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Originally published In Press as doi:10.1074/jbc.M404051200 on June 7, 2004

J. Biol. Chem., Vol. 279, Issue 33, 34595-34602, August 13, 2004
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Protein 4.1R, a Microtubule-associated Protein Involved in Microtubule Aster Assembly in Mammalian Mitotic Extract*

Shu-Ching Huang{ddagger}§, Ramasamy Jagadeeswaran{ddagger}, Eva S. Liu{ddagger}, and Edward J. Benz, Jr.{ddagger}§||**{ddagger}{ddagger}

From the {ddagger}Department of Medical Oncology, Dana Farber Cancer Institute, the §Department of Medicine, Harvard Medical School, the ||Department of Medicine, Brigham and Women's Hospital, the **Department of Pediatrics, Children's Hospital of Boston, Boston, and the {ddagger}{ddagger}Department of Pathology, Harvard Medical School, Boston, Massachusetts 02115

Received for publication, April 12, 2004 , and in revised form, May 18, 2004.


   ABSTRACT
TOP
 ABSTRACT
INTRODUCTION
 EXPERIMENTAL PROCEDURES
 RESULTS
 DISCUSSION
 REFERENCES
 
Non-erythroid protein 4.1R (4.1R) consists of a complex family of isoforms. We have shown that 4.1R isoforms localize at the mitotic spindle/spindle poles and associate in a complex with the mitotic-spindle organization proteins Nuclear Mitotic Apparatus protein (NuMA), dynein, and dynactin. We addressed the mitotic function of 4.1R by investigating its association with microtubules, the main component of the mitotic spindles, and its role in mitotic aster assembly in vitro. 4.1R appears to partially co-localize with microtubules throughout the mitotic stages of the cell cycle. In vitro sedimentation assays showed that 4.1R isoforms directly interact with microtubules. Glutathione S-transferase (GST) pull-down assays using GST-4.1R fusions and mitotic cell extracts further showed that the association of 4.1R with tubulin results from both the membrane-binding domain and C-terminal domain of 4.1R. Moreover, 4.1R, but not actin, is a mitotic microtubule-associated protein; 4.1R associates with microtubules in the microtubule pellet of the mitotic asters assembled in mammalian cell-free mitotic extract. The organization of microtubules into asters depends on 4.1R in that immunodepletion of 4.1R from the extract resulted in randomly dispersed microtubules. Furthermore, adding a 135-kDa recombinant 4.1R reconstituted the mitotic asters. Finally, we demonstrated that a mitotic 4.1R isoform appears to form a complex in vivo with tubulin and NuMA in highly synchronized mitotic HeLa extracts. Our results suggest that a 135-kDa non-erythroid 4.1R is important to cell division, because it participates in the formation of mitotic spindles and spindle poles through its interaction with mitotic microtubules.


   INTRODUCTION
TOP
 ABSTRACT
 INTRODUCTION
EXPERIMENTAL PROCEDURES
 RESULTS
 DISCUSSION
 REFERENCES
 
Protein 4.1R is an 80-kDa structural component of the red blood cell cytoskeleton. 4.1R is critical to the formation of the spectrin/actin/4.1R junctional complex, whose integrity is vital for the mechanical stability and elasticity of the red blood cells (reviewed in Ref. 1). The 80-kDa 4.1R of mature red blood cells is the prototype of a large array of 4.1R isoforms arising from a single gene by utilizing different promoters (2), alternative mRNA splicing (3, 4), two translation initiation sites (5, 6), and post-translational modifications (7). Three homologues of 4.1R, namely 4.1G, 4.1N, and 4.1B, have been identified (8–11). They share a common structural organization with 4.1R: highly conserved protein interaction domains (the 30-kDa membrane-binding domain (MBD1), the 10-kDa spectrin/actin-binding domain (SAB), and the 22- to 24-kDa C-terminal domain (CTD)) interspersed with unique domains. The N-terminal extension domain (head-piece, or HP) and exon 13 in the 16-kDa domain are unique to 4.1R. Thus, 4.1R function(s) in non-erythroid cells may be specific or sustainable by redundant systems involving other family members.

Regulated alternative splicing is a characteristic protein 4.1 family feature (3, 4, 12). Multiple isoforms of 4.1R are present in many non-erythroid cell types. The prevalence and homology of these proteins in many species implies their basic importance to cell structure and function. 4.1R isoforms appear to be critical components of many important supramolecular complexes. 4.1R isoforms have been shown to interact with interphase microtubules in human T cells (13), the components of the contractile apparatus in skeletal myofibers (14), and the tight junction proteins in epithelial cells (15). 4.1R isoforms have also been shown to be the components of the nuclear matrix (16, 17) and may be involved in splicing processes (18).

4.1R is reorganized during the cell cycle; it localizes in the nucleus and cytoplasm of interphase cells and rapidly redistributes to the developing spindle poles when the nuclear envelope dissembles in prometaphase (16, 17, 19, 20). In keeping with the key transitions in the cell cycle controlled by the cyclin-dependent kinases, the redistribution of 4.1R to the mitotic spindle and spindle poles is regulated by a phosphorylation event that occurs at Thr-60 and Ser-679 sites by cyclin-dependent cdc2 kinase.2 We (20) previously showed that a 135-kDa 4.1R isoform may participate in mitosis via its association with the non-centrosomal proteins NuMA, dynein, and dynactin, which are essential to the organization of functional spindle poles and tethering of the centrosomes to the spindle pole (21). From these results, we hypothesize that 4.1R plays an important role in organizing mitotic spindle and spindle poles.

A central event during cell division is the transformation of an interphase network of microtubules into a bipolar spindle that mediates the accurate segregation of chromosomes during both mitosis and meiosis. Microtubules in the spindle are organized such that the minus ends are at or near the poles while the plus ends extend toward the cell cortex or chromosomes (22, 23). Recent experiments have begun to define the mechanisms and molecules involved in organizing microtubules into spindles (reviewed in Ref. 24). In somatic cells, centrosomes are the dominant centers of microtubule nucleation. However, centrosomes and the microtubule arrays nucleated from them are not sufficient to act as functional spindle poles (25). The organization of microtubules into spindles is governed largely by the interaction of microtubules and microtubule ends with accessory proteins that regulate microtubule dynamics. Several non-centrosomal proteins such as cytoplasmic dynein (26), dynactin (27), Eg5 (28), HSET (29), ch-TOP (30), cohesin (31), and astrin (32), as well as the structural protein NuMA (33) are involved in focusing microtubules at spindle poles. Researchers are now actively searching for additional proteins that may associate only transiently with spindle poles and for the proteins that are minor components of the spindle poles.

In this study, we investigate the association of 4.1R with microtubules, the main component of the mitotic spindles, and the role of 4.1R in mitotic aster assembly in vitro. We demonstrate that 4.1R is a mitotic microtubule-associated protein and that 4.1R is critical to the organization of microtubules into asters in HeLa mitotic extracts. Our findings suggest that a non-erythroid 135-kDa 4.1R is an important component of cell division by participating in the formation of mitotic spindles and spindle poles through its interaction with mitotic microtubules.


   EXPERIMENTAL PROCEDURES
TOP
 ABSTRACT
 INTRODUCTION
 EXPERIMENTAL PROCEDURES
RESULTS
 DISCUSSION
 REFERENCES
 
Antibody Production—Antisera to synthetic peptides of exon 13 of 4.1R (DSADRSPRPTSAPAI) (anti-exon 13) and the recombinant HP of 4.1R (anti-HP) were prepared as described previously (20). The sera were purified on immunoaffinity columns using the Sulfolink kit (Pierce) covalently cross-linked to the synthetic peptides or fusion peptides used for immunization. The purified antibodies were eluted from the columns with 0.1 N glycine (pH 2.8), neutralized with Tris-HCl, pH 9.5, and dialyzed into phosphate-buffered saline. Anti-NuMA mAb was purchased from Oncogene. Anti-dynein mAb (intermediate chain, clone 70.1), anti-actin mAb, and anti-{alpha}-tubulin mAb DM1A were purchased from Sigma. Anti-p150glued mAb (the largest subunit of dynactin) was purchased from BD Transduction.

