Abstract
Highly charged intrinsically disordered proteins are essential regulators of chromatin structure and transcriptional activity. Here we identify a surprising mechanism of molecular competition that relies on the pronounced dynamical disorder present in these polyelectrolytes and their complexes. The highly positively charged human linker histone H1.0 (H1) binds to nucleosomes with ultrahigh affinity, implying residence times incompatible with efficient biological regulation. However, we show that the disordered regions of H1 retain their large-amplitude dynamics when bound to the nucleosome, which enables the highly negatively charged and disordered histone chaperone prothymosin α to efficiently invade the H1–nucleosome complex and displace H1 via a competitive substitution mechanism, vastly accelerating H1 dissociation. By integrating experiments and simulations, we establish a molecular model that rationalizes the remarkable kinetics of this process structurally and dynamically. Given the abundance of polyelectrolyte sequences in the nuclear proteome, this mechanism is likely to be widespread in cellular regulation.
This is a preview of subscription content, access via your institution
Access options
Access Nature and 54 other Nature Portfolio journals
Get Nature+, our best-value online-access subscription
$29.99 / 30 days
cancel any time
Subscribe to this journal
Receive 12 print issues and online access
$259.00 per year
only $21.58 per issue
Buy this article
- Purchase on Springer Link
- Instant access to full article PDF
Prices may be subject to local taxes which are calculated during checkout
Similar content being viewed by others
Data availability
Data supporting the findings of this study are available within the paper and its Supplementary Information. Source data are provided with this paper.
Code availability
A custom WSTP add-on for Mathematica (Wolfram Research) used for the analysis of single-molecule fluorescence data is available upon request and at https://schuler.bioc.uzh.ch/programs. A modified version of GROMACS was used for coarse-grained simulations, which is available at https://github.com/bestlab/gromacs-2019.4.git.
References
Habchi, J., Tompa, P., Longhi, S. & Uversky, V. N. Introducing protein intrinsic disorder. Chem. Rev. 114, 6561–6588 (2014).
Watson, M. & Stott, K. Disordered domains in chromatin-binding proteins. Essays Biochem. 63, 147–156 (2019).
Wright, P. E. & Dyson, H. J. Intrinsically disordered proteins in cellular signalling and regulation. Nat. Rev. Mol. Cell Biol. 16, 18–29 (2014).
Fuxreiter, M. et al. Malleable machines take shape in eukaryotic transcriptional regulation. Nat. Chem. Biol. 4, 728–737 (2008).
Vuzman, D. & Levy, Y. Intrinsically disordered regions as affinity tuners in protein–DNA interactions. Mol. Biosyst. 8, 47–57 (2012).
Borgia, A. et al. Extreme disorder in an ultrahigh-affinity protein complex. Nature 555, 61–66 (2018).
Turner, A. L. et al. Highly disordered histone H1–DNA model complexes and their condensates. Proc. Natl Acad. Sci. USA 115, 11964–11969 (2018).
Srivastava, S. & Tirrell, M. V. Polyelectrolyte complexation. Adv. Chem. Phys. 161, 499–544 (2016).
van der Gucht, J., Spruijt, E., Lemmers, M. & Cohen Stuart, M. A. Polyelectrolyte complexes: bulk phases and colloidal systems. J. Colloid Interface Sci. 361, 407–422 (2011).
Gibbs, E. B. & Kriwacki, R. W. Linker histones as liquid-like glue for chromatin. Proc. Natl Acad. Sci. USA 115, 11868–11870 (2018).
Larson, A. G. et al. Liquid droplet formation by HP1α suggests a role for phase separation in heterochromatin. Nature 547, 236–240 (2017).
Schuler, B. et al. Binding without folding – the biomolecular function of disordered polyelectrolyte complexes. Curr. Opin. Struct. Biol. 60, 66–76 (2019).
Korolev, N., Allahverdi, A., Lyubartsev, A. P. & Nordenskiold, L. The polyelectrolyte properties of chromatin. Soft Matter 8, 9322–9333 (2012).
