Search tips
Search criteria 


Logo of mbcLink to Publisher's site
Mol Biol Cell. 2008 October; 19(10): 4534–4544.
PMCID: PMC2555953

Two Microtubule-associated Proteins of Arabidopsis MAP65s Promote Antiparallel Microtubule Bundling

David G. Drubin, Monitoring Editor


The Arabidopsis MAP65s are a protein family with similarity to the microtubule-associated proteins PRC1/Ase1p that accumulate in the spindle midzone during late anaphase in mammals and yeast, respectively. Here we investigate the molecular and functional properties of AtMAP65-5 and improve our understanding of AtMAP65-1 properties. We demonstrate that, in vitro, both proteins promote the formation of a planar network of antiparallel microtubules. In vivo, we show that AtMAP65-5 selectively binds the preprophase band and the prophase spindle microtubule during prophase, whereas AtMAP65-1-GFP selectively binds the preprophase band but does not accumulate at the prophase spindle microtubules that coexists within the same cell. At later stages of mitosis, AtMAP65-1 and AtMAP65-5 differentially label the late spindle and phragmoplast. We present evidence for a mode of action for both proteins that involves the binding of monomeric units to microtubules that “zipper up” antiparallel arranged microtubules through the homodimerization of the N-terminal halves when adjacent microtubules encounter.


In higher plant cells, interphase microtubules occur predominantly at the cell cortex as ordered bundles in close association with the plasma membrane. These so-called cortical microtubules (CMTs) play crucial roles in cell morphogenesis (Wasteneys and Fujita, 2006 blue right-pointing triangle). In rapidly elongating cells, CMTs are linear bundles that are usually transversely oriented relative to the longest cell axis. When cell expansion slows down, the transverse organization is lost and CMTs become oblique (Lloyd, 1994 blue right-pointing triangle; Dixit and Cyr, 2004 blue right-pointing triangle). CMTs are highly dynamic and show higher (de)-polymerization rates than interphase mammalian microtubules (Shaw et al., 2003 blue right-pointing triangle; Dixit et al., 2006 blue right-pointing triangle). In contrast to animal and yeast microtubules (MTs), CMTs do not emanate from a well-defined nucleating center. Instead, the MT nucleation activity in interphase plant cells mostly occurs at dispersed sites along pre-existing MTs at the cell's cortex (Murata et al., 2005 blue right-pointing triangle) in a γ-tubulin–dependent manner (Pastuglia et al., 2006 blue right-pointing triangle). This MT-dependent nucleation results in branching patterns of CMTs (Murata et al., 2005 blue right-pointing triangle) that are subsequently resolved into coaligned CMTs. After nucleation, the majority of the MTs are released from their nucleation site, move in the cell cortex by a hybrid treadmilling mechanism leading to polymer interactions (Shaw et al., 2003 blue right-pointing triangle), and are incorporated into bundles (Dixit and Cyr, 2004 blue right-pointing triangle). Significantly, the CMT bundles are not anchored and consequently both MT ends are dynamic. Thus, the ordered patterns of CMT arrays are not correlated with the patterns of the CMT nucleation sites (Dixit et al., 2006 blue right-pointing triangle) and depend on a yet-to-be-discovered mechanism.

To accommodate for the transverse network observed in expanding cells, CMTs form bundles. How these bundles are organized is not clear, and for instance, the polarity of CMTs within bundles is not yet solved. Using an in vitro model that provides good access to the cortex combined with the hook decoration of MTs, Tian et al. (2004) blue right-pointing triangle demonstrated that the MTs in the cortical array are predominantly oriented in a mixed polarity. This organization is in agreement with opposing growth directionalities of green fluorescent protein (GFP)-labeled MTs observed in the cortical array (Chan et al., 2003 blue right-pointing triangle; Shaw et al., 2003 blue right-pointing triangle). In contrast, Dixit et al. (2006) blue right-pointing triangle reported that ~70% of CMTs have the same polarity and that this polar arrangement of CMTs occurs simultaneously with the coalignment of CMTs. This bias toward copolarity might be the net result of sectorial fields of copolymerizing MTs observed in spinning-disk confocal microscopic records (Chan et al., 2007 blue right-pointing triangle).

At the molecular level, putative candidate proteins stimulating the cross-linking of MTs in vitro and in vivo have been identified. They are mainly members of the MT-associated family MAP65s (Smertenko et al., 2004 blue right-pointing triangle; Wicker-Planquart et al., 2004 blue right-pointing triangle; Li et al., 2007a blue right-pointing triangle). MAP65 proteins are evolutionarily conserved, nonmotor microtubule-associated proteins (MAPs) that in animal and yeast cells accumulate in the spindle midzone during late anaphase to stabilize overlapping antiparallel arranged MTs (Verni et al., 2004 blue right-pointing triangle; Zhu et al., 2006 blue right-pointing triangle; Janson et al., 2007 blue right-pointing triangle). In Arabidopsis nine AtMAP65 family members were identified (Hussey et al., 2002 blue right-pointing triangle). These all possess a conserved sequence of 16 amino acids located at the C-terminus and coiled-coil sequences with putative protein–protein interaction activity (Schuyler et al., 2003 blue right-pointing triangle; Verni et al., 2004 blue right-pointing triangle). Overall sequence identity is poorly conserved, suggesting that AtMAP65 proteins have adopted separate properties. AtMAP65-1 is so far the more studied and was shown to colocalize with bundled CMTs and the spindle midzone in anaphase (Van Damme et al., 2004a blue right-pointing triangle; Mao et al., 2005a blue right-pointing triangle; Smertenko et al., 2006 blue right-pointing triangle). In vitro, AtMAP65-1 promotes MT bundling and appears as filamentous cross-bridges regularly spaced along the MT wall (Smertenko et al., 2004 blue right-pointing triangle; Mao et al., 2005b blue right-pointing triangle). Other GFP-tagged AtMAP65 proteins have different localizations. AtMAP65-3 is associated with the mitotic MT array during both early and late mitosis in all Arabidopsis organs (Caillaud et al., 2008 blue right-pointing triangle). AtMAP65-4 associates with the prophase spindle MTs and labels the spindle MTs until anaphase (Van Damme et al., 2004a blue right-pointing triangle). AtMAP65-6 colocalizes with mitochondria (Mao et al., 2005b blue right-pointing triangle). Finally, AtMAP65-5 associates with a subset of transversely organized CMT bundles in interphase as well as the phragmoplast during cytokinesis (Van Damme et al., 2004a blue right-pointing triangle). On the basis of the their diverse localization patterns, we postulate that AtMAP65s exhibit differential molecular and functional properties which still remain to be identified.

