In vitro gliding assay of microtubules (MTs) on kinesins has provided us with valuable biophysical and chemo-mechanical insights of this biomolecular motor system. Visualization of MTs in an in vitro gliding assay has been mainly dependent on optical microscopes, limited resolution of which often render them insufficient sources of desired information. In this work, using high speed atomic force microscopy (HS-AFM), which allows imaging with higher resolution, we monitored MTs and protofilaments (PFs) of tubulins while gliding on kinesins. Moreover, under the HS-AFM, we also observed splitting of gliding MTs into single PFs at their leading ends. The split single PFs interacted with kinesins and exhibited translational motion, but with a slower velocity than the MTs. Our investigation at the molecular level, using the HS-AFM, would provide new insights to the mechanics of MTs in dynamic systems and their interaction with motor proteins.
Microtubule (MT)-kinesin, a cytoskeletal component, plays crucial roles in cell through its various spatial and mechanical functions1,2,3,4,5,6. This biomolecular motor system actively participate in cell contractility4, development and maintenance of cell polarity7 and also in a number of intracellular events such as intracellular transport, regulation of cell morphology and cell mechanics8, 9. In vitro gliding assay, where kinesins are adhered to a substrate and MTs are propelled by the kinesins through consumption of adenosine triphosphate (ATP)5, has been a useful means in unveiling physiological and chemo-mechanical characteristics of this biomolecular motor system10,11,12. Based on the in vitro gliding assay nowadays the MT-kinesin system is finding applications for nanotransport, detection, sensing, imaging, etc.13, 14. In those works, observation of MTs in the in vitro gliding assay has been mainly dependent on the employment of optical microscopes, limited resolution of which often hinders detail exploration and fails to provide adequate information from the gliding assay. In this work, we performed in vitro gliding assay of MTs on lipid bilayer and monitored the gliding MTs and PFs of tubulins under a high speed atomic force microscope (HS-AFM). Moreover, utilizing the advantage of the HS-AFM in monitoring a specimen at the molecular level15,16,17, we for the first time directly observed splitting of gliding MTs into single PFs. Upon splitting, the motile MTs were found to abruptly change their direction of movement. The split single PFs also interacted with kinesins and exhibited translational motion like the intact MTs, but with relatively lower velocity. Recently structural disintegration of MTs in the in vitro gliding assay has started to draw attention where, based on the investigations under fluorescence microscopy, wear or breakage of MTs into smaller parts18 or protofilament bundles (PFBs)19 were reported. Using the HS-AFM our direct observation at the molecular level provides new insights to the structural degradation of MTs in an in vitro gliding assay. This work would contribute to our current understanding of the mechanics of MTs in dynamic systems, and at the same time would help promote sustainable applications of biomolecular motor systems in synthetic world20,21,22.
Results and Discussion
Observation of gliding MTs and tubulin PFs on a kinesin coated substrate
We monitored gliding MTs and PFs of tubulins under HS-AFM by demonstrating an in vitro gliding assay of MTs on kinesins fixed to a streptavidin coated lipid bilayer on mica (Fig. 1a). The mica-supported biotinylated lipid bilayer was prepared as described in a previous report23. In brief, first unilamellar vesicles were prepared from 1,2-Dihexadecanoyl-sn-glycero-3-phosphocholine (DPPC), 1,2-Dipalmitoyl-3-trimethylammonium-propane (DPTAP) and 1,2-dipalmitoyl-sn-glycero-3- phosphoethanolamine-N-(cap biotinyl) (biotin-cap DPPE) (see the experimental section for detail). The vesicles were deposited to freshly cleaved mica disks followed by the addition of streptavidin to the lipid bilayer surface. It was observed that upon application of the streptavidin solution, the streptavidin molecules started to form small crystal islands on the biotinylated lipid bilayer (Fig. S1). After decorating the lipid bilayer with streptavidin, biotinylated kinesin solution was added onto the surface. Subsequently, taxol-stabilized MTs were applied and next by adding ATP, the motility of MTs on the kinesin coated substrate was initiated. We monitored the motility of the MTs by HS-AFM, which allowed real time imaging of the motile MTs with a high resolution. As