Hergeth, S. P. & Schneider, R. The H1 linker histones: multifunctional proteins beyond the nucleosomal core particle. EMBO Rep. 16, 1439–1453 (2015).
Cutter, A. R. & Hayes, J. J. A brief review of nucleosome structure. FEBS Lett. 589, 2914–2922 (2015).
Öztürk, M. A., De, M., Cojocaru, V. & Wade, R. C. Chromatosome structure and dynamics from molecular simulations. Annu. Rev. Phys. Chem. 71, 101–119 (2020).
Willcockson, M. A. et al. H1 histones control the epigenetic landscape by local chromatin compaction. Nature 589, 293–298 (2021).
Gibson, B. A. et al. Organization of chromatin by intrinsic and regulated phase separation. Cell 179, 470–484, e421 (2019).
Flanagan, T. W. & Brown, D. T. Molecular dynamics of histone H1. Biochim. Biophys. Acta 1859, 468–475 (2016).
George, E. M. & Brown, D. T. Prothymosin α is a component of a linker histone chaperone. FEBS Lett. 584, 2833–2836 (2010).
Gomez-Marquez, J. & Rodríguez, P. Prothymosin α is a chromatin-remodelling protein in mammalian cells. Biochem. J. 333, 1–3 (1998).
Karetsou, Z. et al. Prothymosin α modulates the interaction of histone H1 with chromatin. Nucleic Acids Res. 26, 3111–3118 (1998).
Peng, B. & Muthukumar, M. Modeling competitive substitution in a polyelectrolyte complex. J. Chem. Phys. 143, 243133 (2015).
Mao, A. H., Crick, S. L., Vitalis, A., Chicoine, C. L. & Pappu, R. V. Net charge per residue modulates conformational ensembles of intrinsically disordered proteins. Proc. Natl Acad. Sci. USA 107, 8183–8188 (2010).
Müller-Späth, S. et al. Charge interactions can dominate the dimensions of intrinsically disordered proteins. Proc. Natl Acad. Sci. USA 107, 14609–14614 (2010).
Lowary, P. T. & Widom, J. New DNA sequence rules for high affinity binding to histone octamer and sequence-directed nucleosome positioning. J. Mol. Biol. 276, 19–42 (1998).
Fang, H., Clark, D. J. & Hayes, J. J. DNA and nucleosomes direct distinct folding of a linker histone H1 C-terminal domain. Nucleic Acids Res. 40, 1475–1484 (2012).
White, A. E., Hieb, A. R. & Luger, K. A quantitative investigation of linker histone interactions with nucleosomes and chromatin. Sci. Rep. 6, 19122 (2016).
Bednar, J. et al. Structure and dynamics of a 197 bp nucleosome in complex with linker histone H1. Mol. Cell 66, 384–397.e8 (2017).
Sridhar, A. et al. Emergence of chromatin hierarchical loops from protein disorder and nucleosome asymmetry. Proc. Natl Acad. Sci. USA 117, 7216–7224 (2020).
Syed, S. H. et al. Single-base resolution mapping of H1–nucleosome interactions and 3D organization of the nucleosome. Proc. Natl Acad. Sci. USA 107, 9620–9625 (2010).
Record, M. T. Jr, Anderson, C. F. & Lohman, T. M. Thermodynamic analysis of ion effects on the binding and conformational equilibria of proteins and nucleic acids: the roles of ion association or release, screening, and ion effects on water activity. Q. Rev. Biophys. 11, 103–178 (1978).
Anderson, C. F. & Record, M. T. Jr. Salt-nucleic acid interactions. Annu. Rev. Phys. Chem. 46, 657–700 (1995).
Brown, D. T., Izard, T. & Misteli, T. Mapping the interaction surface of linker histone H10 with the nucleosome of native chromatin in vivo. Nat. Struct. Mol. Biol. 13, 250–255 (2006).
Gansen, A. et al. High precision FRET studies reveal reversible transitions in nucleosomes between microseconds and minutes. Nat. Commun. 9, 4628 (2018).