Plasmid Construction and Fusion Protein Production—cDNAs were generated by restriction digestion of 4.1R cDNAs (34) or by PCR using an amplification kit (Promega Corp.) and a thermocycler (PCR System 480, PerkinElmer Life Sciences). The 135-kDa/GST fusion construct was generated by cloning a human 4.1R cDNA containing all exons (35) except exons 3, 14, 15, 17a/a', and 17b in-frame into EcoRI and SalI sites of pGEX-6P1 (Amersham Biosciences). For 80-kDa/GST and its different domains in vector pGEX-6P1, custom primer sets with EcoRI or SalI at their 5' or 3' ends, respectively, were used to amplify the corresponding cDNA sequences, digested with EcoRI and SalI, and subcloned in-frame into pGEX-6P1. The primers designed for generation of 4.1R domains (GenBankTM accession number J03796 [GenBank] ) were as follows: 80-kDa/pGEX (674–696/2354–2374), Hp/pGEX (47–69/651–673), MBD/pGEX (674–696/1539–1461), 16-kDa/pGEX (1462–1484/1762–1784), SAB/pGEX (1785–1807/1900–1922), and CTD/pGEX (1923–1942/2354–2374). In some cases, recombinant 4.1R protein was produced using pET-31b(+) vector (Novagen) with a stop codon inserted before the His tag to increase the solubility of the protein. To ensure correctness of the reading frame, the 5'-junction of each construct was sequenced.

Recombinant GST-4.1R was produced according to the manufacturer's protocol (Amersham Biosciences). When vector pET-31b(+) was used, the cDNA was transformed into Escherichia coli BL21(DE3) for protein production. Expression and purification of 4.1R were accomplished as follows. Bacteria were grown in 500 ml of LB medium at 37 °C until A650 reached ~0.7, and the expression of 4.1R was induced by 0.1 mM isopropyl-1-thio-{beta}-D-galactopyranoside at 18 °C overnight. Bacteria were resuspended in 25 ml of phosphate-buffered saline-T (10 mM Na2HPO4/NaH2PO4, pH 7.4, 150 mM NaCl, 0.05% Triton X-100) containing protease inhibitors (4 µg/ml aprotinin, 4 µg/ml leupeptin, 4 µg/ml antipain, 12.5 µg/ml chymostatin, 12 µg/ml pepstatin, 130 µg/ml {epsilon}-aminocaproic acid, 200 µg/ml p-aminobenzamidine, and 1 mM phenylmethylsulfonyl fluoride). The bacterial lysate was passed through a gel filtration column (Superdex-200, 2.5 x 125 cm) pre-equilibrated with gel filtration buffer (10 mM Na2HPO4/NaH2PO4, pH 7.4, 1 M NaCl, 1 mM EDTA, 1 mM DTT, 0.05% Triton X-100, 1 mM NaN3). The fractions containing 4.1R were pooled and dialyzed against an ion-exchange buffer (10 mM Na2HPO4/NaH2PO4, pH 7.4, 70 mM KCl, 1 mM EDTA). 4.1R was then eluted from the Q-Sepharose ion-exchange column by a salt gradient from 100 mM to 500 mM KCl in the above ion-exchange buffer. Pure recombinant 4.1R was then concentrated using Centricon Plus-20 centrifugal filter (Millipore). The protein contents were determined using a standard BCA assay determination kit (Pierce Chemical Co.).

In Vitro Microtubule Binding and GST-pull-down Assay—The microtubule binding assay was performed using the Microtubule Binding Protein Assay kit (Cytoskeleton, Inc.) according to the manufacturer's instructions. Equivalent aliquots of supernatants and pellets were analyzed on Coomassie-stained gels.

For the GST-pull-down assay, mitotic cell lysates were prepared in lysis buffer (25 mM Tris-HCl, 100 mM NaCl, 0.2 mM EDTA, 1 mM DTT, 1.0% Nonidet P-40, pH 7.5) supplemented with protease inhibitors and phosphatase inhibitors (5 mM {beta}-glycerophosphate, 10 mM NaF, 10 mM Na4P2O7). The cell lysate was then pre-cleared by mixing with 100 µlof GST-Sepharose beads at 4 °C for 1 h. Equal amounts of recombinant 135-kDa/GST, 80-kDa/GST, HP/GST, MBD/GST, 16-kDa/GST, SAB/GST, and CTD/GST fusion proteins bound to glutathione-Sepharose were mixed with 0.5 mg of GST-Sepharose bead pre-cleared mitotic cell lysates at 4 °C for 16 h. Beads were washed six times in 4 °C with lysis buffer and immunoblotted with antibodies to {alpha}-tubulin. To verify the quantity and quality of GST and GST-4.1R fusions used in the experiments, a gel loaded with the same amount of fusion proteins was stained with Coomassie Blue.

In Vitro Mitotic Aster Assembly Assay—HeLa (ATCC CCL 2, human cervix epithelioid carcinoma) cells were grown in Dulbecco's modified Eagle's medium supplemented with 10% heat-inactivated fetal bovine serum (Sigma). Highly enriched mitotic HeLa cells were prepared by synchronization of the cells at the G1/S boundary of the cell cycle by a double thymidine block (36). Cells were grown in complete medium after being released from the second thymidine block for 4 h, and the mitotic population was enriched by addition of 60 ng/ml of nocodazole for 6 h. The in vitro aster assembly assay was performed using an established protocol (25, 30). Briefly, mitotic cells were collected by shake-off and incubated with 20 µg/ml cytochalasin B for 30 min at 37 °C. Cells were then washed with phosphate-buffered saline and resuspended at a concentration of ~3 x107 cells/ml in KHM buffer (78 mM KCl, 50 mM Hepes, pH 7.0, 4 mM MgCl2, 2 mM EGTA, 1 mM DTT) containing cytochalasin B and protease inhibitors. Cells were Dounce-homogenized, and the crude extract was subjected to ultracentrifugation at 100,000 x g for 15 min at 4 °C. The supernatant was collected, and latrunculin B (5 µg/ml) was added to reduce actin polymerization and the contamination of microtubule pellets with actin and actin-associated proteins. The supernatant was then supplemented with 10 µM taxol and 2.5 mM ATP, and microtubule asters were assembled by incubation at 30 °C for 60 min. After incubation, samples were processed for indirect immunofluorescence microscopy. The remaining samples were centrifuged through 50% sucrose cushions prepared in KHM at 100,000 x g for 2 h at 4 °C to collect mitotic microtubule-associated proteins in the pellet. Both supernatant and insoluble pellet were collected directly in Laemmli sample buffer for Western blot analysis.

Immunodepletion and Reconstitution Assay—latrunculin B-treated HeLa mitotic extracts described above were subjected to immunodepletion. Thirty micrograms of pre-immune rabbit IgG or 4.1R affinity-purified anti-HP antibodies were coupled to protein A beads and incubated with mitotic extracts for 20 min at 4 °C. The beads were spun down, the supernatants were collected, and the depletion process was repeated twice. Both beads and supernatants in each successive depletion were subjected to Western blotting to verify the effectiveness of depletion of 4.1R and the co-depletion of NuMA and tubulin in these extracts. The final supernatants were subjected to the in vitro aster assembly as described under "In Vitro Mitotic Aster Assembly Assay" above. For reconstitution assays, recombinant 4.1Rs were added to 4.1R-immunodepeleted mitotic extracts and subjected to an in vitro aster assembly as described above.