In this report we investigated the molecular and functional properties of AtMAP65-5 and further investigated biochemical mechanisms of AtMAP65-1 MT binding and MT bundling. We found that in vivo AtMAP65-1 and AtMAP65-5 differentially associate with MTs during prophase preceding the initiation and formation of a bipolar spindle and at the end of metaphase and during anaphase. In vitro, we demonstrate that AtMAP65-1 and AtMAP65-5 are monomeric in solution and promote the bundling of antiparallel aligned MTs. The presented data are in favor of their binding to MTs as monomers followed by their homodimerization through their N-terminal regions when adjacent MTs encounter.


Recombinant Protein, Expression, and Purification

AtMAP65-1 (At5g55230), AtMAP65-5 (At2g38720), domains of AtMAP65-1 and AtMAP65-5, AtMAP65-1, and AtMAP65-5 deleted of one domain were purified as tagged proteins with either His tag at N- and C-termini, or GFP at the N-terminus and His tag at the C-terminus using homemade vectors. Primers used to amplify cDNAs are given in Supplemental Table S1.

For AtMAP65-1 and AtMAP65-5 three domains were defined: 1) for AtMAP65-1: the domain 1 (aa 1-150), the domain 2 (aa 151-339), and the domain 3 (aa 340-587); for AtMAP65-5: the domain 1 (aa 1-140), the domain 2 (aa 141-328), and the domain 3 (aa 329-550). These domains and AtMAP65-5 or AtMAP65-1 deleted of one domain were further referred to as AtMAP65-5(1), AtMAP65-5(2), AtMAP65-5(3), and AtMAP65-5(13) and as AtM65-5(23), AtMAP65-1(1), AtMAP65-1(2), AtMAP65-1(3), AtMAP65-1(23), and AtMAP65-1(13). All sequences were verified by sequencing.

Recombinant AtMAP65s proteins were purified on Ni Sepharose columns and stored at −80°C in 10% (vol/vol) glycerol, 50 mM NaPi, 0.1 M NaCl, and 0.5 mM DTT, pH 7.9. A detailed protocol is given in Supplemental Data.

Tubulin Polymerization and MT-binding Assays

Purified bovine tubulin (Vantard et al., 1994 blue right-pointing triangle) was assembled in G-BRB80 buffer (BRB buffer: 80 mM Pipes, pH 6.8, 1 mM EGTA, and 1 mM MgCl2 plus 1 mM GTP). Polymerization was monitored at 350 nm at 37 or 4°C. For experiments using preformed MTs, MTs were assembled from 20 μM tubulin in presence of 20 μM of taxotere (Sigma, St. Louis, MO) in G-BRB80 at 37°C for 30 min and further diluted in G-BRB80 supplemented with 10 μM taxotere. MTs were incubated with AtMAP65s at 20°C for 20 min. For cosedimentation assays, reaction mixtures were spun (10 min, 100,000 × g) through a glycerol cushion (30% [vol/vol] glycerol in G-BRB80 plus 10 μM taxotere). Supernatants and pellets were analyzed on western blot probed with anti-AtMAP65-1 or anti-AtMAP65-5 antibodies. For analyses of the relative efficiencies of full-length and constructs of AtMAP65s to bundle MTs, cosedimentation assays were done at low-speed centrifugation (10 min, 4000 × g).

Imaging Assays

Fluorescent MTs assembled from a mixture of 5 μM rhodamine-labeled tubulin (prepared according to Hyman et al., 1991 blue right-pointing triangle) and 10 μM unlabeled tubulin were incubated at 20°C with AtMAP65s and observed according to Stoppin et al. (1996) blue right-pointing triangle.

For AtMAP65s binding on MTs, rhodamine MTs (0.2 μM) were incubated for 5 min with GFP-AtMAP65s (0.5 μM), and a 1-μl sample was observed on fluorescence microscope (Axioplan 2 microscope, 63× NA 1.3 objective; Zeiss, Thornwood, NY) and a Hamamastu CCD Orca camera (Bridgewater, NJ) and Metaview image processing (Molecular Devices, Downingtown, PA).

For negative-stain electron microscopy (EM) observations, MTs (1 μM) were incubated at 20°C for 20 min with AtMAP65s (1 μM). Samples were stained with 2% (wt/vol) uranyl acetate and observed on a CM12 microscope (FEI, The Netherlands, Eindhoven) operating at 120 kV. The polarity of MTs within bundles was determined by cryo-EM as described by Chrétien et al. (1996) blue right-pointing triangle. With this method MTs show fringe patterns produced by the superposition of protofilaments from the front and back of the MT wall in projection. To increase the contrast of fringes observed in vitrified MTs images, we computed filtered images using the J0 and JN terms in the Fourier transform of the images. Arrowhead patterns formed by the dark fringes are then clearly visible on these filtered images.

These differences between the values (inter-MT distance, cross-bridges angles) calculated from negative-stain EM or cryo-EM micrographs are inherent to the two methods of sample preparation for EM and are explained by the fact that with negative staining procedure, we only observe surface information (the footprint of the object in the stain). Furthermore after this procedure, MT bundles may be flattened, whereby errors are introduced that account for an apparent shorter inter-MT distance and a smaller angle. On the other hand, the cryo-EM method preserves much better the native form and the structure of the specimen (Dubochet et al., 1988 blue right-pointing triangle), and images contain information all along the thickness of the vitreous sample, contributing thus to a larger distribution of MT interspace lengths. Via cryo-EM, a projection of a 3D object is obtained, allowing the calculation of internal positional information of the specimen (see Figure 9B). Because the specimen preparation procedure preserves better the original structure, data are more reliable.

Figure 9.
Schematic representation of AtMAP65-5 or AtMAP65-1 binding along the MT protofilaments. (A) Schematic view of MTs cross-linked by either AtMAP65-5 or AtMAP65-1. AtMAP65-5 or AtMAP65-1 dimerize via domains 1 and 2. The proximal region of domain 3 (red) ...

Oligomerization Determination

Analytical ultracentrifugation sedimentation velocity experiments were performed at 20°C and 42,000 rpm in two channel centerpiece cells loaded in a rotor ANTi50 in a Beckman XLI (Fullerton, CA). Samples were obtained from gel filtration eluted with 10% glycerol, 0.1 M NaCl, 0.5 mM DDT, and 50 mM NaPi, pH 8. Scans were recorded overnight at 280 nm. Analysis, done with the program Sedfit (available free at, were performed in terms of continuous distribution, c(s), of sedimentation coefficients, s,(Ebel, 2007 blue right-pointing triangle) and in terms of noninteracting species allowing the independent determination of s and molecular weight (MW; Schuck, 2000 blue right-pointing triangle). Equations for calculation of s20,w and MW are given in Supplemental Data. The disordered regions were determined using the DisEMBL1.5 software (

Polyclonal Antibody Production and Purification

Recombinant purified AtMAP65-1 and AtMAP65-5 were used as antigens to raise antibodies. Antisera were produced at a commercial facility (Charles River Laboratories, Wilmington, MA). IgG was isolated from the antisera by the method described by Vantard et al. (1994) blue right-pointing triangle.

