Abstract
The dynamic architecture of the microtubule cytoskeleton is crucial for cell division, motility and morphogenesis. The dynamic properties of microtubules—growth, shrinkage, nucleation, and severing—are regulated by an arsenal of microtubule-associated proteins (MAPs). The activities of many of these MAPs have been reconstituted in vitro using microscope assays. As an alternative to fluorescence microscopy, interference-reflection microscopy (IRM) has been introduced as an easy-to-use, wide-field imaging technique that allows label-free visualization of microtubules with high contrast and speed. IRM circumvents several problems associated with fluorescence microscopy including the high concentrations of tubulin required for fluorescent labeling, the potential perturbation of function caused by the fluorophores, and the risks of photodamage. IRM can be implemented on a standard epifluorescence microscope at low cost and can be combined with fluorescence techniques like total-internal-reflection-fluorescence (TIRF) microscopy. Here we describe the experimental procedure to image microtubule dynamics and severing using IRM , providing practical tips and guidelines to resolve possible experimental hurdles.
Access this chapter
Tax calculation will be finalised at checkout
Purchases are for personal use only
References
Howard J, Hyman AA (2003) Dynamics and mechanics of the microtubule plus end. Nature 422:753–758. https://doi.org/10.1038/nature01600
Akhmanova A, Steinmetz MO (2015) Control of microtubule organization and dynamics: two ends in the limelight. Nat Rev Mol Cell Biol 16:711–726. https://doi.org/10.1038/nrm4084
Kuo Y-W, Howard J (2020) Cutting, amplifying, and aligning microtubules with severing enzymes. Trends Cell Biol 31:50–61. https://doi.org/10.1016/j.tcb.2020.10.004
Roostalu J, Surrey T (2017) Microtubule nucleation: beyond the template. Nat Rev Mol Cell Biol 18:702–710. https://doi.org/10.1038/nrm.2017.75
Brouhard GJ, Rice LM (2018) Microtubule dynamics: an interplay of biochemistry and mechanics. Nat Rev Mol Cell Biol 19:451–463. https://doi.org/10.1038/s41580-018-0009-y
Goodson HV, Jonasson EM (2018) Microtubules and microtubule-associated proteins. Cold Spring Harbor Perspect Biol 10:a022608. https://doi.org/10.1101/cshperspect.a022608
Brouhard GJ, Stear JH, Noetzel TL et al (2008) XMAP215 is a processive microtubule polymerase. Cell 132:79–88. https://doi.org/10.1016/j.cell.2007.11.043
Helenius J, Brouhard G, Kalaidzidis Y et al (2006) The depolymerizing kinesin MCAK uses lattice diffusion to rapidly target microtubule ends. Nature 441:115–119. https://doi.org/10.1038/nature04736
Varga V, Helenius J, Tanaka K et al (2006) Yeast kinesin-8 depolymerizes microtubules in a length-dependent manner. Nat Cell Biol 8:957–962. https://doi.org/10.1038/ncb1462
Gardner MK, Zanic M, Gell C et al (2011) Depolymerizing kinesins Kip3 and MCAK shape cellular microtubule architecture by differential control of catastrophe. Cell 147:1092–1103. https://doi.org/10.1016/j.cell.2011.10.037
Bieling P, Laan L, Schek H et al (2007) Reconstitution of a microtubule plus-end tracking system in vitro. Nature 450:1100–1105. https://doi.org/10.1038/nature06386
Vale RD, Funatsu T, Pierce DW et al (1996) Direct observation of single kinesin molecules moving along microtubules. Nature 380:451–453. https://doi.org/10.1038/380451a0
Fink G, Hajdo L, Skowronek KJ et al (2009) The mitotic kinesin-14 Ncd drives directional microtubule–microtubule sliding. Nat Cell Biol 11:717–723. https://doi.org/10.1038/ncb1877
Dixit R, Ross JL, Goldman YE, Holzbaur ELF (2008) Differential regulation of dynein and kinesin motor proteins by Tau. Science 319:1086–1089. https://doi.org/10.1126/science.1152993
Korten T, Nitzsche B, Gell C et al (2011) Single molecule analysis, methods and protocols. Meth Mol Biol 783:121–137. https://doi.org/10.1007/978-1-61779-282-3_7
