Abstract
Intercellular calcium waves (ICW) are complex signalling phenomena that control many essential biological activities, including smooth muscle contraction, vesicle secretion, gene expression and changes in neuronal excitability. Accordingly, the remote stimulation of ICW could result in versatile biomodulation and therapeutic strategies. Here we demonstrate that light-activated molecular machines (MM)—molecules that perform mechanical work on the molecular scale—can remotely stimulate ICW. MM consist of a polycyclic rotor and stator that rotate around a central alkene when activated with visible light. Live-cell calcium-tracking and pharmacological experiments reveal that MM-induced ICW are driven by the activation of inositol-triphosphate-mediated signalling pathways by unidirectional, fast-rotating MM. Our data suggest that MM-induced ICW can control muscle contraction in vitro in cardiomyocytes and animal behaviour in vivo in Hydra vulgaris. This work demonstrates a strategy for directly controlling cell signalling and downstream biological function using molecular-scale devices.
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
All data supporting the findings of this study are available within the article and its supplementary information. Source data are provided with this paper. Additional raw data and analysis code are available via GitHub at https://github.com/jlb48249/MM-ICW.
Code availability
Data analysis scripts are available via GitHub at https://github.com/jlb48249/MM-ICW.
References
Clapham, D. E. Calcium signaling. Cell 131, 1047–1058 (2007).
Tsutsumi, M. et al. Mechanical-stimulation-evoked calcium waves in proliferating and differentiated human keratinocytes. Cell Tissue Res. 338, 99–106 (2009).
Screaton, R. A. et al. The CREB coactivator TORC2 functions as a calcium- and cAMP-sensitive coincidence detector. Cell 119, 61–74 (2004).
Carrasco, M. A. & Hidalgo, C. Calcium microdomains and gene expression in neurons and skeletal muscle cells. Cell Calcium 40, 575–583 (2006).
Glaser, T. et al. ATP and spontaneous calcium oscillations control neural stem cell fate determination in Huntington’s disease: a novel approach for cell clock research. Mol. Psychiatry 26, 2633–2650 (2021).
Tada, M. & Concha, M. L. Vertebrate gastrulation: calcium waves orchestrate cell movements. Curr. Biol. 11, R470–R472 (2001).
McCormack, J. G., Halestrap, A. P. & Denton, R. M. Role of calcium ions in regulation of mammalian intramitochondrial metabolism. Phys. Rev. 70, 391–425 (1990).
Leybaert, L. & Sanderson, M. J. Intercellular Ca2+ waves: mechanisms and function. Phys. Rev. 92, 1359–1392 (2012).
Eng, G. et al. Autonomous beating rate adaptation in human stem cell-derived cardiomyocytes. Nat. Commun. 7, 10312 (2016).
Llano, I. et al. Presynaptic calcium stores underlie large-amplitude miniature IPSCs and spontaneous calcium transients. Nat. Neurosci. 3, 1256–1265 (2000).
Takano, T. et al. Astrocyte-mediated control of cerebral blood flow. Nat. Neurosci. 9, 260–267 (2006).
Drumm, B. T. et al. The effects of mitochondrial inhibitors on Ca2+ signalling and electrical conductances required for pacemaking in interstitial cells of Cajal in the mouse small intestine. Cell Calcium 72, 1–17 (2018).
Gourine, A. V. et al. Astrocytes control breathing through pH-dependent release of ATP. Science 329, 571–575 (2010).
Berridge, M. J. Calcium signaling remodeling and disease. Biochem. Soc. Trans. 40, 297–309 (2012).
Stewart, T. A., Yapa, K. T. D. S. & Monteith, G. R. Altered calcium signaling in cancer cells. Biochim. Biophys. Acta Biomembr. 1848, 2502–2511 (2015).
Berridge, M. J., Lipp, P. & Bootman, M. D. The versatility and universality of calcium signaling. Nat. Rev. Mol. Cell Biol. 1, 11–21 (2000).
Cornell-Bell, A. H. et al. Glutamate induces calcium waves in cultured astrocytes: long-range glial signaling. Science 247, 470–473 (1990).
Sanderson, M. J., Charles, A. C. & Dirksen, E. R. Mechanical stimulation and intercellular communication increases intracellular Ca2+ in epithelial cells. Cell Regul. 1, 585–596 (1990).