In Vivo Confocal Imaging

AtMAP65-1-GFP, AtMAP65-5-GFP, and red fluorescent protein (RFP)-TUA6 constructs are already described (Van Damme et al., 2004a blue right-pointing triangle). AtMAP65-GFP constructs were supertransformed into a BY-2 suspension culture stably expressing RFP-TUA6 as described (Geelen and Inzé, 2001 blue right-pointing triangle). The BY-2 cells were imaged using a chambered coverglass system (Labtek, Nunc, Naperville, IL) and immobilized in BY-2 medium with added vitamins and 0.8% of low melting point agarose (Invitrogen, Carlsbad, CA). Images were captured on using a 60× water corrected lens with an NA of 1.2 and 3× zoom on an Olympus Fluoview 1000 inverted confocal microscope, with standard enhanced GFP (eGFP) and monomeric RFP (mRFP) settings (15% 488-nm Argon laser power, 15% 559-nm diode laser power; DM405/488/559/635 excitation filter, SDM 560 beam splitter; 500–545-nm emission window for eGFP and 570–670-nm emission window for mRFP) using consecutive line capturing mode and four times Laman line averaging. 3D reconstruction was performed using the 3D software module of the FV1000 software.


AtMAP65-5 Cross-Link MTs in a Fishbone Pattern

When AtMAP65-5 was incubated with rhodamine-labeled MTs, MT bundles were observed (Figure 1b). As already reported, AtMAP65-1 produced similar MT bundles (Figure 1c; Smertenko et al., 2004 blue right-pointing triangle). AtMAP65-5 and AtMAP65-1 were both localized along the entire length of the bundles (Supplemental Figure S1). Electronmicrographs of AtMAP65-5–induced bundles show that MTs are parallel-arranged and separated by cross-bridges at an average distance of 25 nm (Figure 1e). The cross-bridges form a lattice that is equally spaced along the MT walls and diagonally oriented between two adjacent parallel MTs. The angle between the cross-bridges relative to the MT axis was 50° on average (n = 95; Figure 1g). Comparable data were obtained with AtMAP65-1 (Figure 1, f and h) as described for carrot MAP65-1 by Chan et al. (1999) blue right-pointing triangle.

Figure 1.
AtMAP65-5 bundles MTs in vitro. (a–c) Observations of rhodamine-labeled taxol-stabilized MTs (1 μM) incubated in the absence (a) or in the presence of AtMAP65-5 (b) and AtMAP65-1 (c) at 0.5 μM. AtMAP65-1 and AtMAP65-5 induce MT ...

AtMAP65-5 and AtMAP65-1 Bundle MTs through Their N-terminal Part

To locate the domains of AtMAP65-5 and AtMAP65-1 required for MT bundling and cross-bridge formation, we defined three different domains on the basis of the amino acid sequence alignment of the AtMAP65s (Figures 2 and and3).3). Roughly the domains correspond to the N-terminal, the central and the C-terminal regions of the AtMAP65-5 and AtMAP65-1 proteins (referred as to domains 1, 2, and 3, respectively). In addition, the domain 3 (C-terminal region) was subdivided in two domains: the N-terminal part including the most evolutionarily conserved domain of MAP65 family (referred as to 3N) and the C-terminal part, which is divergent among the AtMAP65 members (referred as to 3C). The separate fragments as well as combinations thereof, were purified as His-tagged recombinant proteins [designated AtMAP65(2), AtMAP65(3), AtMAP65(13), AtMAP65(23), AtMAP65(3N), AtMAP65(3C), and AtMAP65(Δ3C); Figures 2A and and33A].

Figure 2.
Analysis of functional domains of AtMAP65-1 on MT bundling in vitro. (A) Diagrams of the AtMAP65-1 domains and their combinations. The conserved motif through evolution is underlined. (B) Bundled MTs and individual MTs were separated by low-speed centrifugation. ...
Figure 3.
Analysis of functional domains of AtMAP65-5 on MT bundling in vitro. (A) Diagrams of the AtMAP65-5 domains and their combinations. The conserved motif through evolution is underlined. (B) Bundled MTs and individual MTs were separated by low-speed centrifugation. ...

High speed centrifugation of both AtMAP65s and their different constructs [AtMAP65(2), AtMAP65(3), AtMAP65(13), AtMAP65(23), AtMAP65(Δ3C), and AtMAP65(3C)] after incubation with MTs led to the sedimentation of the proteins carrying the domain 3N of either AtMAP65-5 or AtMAP65-1 (Supplemental Figure S2). The proteins AtMAP65(2) and AtMAP65(3C) did not sedimented with MTs. These results indicate that the MT-binding domain of AtMAP65-5 and AtMAP65-1 is located in the domain 3N corresponding to the conserved part of the C-terminal domain of these two MAPs, in agreement with previous reports on MAP65 members (Mollinari et al., 2002 blue right-pointing triangle; Smertenko et al., 2004 blue right-pointing triangle; Loïdice et al., 2005 blue right-pointing triangle).

The efficiency of MT bundling by the different AtMAP65 proteins was assayed by low-speed centrifugations that allow single MTs to remain in the supernatant, while bundled MTs sediment. Analysis of the supernatant and pellets (Figures 2B and and3B)3B) showed that the MTs cosedimented with the constructs AtMAP65(13), AtMAP65(23), and AtMAP65(Δ3C) but not with AtMAP65(3). These results demonstrate that the N-terminal and the central domain of both AtMAP65-1 and AtMAP65-5 are independently able to promote MT bundling in vitro, that the domain 3, carrying the MT-binding domain (3N), is not able by itself to induce microtubule bundling, and that the domain 3C (C-terminal domain) is not required for such activity.

Observations of rhodamine-labeled MTs incubated with AtMAP65(13), AtMAP65(23), and AtMAP65(Δ3C) (Figures 2C and and3C)3C) confirmed the cross-linking activity of the N-terminus and the central domains independently from each other. Measurements at the EM level of the distance between MTs into bundles (Figures 2D and and3D)3D) showed that the inter-MT space was narrower in the presence of AtMAP65 fragments than with the full-length AtMAP65-1 and AtMAP65-5 (<10 vs. ~ 20–30 nm) except for AtMAP65-1(Δ3C), which induced the same inter-MT spacing than full-length AtMAP65-1 (Figure 2Dd).