Coimmunoprecipitation and Immunoblotting—Coimmunoprecipitation of 4.1R, tubulin, and NuMA was performed using HeLa mitotic extracts as described previously (20). In brief, mitotic HeLa cells were homogenized in coimmunoprecipitation buffer (25 mM Tris-HCl, pH 7.5, 100 mM NaCl, 1 mg/ml bovine serum albumin, 0.2 mM EDTA, 5 mM iodoacetamide, 2% CHAPS, protease inhibitors, phosphatase inhibitors), and given 20 strokes in a tight-fitting glass homogenizer. The homogenate was centrifuged at 10,000 x g for 10 min at 4 °C, and the supernatant was pre-cleared with pre-immune rabbit IgG. Subsequently, the supernatant was immunoprecipitated with pre-immune rabbit IgG, affinity-purified anti-HP Ab, anti-NuMA mAb, or anti-{alpha}-tubulin mAb. The immunoprecipitated samples were examined for the presence of 4.1R, NuMA, or tubulin using its respective antibody. Some chemiluminograms were scanned using the Adobe Photoshop software (Adobe Systems, Inc.), and the protein bands of interest were quantitated by using the National Institutes of Health Image software for the Apple Macintosh computer.

Indirect Immunofluorescence and Imaging—HeLa cells were grown on poly-D-lysine-coated coverslips and subjected to immunofluorescence staining as described previously (20). Mitotic asters assembled in vitro were spotted on poly-D-lysine-coated coverslips, fixed in methanol, and then subjected to immunofluorescent staining as described before (25). The samples were viewed with an Axiovert 200M inverted microscope (Zeiss, Inc.). Asters were viewed under a x100 oil objective. Images were collected using SlideBook4 software and processed using Photoshop.


   RESULTS
TOP
 ABSTRACT
 INTRODUCTION
 EXPERIMENTAL PROCEDURES
 RESULTS
DISCUSSION
 REFERENCES
 
Protein 4.1R and Tubulin Partially Co-localize Throughout the Cell Cycle—We (20) reported earlier that a 135-kDa 4.1R isoform specifically interacts with NuMA and associates in a complex containing NuMA, dynein, and dynactin. The cytoplasmic complex dynein/dynactin/NuMA is known to localize to the spindle poles and tether centrosomes to spindle microtubules (21). NuMA binds directly to tubulin and organizes the spindle poles by stable cross-linking to the microtubule fibers at the poles (37). Because NuMA co-localizes and interacts with both 4.1R and tubulin, we tested the association of 4.1R with tubulin. To examine their topography with respect to the mitotic apparatus, we used antibodies specific to 4.1R and {alpha}-tubulin to examine their localization at different stages of cell cycle.

Immunofluorescence microscopy of HeLa cells during interphase revealed that 4.1R was diffusely distributed throughout the cytoplasm but predominantly resided in the nucleus (Fig. 1, Interphase, 4.1R), whereas tubulin localized mainly in the cytoplasm (Fig. 1, Interphase, Tubulin). Co-localization of 4.1R and tubulin in interphase cytoplasm is most intense around the nucleus (yellow areas), which is produced by superimposing green and red (Fig. 1, Interphase, Merged). At early prophase, 4.1R and microtubules are concentrated at the vertices of the developing spindle poles (Fig. 1, Early prophase). From late prophase throughout anaphase, 4.1R and tubulin are enriched in a crescent-shaped area and are intensely stained at the spindle and spindle poles (Fig. 1, Late prophase, Metaphase, Anaphase). At telophase, 4.1R was apparent in the cytoplasm as well as in the newly developed nuclei, whereas tubulin was mainly associated with midzone microtubules (Fig. 1, Telophase). No labeling was apparent when primary antibodies were replaced by pre-immune rabbit or mouse IgG or when anti-HP antibodies were pre-absorbed with its antigen (data not shown). We examined the endogenous 4.1R in ~100 interphase cells and ~50 cells in each stage of mitosis in three separate experiments. The anti-HP Ab consistently stained the endogenous 4.1R as shown in Fig. 1. Thus, the results suggest that 4.1R partially and reversibly co-localizes with tubulin in the cytoplasm of interphase cells and in the spindle and spindle poles during mitosis.



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  		FIG. 1.
Subcellular localization of 4.1R and tubulin at various stages of the HeLa cell cycle. HeLa cells were fixed and double stained for endogenous 4.1R and tubulin, and for nucleic acids (DNA). Green represents anti-HP epitopes, red represents anti-tubulin epitopes, yellow indicates the co-localization of 4.1R and tubulin, and blue represents DNA stained with DAPI. Bar, 10 µm.

 
Protein 4.1R Interacts with Tubulin in Vitro and in Mitotic Homogenates—The co-localization of 4.1R and tubulin at the spindle and spindle poles of mitotic cells prompted us to investigate whether mitotic 4.1R isoforms interact with microtubules. Our analysis of 4.1R mRNA expression in HeLa cells2 indicated that a 135-kDa isoform (4.1R135), containing all of the alternatively spliced exons except exons 3, 14, 15, 17a, and 17b, is a predominant isoform that is expressed in mitotic cells. To determine whether 4.1R135 interacts directly with microtubules, we used purified recombinant 4.1R135 protein and pure microtubules in microtubule sedimentation assays to analyze the interaction between 4.1R135 and tubulin. An 80-kDa 4.1R isoform (4.1R80) that has been shown to interact with microtubules (38) served as a positive control. Taxol-polymerized microtubules were incubated with recombinant 4.1R135 or 4.1R80 and sedimented through a 50% glycerol cushion. Although 4.1R135 and 4.1R80 alone did not sediment to the pellet (data not shown), both forms were readily detected in the pellet fraction with polymerized microtubules (Fig. 2B, pellet) but not in the supernatant fraction (Fig. 2B, sup), suggesting their interaction with microtubules in vitro. This interaction was specific: a well characterized MAP2 was bound to microtubules, whereas bovine serum albumin did not bind (data not shown).



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  		FIG. 2.
Interaction of 4.1R and microtubules in vitro and in GST pull-down assays using GST-4.1R and HeLa mitotic cell lysate. A, schematic representation of different domains of 4.1R: the HP, MBD, 16 kDa, SAB, and CTD. B, microtubule sedimentation assay with purified recombinant 4.1R135 or 4.1R80 and pure microtubules sedimented through a 50% glycerol cushion. Recovery of 4.1R in the microtubule pellet (pellet) fraction and the soluble supernatant (sup) fraction was fractionated on a 10% SDS-PAGE gel and determined by Coomassie Blue staining. C, purified GST-4.1R fusion proteins are visible by Coomassie Blue staining. D, GST pull-down was performed as described under "Experimental Procedures." After incubation of GST-4.1R fusion protein with mitotic HeLa cell lysate, the bound protein complexes were washed and analyzed by SDS-PAGE and visualized by immunoblotting with anti-{alpha}-tubulin antibody.