mentioned above, the surface was divided into small islands after addition of streptavidin creating an inhomogeneous surface. As the distance between two islands was much smaller than the length of MTs, we continued the observation of motility of MTs on such surface. The motility of MTs over kinesin coated lipid bilayer substrate can be observed from the images showing their displacement with time (Fig. 1b). While monitoring the gliding MTs under HS-AFM, we also observed smaller and thinner filaments, as shown in Fig. 1c (n~30), with length of 80 ± 30 nm (mean ± S.D.) (Fig. S2) and height (~2.3 nm) (Fig. 1d), gliding around the MTs (Movie S1). From the height profile the smaller and thinner filaments appear to be protofilaments (PFs) of tubulins. The PFs might have been produced during MT polymerization but did not participate in the formation of MTs24. While the MTs were moving with a velocity of ~100 nm s−1 (n = 8), the PFs were moving with slower velocity (~40 nm s−1) (n = 18) (Fig. 2). This difference in velocity is in agreement to a previous report where a difference in velocity between MTs and protofilament bundles (PFBs) was observed under fluorescence microscope19. Such difference in velocity of MTs and PFs might be related to the fluctuation of kinesins on the surface, and consequent difference in the extent of force production by the kinesins at MTs or PFs25.
An important observation in the present experimental system is the relatively slower velocity of MTs on the lipid layer, compared to that observed in a conventional gliding assay on glass. To investigate the origin of the low velocity of MTs, we performed gliding assay of MTs by changing the substrate and monitored the MTs under HS-AFM. We demonstrated an in vitro gliding assay on collodion (nitrocellulose) coated mica substrate which is a hydrophobic surface26 (see experimental section). The velocity of MTs was found ~590 nm s−1 on the collodion coated mica substrate, which is very close to the velocity of MTs on glass observed in a conventional gliding assay under fluorescence microscope27. This result suggests that the slow movement of MTs on lipid bilayer coated mica substrate might be related to the nature of substrate which can affect the specific binding of motor protein on the surface. This was further confirmed when an in vitro gliding assay was performed on lipid coated mica substrate prepared from a lipid and composition other than used above. Here we prepared lipid layer on mica using vesicles prepared from 1,2-dioleoyl-sn-glycero-3-phosphocholine (DOPC), 1,2-dioleoyl-sn-glycero-3-phospho-L-serine (DOPS) and 1,2-dioleoyl-sn-glycero-3-phosphoethanolamine-N-(cap biotinyl) (biotin-cap DOPE)28 (see the experimental section for detail). On this lipid layer the velocity of MTs was ~150 nm s−1 (n = 50), which is slightly higher than that observed for the DPPC/DPTAP/biotin-cap DPPE system. Collectively these results confirm the effect of substrate on the velocity of MTs, suggesting the mechanical process of scanning during observation under HS-AFM not to be the main factor behind the slow velocity of MTs. It should be noted that, while preparing lipid layer using DOPC/DOPS/biotin-cap DOPE lipid system at the prescribed composition (see experimental section), we observed noticeable difference in the topography of streptavidin crystals compared to that for DPPC/DPTAP/biotin-cap DPPE system. While there was an incomplete and fractionate appearance of the streptavidin crystals for the DPPC/DPTAP/biotin-cap DPPE system (Fig. S1), we obtained a much uniform layer of streptavidin crystals (Fig. S3a, S3b) for the DOPC/DOPS/biotin-cap DOPE system. On such a uniform crystal layer of streptavidin, we were able to observe the anchored single kinesins using the HS-AFM (Fig. S4a) with a density ~1200 µm−2 (Fig. S4b, Movie S2). The density of kinesins on the lipid layer is found much lower than that on a glass surface29. On this lipid layer we observed MTs, confirmed from their height profile (23 ± 1 nm) (Fig. S5), which also exhibited motility (Movie S3). Despite the formation of homogeneous streptavidin crystal layer on the DPPC/DPTAP/biotin-cap DPPE system, the velocity of MTs remained quite slow (~150 nm s−1, n = 50), which could be attributed to the low density of kinesin on the streptavidin/lipid surface. Similar to the DPPC/DPTAP/biotin-cap DPPE system difference in velocity between PFs (~60 nm s−1, n = 20) and MTs was also observed for the DOPC/DOPS/biotin-cap DOPE system. The path length of PFs was found to be much smaller than MTs and they showed pausing events during their motility (Fig. S6).