Klok, M. et al. MHz unidirectional rotation of molecular rotary motors. J. Am. Chem. Soc. 130, 10484–10485 (2008).
García-López, V. et al. Unimolecular submersible nanomachines. synthesis, actuation, and monitoring. Nano Lett. 15, 8229–8239 (2015).
García-López, V. et al. Molecular machines open cell membranes. Nature 548, 567–572 (2017).
Zheng, Y. et al. Optoregulated force application to cellular receptors using molecular motors. Nat. Commun. 12, 3580 (2021).
García-López, V., Liu, D. & Tour, J. M. Light-activated organic molecular motors and their applications. Chem. Rev. 120, 79–124 (2020).
Pollard, M. M., Klok, M., Pijper, D. & Feringa, B. L. Rate acceleration of light-driven rotary molecular motors. Adv. Func. Mater. 17, 718–729 (2007).
Alaya-Orozco, C. et al. Visible-light-activated molecular nanomachines kill pancreatic cancer cells. ACS Appl. Mater. Int. 12, 410–417 (2020).
Kepp, O., Galluzzi, L., Lipinski, M., Yuan, J. & Kroemer, G. Cell death assays for drug discovery. Nat. Rev. Drug Discov. 10, 221–237 (2011).
Galbadage, T. et al. Molecular nanomachines disrupt bacterial cell wall, increasing sensitivity of extensively drug-resistant Klebsiella pneumoniae to meropenem. ACS Nano 13, 14377–14387 (2019).
Santos, A. L. et al. Light-activated molecular machines are fast-acting broad-spectrum antibacterials that target the membrane. Sci. Adv. 8, eabm2055 (2022).
Vriens, J., Appendino, G. & Nilius, B. Pharmacology of vanilloid transient receptor potential cation channels. Mol. Pharmacol. 75, 1262–1279 (2009).
Hamill, O. P. & McBride, D. W. Jr The pharmacology of mechanogated membrane ion channels. Pharmacol. Rev. 48, 231–252 (1996).
Thastrup, O., Cullen, P. J., Drøbak, B. K., Hanley, M. R. & Dawson, A. P. Thapsigargin, a tumor promoter, discharges intracellular Ca2+ stores by specific inhibition of the endoplasmic reticulum Ca2+-ATPase. Proc. Natl Acad. Sci. USA 87, 2466–2470 (1990).
Bock, G. R. & Ackrill, K. Calcium Waves, Gradients and Oscillations (Wiley, 2008).
Gafni, J. et al. Xestospongins: potent membrane permeable blockers of the inositol 1,4,5-trisphosphate receptor. Neuron 19, 723–733 (1997).
Ribeiro, C. M. P., Reece, J. & Putney, J. W. Role of the cytoskeleton in calcium signaling in NIH 3T3 cells. J. Biol. Chem. 272, 26555–26561 (1997).
Xu, J. et al. GPR68 senses flow and is essential for vascular physiology. Cell 173, 762–775.e16 (2018).
Feher, J. Quantitative Human Physiology: An Introduction 351–361 (Elsevier, 2007).
Stuyvers, B. D., Boyden, P. A. & ter Keurs, H. E. D. J. Calcium waves. Circ. Res. 86, 1016–1018 (2000).
Wang, H. et al. A complete biomechanical model of Hydra contractile behaviors, from neural drive to muscle to movement. Proc. Natl Acad. Sci. 120, e2210439120 (2023).
Goel, T., Wang, R., Martin, S. & Collins, E.-M. S. Linalool acts as a fast and reversible anesthetic in Hydra. PLoS ONE 14, e0224221 (2019).
Takaku, Y. et al. Innexin gap junctions in nerve cells coordinate spontaneous contractile behavior in Hydra polyps. Sci. Rep. 4, 3573 (2014).
Kinnamon, J. C. & Westfall, J. A. A three dimensional serial reconstruction of neuronal distributions in the hypostome of a Hydra. J. Morphol. 168, 321–329 (1981).
Kinnamon, J. C. & Westfall, J. A. Types of neurons and synaptic connections at hypostome-tentacle junctions in Hydra. J. Morphol. 173, 119–128 (1982).