 
To confirm the specificity of the interaction between 4.1R and native tubulin in mitotic cells and to identify the domains of 4.1R responsible for the interaction, we performed a GST pull-down assay using homogenates of mitotic HeLa cells. We expressed either the full-length (135 and 80 kDa) of 4.1R or its individual domain (HP, MBD, 16 kDa, SAB, and CTD) (Fig. 2A) as GST fusion proteins (Fig. 2C). GST-HP migrated with an apparent molecular mass of ~80 kDa instead of the calculated ~55 kDa, most likely because of post-translational modification. Equivalent amounts of the GST fusions and control GST were bound to glutathione matrices and incubated with homogenates of HeLa mitotic lysates. After extensive washing, we used Western blotting to examine the matrix-bound GST fusion proteins for their ability to absorb native tubulin. Consistent with the in vitro sedimentation analysis, this blotting revealed that tubulin was specifically associated with the GST-4.1R135 and GST-4.1R80 (Fig. 2D). When individual domains were tested, only GST-MBD and GST-CTD specifically retained native tubulin (Fig. 2D), suggesting that the MBD and CTD of 4.1R are responsible for its binding to tubulin in mitotic HeLa cells. The binding between the MBD or CTD with native mitotic tubulin was specific in that GST alone did not interact with tubulin. At this time, we do not know what type of post-translational modification is involved in GST-HP. However, it appears that the modification at the HP region does not contribute to the tubulin binding ability of 4.1R, because both the 80-kDa isoform, without the HP, and the 135-kDa isoform, with the addition of the HP, bind to tubulin efficiently.

Protein 4.1R Is a Component of Mitotic Asters Assembled in a Cell-free Mitotic Extract—To determine whether 4.1R plays an active role in organizing the mitotic spindle assembly, we first asked whether 4.1R is a component of mitotic asters assembled in a well established in vitro mitotic aster assembly system (25, 30, 32). In addition to the spectrin-actin-4.1R ternary complex interaction (39, 40), 4.1R exhibits a binary interaction with spectrin (39, 41) or actin (42). We reduced actin polymerization and eliminated the possible interaction between actin and 4.1R by the addition of latrunculin B to mitotic extracts prior to the assembly process. Microtubules were induced to polymerize with 10 µM taxol in the presence of 2.5 mM ATP in the HeLa mitotic extract. Under incubation at 30 °C for 60 min, mitotic asters organized into aster-like arrays in a centrosome-independent process that is driven by microtubule motors and structural proteins. Mitotic asters assembled in this extract are composed of microtubules arranged in a radial array that contain NuMA at the central core (Fig. 3A, +ATP) (25). Consistent with the report of Gaglio and coworkers (33), the microtubules were arranged in poorly organized aggregates rather than astral arrays in the absence of ATP (Fig. 3A, –ATP). NuMA did not concentrate at the central core in these aggregates.



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  		FIG. 3.
Mitotic asters assembled in a cell-free mitotic extract. A, mitotic asters assembled under optimal conditions with taxol and with (+ATP) or without (–ATP) 2.5 mM ATP for 60 min at 30 °C and processed for indirect immunofluorescence using anti-{alpha}-tubulin (green) or anti-NuMA (red) antibodies. Co-localization of tubulin and NuMA is demonstrated through the superimposition of green and red. Bar, 5 µm. B, 4.1R is a mitotic microtubule-associated protein in the microtubule pellet. After a 60-min incubation, the extracts were subjected to centrifugation through a 50% sucrose cushion, separated into soluble (S), and insoluble (P) fractions, and subjected to immunoblotting using anti-NuMA, anti-HP, anti-dynactin, anti-dynein, anti-{alpha}-tubulin, and anti-actin antibodies.

 
We separated the asters from the soluble components of the extract by centrifugation through a 50% sucrose cushion, which allows for the sedimentation of microtubule asters with sufficient mass (32). Under this condition, a portion of 4.1R, but not actin, was co-sedimented with NuMA, dynactin, and tubulin (Fig. 3B, lane P); the latter three proteins are known to associate with microtubules in the microtubule pellet. The inclusion of latrunculin B and the use of 50% sucrose cushions eliminated the contamination of actin in the insoluble pellet (Fig. 3B, actin) and ruled out the possibility of 4.1R interacting with actin. These results demonstrate that 4.1R is a mitotic microtubule-associated protein.

The efficiency of the aster formation is calculated as the conversion of both NuMA and tubulin from a soluble form to an insoluble form (33) as judged by the amount of NuMA and tubulin sedimented into the pellet of the 50% sucrose cushion. It is worth noting that there is a high correlation between the morphology of the aster and the efficiency of aster formation. We standardized our assay conditions as described in the "Experimental Procedures" section and analyzed the asters formed from extracts that exhibit assembly efficiencies ranging between 70 to 85%. With such efficiency, we usually observed ~20 clear asters per field under a x100 oil objective. In each separate experiment, we viewed ~20 fields. Thus, a total of ~400 asters examined display approximately the same size and morphology as shown in Fig. 3A.

Protein 4.1R Is Required for Mitotic Aster Assembly in Vitro —To determine whether the formation of mitotic microtubule asters in synchronized mitotic HeLa extracts requires 4.1R, we examined whether the assembly of mitotic asters was perturbed by the depletion of 4.1R from the extract. In three successive depletions prior to the assembly reaction, the extracts were immunodepleted with 30 µg of affinity-purified anti-HP antibodies or purified pre-immune rabbit IgG. We used Western blotting to examine the degree to which 4.1R, as well as its associated proteins NuMA and tubulin, were depleted from the extracts. Pre-immune IgG did not immunodeplete any 4.1R, NuMA, or tubulin from the cell lysate, because each successive depletion showed that these proteins were absent in protein A Sepharose-bound fractions (Fig. 4A, Pre-immune depleted, lanes P-1, P-2, and P-3). Analysis of the supernatant fractions confirmed that 4.1R, NuMA, and tubulin were present in the supernatant in all three pre-immune IgG depletions (Fig. 4A, Pre-immune depleted, lanes Sup-1, Sup-2, and Sup-3). Anti-HP antibodies efficiently depleted ~95% of 4.1R and ~5% each of NuMA and tubulin in the first depletion (Fig. 4B, 4.1R-depleted, lane P-1). The second depletion removed the remaining ~5% of 4.1R and a small fraction of NuMA as well as tubulin (Fig. 4A, 4.1R-depleted, lane P-2). The third depletion did not remove any 4.1R, NuMA, or tubulin (Fig. 4A, 4.1R-depleted, lane P-3). 4.1R was completely absent from the final supernatant, whereas ~95% of NuMA and tubulin were still present in the final supernatant (Fig. 4A, 4.1R-depleted, lane Sup-3). The in vitro aster assembly was carried out using the supernatant from the third immunoprecipitation.



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  		FIG. 4.
Depletion of 4.1R from mitotic extract inhibited mitotic aster assembly in vitro. A, Western blot analysis of immunodepleted mitotic extracts. Extracts were successively depleted three times with 30 µg of pre-immune IgG or anti-HP antibodies. The degree of 4.1R depletion and co-depletion of NuMA and tubulin was determined by the presence of its respective protein in protein A-Sepharose-bound fractions as indicated (protein A-Sepharose-bound fractions are indicated by P-1, P-2, and P-3; unbound fractions by Sup-1, Sup-2, and Sup-3). For control, 25 µg of mitotic cell lysates was loaded. B, efficiency of aster assembly in mitotic extracts immunodepleted with rabbit preimmune IgG (Pre-immune) and anti-HP IgG (4.1R-depleted). The immunodepleted extracts were used to assemble asters in vitro. The same volumes of reaction mixtures were placed on coverslips and processed for indirect immunofluorescence using anti-{alpha}-tubulin (green) and anti-NuMA (red) antibodies. The merged yellow color indicates the superimposition of tubulin and NuMA. Bar, 5 µm.

 
We spotted equal amounts of assembly reactions from pre-immune-depleted and 4.1R-depleted extracts on coverslips and co-stained them for {alpha}-tubulin and NuMA to examine the efficiency of aster assembly. Three separate aster assemblies were performed. Treatment of the extracts with pre-immune rabbit IgG did not alter either the morphology of the mitotic asters or the distribution of the NuMA protein at the core of these structures (Fig. 4B, Pre-immune). The asters assembled from the pre-immune depleted lysates have similar size and morphology to the untreated control lysates. The assembly efficiency is also comparable to that of the control, in which ~20 asters were observed per field. We routinely examined ~400 asters per experiment.