These results suggest that the length of the proteins upstream of the MT-binding domain is determinant for the interspacing between MTs within bundles. Noticeably, even if the domain 3C of AtMAP65-5 does not interact with MTs, it might play a role in the conformation of the binding domain because the distance between MTs in the presence of full-length AtMAP65-5 is at two times longer than for AtMAP65-5(Δ3C).

Soluble AtMAP65-5 and AtMAP65-1 Are Monomeric and Display Conformational Flexibility

The EM observations of MT bundles induced by AtMAP65-5 and AtMAP65-1 full-length proteins and the different fragments suggested that the inter-MT space depended on the protein size. As the measured distances for the full-length proteins of 20–40 nm on average are too large for a single protein to cover, oligomerization of the MAP65s was suspected. Therefore, we determined their degree of oligomerization in solution by sedimentation velocity (SV) analytical ultracentrifugation and size exclusion chromatography. The sedimentation coefficient (s20w) of AtMAP65-1 at 8 and 30 μM and of AtMAP65-5 at 9 μM were 3.7 ± 0.25 S (Figure 4A). The calculated theoretic s20,w values for hydrated globular compact monomers of AtMAP65-1 is 4.7 and 5 S for AtMAP65-5, i.e., significantly larger than experimental values. The MW was roughly estimated from SV boundary spreading to be 60 kDa for the two proteins, in agreement with the predicted values of 65 and 73 kDa for AtMAP65-1 and AtMAP65-5, respectively. The results indicate that AtMAP65-1 and AtMAP65-5 are monomeric in solution and that they adopt extended conformations. The hydrodynamic radii (RH) of AtMAP65-1 and AtMAP65-5 were calculated to be 42 and 46Å, respectively, corresponding to a frictional ratio f/fmin of ~1.6. SV experiments with the different AtMAP65 peptides provided s-values corresponding as well to monomers with f/fmin of ~1.5 (unpublished data).

Figure 4.
Determination of the oligomerization degree of AtMAP65-1 and AtMAP65-5. (A) Sedimentation velocity analytical ultracentrifugation of purified recombinant AtMAP65-1 and AtMAP65-5. (A1) Superimposition of selected experimental and modeled profiles obtained ...

Gel filtration chromatography showed an apparent MW in a range of 500 kDa for both AtMAP65-5 and AtMAP65-1, much larger than the expected ~70 kDa. Likewise, AtMAP65 fragments produced apparent molecular sizes exceeding the values predicted from sequence data. As proteins with a high intrinsic disorder tend to show reduced mobility in gel-filtration columns (Receveur-Bréchot et al., 2006 blue right-pointing triangle) and because the experimentally determined MWs deviated from the predicted values, we suggest that AtMAP65-5 and AtMAP65-1 are possibly disordered and might adopt an elongated shape in solution. Indeed, according to their hydrodynamic properties (RH = ~45Å, f/fmin = ~1.6), AtMAP65-1 and AtMAP65-5 behaved as random coils (Uversky, 2002 blue right-pointing triangle). Using DisEMb1 software (Linding et al., 2003 blue right-pointing triangle), several disordered domains in AtMAP65-1 and AtMAP65-5 sequences were identified (Figure 4B). Because disordered domains generally lack tertiary structure and fold only upon interaction with other proteins, the presence of such domains in AtMAP65-5 and AtMAP65-1 support the viewpoint that they undergo conformational changes upon interaction with microtubules, themselves, and/or regulatory proteins.

Having determined that in solution both AtMAP65-1 and AtMAP65-5 are monomeric and postulating that at least a homo-dimer may be necessary to bundle two MTs together, we considered that AtMAP65-5 and AtMAP65-1 may bind to MTs as monomers and that this binding is not stable until they interact with a partner localized to a parallel MT. To address this question, we incubated single MTs with GFP-tagged AtMAP65-1 or AtMAP65-5 (Figure 4C). We observed that GFP-AtMAP65-1 and GFP-AtMAP65-5 localized along the MT bundles (detected as thick MTs, arrows in Figures 4C, a and d), whereas no significant accumulation of either AtMAP65-1 or AtMAP65-5 along MTs could be detected (n = ~100).

AtMAP65-5 and AtMAP65-1 Promote the Bundling of Antiparallel MTs

A key issue of the organization of MT bundles is their polarity (Ehrhardt and Shaw, 2006 blue right-pointing triangle). Here we determined the polarity of MTs within AtMAP65-5– and AtMAP65-1– induced bundles in vitro using cryo-EM as described by Chrétien et al. (1996) blue right-pointing triangle. Observed in vitreous ice, MTs with skewed protofilaments show arrowhead moiré patterns, the origin of which is related to an asymmetry of the mass distribution of the tubulin molecules in the MT wall. The arrowheads point toward the plus end of MTs when protofilaments show a right-handed skew and toward the minus end of MTs when protofilaments show a left-handed skew. Cryo-EM observation of in vitro AtMAP65-1 and AtMAP65-5–induced MT bundles confirmed the diagonal cross-linking pattern between adjacent MTs as detected by classic EM (~60 ± 5° relative to the MT axis, n = 40; Figure 5, A, a and b, and B, a and b). The inter-MT space in AtMAP65-1 bundles was in the range of 30–40 nm and was more regular in comparison to AtMAP65-5 bundles, which displayed MT separations varying between 15 and 40 nm. Note that for technical reasons, values obtained with cryo-EM are different from those calculated from EM micrographs. This point is explained in details in Material and Methods. The moiré patterns of AtMAP65-1– and AtMAP65-5–bundled MTs showed that the orientation of adjacent MTs in bundles induced by AtMAP65-1 or AtMAP65-5 was antiparallel (17 and 38 MTs were analyzed, respectively, for AtMAP65-1 and AtMAP65-5; Figure 5, Ac and Bc). Because no parallel arranged MTs were detected that are connected via AtMAP65-5 or AtMAP65-1 cross-bridges, we conclude that these two AtMAP65 specifically promote antiparallel bundling of MTs. A much more complete description of the methodology used is explained in detail in Supplemental Materials.

Figure 5.
Determination of the polarity of MTs within bundles induced by AtMAP65-1 and AtMAP65-5. Cryo-EM of vitreous ice-embedded MTs incubated with AtMAP65-1 (A) and AtMAP65-5 (B). (Aa and Ba). View of aligned MTs showing AtMAP65-1 and AtMAP65-5 as extensive ...

