monomeric on membranes over a wide range of surface densities and lipid compositions. Biophys. J. 114, 137–145 (2018).
Shi, T. et al. Conservation of protein abundance patterns reveals the regulatory architecture of the EGFR-MAPK pathway. Sci. Signal 9, rs6 (2016).
Zheng, Y. et al. Structural insights into Ras regulation by SIN1. Proc. Natl. Acad. Sci. U.S.A. 119, e2119990119 (2022).
Lee, H.-W. et al. Real-time single-molecule co-immunoprecipitation analyses reveal cancer-specific Ras signalling dynamics. Nat. Commun. 4, 1505 (2013).
Li, L., Möbitz, S. & Winter, R. Characterization of the spatial organization of Raf isoforms interacting with K-Ras4B in the lipid membrane. Langmuir 36, 5944–5953 (2020).
Shrestha, R. et al. Membrane lipids drive formation of KRAS4b-RAF1 RBDCRD nanoclusters on the membrane. Commun. Biol. 7, 242 (2024).
Lavoie, H. et al. BRAF oncogenic mutants evade autoinhibition through a common mechanism. Science 388, eadp2742 (2025).
Li, S., Jang, H., Zhang, J. & Nussinov, R. Raf-1 cysteine-rich domain increases the affinity of K-Ras/Raf at the membrane, promoting MAPK signaling. Structure 26, 513–525.e2 (2018).
Nguyen, K. et al. Exploring CRD mobility during RAS/RAF engagement at the membrane. Biophys. J. 121, 3630–3650 (2022).
Ziemba, B. P. & Falke, J. J. Lateral diffusion of peripheral membrane proteins on supported lipid bilayers. Chem. Phys. Lipids 172-173, 67–77 (2013).
Travers, T. et al. Anionic lipids impact RAS-binding site accessibility and membrane binding affinity of CRAF RBD-CRD. Biophys. J. 119, 525–538 (2020).
Leonard, T. A. & Hurley, J. H. Regulation of protein kinases by lipids. Curr. Opin. Struct. Biol. 21, 785–791 (2011).
Hopfield, J. J. Kinetic proofreading: a new mechanism for reducing errors in biosynthetic processes requiring high specificity. Proc. Natl. Acad. Sci. U.S.A. 71, 4135–4139 (1974).
Huang, W. Y. C. et al. Phosphotyrosine-mediated LAT assembly on membranes drives kinetic bifurcation in recruitment dynamics of the Ras activator SOS. Proc. Natl. Acad. Sci. U.S.A. 113, 8218–8223 (2016).
Huang, W. Y. C. et al. A molecular assembly phase transition and kinetic proofreading modulate Ras activation by SOS. Science 363, 1098–1103 (2019).
Duewell, B. R., Wilson, N. E., Bailey, G. M., Peabody, S. E. & Hansen, S. D. Molecular dissection of PI3Kβ synergistic activation by receptor tyrosine kinases, GβGγ, and Rho-family GTPases. eLife 12, RP88991 (2023).
Oh, D. et al. Fast rebinding increases dwell time of Src homology 2 (SH2)-containing proteins near the plasma membrane. Proc. Natl. Acad. Sci. U.S.A. 109, 14024–14029 (2012).
Gureasko, J. et al. Membrane-dependent signal integration by the Ras activator Son of sevenless. Nat. Struct. Mol. Biol. 15, 452–461 (2008).
Song, Y., Rodgers, V. G. J., Schultz, J. S. & Liao, J. Protein interaction affinity determination by quantitative FRET technology. Biotechnol. Bioeng. 109, 2875–2883 (2012).
Tinevez, J.-Y. et al. TrackMate: an open and extensible platform for single-particle tracking. Methods 115, 80–90 (2017).
Lee, Y. K.SPT_Kon_StepSize: MATLAB script for association kinetics and step size distribution analysis. GitHub. https://doi.org/10.5281/zenodo.18126517 (2026).
Acknowledgements
We thank Tom Huxford for his constructive feedback on the manuscript and helpful discussions on protein analysis. We acknowledge the Scientific Instrumentation Facilities in the Department of Chemistry and Biochemistry at the University of San Diego, and Scientific Instrument Specialist Joseph Avila, for providing access to the Jasco J-1100 Circular Dichroism Spectrophotometer (CD) and for technical support. This study was supported by an NSF CAREER Award MCB-2145852 to Y.K.L. A.J.S. was supported in part as a Fellow of the Rees-Stealy Research Foundation.
Author information
Authors and Affiliations
Contributions
A.J.S. expressed and purified all proteins, with assistance from K.T. and A.C. A.J.S., K.T., and Y.K.L. performed and analyzed ensemble and single-molecule binding assays, with assistance from J.G., A.C., and A.M. J.G. performed FCS experiments. Y.K.L. designed the experiments and directed the project. A.J.S. and Y.K.L. drafted the manuscript with input from all authors.
Corresponding author
Ethics declarations
Competing interests
The authors declare no competing interests.
Peer review
Peer review information
Nature Communications thanks Joseph Falke and the other, anonymous, reviewer(s) for their contribution to the peer review of this work. A peer review file is available.
Additional information
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Supplementary information
Source data
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution-NonCommercial-NoDerivatives 4.0 International License, which permits any non-commercial use, sharing, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if you modified the licensed material. You do not have permission under this licence to share adapted material derived from this article or parts of it. The images or other third party material in this article are included in the article’s Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by-nc-nd/4.0/.
About this article
Cite this article
Jimenez Salinas, A., Tevdorashvili, K., Grim, J. et al. Positive cooperativity between RAS-binding and cysteine-rich domains regulates RAF membrane binding kinetics via lateral rebinding. Nat Commun (2026). https://doi.org/10.1038/s41467-026-69437-6
Received:
Accepted:
Published:
DOI: https://doi.org/10.1038/s41467-026-69437-6