However, depletion of 4.1R from the extract with the anti-HP antibody inhibited the assembly of the mitotic asters and yielded randomly arranged microtubules (Fig. 4B, 4.1R-depleted). There were no visible organized asters in all three experiments performed. The failure of aster assembly in the 4.1R-depleted extracts was apparently not due to indirect depletion of NuMA or {alpha}-tubulin, because Western blotting showed that the amounts of NuMA and {alpha}-tubulin were comparable in the control (Fig. 4A, Pre-immune depleted, lane Sup-3) and experimental (Fig. 4A, 4.1R-depleted, lane Sup-3) extracts. These results demonstrated that organization of microtubules into asters required 4.1R or a 4.1R-containing complex in a cell-free system.

To determine whether 4.1R is the functional component depleted from the extract using the anti-HP antibody, we tested whether the purified recombinant 4.1R protein would reconstitute mitotic aster formation in the 4.1R-depleted extracts. We first verified the amount of 4.1R to be added into the reconstruction assay by examining the number of copies of 4.1R135 in a single mitotic cell. For this reason, we immunoblotted known amounts of recombinant 4.1R-HP and serial dilutions of mitotic HeLa extract with anti-HP antibody (Fig. 5A). We used Photoshop to scan the anti-HP chemiluminograms and quantified the protein bands with the NIH Image software for the Macintosh computer. We estimate that each mitotic HeLa cell has ~5 x 104 copies of 4.1R135 (Fig. 5A). The amount of recombinant 4.1R135 at a concentration of 0.35 µg is equal to that of endogenous 4.1R135 from 3 x 107 mitotic HeLa cells.



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  		FIG. 5.
Reconstitution of mitotic aster formation in the 4.1R-depleted mitotic extract using the purified recombinant 135-kDa 4.1R. A, analysis of the number of copies of 4.1R135 expressed in mitotic HeLa cells. Known amount of GST-HP fusion protein were used as standards for the analysis of 4.1R expression in serial dilutions of mitotic HeLa lysates. Both standard and HeLa lysate blots were probed with anti-HP antibody. The anti-HP chemiluminograms were scanned using Photoshop, and the protein bands were quantified using NIH Image software for Macintosh. B, mitotic asters were assembled in the 4.1R-depleted mitotic extract under optimal conditions with taxol and ATP at 30 °C. At initiation of microtubule polymerization, the purified recombinant 4.1R protein was added in amounts equivalent to one time (1X), five times (5X), or 10 times (10X) endogenous 4.1R. The samples were then processed for indirect immunofluorescence with anti-{alpha}-tubulin (green) or anti-NuMA (red) antibodies. Approximately 20 asters per field were assembled from all of the reconstitution assays. A total of ~400 asters per sample were examined. Bar, 5 µm. C, after 60 min of incubation, the extracts that were supplemented with recombinant 4.1R135 equivalent to (1X) or 5 times (5X) the amount of endogenous 4.1R were centrifuged through a 50% sucrose cushion and separated into soluble (S) and insoluble (P) fractions and subjected to immunoblotting using anti-HP 4.1, anti-{alpha}-tubulin, and anti-NuMA antibodies. To avoid overloading of 4.1R from the 5X sample, only one-fifth of the supernatant was loaded in the 4.1R lane.

 
The reconstitution assays were performed using extracts isolated from 3 x 107 mitotic HeLa cells that have been subjected to immunodepletion with anti-HP antibodies. Supplementation of the 4.1R-depleted extract with purified recombinant 4.1R135 at concentrations equivalent to 1- to 10-fold of endogenous 4.1R135 restored mitotic aster formation (Fig. 5B, 1X). The reconstituted assembly reactions exhibited ~75% assembly efficiency and resulted in ~20 asters per field. The addition of recombinant 4.1R135 to the 4.1R-depleted extract at quantities exceeding normal endogenous levels (5 times and 10 times molar excess) did not appear to increase the number of aster formations or alter the morphology of the asters (Fig. 5B, 5X and 10X). When centrifuged through a 50% sucrose cushion, recombinant 4.1R135 was recovered along with NuMA and tubulin from the mitotic microtubule pellets (Fig. 5C). These results suggest that a 135-kDa 4.1R isoform is required for mitotic aster formation in a cell-free system.

Protein 4.1R and Tubulin Associate in Vivo —The co-localization of 4.1R and tubulin at the spindle and spindle poles, the interaction of 4.1R with microtubules in vitro, and the involvement of 4.1R in mitotic aster assembly prompted us to investigate whether the native 4.1R can associate with native tubulin in vivo. We performed co-immunoprecipitation assays using mitotic extracts from highly synchronized HeLa cells with anti-HP or anti-{alpha}-tubulin antibodies. Anti-NuMA mAb, known to co-immunoprecipitate with 4.1R (20) and tubulin (37), and pre-immune rabbit IgG served as positive and negative controls, respectively. Immunoblot staining using anti-4.1R (anti-HP and anti-exon 13), anti-{alpha}-tubulin, or anti-NuMA antibodies revealed co-precipitated polypeptides (Fig. 6, Bound, upper panel) and their supernatants (Fig. 6, Unbound, lower panel). Anti-HP antibody efficiently immunoprecipitated a 135-kDa 4.1R isoform (Fig. 6A, {alpha}-HP, lane {alpha}-HP), whereas control rabbit IgG did not precipitate any immunoreactive band (Fig. 6A, {alpha}-HP, lane Pre-immune). Analysis of anti-tubulin and anti-NuMA immunoprecipitates for the presence of 4.1R allowed ready detection of a 135-kDa 4.1R isoform in both immunoprecipitates, although at much less intensity (Fig. 6A, {alpha}-HP, lanes {alpha}-tubulin and {alpha}-NuMA). These results suggest that a 135-kDa 4.1R isoform occurs in vivo in a complex with NuMA and tubulin.



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  		FIG. 6.
Co-immunoprecipitation of 4.1R, tubulin, and NuMA from HeLa mitotic extracts. HeLa mitotic extracts were prepared as described under "Experimental Procedures" and were subjected to immunoprecipitation using rabbit preimmune IgG, anti-HP, anti-{alpha}-tubulin mAb, and anti-NuMA mAb. Immunoprecipitate analysis entailed immunoblotting using anti-HP Ab (A), anti-{alpha}-tubulin mAb (B), anti-NuMA mAb (C), or anti-exon 13 Ab (D). The arrows denote the migration position of the 135-kDa 4.1R isoform (A and D), tubulin (B), and NuMA (C). One-third of the immunoprecipitates (Bound) and one-eighth of the supernatant fractions (Unbound) were loaded onto the lanes as indicated. For control, 25 µg of cell lysates was loaded.

 
We further confirmed the association of 4.1R, NuMA, and tubulin by blotting the immunoprecipitates with anti-{alpha}-tubulin or anti-NuMA antibodies. Analysis of a duplicated co-precipitated blot using anti-{alpha}-tubulin antibody revealed a strong immunoreactive tubulin band from anti-tubulin immunoprecipitates and a less intense tubulin band from both anti-HP and anti-NuMA precipitates (Fig. 6B, {alpha}-tubulin, upper panel). Similarly, the anti-NuMA antibody detected a strong immunoreactive NuMA band from anti-NuMA precipitates and a less intense band from both anti-HP and anti-tubulin precipitates (Fig. 6C, {alpha}-NuMA, upper panel). In keeping with our earlier report (20) and that of Gregson and associates (31), our results indicate that NuMA and 4.1R as well as NuMA and tubulin co-precipitated in a complex in vivo. These results also demonstrate that 4.1R, tubulin, and NuMA associate together during the mitotic stage of the cell cycle. The co-precipitation of tubulin by anti-HP antibodies, the detection of 4.1R that co-precipitated with tubulin by anti-HP antibodies, and the molecular mass of the 4.1R isoform that co-precipitates with tubulin all suggest that a 135-kDa 4.1R isoform derived from the upstream translation initiation site associates with tubulin in vivo.