Saper G, Hess H (2020) Kinesin-propelled label-free microtubules imaged with interference reflection microscopy. New J Phys 22:095002. https://doi.org/10.1088/1367-2630/abb47b
Howard J, Hyman AA (1993) Chapter 7 preparation of marked microtubules for the assay of the polarity of microtubule-based motors by fluorescence microscopy. Meth Cell Biol 39:105–113. https://doi.org/10.1016/s0091-679x(08)60164-8
Vigers GP, Coue M, McIntosh JR (1988) Fluorescent microtubules break up under illumination. J Cell Biol 107:1011–1024. https://doi.org/10.1083/jcb.107.3.1011
Aumeier C, Schaedel L, Gaillard J et al (2016) Self-repair promotes microtubule rescue. Nat Cell Biol 18:1054–1064. https://doi.org/10.1038/ncb3406
Ti S-C, Pamula MC, Howes SC et al (2016) Mutations in human tubulin proximal to the kinesin-binding site alter dynamic instability at microtubule plus- and minus-ends. Dev Cell 37:72–84. https://doi.org/10.1016/j.devcel.2016.03.003
Johnson V, Ayaz P, Huddleston P, Rice LM (2011) Design, overexpression, and purification of polymerization-blocked yeast αβ-tubulin mutants. Biochemistry 50:8636–8644. https://doi.org/10.1021/bi2005174
Orbach R, Howard J (2019) The dynamic and structural properties of axonemal tubulins support the high length stability of cilia. Nat Commun 10:1838. https://doi.org/10.1038/s41467-019-09779-6
Ayukawa R, Iwata S, Imai H et al (2020) GTP-dependent formation of straight oligomers leads to nucleation of microtubules. Biorxiv. 2020.03.05.979989. https://doi.org/10.1101/2020.03.05.979989
Sackett DL, Werbovetz KA, Morrissette NS (2010) Isolating tubulin from nonneural sources. Meth Cell Biol 95:17–32. https://doi.org/10.1016/s0091-679x(10)95002-4
Widlund PO, Podolski M, Reber S et al (2012) One-step purification of assembly-competent tubulin from diverse eukaryotic sources. Mol Biol Cell 23:4393–4401. https://doi.org/10.1091/mbc.e12-06-0444
Hotta T, Fujita S, Uchimura S et al (2016) Affinity purification and characterization of functional tubulin from cell suspension cultures of arabidopsis and tobacco. Plant Physiol 170:1189–1205. https://doi.org/10.1104/pp.15.01173
Vemu A, Atherton J, Spector JO et al (2016) Structure and dynamics of single-isoform recombinant neuronal human tubulin. J Biol Chem 291:12907–12915. https://doi.org/10.1074/jbc.c116.731133
Souphron J, Bodakuntla S, Jijumon AS et al (2019) Purification of tubulin with controlled post-translational modifications by polymerization–depolymerization cycles. Nat Protoc 14:1634–1660. https://doi.org/10.1038/s41596-019-0153-7
Hirst WG, Biswas A, Mahalingan KK, Reber S (2020) Differences in Intrinsic tubulin dynamic properties contribute to spindle length control in xenopus species. Curr Biol 30:2184–2190.e5. https://doi.org/10.1016/j.cub.2020.03.067
Hotani H, Horio T (1988) Dynamics of microtubules visualized by darkfield microscopy: treadmilling and dynamic instability. Cell Motil Cytoskel 10:229–236. https://doi.org/10.1002/cm.970100127
Walker RA, O’Brien ET, Pryer NK et al (1988) Dynamic instability of individual microtubules analyzed by video light microscopy: rate constants and transition frequencies. J Cell Biol 107:1437–1448. https://doi.org/10.1083/jcb.107.4.1437
Bormuth V, Howard J, Schäffer E (2007) LED illumination for video-enhanced DIC imaging of single microtubules. J Microsc 226:1–5. https://doi.org/10.1111/j.1365-2818.2007.01756.x
Mahamdeh M, Simmert S, Luchniak A et al (2018) Label-free high-speed wide-field imaging of single microtubules using interference reflection microscopy. J Microsc 1991:95. https://doi.org/10.1111/jmi.12744
Simmert S, Abdosamadi MK, Hermsdorf G, Schäffer E (2018) LED-based interference-reflection microscopy combined with optical tweezers for quantitative three-dimensional microtubule imaging. Opt Express 26:14499. https://doi.org/10.1364/oe.26.014499