Generally, taxol-stabilized PFs are known to form curled structures as reported in a previous AFM study24. In fact, bundles of PFs form ring shaped structure when detaching from the MTs19. However, in our experiment, we didn’t observe such curled shape of single PFs during gliding on the surface. Usually, when a PF starts to be bent, kinesin binding surface of the PF goes inside the PF ring and inner part of the MT is exposed to the outside ring. But here if the kinesin binding side of PF is fixed on a flat kinesin coated surface, PF cannot be bent to form ring anymore and should keep straight structure (Fig. S7). On the other hand, if PFs form bundle, it may produce more force to bend PFs. Therefore, single PFs are found to exhibit translational motion, unlike the PFBs which exhibit circular motion on the kinesin coated surface19. To confirm further, we imaged MTs and PFs of tubulins fixed to mica substrate through electrostatic interaction (Fig. 3a–g). A magnified HS-AFM image shows helical lattice of MT filaments with a helix angle ~1 degree where the number of observed PFs was 16 (Fig. 3b). Short and thin filaments with length of 50 ± 20 nm (n~60, Fig. S2) and circular, curled and straight conformation were also observed (Fig. 3c). From the topographic image and height profile, the height of a MT filament was obtained as ~25 nm (Fig. 3d, e). On the other hand, for the thinner filaments the height was ~4 nm (Fig. 3f, g), and these findings agree well with the literature24. Based on this discussion, we can confer that the gliding thinner filaments observed under HS-AFM in the in vitro gliding assay are PFs of tubulins.
Observation of splitting of gliding MTs into single PFs
Motility of MTs on a kinesin coated substrate has been reported to be associated with molecular wear, breakage or splitting of MTs into PFBs18, 19. The broken and split MTs exhibited translational and circular motion respectively on the kinesin coated substrate18, 19. Here taking the advantage of high resolution imaging of gliding MTs by HS-AFM, we directly observe the splitting of gliding MTs into single PFs on lipid coated mica substrate (Movie S4, S5). While monitoring the motile MTs by HS-AFM, we observed that the MTs suddenly changed their moving direction after a short pause. Such abrupt change in direction of motion of the MTs was also observed under fluorescence microscope, although the reason has remained obscure. Our high resolution imaging by HS-AFM revealed that after pausing, a gliding MT was split into two fragments (Fig. 4a). This result suggests that, the sudden change in direction of motile MTs is related to such splitting of the MTs. Probably, the leading end of a MT has tapered-part30 (Fig. S8) and when PFs at the tapered leading end of MT collides with dead kinesins or some obstacles, the PFs might be bent, and being pushed by the lagging part of the MT. Finally, the tapered PFs are broken and separated from the leading end of MTs. Consequently, MTs might change their moving direction due to the buckling force from the PF (Fig. 4b). Additionally, taking into account the difference in the velocity between PFs and MTs, PFs tapered at the leading end of a MT might also cause bending of tapered-PFs due to the mismatch of the velocity and subsequently causing directional change of MTs. Thus, from our observation under HS-AFM, we revealed that splitting of PFs from the leading end of MTs influences the motility of MTs. However, we can see splitting of MTs into PFs on the lipid bilayer surface with some fractionate appearance of streptavidin crystals (DPPC/DPTAP/biotin-cap DPPE) (Fig. 4). We also observed such splitting on the uniform large areas of streptavidin crystals using the other lipid bilayer (DOPC/DOPS/biotin-cap DOPE) surface (Movie S5) which indicates that incomplete or fractionate appearance of streptavidin crystals might have no considerable effect on the splitting of gliding MTs into PFs. The PF split from the motile MTs showed translational motion, which is in contrary to the circular motion exhibited by PFBs19.