To examine the possible interaction of other isoforms of 4.1R with tubulin, we used a second antibody specific to 4.1R to examine immunoprecipitates of anti-tubulin mAb. A constitutively expressed exon 13 within the 16-kDa domain has been shown to be unique to 4.1R. Exon 13 does not exhibit sequence homology with other 4.1 family members (8–11), so we used an exon 13-specific antibody to examine 4.1R isoforms that interact with tubulin. We included rabbit pre-immune IgG and anti-NuMA mAb immunoprecipitates as controls. Anti-exon 13 antibody did not detect any band from the pre-immune precipitates, whereas anti-HP precipitates showed a strong 135-kDa 4.1R band (Fig. 6D, {alpha}-exon 13, lanes Pre-immune and {alpha}-HP, upper panel). Consistent with our previous report (20) that a 135-kDa 4.1R isoform associates with NuMA in a mitotic complex, anti-exon 13 detected a 135-kDa 4.1R in NuMA immunoprecipitates (Fig. 6D, {alpha}-exon 13, lane {alpha}-NuMA, upper panel). Analysis of anti-tubulin immunoprecipitates with the anti-exon 13 Ab (Fig. 6D, {alpha}-exon 13, lane {alpha}-tubulin, upper panel) revealed an immunoreactive band of 135 kDa. These data further suggest that a 135-kDa isoform of 4.1R interacts with tubulin and NuMA in mitotic HeLa cells.

The results obtained so far suggest that a small fraction of a 135-kDa 4.1R isoform occurs in vivo in a complex with a small fraction of the mitotic apparatus proteins tubulin and NuMA. To estimate what fractions of 4.1R and tubulin associate together, we determined the efficiencies of immunoprecipitation and co-precipitation by analyzing both the protein A Sepharose-bound (Fig. 6, Bound) and unbound (Fig. 6, Unbound) fractions. We used cell lysates from 107 mitotic cells with 10 µg each of anti-HP, anti-{alpha}-tubulin, and anti-NuMA IgGs for each immunoprecipitation assay. Quantitation from three separate experiments shows that ~80% of 4.1R was precipitated by anti-HP Ab that co-precipitated ~1% of tubulin and that ~50% of tubulin was precipitated by anti-tubulin mAb, which in turn brought down ~5% of 4.1R. Consistent with our previous report (20), 4.1R and NuMA co-immunoprecipitated with limited efficiency; ~50% of NuMA was precipitated by anti-NuMA mAb that brought down ~5% 4.1R. The lower efficiency of co-immunoprecipitation compared with immunoprecipitation suggests that only a fraction of these molecules associate together in vivo. This is consistent with our immunofluorescent staining results, suggesting that subpopulations of 4.1R and tubulin partially co-localize together.


   DISCUSSION
TOP
 ABSTRACT
 INTRODUCTION
 EXPERIMENTAL PROCEDURES
 RESULTS
 DISCUSSION
REFERENCES
 
Protein 4.1R has been known to localize at the spindle and spindle poles of mitotic cells (17, 19, 20); however, little is known about the topography and relation of 4.1R to the major constituent of the mitotic apparatus, the microtubules, or about its function in spindle/spindle poles. In this report, we demonstrate that 4.1R co-localizes with microtubules at the mitotic spindle and spindle poles, co-sediments with microtubules in vitro, co-immunoprecipitates with tubulin in vivo, and associates with tubulin in mitotic HeLa cell extracts through its MBD and CTD. Furthermore, we show that 4.1R is a mitotic microtubule-associated protein and is essential to mitotic aster assembly in vitro in a cell-free extract prepared from synchronized HeLa cells. Based on these results, we propose that non-erythroid 4.1R may contribute to the organization of mitotic spindles.

The cell cycle-dependent localization of 4.1R is unique; it localizes to the nucleus and cytoplasm during interphase and redistributes to the spindle poles during mitosis, at which point 4.1R partially co-localizes with two major constituents of the mitotic apparatus, NuMA, and microtubules. We (20) previously showed that 4.1R directly interacts with NuMA through its C-terminal domain and forms a complex with the spindle pole-organizing proteins NuMA, dynein, and dynactin during cell division. We now show that, in addition to its interaction with NuMA, 4.1R interacts with tubulin in mitotic cells and is a mitotic microtubule-associated protein. It has been previously documented that purified 4.1R from red blood cells interacts specifically with the C-terminal domain of tubulin (38). In human T cells, 4.1R isoforms lacking exon 16 co-localize and interact with interphase microtubules through a 22-amino acid sequence located within exon 10 of the MBD domain (13). Consistent with these reports, our immunofluorescent staining showed a partial co-localization of 4.1R and tubulin in interphase HeLa cells, and in vitro sedimentation experiments confirmed the interaction of an erythrocyte 4.1R80 isoform with purified microtubules. Moreover, we showed that a major HeLa 4.1R135 isoform containing all of the alternatively spliced exons except exons 3, 14, 15, 17a, and 17b2 also sedimented with purified microtubules. Furthermore, we demonstrated that both 4.1R80 and 4.1R135 isoforms associate with tubulin in a GST pull-down assay using HeLa mitotic extracts. In contrast to the interaction of 4.1R isoforms with interphase T-cell tubulin (13), an interaction that requires only the MBD, we found that both the MBD and the CTD of 4.1R contribute to its binding to tubulin in HeLa mitotic extracts. Post-translational modifications of tubulin have been shown to regulate its association with microtubule-associated proteins (43). Polyglutamylated tubulin was detected in proliferating cells of different origins (HeLa, KE37, and NIH 3T3), where it associates with the centrioles, the spindle, and the midbody (44). The localization of 4.1R coincides with that of tubulin during mitosis; thus, it is possible that the post-translational modification of tubulin in mitotic cells might facilitate their selective recruitment of 4.1R isoforms through their MBD as well as their CTD into distinct microtubule populations, hence modulating their functional properties.

Alternatively, a third protein may be involved in the indirect interaction of mitotic tubulin and the CTD of 4.1R. A good candidate protein is NuMA, because NuMA interacts with tubulin through amino acids 1868–1967 (37) and with the CTD of 4.1R through amino acids 1788–1810 (20). This suggests that the same population of NuMA may link 4.1R molecules to tubulin; thus, these proteins can form a three-way complex. Using a complementary assay, co-immunoprecipitation, we also demonstrated that 4.1R appears to interact in vivo with NuMA as well as with tubulin. However, binary interactions between NuMA and tubulin also occur; the depletion of 4.1R from the mitotic HeLa extracts did not dissociate the interaction of NuMA and tubulin, as shown through their association in randomly dispersed microtubules assembled in 4.1R-immunodepleted extracts (see Fig. 4B, 4.1R-depleted). Further experiments are required to determine whether 4.1R associates with NuMA and tubulin simultaneously or individually. Nevertheless, the association of 4.1R, NuMA, and tubulin suggests that 4.1R may play a role in organizing mitotic spindles.