Gansen, A. et al. Nucleosome disassembly intermediates characterized by single-molecule FRET. Proc. Natl Acad. Sci. USA 106, 15308–15313 (2009).
Gopich, I. V. & Szabo, A. Decoding the pattern of photon colors in single-molecule FRET. J. Phys. Chem. B 113, 10965–10973 (2009).
Lever, M. A., Th’ng, J. P., Sun, X. & Hendzel, M. J. Rapid exchange of histone H1.1 on chromatin in living human cells. Nature 408, 873–876 (2000).
Misteli, T., Gunjan, A., Hock, R., Bustin, M. & Brown, D. T. Dynamic binding of histone H1 to chromatin in living cells. Nature 408, 877–881 (2000).
Bednar, J., Hamiche, A. & Dimitrov, S. H1–nucleosome interactions and their functional implications. Biochim. Biophys. Acta 1859, 436–443 (2015).
Bryan, L. C. et al. Single-molecule kinetic analysis of HP1-chromatin binding reveals a dynamic network of histone modification and DNA interactions. Nucleic Acids Res. 45, 10504–10517 (2017).
Papamarcaki, T. & Tsolas, O. Prothymosin α binds to histone H1 in vitro. FEBS Lett. 345, 71–75 (1994).
Sottini, A. et al. Polyelectrolyte interactions enable rapid association and dissociation in high-affinity disordered protein complexes. Nat. Commun. 11, 5736 (2020).
Haritos, A. A., Salvin, S. B., Blacher, R., Stein, S. & Horecker, B. L. Parathymosin alpha: a peptide from rat tissues with structural homology to prothymosin alpha. Proc. Natl Acad. Sci. USA 82, 1050–1053 (1985).
Chen, T. Y., Cheng, Y. S., Huang, P. S. & Chen, P. Facilitated unbinding via multivalency-enabled ternary complexes: new paradigm for protein–DNA interactions. Acc. Chem. Res. 51, 860–868 (2018).
Gibb, B. et al. Concentration-dependent exchange of replication protein A on single-stranded DNA revealed by single-molecule imaging. PLoS ONE 9, e87922 (2014).
Kamar, R. I. et al. Facilitated dissociation of transcription factors from single DNA binding sites. Proc. Natl Acad. Sci. USA 114, E3251–E3257 (2017).
Lewis, J. S. et al. Single-molecule visualization of fast polymerase turnover in the bacterial replisome. eLife 6, e23932 (2017).
Potoyan, D. A., Zheng, W. H., Komives, E. A. & Wolynes, P. G. Molecular stripping in the NF-κB/IκB/DNA genetic regulatory network. Proc. Natl Acad. Sci. USA 113, 110–115 (2016).
Wu, H., Dalal, Y. & Papoian, G. A. Binding dynamics of disordered linker histone H1 with a nucleosomal particle. J. Mol. Biol. 433, 166881 (2021).
Fang, H., Wei, S., Lee, T. H. & Hayes, J. J. Chromatin structure-dependent conformations of the H1 CTD. Nucleic Acids Res. 44, 9131–9141 (2016).
Soranno, A. et al. Quantifying internal friction in unfolded and intrinsically disordered proteins with single-molecule spectroscopy. Proc. Natl Acad. Sci. USA 109, 17800–17806 (2012).
Nettels, D., Gopich, I. V., Hoffmann, A. & Schuler, B. Ultrafast dynamics of protein collapse from single-molecule photon statistics. Proc. Natl. Acad. Sci. USA 104, 2655–2660 (2007).
Kenzaki, H. & Takada, S. Partial unwrapping and histone tail dynamics in nucleosome revealed by coarse-grained molecular simulations. PLoS Comput. Biol. 11, e1004443 (2015).
Zhang, B., Zheng, W., Papoian, G. A. & Wolynes, P. G. Exploring the free energy landscape of nucleosomes. J. Am. Chem. Soc. 138, 8126–8133 (2016).
Holmstrom, E. D., Liu, Z. W., Nettels, D., Best, R. B. & Schuler, B. Disordered RNA chaperones can enhance nucleic acid folding via local charge screening. Nat. Commun. 10, 245 (2019).