In conclusion, exploiting the advantage of high resolution imaging by HS-AFM at molecular scale, we have successfully observed gliding motion of MTs and single PFs in an in vitro gliding assay. Moreover, splitting of the gliding MTs into single PFs has also been observed directly for the first time, which can account for the sudden directional change of the gliding MTs in the gliding assay. Our investigation thus provides an answer to the long standing mystery of sudden directional change of gliding MTs in an in vitro gliding assay, which has been observed under epi-fluorescence microscopy. From the detail investigation of motile MTs at the molecular level using HS-AFM, detail of the relationship between structure of MTs and their motility behavior would be understandable. High resolution imaging by HS-AFM might be advantageous in the study of MT dynamics or interaction between motor proteins and MTs with defects in their lattice31,32,33,34 and impact of structural change of MTs by MAPs35, motor proteins36, 37 or post translational modification38 on their functionality in a dynamic system.
Materials and Methods
Purification of tubulin and kinesin
Tubulin was purified from porcine brain using a high-concentration PIPES buffer (1 M PIPES, 20 mM EGTA, and 10 mM MgCl2; pH adjusted to 6.8 using KOH). The high-concentration PIPES buffer and Brinkley Buffer 80 (BRB80) (80 mM PIPES, 1 mM EGTA, 1 mM MgCl2, pH 6.8) were prepared using PIPES from Sigma, and the pH was adjusted using KOH39. Kinesin construct consisting of human kinesin (residues 1-465), with an N-terminal histidine tag, and a C-terminal avi-tag were prepared as described in previously published reports by partially modifying the expression and purification methods40, 41.
Preparation of MTs
For preparation of MTs, 56 µM tubulin was incubated at 37 °C for 30 min using polymerization buffer including guanosine-5′-triphosphate (GTP) (80 mM PIPES, 1 mM EGTA, 1 mM MgCl2, 1 mM GTP, pH ~6.8). Tubulin and polymerization buffer were mixed at a 4:1 volume ratio. Finally polymerized MTs were stabilized with taxol buffer (80 mM PIPES, 1 mM EGTA, 1 mM MgCl2, 10 µM Paclitaxel, 5% DMSO).
Observation of MTs and PFs on mica surface
1 µM MT was directly deposited on the mica surface and washed with 40 µL taxol buffer including 3 µM paclitaxel to avoid the crystals of taxol during observation and observed by HS-AFM.
Preparation of streptavidin coated lipid bilayer surface
Lipid system 1: Biotinylated mica-supported lipid bilayers were prepared as described in a previous report23. Briefly, solution of 1,2-Dihexadecanoyl-sn-glycero-3-phosphocholine (DPPC) in chloroform, 1,2-Dipalmitoyl-3-trimethylammonium-propane (DPTAP) and 1,2-dipalmitoyl-sn-glycero-3- phosphoethanolamine-N-(cap biotinyl) (biotin-cap DPPE) (Avanti Polar Lipids) were mixed at a weight ratio of 0.85:0.05:0.10. The chloroform was then evaporated under a stream of nitrogen gas, and the lipids were redissolved in MilliQ H2O at a concentration of 1 mg mL−1. Solubilized lipid was diluted to ~0.05 mg mL−1 by MilliQ H2O and sonicated to obtain small unilamellar vesicles. A drop of the vesicle solution (3 μL) was deposited on freshly cleaved mica disks. After ~3 h of incubation in a sealed container, in which a Kimwipe wetted with MilliQ H2O was placed, the surface was rinsed with crystallization buffer 1 (20 mM Tris-HCl, 1 mM EDTA, 10 mM MgCl2, pH~7.6). Then, a drop (3 μL) of streptavidin in crystallization buffer 1 (1 μg mL−1) was deposited on the bilayer surface. After 30 min of incubation, the surface was rinsed again with crystallization buffer 1 to remove the excess streptavidin.