Centrosome-free spindle-pole formation that depends on the action of non-centrosomal structural and microtubule motor proteins was directly demonstrated during spindle assembly in extracts from metaphase-arrested frog eggs (45). Dynein-dependent and centrosome-free spindle-pole formation was mimicked by the induction of microtubule asters in the presence of the drug taxol in both Xenopus (46) and mammalian systems (25). An in vitro aster assembly assay using HeLa mitotic extracts, an assay that recapitulates many of the structural events in mitosis, has been used widely to characterize the function of a number of proteins localized at the spindle poles (29–33). We used this assay to show that mitotic aster assembly was inhibited in a 4.1R depletion-specific manner and that assembly could be re-initiated with purified recombinant 4.1R135. These results suggest that 4.1R is essential to the assembly of mitotic asters in vitro.

Our immunoprecipitation/co-precipitation assays showed that only a subpopulation of NuMA and {alpha}-tubulin interacts with 4.1R. Consistent with these results, the immunodepletion assays further confirmed that 4.1R antibodies failed to co-deplete significant amounts of NuMA and {alpha}-tubulin. These results imply that aster assembly is not abolished because of the lack of NuMA or {alpha}-tubulin. This idea is further supported by the observation that NuMA still associates with the irregularly shaped microtubules in the 4.1R-depleted assembly reactions. Thus, depletion of 4.1R does not seem to affect the association of NuMA with tubulin. Rather, recruitment of 4.1R to the astral arrays by tubulin and/or NuMA could be functionally necessary for assembly or maintenance of astral arrays.

The biological significance of 4.1R in centrosome-dependent spindle-pole formation in somatic cells is unclear. 4.1R might stabilize the interaction among NuMA, dynein, dynactin, and microtubules in a manner analogous to its role in the stabilization of the association of spectrin, actin, and integral proteins in red blood cells. Viable homozygous 4.1R knockout mice have been generated (47). The viability of these mice is perplexing, given the wide tissue distribution of 4.1R and its possible involvement in cell division. However, it is not unprecedented that germ line alterations that activate or inactivate genes of interest might have effects other than somatic mutations because of developmental compensation (48, 49). For example, the acute loss of Rb in primary quiescent cells has phenotypic consequences that differ from germ line loss of Rb function (50). In cell division, the function of 4.1R in 4.1R null mice may be sustained by redundant systems and might involve other 4.1 family members. It is worth noting that 4.1B does not express in HeLa cells, and 4.1N expresses in minute amounts. 4.1G is highly expressed in HeLa. Therefore, 4.1G would be the most likely candidate for redundancy. We2 note that a complicated transcription coupling splicing mechanism exists in 4.1 family members. Further identification of the 4.1G or N isoforms most likely to be involved in mitosis is necessary to assess the possible functional redundancy of these 4.1 family members. Regardless, the ability of 4.1R to interact with mitotic tubulin and the fact that mitotic aster assembly in vitro requires 4.1R suggest that 4.1R may be pivotal to the structural organization and maintenance of the mitotic apparatus during cell division. This idea is supported by an in vitro aster assembly assay using Xenopus egg extracts (51) that indicates that the SAB and CTD peptides significantly deranged the normal symmetrical microtubule array and dispersed the tight focus of NuMA. Furthermore, small interference RNA-caused knockout of 4.1R in HeLa cells also resulted in poorly focused spindle poles in mitotic cells.2 Additional work will establish the precise role of cytoskeletal 4.1R in the mechanochemistry of the mitotic spindle. This report, however, suggests that 4.1R is crucial and is related to mitotic tubulin binding.


   FOOTNOTES
 
* This work was supported by National Institutes of Health Grants HL61295 (to S.-C. H.) and HL44985 (to E. J. B.). The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact. Back

To whom correspondence should be addressed: Dept. of Medical Oncology, Dana Farber Cancer Institute, D610, 44 Binney St., Boston, MA 02115. Tel.: 617-632-6965; Fax: 617-632-2662; E-mail: shu-ching_huang{at}dfci.harvard.edu.

1 The abbreviations used are: MBD, membrane-binding domain; NuMA, Nuclear Mitotic Apparatus protein; SAB, spectrin/actin binding; CTD, C-terminal domain; HP, head-piece; GST, glutathione S-transferase; DTT, dithiothreitol; Ab, rabbit polyclonal antibodies; mAb, mouse monoclonal antibodies; CHAPS, 3-[(3-cholamidopropyl)dimethylammonio]-1-propanesulfonic acid. Back

2 S.-C. Huang, E. S. Liu, S.-H. Chan, I. D. Munagala, H. T. Cho, and E. J. Benz, Jr., unpublished data. Back


   ACKNOWLEDGMENTS
 
We thank Julia Hartenstein and Dr. Siu-Hong Chan for their early studies that contributed to this work. We acknowledge Indira Munagala for her assistance with the analysis of number copies of 4.1R in mitotic HeLa cells. We thank Drs. Narla Mohandas and Xiuli An (New York Blood Center) for providing a 4.1R/pET-31b(+) construct and the procedure for the purification of 4.1R from pET-31b(+) vector.