Korolev, N., Fan, Y., Lyubartsev, A. P. & Nordenskiold, L. Modelling chromatin structure and dynamics: status and prospects. Curr. Opin. Struct. Biol. 22, 151–159 (2012).
Lu, X., Hamkalo, B., Parseghian, M. H. & Hansen, J. C. Chromatin condensing functions of the linker histone C-terminal domain are mediated by specific amino acid composition and intrinsic protein disorder. Biochemistry 48, 164–172 (2009).
Shoemaker, B. A., Portman, J. J. & Wolynes, P. G. Speeding molecular recognition by using the folding funnel: the fly-casting mechanism. Proc. Natl Acad. Sci. USA 97, 8868–8873 (2000).
Vareli, K., Tsolas, O. & Frangou-Lazaridis, M. Regulation of prothymosin α during the cell cycle. Eur. J. Biochem. 238, 799–806 (1996).
Wang, S. et al. Linker histone defines structure and self-association behaviour of the 177 bp human chromatosome. Sci. Rep. 11, 380 (2021).
Catez, F., Ueda, T. & Bustin, M. Determinants of histone H1 mobility and chromatin binding in living cells. Nat. Struct. Mol. Biol. 13, 305–310 (2006).
Annalisa, I. & Robert, S. The role of linker histone H1 modifications in the regulation of gene expression and chromatin dynamics. Biochim. Biophys. Acta 1859, 486–495 (2015).
Privalov, P. L., Dragan, A. I. & Crane-Robinson, C. Interpreting protein/DNA interactions: distinguishing specific from non-specific and electrostatic from non-electrostatic components. Nucleic Acids Res. 39, 2483–2491 (2011).
Shakya, A., Park, S., Rana, N. & King, J. T. Liquid-liquid phase separation of histone proteins in cells: role in chromatin organization. Biophys. J. 118, 753–764 (2020).
Scott, K. A., Steward, A., Fowler, S. B. & Clarke, J. Titin; a multidomain protein that behaves as the sum of its parts. J. Mol. Biol. 315, 819–829 (2002).
Kilic, S., Bachmann, A. L., Bryan, L. C. & Fierz, B. Multivalency governs HP1α association dynamics with the silent chromatin state. Nat. Commun. 6, 7313 (2015).
Lowary, P. T. & Widom, J. New DNA sequence rules for high affinity binding to histone octamer and sequence-directed nucleosome positioning. J. Mol. Biol. 276, 19–42 (1998).
Dyer, P. N. et al. Reconstitution of Nnucleosome core particles from recombinant histones and DNA. Methods Enzymol. 375, 23–44 (2004).
Müller, B. K., Zaychikov, E., Bräuchle, C. & Lamb, D. C. Pulsed interleaved excitation. Biophys. J. 89, 3508–3522 (2005).
Klehs, K. et al. Increasing the brightness of cyanine fluorophores for single-molecule and superresolution imaging. ChemPhysChem 15, 637–641 (2014).
Aitken, C. E., Marshall, R. A. & Puglisi, J. D. An oxygen scavenging system for improvement of dye stability in single-molecule fluorescence experiments. Biophys. J. 94, 1826–1835 (2008).
Ha, T. & Tinnefeld, P. Photophysics of fluorescence probes for single-molecule biophysics and super-resolution imaging. Ann. Rev. Phys. Chem. 63, 595–617 (2012).
Schuler, B. Application of single molecule Förster resonance energy transfer to protein folding. Methods Mol. Biol. 350, 115–138 (2007).
Nettels, D., Gopich, I. V., Hoffmann, A. & Schuler, B. Ultrafast dynamics of protein collapse from single-molecule photon statistics. Proc. Natl Acad. Sci. USA 104, 2655–2660 (2007).
Gopich, I. V., Nettels, D., Schuler, B. & Szabo, A. Protein dynamics from single-molecule fluorescence intensity correlation functions. J. Chem. Phys. 131, 095102 (2009).