Lipid system 2: For the DOPC/DOPS/biotin-cap DOPE system, solution of 1,2-dioleoyl-sn-glycero-3-phosphocholine (DOPC) in chloroform, 1,2-dioleoyl-sn-glycero-3-phospho-L-serine (DOPS) and 1,2-dioleoyl-sn-glycero-3-phosphoethanolamine-N-(cap biotinyl) (biotin-cap DOPE) (Avanti Polar Lipids) were mixed at a weight ratio of 7:2:1. The chloroform was then evaporated under a stream of nitrogen gas, and the lipids were redissolved in MilliQ H2O at a concentration of 1 mg mL−1. Solubilized lipid was diluted to ~0.05 mg mL−1 by MilliQ H2O and sonicated to obtain small unilamellar vesicles. A drop of the vesicle solution (3 μL) was deposited on freshly cleaved mica disks. After ~3 h of incubation in a sealed container, in which a Kimwipe wetted with MilliQ H2O was placed, the surface was rinsed with crystallization buffer 2 (10 mM HEPES-NaOH, 150 mM NaCl, 2 mM CaCl2, pH 7.4). Then, a drop (3 μL) of streptavidin in crystallization buffer 2 (1 mg mL−1) was deposited on the bilayer surface. After 3 h of incubation, the surface was rinsed again with crystallization buffer 2 to remove the excess streptavidin. For the chemical fixation of the streptavidin crystals, a 10 mM glutaraldehyde-containing crystallization solution 2 was applied and incubated for 5 min. The reaction was quenched using 20 mM Tris buffer mixed in the crystallization buffer 2.
Preparation of motility assay of MTs on lipid bilayer coated mica substrate
A drop (2 μL) of biotinylated kinesin (6 μM and 200 nM for Lipid system 1 and 2 respectively) in BRB80 with 1 mM DTT (80 mM PIPES, 1 mM EGTA, 1 mM MgCl2, 1 mM DTT, pH 6.8) was deposited on the 2D streptavidin crystal surface. After 2~3 min incubation the surface was rinsed with 20 μL BRB80 to remove excess kinesin and then a drop of 1 μM MT solution in BRB80 with 3 μM paclitaxel (80 mM PIPES, 1 mM EGTA, 1 mM MgCl2, 1 mM DTT, 3 μM paclitaxel/DMSO; pH 6.8) was deposited on the surface. After 3 min of incubation, the surface was rinsed with 20 μL taxol buffer and imaged by AFM in ~120 μL of the taxol buffer containing 2 mM ATP.
Preparation of motility assay on the nitrocellulose coated glass surface
2% nitrocellulose (NC) in isoamyl acetate (0.5 µL) was deposited on a freshly cleaved mica surface for 15 min to completely dry. Then 200 nM kinesin-1 (2 µL) in BRB80 with 1 mM DTT (80 mM PIPES, 1 mM EGTA, 1 mM MgCl2, 1 mM DTT, pH 6.8) was deposited on the surface for 5 min. After that washed by excess amount of BRB80 with DTT (~100 µL) buffer. 1 mg mL−1 casein in BRB80 (2 µL) was deposited on the surface for 3 min. Then rinsed with taxol buffer (BRB80 with 3 µM paclitaxel) (20 µL). 1 µM of MT in taxol buffer was deposited and waited for 5 min. Finally rinsed with taxol buffer ~60 µL and imaged by AFM in ~120 µL of the taxol buffer containing 2 mM ATP.
AFM imaging was performed using a tip scan high-speed AFM imaging system (BIXAM, olympus, Tokyo, Japan) that was improved based on a previously developed machine42 and laboratory-made high-speed AFM imaging system15. Silicon nitride cantilevers (resonant frequency = 0.4–1.0 MHz in water, spring constant = 0.1 Nm−1, electron-beam-deposited tip radius <15 nm; Olympus BLAC10EGS-A2). AFM images were analyzed using the AFM Scanning System Software (Olympus, Tokyo, Japan), laboratory made software, Adobe Photoshop CC and ImageJ43.