   REFERENCES
TOP
 ABSTRACT
 INTRODUCTION
 EXPERIMENTAL PROCEDURES
 RESULTS
 DISCUSSION
 REFERENCES
 

  1. Benz, E. J., Jr. (1994) in The Molecular Basis of Blood Diseases (Stamatoyannopoulos, G., Neinhuis, A. W., Majerus, P., Varmus, H., eds) 2nd Ed., pp. 257–292
  2. Parra, M. K., Gee, S. L., Koury, M. J., Mohandas, N., and Conboy, J. G. (2003) Blood 101, 4164–4171[Abstract/Free Full Text]
  3. Conboy, J. G., Chan, J., Mohandas, N., and Kan, Y. W. (1988) Proc. Natl. Acad. Sci. U. S. A. 85, 9062–9065[Abstract/Free Full Text]
  4. Tang, T. K., Quin, Z., Marchesi, V. T., and Benz, E. J., Jr. (1990) J. Cell Biol. 110, 617–624[Abstract/Free Full Text]
  5. Huang, S. C., Baklouti, F., Tang, T. K., and Benz, E. J., Jr. (1992) Trans. Assoc. Am. Phys. Vol. CV, 165–171
  6. Chasis, J. A., Coulombel, L., McGee, S., Lee, G., Tchernia, G., Conboy, J. G., and Mohandas, N. (1996) Blood 87, 5324–5331[Abstract/Free Full Text]
  7. Subrahmanyam, G., Bertics, P. J., and Anderson, R. A. (1991) Proc. Natl. Acad. Sci. U. S. A. 88, 5222–5226[Abstract/Free Full Text]
  8. Walensky, L. D., Blackshaw, S., Liao, D., Watkins, C. C., Weier, H. U., Parra, M., Huganir, R. L., Conboy, J. G., Mohandas, N., and Snyder, S. H. (1999) J. Neurosci. 19, 6457–6467[Abstract/Free Full Text]
  9. Ohara, R., Yamakawa, H., Nakayama, M., Yuasa, S., and Ohara, O. (1999) Brain Res. Dev. Brain Res. 117, 127–138[CrossRef][Medline] [Order article via Infotrieve]
  10. Tran, Y. K., Bogler, O., Gorse, K. M., Wieland, I., Green, M. R., Newahsm, I. F. (1999) Cancer Res. 59, 35–43[Abstract/Free Full Text]
  11. Parra, M., Gascard, P., Walensky, L. D., Gimm, J. A., Blackshaw, S., Chan, N., Takakuwa, Y., Berger, T., Lee, G., Chasis, J. A., Snyder, S. H., Mohandas, N., and Conboy, J. G. (2000) J. Biol. Chem. 275, 3247–3255[Abstract/Free Full Text]
  12. Ramez, M., Blot-Chabaud, M., Cluzeaud, F., Chanan, S., Patterson, M., Walensky, L. D., Marfatia, S., Baines, A. J., Chasis, J. A., Conboy, J. G., Mohandas, N., and Gascard, P. (2003) Kidney Int. 63, 1321–1337[CrossRef][Medline] [Order article via Infotrieve]
  13. Perez-Ferreiro, C. M., Luque, C. M., and Correas, I. (2001) J. Biol. Chem. 276, 44785–44791[Abstract/Free Full Text]
  14. Kontrogianni-Konstantopoulos, A., Huang, S. C., and Benz, E. J., Jr. (2000) Mol. Biol. Cell 11, 3805–3817[Abstract/Free Full Text]
  15. Mattagajasingh, S. N., Huang, S. C., Hartenstein, J. S., and Benz, E. J., Jr. (2000) J. Biol. Chem. 275, 30573–30585[Abstract/Free Full Text]
  16. De Carcer, G., Lallena, M. J., and Correas, I. (1995) Biochem. J. 312, 871–877
  17. Krauss, S. W., Larabell, C. A., Lockett, S., Gascard, P., Penman, S., Mohandas N., and Chasis, J. A. (1997) J. Cell Biol. 137, 275–289[Abstract/Free Full Text]
  18. Lallena, M. J., and Correas, I. (1997) J. Cell Sci. 110, 239–247[Abstract]
  19. Krauss, S. W., Chasis, J. A., Rogers, C., Mohandas, N., Krockmalnic, G., and Penman, S. (1997) Proc. Natl. Acad. Sci. U. S. A. 94, 7297–7302[Abstract/Free Full Text]
  20. Mattagajasingh, S. N., Huang, S. C., Hartenstein, J. S., Snyder, M., Marchesi, V. T., and Benz, E. J., Jr. (1999) J. Cell Biol. 145, 29–43[Abstract/Free Full Text]
  21. Merdes, A., Ramyar, K., Vechio, L. D., and Cleveland, D. W. (1996) Cell 87, 447–458[CrossRef][Medline] [Order article via Infotrieve]
  22. Heidemann, S. R., and McIntosh, J. R. (1980) Nature 286, 517–519[CrossRef][Medline] [Order article via Infotrieve]
  23. McIntosh, J. R., and Euteneuer, U. (1984) J. Cell Biol. 98, 525–533[Abstract/Free Full Text]
  24. Compton, D. A. (2000) Annu. Rev. Biochem. 69, 95–114[CrossRef][Medline] [Order article via Infotrieve]
  25. Gaglio, T., Dionne, M. A., and Compton, D. A. (1997) J. Cell Biol. 138, 1055–1066[Abstract/Free Full Text]
  26. Rusan, N. M., Tulu, U. S., Fagerstrom, C., and Wadsworth, P. (2002) J. Cell Biol. 158, 997–1003[Abstract/Free Full Text]
  27. Quintyne, N. J., Gill, S. R., Eckley, D. M., Crego, C. L., Compton, D. A., and Schroer, T. A. (1999) J. Cell Biol. 147, 321–334[Abstract/Free Full Text]
  28. Whitehead, C. M., and Rattner, J. B. (1998) J. Cell Sci. 111, 2551–2561[Abstract]
  29. Mountain, V., Simerly, C., Howard, L., Ando, A., Schatten, G., and Compton, D. A. (1999) J. Cell Biol. 147, 351–366[Abstract/Free Full Text]
  30. Dionne, M. A., Sanchez, A., and Compton, D. A. (2000) J. Biol. Chem. 275, 12346–12352[Abstract/Free Full Text]
  31. Gregson, H. C., Schmiesing, J. A., Kim, J. S., Kobayashi, T., Zhou, S., and Yokomori, K. (2001) J. Biol. Chem. 276, 47575–47582[Abstract/Free Full Text]
  32. Mack, G. J., and Compton, D. A. (2001) Proc. Natl. Acad. Sci. U. S. A. 98, 14434–14439[Abstract/Free Full Text]
  33. Gaglio, T., Saredi, A., and Compton, D. A. (1995) J. Cell Biol. 131, 693–708[Abstract/Free Full Text]
  34. Tang, T. K., Leto, T. L., Correas, I., Alonso, M. A., Marchesi, V. T., and Benz, E. J., Jr. (1988) Proc. Natl. Acad. Sci. U. S. A. 85, 3713–3717[Abstract/Free Full Text]
  35. Baklouti, F., Huang, S. C., Vulliamy, T. J., Delaunay, J. D., and Benz, E. J., Jr. (1997) Genomics 39, 289–302[CrossRef][Medline] [Order article via Infotrieve]
  36. O'Conner, P. M., and Jackman, J. (1995) in Cell Cycle: Experimental Procedures (Pogans, M., ed) pp. 63–74 Springer-Verlag, New York
  37. Haren, L., and Merdes, A. (2002) J. Cell Sci. 115, 1815–1824[Abstract/Free Full Text]
  38. Correas, I., and Avila, J. (1988) Biochem. J. 255, 217–221[Medline] [Order article via Infotrieve]
  39. Discher, D. E., Winardi, R., Schischmanoff, P. O., Parra, M., Conboy, J. G., and Mohandas, N. (1995) J. Cell Biol. 130, 897–907[Abstract/Free Full Text]
  40. Kontrogianni-Konstantopoulos, A., Frye, C. S., Benz, E. J., Jr., and Huang, S. C. (2001) J. Biol. Chem. 276, 20679–20687[Abstract/Free Full Text]
  41. Schischmanoff, P. O., Winardi, R., Discher, D. E., Parra, M. K., Bicknese, S. E., Witkowska, H. E., Conboy, J. G., and Mohandas, N. (1995) J. Biol. Chem. 270, 21243–21250[Abstract/Free Full Text]
  42. Gimm, J. A., An, X., Nunomura, W., and Mohandas, N. (2002) Biochemistry 41, 7275–7282[CrossRef][Medline] [Order article via Infotrieve]
  43. Bonnet, C., Boucher, D., Lazereg, S., Pedrotti, B., Islam, K., Denoulet, P., and Larcher, J. C. (2001) J. Biol. Chem. 276, 12839–12848[Abstract/Free Full Text]
  44. Bobinnec, Y., Moudjou, M., Fouquet, J.-P., Desbruyeres, E., Edde, B., and Bornens, M. (1998) Cell Motil. Cytoskel 39, 223–232[CrossRef][Medline] [Order article via Infotrieve]
  45. Heald, R., Tournebize, R., Blank, T., Sandaltzopoulos, R., Becker, P., Hyman, A., and Karsenti, E. (1996) Nature 382, 420–425[CrossRef][Medline] [Order article via Infotrieve]
  46. Verde, F., Berrez, J. M., Antony, C., and Karsenti, E. (1991) J. Cell Biol. 112, 1177–1187[Abstract/Free Full Text]
  47. Shi, Z. T., Afzal, V., Coller, B., Patel, D., Chasis, J. A., Parra, M., Lee, G., Paszty, C., Stevens, M., Walensky, L., Peters, L. L., Mohandas, N., Rubin, E., and Conboy, J. G. (1999) J. Clin. Invest. 103, 331–340[Medline] [Order article via Infotrieve]
  48. Jonkers, J., and Berns, A. (2002) Nat. Rev. Cancer 2, 251–265[CrossRef][Medline] [Order article via Infotrieve]
  49. Van Dyke, T., and Jacks, T. (2002) Cell 108, 135–144[CrossRef][Medline] [Order article via Infotrieve]
  50. Sage, J., Miller, A. L., Perez-Mancera, P. A., Wysocki, J. M., and Jacks, T. (2003) Nature 424, 223–228[CrossRef][Medline] [Order article via Infotrieve]
  51. Krauss, S. W., Lee, G., Chasis, J. A., Mohandas, N., and Heald, R. (2004) J. Biol. Chem. 279, 27591–27598[Abstract/Free Full Text]

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