Holmstrom, E. D. et al. Accurate transfer efficiencies, distance distributions, and ensembles of unfolded and intrinsically disordered proteins from single-molecule FRET. Methods Enzymol. 611, 287–325 (2018).
Zheng, W. et al. Inferring properties of disordered chains from FRET transfer efficiencies. J. Chem. Phys. 148, 123329 (2018).
Gopich, I. V. & Szabo, A. Theory of the energy transfer efficiency and fluorescence lifetime distribution in single-molecule FRET. Proc. Natl Acad. Sci. USA 109, 7747–7752 (2012).
Sisamakis, E., Valeri, A., Kalinin, S., Rothwell, P. J. & Seidel, C. A. M. Accurate single-molecule FRET studies using multiparameter fluorescence detection. Methods Enzymol. 475, 455–514 (2010).
Hellenkamp, B. et al. Precision and accuracy of single-molecule FRET measurements—a multi-laboratory benchmark study. Nat. Methods 15, 669–676 (2018).
Zosel, F., Mercadante, D., Nettels, D. & Schuler, B. A proline switch explains kinetic heterogeneity in a coupled folding and binding reaction. Nat. Commun. 9, 3332 (2018).
Chung, H. S. et al. Extracting rate coefficients from single-molecule photon trajectories and FRET efficiency histograms for a fast-folding protein. J. Phys. Chem. A 115, 3642–3656 (2011).
Viterbi, A. J. Error bounds for convolutional codes and an asymptotically optimum decoding algorithm. IEEE Trans. Inf. Theory 13, 260–269 (1967).
Karanicolas, J. & Brooks, C. L. III The origins of asymmetry in the folding transition states of protein L and protein G. Protein Sci. 11, 2351–2361 (2002).
Kim, Y. C. & Hummer, G. Coarse-grained models for simulations of multiprotein complexes: application to ubiquitin binding. J. Mol. Biol. 375, 1416–1433 (2008).
Yakovchuk, P., Protozanova, E. & Frank-Kamenetskii, M. D. Base-stacking and base-pairing contributions into thermal stability of the DNA double helix. Nucleic Acids Res. 34, 564–574 (2006).
Zhou, B. R. et al. Structural insights into the histone H1–nucleosome complex. Proc. Natl Acad. Sci. USA 110, 19390–19395 (2013).
Zhou, Y. B., Gerchman, S. E., Ramakrishnan, V., Travers, A. & Muyldermans, S. Position and orientation of the globular domain of linker histone H5 on the nucleosome. Nature 395, 402–405 (1998).
Berendsen, H. J. C., van der Spoel, D. & van Drunen, R. GROMACS: a message-passing parallel molecular dynamics implementation. Comp. Phys. Comm. 91, 43–56 (1995).
van der Spoel, D. et al. GROMACS: fast, flexible, and free. J. Comput. Chem. 26, 1701–1718 (2005).
Aznauryan, M. et al. Comprehensive structural and dynamical view of an unfolded protein from the combination of single-molecule FRET, NMR, and SAXS. Proc. Natl Acad. Sci. USA 113, E5389–E5398 (2016).
Lin, L. I. A concordance correlation coefficient to evaluate reproducibility. Biometrics 45, 255–268 (1989).
Tribello, G. A., Bonomi, M., Branduardi, D., Camilloni, C. & Bussi, G. Plumed 2: new feathers for an old bird. Comput. Phys. Commun. 185, 604–613 (2014).
Sugita, Y., Kitao, A. & Okamoto, Y. Multidimensional replica-exchange method for free-energy calculations. J. Chem. Phys. 113, 6042–6051 (2000).
Kumar, S., Rosenberg, J. M., Bouzida, D., Swendsen, R. H. & Kollman, P. A. The weighted histogram analysis method for free-energy calculations on biomolecules. I. The method. J. Comp. Chem. 13, 1011–1021 (1992).
Shoup, D. & Szabo, A. Role of diffusion in ligand binding to macromolecules and cell-bound receptors. Biophys. J. 40, 33–39 (1982).