Alberts, B. et al. In Molecular Biology of the Cell. (5th Edition) 965–1114 (Garland Science, 2008).
Sharp, D. J., Rogers, D. C. & Scholey, J. M. Microtubule motors in mitosis. Nature 407, 41–47 (2000).
Tay, C. Y. et al. Nanoparticles strengthen intracellular tension and retard cellular migration. Nano Lett. 14, 83–88 (2014).
Bershadsky, A. D., Balaban, N. Q. & Geiger, B. Adhesion-dependent cell mechanosensitivity. Annu. Rev. Cell Dev. Biol. 19, 677–695 (2003).
Howard, J. In Mechanics of motor protein and the cytoskeleton. 111–112 (Sinauer Associates, Inc., Sunderland, Massachusetts, 2001).
Kurachi, M., Hoshi, M. & Tashiro, H. Buckling of a single microtubule by optical trapping forces: direct measurement of microtubule rigidity. Cell Motil. Cytoskeleton 30, 221–228 (1995).
Zhang, J., Guo, W. H. & Wang, Y. L. Microtubules stabilize cell polarity by localizing rear signals. PNAS 18, 16383–6388 (2014).
Stamenovic, D., Mijailovich, S. M., Tolic-Norrelykke, I. M., Chen, J. & Wang, N. Cell prestress II. Contribution of microtubules. Am J Physiol Cell Physiol 282, C617–C624 (2002).
Wang, N., Butler, J. P. & Ingber, D. E. Mechanotransduction across the cell surface and through the cytoskeleton. Science 260, 1124–1127 (1993).
Howard, J., Hudspeth, A. J. & Vale, R. D. Movement of microtubules by single kinesin molecules. Nature 342, 154–158 (1989).
Hunt, A. J. & Howard, J. Kinesin swivels to permit microtubule movement in any direction. PNAS 90, 11653–11657 (1993).
Jiang, M. Y. & Sheetz, M. P. Cargo activated ATPase activity of kinesin. Biophys. J. 68, 283–285 (1995).
Diez, S. & Howard, J. Nanotechnological applications of biomolecular motor systems. Physics in Canada 65, 7–12 (2009).
Hess, H. & Vogel, V. Molecular shuttles based on motor proteins: active transport in synthetic environments. Rev. Mol. Biotechnol. 82, 67–85 (2001).
Ando, T. et al. A high-speed atomic force microscope for studying biological macromolecules. PNAS 98, 12468–12472 (2001).
Ando, T. et al. A high-speed atomic force microscope for studying biological macromolecules in action. Chemphyschem 4, 1196–1202 (2003).
Ando, T. et al. High-speed atomic force microscopy for studying the dynamic behavior of protein molecules at work. Japanese journal of applied physics 45, 1897–1903 (2006).
Dumont Emmanuel, L. P., Do, C. & Hess, H. Molecular wear of microtubules propelled by surface-adhered kinesins. Nat. Nanotechnol. 10, 166–169 (2015).
Delinder, V. V., Adams, P. G. & Bachand, G. D. Mechanical splitting of microtubules into protofilament bundles by surface-bound kinesin-1. Sci. Rep. 6, 39408 (2016).
Soong, R. K. et al. Powering an inorganic nanodevice with a biomolecular motor. Science 290, 1555–1558 (2000).
Knoblauch, M. & Peters, W. S. Biomimetic actuators: where technology and cell biology merge. Cell. Mol. Life Sci. 61, 2497–2509 (2004).
Inoue, D. et al. Sensing surface mechanical deformation using active probes driven by motor proteins. Nat. Commun. 7, 12557 (2016).
Kodera, N., Yamamoto, D., Ishikawa, R. & Ando, T. Video imaging of walking myosin V by high-speed atomic force microscopy. Nature 468, 72–76 (2010).