Further inspection of the diffraction patterns calculated from cryo-EM images revealed an additional regular patterning corresponding to the spacing between AtMAP65-1 and AtMAP65-5 cross-bridges in projection (Figures 5A, d and e, and B, d and e). The diffraction patterns are calculated from vitrified MT images, revealing an additional regular patterning at project ~80Å, corresponding to the spacing between AtMAP65-1 and AtMAP65-5 cross-bridges in projection. This spacing corresponds to the tubulin dimer repeat. Nevertheless this further regular patterning corresponds to a feature through the thickness of the sample; thus we cannot conclude that we have one MAP65 bound per tubulin dimer (Figure 9A). In conclusion, these data show that the two ends of cross-bridges observed within MT bundles are linked to adjacent MTs, indicating that at least two MT-binding domains are necessary to link two adjacent MTs.

In Vitro Tubulin Assembly in the Presence of Recombinant AtMAP65-5 and AtMAP65-1

Besides the properties of AtMAP65-1 and AtMAP65-5 to bundle MTs, we further addressed whether AtMAP65-5 could affect tubulin assembly in vitro. We quantified the amount of tubulin that polymerized in the presence of AtMAP65-5 by high-speed cosedimentation assays (Figure 6A) and by time-lapse spectroscopy (Figure 6B; kinetic graphs are shown in Supplemental Figure S3). In both series of experiments, we observed an increased amount of tubulin in the presence of AtMAP65-5, suggesting that AtMAP65-5 has an effect on tubulin assembly. By imaging assays, rhodamine-labeled tubulin, assembly in the presence of AtMAP65-5 showed few MT bundles and often aggregates associated with radiating MTs were observed (Figure 6Cb).

Figure 6.
Effect of AtMAP65-5 on MT assembly in vitro. (A) Quantification of the amount of tubulin (15 μM) that polymerized into MTs in presence of AtMAP65s. MTs and associated AtMAP65s were pelleted by high-speed centrifugation. (B) Tubulin assembly (15 ...

As there is a controversy concerning the effects of AtMAP65-1 and its C-terminal part on tubulin assembly, we performed similar experiments with both full-length AtMAP65-1 and the truncated protein AtMAP65-1(Δ3C). We observed an increase in the amount of the polymerized tubulin in the presence of both AtMAP65-1 and AtMAP65-1(Δ3C) (Figure 6, A and B). AtMAP65-1(Δ3C) had a comparable although reduced activity in tubulin polymerization in comparison with AtMAP65-1. We noted that AtMAP65-5(Δ3C) also has similar effects on tubulin assembly than AtMAP65-5, with AtMAP65-5(Δ3C) being slightly less efficient than the full-length protein (Figure 6B). No polymerization of tubulin in the presence of the domains 3, 3N, and 3C of AtMAP65-1 was observed (unpublished data), in contrast to a recent report by Li et al. (2007b) blue right-pointing triangle or with the domain 3 of AtMAP65-5. AtMAP65-1 and AtMAP65-1(Δ3C) on the other hand did stimulate MT bundling when incubated with tubulin (Figure 6C, d and e). Because AtMAP65-1 and AtMAP65-5 have been shown to protect CMTs from cold-induced depolymerization (Wicker-Planquart et al., 2004 blue right-pointing triangle; our unpublished data), we suggest that the effect on MT polymerization observed in vitro might be mainly due to a stabilization of the MTs. Overall the data suggest that the main activity of AtMAP65-5 and AtMAP65-1 is to induce MT bundling but not to promote MT polymerization in vitro, in line with previous reports on AtMAP65-1 and NtMAP65-1 (Smertenko et al., 2004 blue right-pointing triangle; Wicker-Planquart et al., 2004 blue right-pointing triangle).

AtMAP65-5 Localization during Mitosis

To study AtMAP65-5 MT-binding properties in vivo, we followed its subcellular localization in transformed dividing BY-2 cells expressing AtMAP65-5-GFP and compared it to the AtMAP65-1 localization. Typically, during interphase CMTs were decorated with GFP-AtMAP65-5 (Van Damme et al., 2004a blue right-pointing triangle). We found that during prophase, GFP- AtMAP65-5 strongly labeled the preprophase band, a hallmark for the division zone, and the perinuclear MTs before the initiation of the bipolar spindle (Figure 7A, Video S1). The perinuclear MTs labeled with AtMAP65-5 are coaligned and formed a basket surrounding the nucleus. In some cells, at the polar sides of the cage, MTs emanate toward the distal ends of the cells. These aster-like MTs, when present, were labeled by AtMAP65-5-GFP (Figure 7A). Upon nuclear envelope breakdown, AtMAP65-5-GFP dissociated from the perinuclear MTs to reassociate with the interdigitated MTs at the spindle midzone at the end of metaphase until the end of anaphase (Figure 8A, Video S2). On initiation of the phragmoplast, AtMAP65-5-GFP accumulated in the central zone, displaying discrete filamentous structures between the separating nuclei. A few minutes later when the phragmoplast flattened, AtMAP65-5-GFP concentrated at a narrow zone in the center and at the side of the nucleus that faces the equatorial zone (this study; Van Damme et al., 2004a blue right-pointing triangle). In comparison, AtMAP65-1-GFP, that which colocalizes with the CMTs and the preprophase band (Van Damme et al., 2004a blue right-pointing triangle; Smertenko et al., 2004 blue right-pointing triangle; Mao et al., 2005a blue right-pointing triangle), was absent from the perinuclear area, but did associate with aster-like polar MT bundles when present (Figure 7B, Video S3). Furthermore, AtMAP65-1-GFP showed a limited accumulation at the spindle midzone only in early anaphase (Figure 8B, Video S3), the labeling being stronger in late anaphase. These observations revealed that in vivo the MT binding of AtMAP65-5-GFP is spatially and temporally regulated during the cell cycle and that its subcellular distribution during mitosis is partly different to that of AtMAP65-1.

Figure 7.
Differential localization of AtMAP65-5 and AtMAP65-1 during prophase. Tobacco BY-2 cells expressing AtMAP65-5-GFP and RFP-TUA6 (A) and expressing AtMAP65-1-GFP and RFP-TUA6 (B). Cells are observed in the GFP channel (a and d) and in the RFP channel (b ...
Figure 8.
AtMAP65-5 accumulates in the midzone in metaphase until late anaphase. Time-lapse recording of tobacco BY-2 cells expression AtMAP65-5-GFP and RFP-TUA6 (A) and AtMAP65-1-GFP and RFP-TUA6 (B). The yellow signal in the third rows corresponds to the merged ...


This report expands the analysis of the molecular properties of AtMAP65-5 and provides uncovers previously unknown properties for AtMAP65-1.