Dupre, C. & Yuste, R. Non-overlapping neural networks in Hydra vulgaris. Curr. Biol. 27, 1085–1097 (2017).
Badhiwala, K. N., Primack, A. S., Juliano, C. E. & Robinson, J. T. Multiple neuronal networks coordinate Hydra mechanosensory behavior. eLife 10, e64108 (2020).
Guertin, S. & Kass-Simon, G. Extraocular spectral photosensitivity in the tentacles of Hydra vulgaris. Comp. Biochem. Physiol. A Mol. Integr. Physiol. 184, 163–170 (2015).
van Venrooy, A. et al. Probing the rotary cycle of amine-substituted molecular motors. J. Org. Chem. 88, 762–770 (2023).
Garcia-Lopez, V. et al. Synthesis of light-driven motorized nanocars for linear trajectories and their detailed NMR structural determination. Tetrahedron 73, 4864–4873 (2017).
Sinnecker, D. & Schaefer, M. Real-time analysis of phospholipase C activity during different patterns of receptor-induced Ca2+ responses in HEK293 cells. Cell Calcium 35, 29–38 (2004).
Lancon, A. et al. Human hepatic cell uptake of resveratrol: involvement of both passive diffusion and carrier-mediated process. Biochem. Biophys. Res. Commun. 4, 1132–1137 (2004).
Roke, D. et al. Light-gated rotation in a molecular motor functionalized with a dithienylethene switch. Angew. Chem. Int. Ed. 57, 10515–10519 (2018).
Saywell, A. et al. Light-induced translation of motorized molecules on a surface. ACS Nano 10, 10945–10952 (2016).
Frisch, M. J. et al. Gaussian 16 Rev. A.03 (Wallingford, 2016).
Dennington, R., Keith, T. A and Millam, J. M. GaussView version 6 (Semichem, 2019).
Tao, J., Perdew, J. P., Staroverov, V. N. & Scuseria, G. E. Climbing the density functional theory ladder: nonempirical meta-generalized gradient approximation designed for molecules and solids. Phys. Rev. Lett. 91, 146401 (2003).
Weigend, F. & Ahlrichs, R. Balanced basis sets of split valence, triple zeta valence and quadruple zeta valence quality for H to Rn: design and assessment of accuracy. Phys. Chem. Chem. Phys. 7, 3297–3305 (2005).
Grimme, S., Ehrlich, S. & Georigk, L. Effect of the damping function in dispersion corrected density functional theory. J. Comp. Chem. 32, 1456–1465 (2011).
Dunlap, B. I. Robust and variational fitting: removing the four-center integrals from center stage in quantum chemistry. J. Mol. Struct. THEOCHEM 529, 37–40 (2000).
Grimme, S., Antony, J., Ehrlich, S. & Krieg, H. A consistent and accurate ab initio parametrization of density functional dispersion correction (DFT-D) for the 94 elements H-Pu. J. Chem. Phys. 132, 154104 (2010).
Stratmann, R. E., Scuseria, G. E. & Frisch, M. J. Achieving linear scaling in exchange-correlation density functional quadratures. Chem. Phys. Lett. 257, 213–223 (1996).
Zhao, X., Fan, B., Hassan, S., Veeraraghavan, A. & Robinson, J. T. Near field optical sensing of single cell activity with integrated micro-ring resonators. In Biophotonics Congress 2021 paper BTu3B.4 (Optical Society of America, 2021).
Gunasekera, R. S. et al. Molecular nanomachines can destroy tissue or kill multicellular eukaryotes. ACS Appl. Mater. Int. 12, 13657–13670 (2020).
Hajnoczky, G., Davies, E. & Madesh, M. Calcium signaling and apoptosis. Biochem. Biophys. Ref. Commun. 304, 445–454 (2003).
Cnossen, A., Kistemaker, J. C. M., Kojima, T. & Feringa, B. L. Structural dynamics of overcrowded alkene-based molecular motors during thermal isomerization. J. Org. Chem. 79, 927–935 (2014).
Nagaraja, D. et al. Solvent effect on the relative quantum yield and fluorescence quenching of a newly synthesized coumarin derivative. Luminescence 30, 495–502 (2014).
Tzouanas, C. N. et al. Hydra show stable responses to thermal stimulation despite large changes in the number of neurons. iScience 24, 102490 (2021).