Caille, C. E. et al. Straight GDP-tubulin protofilaments form in the presence of taxol. Current Biology 17, 1765–1770 (2007).
Grover, R. et al. Transport efficiency of membrane-anchored kinesin-1 motors depends on motor density and diffusivity. PNAS 113, E7185–E7193 (2016).
Nicolau, D. V. et al. Surface hydrophobicity modulates the operation of actomyosin-based dynamic nanodevices. Langmuir 23, 10846–10854 (2007).
Kabir, A. M. R., Inoue, D., Kakugo, A., Kamei, A. & Gong, J. P. Prolongation of the active lifetime of a biomolecular motor for in vitro motility assay by using an inert atmosphere. Langmuir 27, 13659–13668 (2011).
Yamamoto, D., Nagura, N., Omote, S., Taniguchi, M. & Ando, T. Streptavidin 2D crystal substrates for visualizing biomolecular processes by atomic force microscopy. Biophys. J. 97, 2358–2367 (2009).
Dumont Emmanuel, L. P., Belmas, H. & Hess, H. Observing the mushroom-to-brush transition for kinesin proteins. Langmuir 29, 15142–15145 (2013).
Kacher, C. M. et al. Imaging microtubules and kinesin decorated microtubules using tapping mode atomic force microscopy in fluids. EurBiophys J. 28, 611–620 (2000).
Aumeier, C. et al. Self-repair promotes microtubule rescue. Nat. Cell Biol. 18, 1054–1064 (2016).
Schaedel, L. et al. Microtubules self-repair in response to mechanical stress. Nat. Mater. 14, 1156–1163 (2015).
de Forges, H. et al. Localized mechanical stress promotes microtubule rescue. Current Biology 26, 3399–3406 (2016).
Liang, W. H. et al. Microtubule defects influence kinesin-based transport in vitro. Biophys. J. 110, 2229–2240 (2016).
Portran, D. et al. MAP65/Ase1 promote microtubule flexibility. MBoC 24, 1964–1973 (2013).
Krebs, A., Goldie, K. N. & Hoenger, A. Complex formation with kinesin motor domains affects the structure of microtubules. J. Mol. Biol. 335, 139–153 (2004).
Kabir, A. M. R. et al. Buckling of microtubules on a 2D elastic medium. Sci. Rep. 5, 17222 (2015).
Robinson, P. et al. Detyrosinated microtubules buckle and bear load in contracting cardiomyocytes. Science 352, aaf0659 (2016).
Castoldi, M. & Popov, A. V. Purification of brain tubulin through two cycles of polymerization-depolymerization in a high-molarity buffer. Protein Expression Purif. 32, 83–88 (2003).
Fujimoto, K. et al. Colocalization of quantum dots by reactive molecules carried by motor proteins on polarized microtubule arrays. ACS Nano 7, 447–455 (2013).
Yokokawa, R., Tarhan, M. C., Kon, T. & Fujita, H. Simultaneous and bidirectional transport of kinesin-coated microspheres and dynein-coated microspheres on polarity-oriented microtubules. Biotechnology and Bioengineering 101, 1–8 (2008).
Suzuki, Y. et al. High-speed atomic force microscopy combined with inverted optical microscopy for studying cellular events. Sci. Rep. 3, 2131 (2013).
“ Ferreira, T. & Rasband, W. ImageJ user guide IJ 1.46r (2012) (17/2/2017)” https://imagej.nih.gov/ij/docs/guide/index.html.
This work was financially supported by Grant-in-Aid for Scientific Research on Innovative Areas “Molecular Robotics” (JSPS KAKENHI Grant Number JP24104004) from Japan Society for the Promotion of Science (JSPS) and New Energy and Industrial Technology Development Organization (NEDO), Japan (PJ22160019).
The authors declare that they have no competing interests.
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Keya, J.J., Inoue, D., Suzuki, Y. et al. High-Resolution Imaging of a Single Gliding Protofilament of Tubulins by HS-AFM. Sci Rep 7, 6166 (2017). https://doi.org/10.1038/s41598-017-06249-1
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