We found that AtMAP65-5 induces MT bundling in vitro and that it binds MTs through the domain conserved among AtMAP65s (referred as domain 3N), this domain alone being unable to induce MT bundling and tubulin assembly. Similarly we found that AtMAP65-1 has only one MT-binding domain (within the domain 3N) and that this domain is not able to stimulate tubulin assembly and MT bundling.

AtMAP65-5 and AtMAP65-1 contain intrinsic disordered domains mostly within their C-terminal domain (domain 3) as suggested by Li et al. (2007a) blue right-pointing triangle for AtMAP65-1. Disordered domains provide a level of structural plasticity by their propensity to form tertiary structure upon binding to physiological partner(s) (Gunasekaran et al., 2003 blue right-pointing triangle; Receveur-Bréchot et al., 2006 blue right-pointing triangle). AtMAP65-5 appears more disordered than AtMAP65-1, suggesting differences in their structure when bound to MTs or other physiological partner(s). Recently, Smertenko et al. (2006) blue right-pointing triangle showed that in vivo, the MT-binding activity of AtMAP65-1 is partly controlled by phosphorylation of nine amino acid residues within its 3C-terminal domain and that phosphorylation weakens interaction of AtMAP65-1 with MTs. Because it does not bind MTs in vitro and is highly disordered, it is possible that upon phosphorylation the 3C-terminal domain is refolded so that the conformation of the 3N- terminal domain changes, resulting in the weakness of AtMAP65-1 binding to MTs. Because only one of the nine phophorylable AtMAP65-1's residues is conserved in AtMAP65-5, the regulation of its MT binding might rely on an alternative mechanism.

AtMAP65-5 Localization Is Cell Cycle Specific

AtMAP65-5 was shown to associate with a subset of transversely organized CMTs and the phragmoplast (Van Damme et al., 2004a blue right-pointing triangle). Our time-lapse analysis of AtMAP65-5's localization shows that during prophase, AtMAP65-5 localizes at the perinuclear area at the onset of spindle formation and at the preprophase band. In comparison, AtMAP65-1 does not associate with the perinuclear array, whereas within the same cell, it does bind the preprophase band. After nuclear envelop breakdown, AtMAP65-5 reappears and labels distinct MTs in the spindle midzone not labeled by AtMAP65-1. These observations indicate that the AtMAP65-1 and AtMAP65-5 MT-binding capacity might be controlled locally and temporally during mitosis.

MT Organization within Bundles Induced by AtMAP65-5 and AtMAP65-1

Using cryo-EM, we observed that in vitro MT bundles induced by AtMAP65-5 and AtMAP65-1 contain coaligned MTs 15–40 and 30–40 nm apart, respectively. This distance is in range of the inter-MT space reported for bundles at the cell cortex (Hardham and Gunning, 1978 blue right-pointing triangle) and for carrot MAP65-1 and AtMAP65-1 in vitro (Chan et al., 1999 blue right-pointing triangle; Smertenko et al., 2004 blue right-pointing triangle). Cross-bridges form a diagonal pattern connected with the MT wall at ~60° relative to the MT axis. Via cryo-EM, a projection of a 3D object is obtained, allowing the calculation of internal positional information of the specimen (Figure 9B). We calculated that AtMAP65-5 or AtMAP65-1 binds with a periodicity of 24 nm along the MT protofilaments, i.e., one molecule per three tubulin heterodimers (Figure 9A).

Each of the two ends of cross-bridges are linked to adjacent MTs, indicating that at least two MT-binding domains are necessary to link two adjacent MTs. As the inter-MT space is too large for a single MAP65 molecule to cross, AtMAP65-1 and AtMAP65-5 must undergo oligomerization to form the cross-bridges. We suggest that a cooperative action of domains 1 and 2 is required to build this link because deletion of one of these domains reduces the inter-MT spacing by half. Cross-bridges generated by AtMAP65-5 were less regular and shorter on average than those generated by AtMAP65-1, suggesting different conformational organization of domain 1 and 2 in two MAP65s. The presence of many short disordered stretches within the domain 1 and 2 in AtMAP65-5 and just one in domain 2 in AtMAP65-1 might be responsible for a difference in cross-bridge length. Therefore, the structural basis of the AtMAP65-1 and AtMAP65-5 interactions to induce MT bundling may be different for AtMAP65-1 and AtMAP65-5.

AtMAP65-1 and AtMAP65-5 behaved as monomers in their soluble forms. This result challenges the findings by Smertenko et al. (2004) blue right-pointing triangle, who proposed that AtMAP65-1 form homodimers in solution. Their conclusions were based on chemical cross-linking, native acrylamide gel electrophoresis and affinity chromatography with cell extracts. In view of the presence of disordered domains and high structural flexibility, we postulate that AtMAP65-1 and AtMAP65-5 dimerization is stimulated at high concentrations or when in contact with a protein-binding matrix. In addition, reduced electrophoretic migration in acrylamide gels is a common feature for unfolded proteins (Receveur-Bréchot et al., 2006 blue right-pointing triangle).

One possible interpretation of our results is that AtMAP65-1 and AtMAP65-5 bind to MTs as monomers and that this binding is not stable until they interact with a partner at an adjacent MT. This hypothesis is supported by the fact that in cryo-EM, no filament of AtMAP65-1 or AtMAP65-5 is seen projecting free from a single MT. In fluorescence assays, AtMAP65-1 and AtMAP65-5 accumulated along MT bundles but not along single MTs (Figure 4C). In comparison, in fission yeast binding of Ase1p to MTs is reinforced when Ase1p binds overlapped MTs (Janson et al., 2007 blue right-pointing triangle). In vivo, Van Damme et al. (2004a) blue right-pointing triangle reported that AtMAP65-1-GFP or AtMAP65-5-GFP associated with coaligned MTs and suggested that AtMAP65-1-GFP may not bind to single MTs. Together, these data suggest a mode of action for AtMAP65s MT bundling that involves the binding of monomeric AtMAP65-5 and AtMAP65-1 to MTs that zipper up through the homodimerization of the N-terminal regions when adjacent MTs encounter.

AtMAP65-5 and AtMAP65-1 Induce MT Bundling of Antiparallel MTs in Vitro

The polarity of MTs within a bundle remains a controversial issue. MTs were shown to polymerize within bundles in two directions, suggesting an antiparallel organization (Chan et al., 2003 blue right-pointing triangle; Shaw et al., 2003 blue right-pointing triangle; Van Damme et al., 2004b blue right-pointing triangle; Vos et al., 2004 blue right-pointing triangle), whereas Dixit et al. (2006) blue right-pointing triangle reported that the majority of cortical MTs have the same polarity and that the polar arrangement of CMTs occurs simultaneously with parallel MT arrangement. Using the hook decoration, Tian et al. (2004) blue right-pointing triangle showed that the polarity of MTs in the cortical array is not uniform. In the present study, we provide by an original way new evidence that AtMAP65-1 and AtMAP65-5 stimulate antiparallel bundling of MTs in vitro.