Grunder, S. & Assmann, M. Peptide-gated ion channels and the simple nervous system of Hydra. J. Exp. Biol. 218, 551–561 (2015).
Grigoryan, B. et al. Development, characterization, and applications of multi-material stereolithography bioprinting. Sci. Rep. 11, 3171 (2021).
Mizuno, K., Kurokawa, K. & Ohkuma, S. Regulation of type 1 IP3 receptor expression by dopamine D2-like receptors via AP-1 and NFATc4 activation. Neuropharmacology 71, 264–272 (2013).
Acknowledgements
This project received funding from the Discovery Institute, the Robert A. Welch Foundation (C-2017-20190330), the National Science Foundation Graduate Research Fellowship Program (J.L.B.), the DEVCOM Army Research Laboratory under Cooperative Agreement W911NF-18-2-0234 (A.R.v.V.) and the European Union’s Horizon 2020 research and innovation programme under the Marie Skłodowska-Curie grant agreement no. 843116 (A.L.S.). The views and conclusions contained in this document are those of the authors and should not be interpreted as representing the official policies, either expressed or implied, of the Army Research Laboratory or the US government. The US government is authorized to reproduce and distribute reprints for government purposes notwithstanding any copyright notation herein. The funders had no role in the study design, data collection and analysis, decision to publish, or preparation of the manuscript. This work was conducted in part using resources from the Light Microscopy Facility and the Shared Equipment Authority at Rice University. We acknowledge Z. C. Sanchez (Vanderbilt University) for useful help and advice regarding the growth and activity of cardiomyocytes.
Author information
Authors and Affiliations
Contributions
Conceptualization: J.L.B., A.R.v.V. and J.M.T. Methodology: J.L.B., G.D., S.K., X.Z. and A.L.S. Organic synthesis: A.R.v.V., G.L., B.L., D.L. and J.M.T. Formal analysis: J.L.B. Investigation: J.L.B., S.K., G.C., D.A. and J.Z. Resources: J.T.R. and J.M.T. Writing (original draft): J.L.B. Writing (reviewing and editing): J.L.B., G.D., S.K., A.L.S., J.T.R. and J.M.T. Software: J.L.B. and J.T.L. Visualization: J.L.B. Supervision: G.D., J.T.R. and J.M.T. Funding acquisition: J.M.T. Project oversight: J.M.T.
Corresponding authors
Ethics declarations
Competing interests
Rice University owns the intellectual property on the use of electromagnetic (light) activation of MM for the stimulation of ICW. Conflicts of interest are managed through regular disclosure to the Rice University Office of Sponsored Projects and Research Compliance. The authors declare no other competing interests.
Peer review
Peer review information
Nature Nanotechnology thanks Carson Bruns, Danijela Gregurec and Gabriela Romero Uribe for their contribution to the peer review of this work.
Additional information
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Supplementary information
Supplementary Information
Supplementary Figs. 1–49, Tables 1 and 4 and Discussion.
Supplementary Video 1
Animation of the intrinsic reaction coordinate trajectory for the rate-limiting thermal helix inversion step in MM 1.
Supplementary Video 2
Animation of the intrinsic reaction coordinate trajectory for the rate-limiting thermal helix inversion step in MM 2.
Supplementary Video 3
Animation of the intrinsic reaction coordinate trajectory for the rate-limiting thermal helix inversion step in MM 3.
Supplementary Video 4
Animation of the intrinsic reaction coordinate trajectory for the rate-limiting thermal helix inversion step in MM 4.
Supplementary Video 5
Animation of the intrinsic reaction coordinate trajectory for an alternative relaxation pathway in MM 4.
Supplementary Video 6
Time lapse of Fluo-4 fluorescence in cardiomyocytes treated with MM 1 (8 µM) and Fluo-4 and stimulated with 400 nm laser light for 250 ms at an irradiance of 5.1 × 102 W cm–2. The cell on the left is stimulated at 30 s.
Supplementary Video 7
Time lapse of fluorescence images of a cardiomyocyte treated with MM 1 (8 µM) and CellLight Actin-GFP BacMam 2.0 and stimulated with 400 nm laser light for 250 ms at an irradiance of 5.1 × 102 W cm–2. Stimulation was applied at 30 s. The inward movement of the z lines demonstrates localized contraction at the point of stimulation on the release of calcium ions from the SR.