Mahamdeh M, Howard J (2019) Implementation of interference reflection microscopy for label-free, high-speed imaging of microtubules. J Vis Exp:e59520. https://doi.org/10.3791/59520
Kuo Y-W, Trottier O, Mahamdeh M, Howard J (2019) Spastin is a dual-function enzyme that severs microtubules and promotes their regrowth to increase the number and mass of microtubules. Proc Natl Acad Sci U S A 116:5533–5541. https://doi.org/10.1073/pnas.1818824116
Zhernov I, Diez S, Braun M, Lansky Z (2020) Intrinsically disordered domain of kinesin-3 Kif14 enables unique functional diversity. Curr Biol 30:3342–3351.e5. https://doi.org/10.1016/j.cub.2020.06.039
Gell C, Bormuth V, Brouhard GJ et al (2010) Microtubule dynamics reconstituted in vitro and imaged by single-molecule fluorescence microscopy. Meth Cell Biol 95:221–245. https://doi.org/10.1016/s0091-679x(10)95013-9
Caplow M, Ruhlen RL, Shanks J (1994) The free energy for hydrolysis of a microtubule-bound nucleotide triphosphate is near zero: all of the free energy for hydrolysis is stored in the microtubule lattice [published erratum appears in J Cell Biol 1995 Apr;129(2):549]. J Cell Biol 127:779–788. https://doi.org/10.1083/jcb.127.3.779
Hyman A, Drechsel D, Kellogg D et al (1991) Preparation of modified tubulins. Meth Enzymol 196:478–485
Kuo Y, Trottier O, Howard J (2019) Predicted effects of severing enzymes on the length distribution and total mass of microtubules. Biophys J 117:2066–2078. https://doi.org/10.1016/j.bpj.2019.10.027
Zanic M (2016) The mitotic spindle, methods and protocols. Met Mol Biol 1413:47–61. https://doi.org/10.1007/978-1-4939-3542-0_4
Ziółkowska NE, Roll-Mecak A (2013) In vitro microtubule severing assays. Met Mol Biol 1046:323–334. https://doi.org/10.1007/978-1-62703-538-5_19
Davis LJ, Odde DJ, Block SM, Gross SP (2002) The importance of lattice defects in katanin-mediated microtubule severing in vitro. Biophys J 82:2916–2927. https://doi.org/10.1016/s0006-3495(02)75632-4
Eckert T, Link S, Le DT-V et al (2012) Subunit interactions and cooperativity in the microtubule-severing AAA ATPase spastin. J Biol Chem 287:26278–26290. https://doi.org/10.1074/jbc.m111.291898
Bailey ME, Sackett DL, Ross JL (2015) Katanin severing and binding microtubules are inhibited by tubulin carboxy tails. Biophys J 109:2546–2561. https://doi.org/10.1016/j.bpj.2015.11.011
Wieczorek M, Chaaban S, Brouhard GJ (2013) Macromolecular crowding pushes catalyzed microtubule growth to near the theoretical limit. Cell Mol Bioeng 6:383–392. https://doi.org/10.1007/s12195-013-0292-9
Katsuki M, Muto E, Cross RA (2011) Microtubule dynamics, methods and protocols. Meth Mol Biol 777:117–126. https://doi.org/10.1007/978-1-61779-252-6_9
Acknowledgments
We thank Dr. Mohammed Mahamdeh and Dr. Anna Luchniak for comments and discussions on the manuscript. This work was supported by NIH grants R01 GM139337, DP1 MH110065, and R01 NS118884 (to J.H.) and a fellowship from the Ministry of Education in Taiwan (to Y-W.K.).
Author information
Authors and Affiliations
Corresponding author
Editor information
Editors and Affiliations
Rights and permissions
Copyright information
© 2022 The Author(s), under exclusive license to Springer Science+Business Media, LLC, part of Springer Nature
About this protocol
Cite this protocol
Kuo, YW., Howard, J. (2022). In Vitro Reconstitution of Microtubule Dynamics and Severing Imaged by Label-Free Interference-Reflection Microscopy. In: Inaba, H. (eds) Microtubules. Methods in Molecular Biology, vol 2430. Humana, New York, NY. https://doi.org/10.1007/978-1-0716-1983-4_5
Download citation
DOI: https://doi.org/10.1007/978-1-0716-1983-4_5
Published:
Publisher Name: Humana, New York, NY
Print ISBN: 978-1-0716-1982-7
Online ISBN: 978-1-0716-1983-4
eBook Packages: Springer Protocols