The subcellular localization of AtMAP65-1-GFP and AtMAP65-5-GFP further supports a preference for antiparallel MT bundling in vivo. During late metaphase and anaphase AtMAP65-5 localizes to the midzone and AtMAP65-1 during late anaphase where numerous nonkinetochore MTs are antiparallel overlapping MT plus ends. Noticeably, Ase1p has the inherent ability to distinguish between parallel and antiparallel MTs (Janson et al., 2007 blue right-pointing triangle). We propose a similar property for AtMAP65-1 and AtMAP65-5 but their ability to control the self-organization of MT bundles in plant cells remain to be addressed.

The question of how AtMAP65-1 or AtMAP65-5 regulate the polarity of MTs in plant living plant cells remains unsolved. Janson et al. (2007) blue right-pointing triangle demonstrated that Ase1p localizes to overlapping (−) ends during interphase and overlapping plus ends in the anaphase spindle, the difference in localization being determined by molecular motors as Klp2p (a minus-end–directed motor) mediates the sliding of newly nucleated MTs along antiparallel MT bundles. In plant cells, ATK5, a plus end tracking protein molecular motor (Ambrose et al., 2005 blue right-pointing triangle) preferentially localizes at regions of overlap between opposing interpolar MTs, suggesting an increased affinity for plus ends in an antiparallel orientation (Ambrose and Cyr, 2007 blue right-pointing triangle). In vitro, ATK5 equally coaligns with parallel or antiparallel MTs. One can postulate that the orientation of MTs is determined by MAPs such as AtMAP65s that stabilize CMT coalignment. It will be important to determine whether AtMAP65-1 or AtMAP65-5 can organize stable regions of MT overlap in combination with the activity of a motor such as ATK5.

Supplementary Material

[Supplemental Materials]


We thank Laurent Blanchoin (iRTSV) and François Parcy (iRTSV) for helpful discussions and advice and Olivier Bastien (iRTSV) for help with computing analysis of AtMAP65 sequences. We thank Richard Wade for advice on microtubule polarity determination and for careful reading of the manuscript. D.V.D. is a postdoctoral fellow of the Research Foundation-Flanders. Most of this work was supported by the French CNRS and CEA.

Abbreviations used:

cortical microtubule
Arabidopsis thaliana microtubule-associated protein 65
green fluorescent protein


This article was published online ahead of print in MBC in Press ( on July 30, 2008.