Supplementary Video 8
Time lapse of bright-field images of cardiomyocytes treated with MM 1 (8 µM) and Fluo-4 and stimulated with 400 nm laser light for 250 ms at an irradiance of 5.1 × 102 W cm–2. The cell on the left is stimulated at 30 s.
Supplementary Video 9
Time lapse of fluorescence images of a cardiomyocyte treated with MM 1 (8 µM) and di-8-Anneps (1 µg ml–1) and stimulated with 400 nm laser light for 250 ms at an irradiance of 5.1 × 102 W cm–2. Stimulation was applied at 30 s. The increase in fluorescence of di-8-Anneps during contraction indicates a change in membrane voltage during an action potential.
Supplementary Video 10
Hydra expressing GCaMP7b in epitheliomuscular cells treated with MM 1 (24 µM) and stimulated with 405 nm laser light for 1 s at an irradiance of 9.0 × 102 W cm–2 (protocol I). Stimulation is applied at 10 s. The blue circle shown at 10 s corresponds to the area of stimulation. The trace shown at the bottom of the video corresponds to the intensity of GCaMP7b fluorescence in the area of stimulation across the timescale of the video. The cyan line in the trace represents the time of stimulus presentation, during which no data were collected.
Supplementary Video 11
Hydra expressing GCaMP7b in epitheliomuscular cells treated with DMSO solvent (0.3% v/v) and stimulated with 405 nm laser light for 1 s at an irradiance of 9.0 × 102 W cm–2 (protocol I). Stimulation is applied at 10 s. The blue circle shown at 10 s corresponds to the area of stimulation. The trace shown at the bottom corresponds to the intensity of GCaMP7b fluorescence in the area of stimulation across the timescale of the video. The cyan line in the trace represents the time of stimulus presentation, during which no data were collected.
Supplementary Video 12
Hydra expressing GCaMP7b in epitheliomuscular cells treated with MM 2 (24 µM) and stimulated with 405 nm laser light for 1 s at an irradiance of 6.8 × 102 W cm–2 (protocol I). Stimulation is applied at 10 s at two distinct locations in the Hydra indicated by the yellow and blue circles that appear during stimulation. The traces shown at the bottom of the video correspond to the intensity of GCaMP7b fluorescence in the areas of stimulation across the timescale of the video.
Supplementary Video 13
Hydra expressing GCaMP7b in epitheliomuscular cells treated with MM 2 (24 µM) and stimulated with 405 nm laser light for 2 s at an irradiance of 9.0 × 102 W cm–2. Light was delivered to the oral region of the Hydra (protocol II) at irregular intervals. The yellow circle around the oral region indicates the region to which stimulation was applied. The trace shown at the bottom of the video corresponds to the intensity of GCaMP7b fluorescence in the whole Hydra across the timescale of the video. The vertical yellow lines in the trace mark times during which the stimulus was presented, during which no data were collected. Contractile and electrophysiological responses were observed on each presentation of stimulus.
Supplementary Video 14
Hydra expressing GCaMP7b in epitheliomuscular cells in the absence of MM or light stimulation. The trace shown at the bottom of the video corresponds to the intensity of GCaMP7b fluorescence in the whole Hydra across the timescale of the video.
Source data
Source Data Fig. 1
Statistical source data.
Source Data Fig. 2
Statistical source data.
Source Data Fig. 3
Statistical source data.
Source Data Fig. 4
Statistical source data.
Source Data Fig. 5
Statistical source data.
Rights and permissions
Springer Nature or its licensor (e.g. a society or other partner) holds exclusive rights to this article under a publishing agreement with the author(s) or other rightsholder(s); author self-archiving of the accepted manuscript version of this article is solely governed by the terms of such publishing agreement and applicable law.
About this article
Cite this article
Beckham, J.L., van Venrooy, A.R., Kim, S. et al. Molecular machines stimulate intercellular calcium waves and cause muscle contraction. Nat. Nanotechnol. 18, 1051–1059 (2023). https://doi.org/10.1038/s41565-023-01436-w
Received:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1038/s41565-023-01436-w
This article is cited by
-
Photolipid excitation triggers depolarizing optocapacitive currents and action potentials
Nature Communications (2024)