Acknowledgements
We thank I. König for providing ProTα, K. Buholzer and F. Sturzenegger for helpful discussion, F. Büchler and N. Wyss for excellent technical assistance and the Functional Genomics Center Zurich for performing mass spectrometry. This work utilized the computational resources of the National Institutes of Health HPC Biowulf cluster (http://hpc.nih.gov) and of Piz Daint at the CSCS Swiss National Supercomputing Centre. This project was funded by the Novo Nordisk Foundation (P.O.H.), the Carlsberg Foundation (P.O.H.), The Boehringer Ingelheim Fonds (S.K.), the Swiss National Science Foundation (B.S. and B.F.), École Polytechnique Fédérale de Lausanne (B.F.) and the Intramural Research Program of the National Institute of Diabetes and Digestive and Kidney Diseases at the National Institutes of Health (R.B.B.).
Author information
Authors and Affiliations
Contributions
P.O.H., D.M., R.B.B. and B.S. designed the research; P.O.H. and S.K. prepared the reconstituted nucleosomes; P.O.H., M.B.B., A.B., A.S., S.K. and B.F. prepared the fluorescently labelled and/or unlabelled proteins; P.O.H. and A.S. performed the single-molecule experiments; P.O.H., A.S., D.N. and B.S. analysed the single-molecule data; D.M. and R.B.B. performed and analysed the simulations; R.B.B., B.F. and B.S. supervised the research; and P.O.H. and B.S. wrote the paper with help from all authors.
Corresponding authors
Ethics declarations
Competing interests
The authors declare no competing interests.
Additional information
Peer review information Nature Chemistry thanks the anonymous reviewers for their contribution to the peer review of this work.
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Supplementary information
Supplementary Information
Supplementary Figs. 1–7, Tables 1–3 and references.
Supplementary Video 1
Ensemble of H1 bound to the nucleosome. H1 is represented in blue, DNA in grey and the core histones in white. The video shows 1,000 conformers of the H1–nucleosome complex, obtained from replica-exchange molecular dynamics simulations as described in the Methods.
Supplementary Video 2
Binding and dissociation trajectories of ProTα and H1 bound to the nucleosome. ProTα is shown in red, H1 in blue, DNA in grey and the core histones in white. The trajectory depicting the association of ProTα to the H1–nucleosome complex is concatenated with a trajectory showing the ProTα–H1 complex dissociating from the nucleosome (as indicated by the text displayed), where a ratchet bias with a force constant of 1 kJ mol−1 nm−2 is applied to the globular domain with respect to the dyad to enable dissociation during the accessible simulation time. The segments of the simulations shown correspond to ~5.0 × 105 time steps for ProTα binding and ~2 × 105 time steps for dissociation. Note that these times are more akin to transition path times for binding and dissociation than first passage times, which would be orders of magnitude longer.
Supplementary Data
Source data supporting information.
Source data
Source Data Fig. 1
Transfer efficiency histograms, binding isotherms and binding affinities.
Source Data Fig. 2
Fluorescence time trajectory, dwell times and association/dissociation rates.
Source Data Fig. 3
Fluorescence time trajectories, association/dissociation rates, transfer efficiency histograms and binding isotherms.
Source Data Fig. 4
The nsFCS data, transfer efficiency histograms and transfer efficiencies from experiment and simulation.
Source Data Fig. 5
Simulation data.
Rights and permissions
About this article
Cite this article
Heidarsson, P.O., Mercadante, D., Sottini, A. et al. Release of linker histone from the nucleosome driven by polyelectrolyte competition with a disordered protein. Nat. Chem. 14, 224–231 (2022). https://doi.org/10.1038/s41557-021-00839-3
Received:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1038/s41557-021-00839-3
This article is cited by
-
DNA binding redistributes activation domain ensemble and accessibility in pioneer factor Sox2
Nature Communications (2024)
-
The molecular basis for cellular function of intrinsically disordered protein regions
Nature Reviews Molecular Cell Biology (2024)
-
Extreme dynamics in a biomolecular condensate
Nature (2023)