  • Ambrose J., Li W., Marcus A., Ma H., Cyr R. A minus-end-directed kinesin with plus-end tracking protein activity is involved in spindle morphogenesis. Mol. Biol. Cell. 2005;16:1584–1592. [PMC free article] [PubMed]
  • Ambrose J., Cyr R. The kinesin ATK5 functions in early spindle assembly in Arabidopsis. Plant Cell. 2007;19:226–236. [PubMed]
  • Caillaud M. C., et al. MAP65-3 microtubule-associated protein is essential for nematode-induced giant cell ontogenesis in Arabidopsis. Plant Cell. 2008 doi: 10.1105/tpc.107.057422. Advanced online publication 8 February 2008; [PubMed] [Cross Ref]
  • Chan J., Jensen C. G., Jensen L. C., Bush M., Lloyd C. W. The 65-kDa carrot microtubule-associated protein forms regularly arranged filamentous cross-bridges between microtubules. Proc. Natl. Acad. Sci. USA. 1999;96:14931–14936. [PubMed]
  • Chan J., Calder G. M., Doonan J. H., Lloyd C. W. EB1 reveals mobile microtubule nucleation sites in Arabidopsis. Nat. Cell Biol. 2003;5:967–971. [PubMed]
  • Chan J., Calder G., Fox S., Lloyd C. W. Cortical microtubule arrays undergo rotary movements in Arabidopsis hypocotyl epidermal cells. Nat. Cell Biol. 2007;9:171–175. [PubMed]
  • Chrétien D., Kenney J., Fuller S., Wade R. Determination of microtubule polarity by cryo-electron microscopy. Structure. 1996;4:1031–1040. [PubMed]
  • Dixit R., Cyr R. Encounters between dynamic cortical microtubules promote ordering of the cortical array through angle-dependent modifications of microtubule behaviour. Plant Cell. 2004;16:3274–3284. [PubMed]
  • Dixit R., Chang E., Cyr R. Establishment of polarity during organization of the acentrosomal plant cortical microtubule array. Mol. Biol. Cell. 2006;17:1298–1305. [PMC free article] [PubMed]
  • Dubochet J., Adrian M., Chand J. J., Homo J. C., Lepault J., McDowall A. W., Schultz P. Cryo-electron microscopy of vitrified specimens. Rev. Biophys. 1988;21:129–228. [PubMed]
  • Ebel C. Analytical ultracentrifugation. State of the art and perspectives. In: Uversky V., Permyakov E. A., editors. Methods in Protein Structure and Stability Analysis: Conformational Stability, Size, Shape and Surface of Protein Molecules. New York: Nova Science Publishers; 2007.
  • Ehrhardt D. W., Shaw S. L. Microtubule dynamics and organization in the plant cortex. Annu. Rev. Plant Biol. 2006;57:859–875. [PubMed]
  • Geelen D. N., Inzé D. G. A bright future for the bright yellow-2 cell culture. Plant Physiol. 2001;127:1375–1379. [PubMed]
  • Gunasekaran K., Tsai C., Kumar S., Zanuy D., Nussinov R. Extended disordered proteins: targeting function with less scaffold. Trends Biochem. Sci. 2003;28:81–85. [PubMed]
  • Hardham A. R., Gunning B. Structure of cortical microtubules in plant cells. J. Cell Biol. 1978;77:14–34. [PMC free article] [PubMed]
  • Hussey P., Hawkins T. J., Igarashi H., Kaloriti D., Smertenko A. The plant cytoskeleton: recent advances in the study of the plant microtubule-associated proteins MAP-65, MAP-190 and the Xenopus MAP215-like protein, MOR1. Plant Mol. Biol. 2002;50:915–924. [PubMed]
  • Hyman A., Dreschel D., Kellog D., Salser S., Sawin K., Steffen P., Wordeman L., Mitchison T. Preparation of modified tubulins. Methods Enzymol. 1991;196:478–485. [PubMed]
  • Janson M., Loughlin R., Loïodice I., Brunner C., Nédelec F., Tran P. T. Crosslinkers and motors organize dynamic microtubules to form stable bipolar arrays in fission yeast. Cell. 2007;128:357–368. [PubMed]
  • Li H., Mao T., Zhang Z., Yuan M. The AtMAP65-1 cross-bridge between microtubules is formed by one dimer. Plant Cell Physiol. 2007a;48:866–874. [PubMed]
  • Li H., Yuan M., Mao T. AtMAP65-1 binds to tubulin dimers to promote tubulin assembly. J. Biochem. Mol. Biol. 2007b;40:218–225. [PubMed]
  • Linding R., Jensen L. J., Diella F., Bork P., Gibson T. J., Russell R. B. Protein disorder prediction: implications for structural proteomics. Structure. 2003;11:1453–1459. [PubMed]
  • Lloyd C. W. Why should stationary plants cells have such dynamic microtubules? Mol. Biol. Cell. 1994;5:1277–1280. [PMC free article] [PubMed]
  • Loïdice I., Staub J., Getty T. G., Hguyen N. T., Paoletti A., Tran P. T. Ase1p organizes antiparallel microtubule arrays during interphase and mitosis in fission yeast. Mol. Biol. Cell. 2005;16:1756–1768. [PMC free article] [PubMed]
  • Mao G., Chan J., Calder G., Doonan J. H., Lloyd C. W. Modulated targeting of GFP-AtMAP65-1 to central spindle microtubules during division. Plant Cell. 2005a;43:469–478. [PubMed]
  • Mao T., Jin L., Liu B., Yuan M. Two microtubule-associated proteins of the Arabidopsis MAP65 family function differently on microtubules. Plant Physiol. 2005b;138:654–662. [PubMed]
  • Mollinari C., Kleman J. P., Jiang W., Schoehn G., Hunter T., Margolis B. PRC1 is a microtubule binding and bundling protein essential to maintain the mitotic spindle midzone. J. Cell Biol. 2002;157:1175–1186. [PMC free article] [PubMed]
  • Murata M., Sonobe S., Baskin T. I., Hyodo S., Hasezawa S., Nagata T., Horio T., Hasebe M. Microtubule-dependent microtubule nucleation based on recruitment of gamma-tubulin in higher plants. Nat. Cell Biol. 2005;7:961–968. [PubMed]
  • Pastuglia M., Azimzadeh J., Goussot M., Camilleri C., Evrard J. L., Schmit A. C., Guerche P., Bouchez D. Gamma-tubulin is essential for microtubule organization and development in Arabidopsis. Plant Cell. 2006;18:1412–1425. [PubMed]
  • Receveur-Bréchot V., Bourhis J. M., Uversky V., Canard B., Longhi S. Assessing protein disorder and induced folding. Proteins. 2006;62:24–45. [PubMed]
  • Schuck P. Size-distribution analysis of macromolecules by sedimentation velocity ultracentrifugation and lamm equation modeling. Biophys. J. 2000;78:1606–1619. [PubMed]
  • Schuyler S., Liu J. Y., Pellman D. The molecular function of Ase1p: evidence for a MAP-dependent midzone-specific spindle matrix. J. Cell Biol. 2003;160:517–528. [PMC free article] [PubMed]
  • Shaw S. L., Kamyar R., Ehrhardt D. W. Sustained microtubule treadmilling in Arabidopsis cortical arrays. Science. 2003;300:1715–1718. [PubMed]
  • Smertenko A., Chang H., Wagner V., Kaloriti D., Fenyk S., Sonobe S., Lloyd C. W., Hauser M., Hussey P. The Arabidopsis microtubule-associated protein AtMAP65-1, molecular analysis of its microtubule bundling activity. Plant Cell. 2004;16:2035–2047. [PubMed]
  • Smertenko A. P., Chang H. Y., Sonobe S., Fenyk S. I., Weingartner M., Bogre L., Hussey P. Control of the AtMAP65-1 interaction with microtubules through the cell cycle. J. Cell Sci. 2006;119:3227–3237. [PubMed]
  • Stoppin V., Lambert A. M., Vantard M. Plant microtubule-associated proteins (MAPs) affect microtubule nucleation and growth at plant nuclei and mammalian centrosomes. Eur. J. Cell Biol. 1996;69:11–23. [PubMed]
  • Tian G. W., Smith D., Gluck S., Baskin T. I. Higher plant cortical microtubule array analyzed in vitro in the presence of the cell wall. Cell Motil. Cytoskelet. 2004;57:26–36. [PubMed]
  • Uversky V. N. What does it mean to be natively unfolded? Eur. J. Biochem. 2002;269:2–12. [PubMed]
  • Van Damme D., Van Poucke K., Boutant E., Ritzenthaler C., Inzé D., Geelen D. In vivo dynamics and differential microtubule-binding activities of MAP65 proteins. Plant Physiol. 2004a;136:3956–3967. [PubMed]
  • Van Damme D., Bouget F. Y., Van Poucke K., Inzé D., Geelen D. Molecular dissection of plant cytokinesis and phragmoplast structure: a survey of GFP-tagged proteins. Plant J. 2004b;40:386–398. [PubMed]
  • Vantard M., Peter C., Fellous A., Schellenbaum P., Lambert A. M. Characterization of a 100-kDa heat-stable microtubule-associated protein from higher plants. Eur. J. Biochem. 1994;220:847–853. [PubMed]
  • Verni F., Somma M. P., Gunsalus C. K., Bonaccorsi S., Belloni G., Goldberg M. L., Gatti M. Feo, the Drosophila homolog of PRC1, is required for central-spindle formation and cytokinesis. Curr. Biol. 2004;14:1569–1575. [PubMed]
  • Vos J. W., Dogterom M., Emons A. M. Microtubules become more dynamic but not shorter during preprophase band formation: a possible “search-and-capture” mechanism for microtubule translocation. Cell Motil. Cytoskelet. 2004;57:246–258. [PubMed]
  • Wasteneys G. O., Fujita M. Establishing and maintaining axial growth: wall mechanical properties and the cytoskeleton. J. Plant Res. 2006;119:5–10. [PubMed]
  • Wicker-Planquart C., Stoppin-Mellet V., Blanchoin L., Vantard M. Interactions of tobacco microtubule-associated protein MAP651b with microtubules. Plant J. 2004;39:126–134. [PubMed]
  • Zhu C., Lau E., Schwarzenbacher R., Bossy-Wetzel E., Jiang W. Spatiotemporal control of spindle midzone formation by PRC1 in human cells. Proc. Natl. Acad. Sci. USA. 2006;18:6196–6201. [PubMed]

Articles from Molecular Biology of the Cell are provided here courtesy of American Society for Cell Biology