Dictyostelium dynamin B modulates cytoskeletal structures and membranous organelles
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Dictyostelium discoideum cells produce five dynamin family proteins. Here, we show that dynamin B is the only member of this group of proteins that is initially produced as a preprotein and requires processing by mitochondrial proteases for formation of the mature protein. Our results show that dynamin B-depletion affects many aspects of cell motility, cell-cell and cell-surface adhesion, resistance to osmotic shock, and fatty acid metabolism. The mature form of dynamin B mediates a wide range and unique combination of functions. Dynamin B affects events at the plasma membrane, peroxisomes, the contractile vacuole system, components of the actin-based cytoskeleton, and cell adhesion sites. The modulating effect of dynamin B on the activity of the contractile vacuole system is unique for the Dictyostelium system. Other functions displayed by dynamin B are commonly associated with either classical dynamins or dynamin-related proteins.
KeywordsDictyostelium discoideum Dynamin Presequence Peroxisome Fission Cell adhesion
Differential interference contrast microscopy
GTPase effector domain
Green fluorescent protein
Mitochondrial targeting sequence
N-terminal sequence or presequence
Proline rich domain
Peroxisomal targeting signal of type 1
Reflection interference contrast microscopy
Total internal reflection fluorescence
Yellow fluorescent protein
Dynamins are high molecular weight GTP-binding proteins with high intrinsic GTPase activity [1, 2, 3]. Classical dynamins comprise five well-defined domains: an N-terminal GTPase domain, a middle domain, a pleckstrin homology (PH) domain, a GTPases effector domain (GED), and a C-terminal proline-rich domain (PRD) . Their function has been best studied in the context of the budding and scission of nascent vesicles from parent membranes [4, 5, 6, 7, 8]. Additional cellular functions include roles in actin-dependent membrane processes, the formation of cell surface extensions, and focal adhesion dynamics [9, 10].
Dynamin-related proteins lack a PRD and a PH domain. They have been classified into several subfamilies such as dynamin-like proteins (Dlps), OPA1/Mgm1p-like proteins, Mx proteins, mitofusins, and guanylate-binding proteins/atlastins . All eukaryotic organisms studied so far possess at least a single dynamin-related protein that is involved in the division of mitochondria and peroxisomes [11, 12, 13]. It was shown for instance that mutations in yeast Dnm1 and human Drp1 strongly affect the distribution of mitochondria, but have little or no effect on membrane trafficking [11, 14, 15]. The mechanism by which these proteins control fission of mitochondria may be similar to that employed by dynamin 1 during vesicle formation . Yeast Dnm1p, the plant dynamin-related proteins ADL2b, DRP3A and DRP3B, and mammalian Drp1 were shown to play a role in peroxisomal as well as mitochondrial fission [13, 17, 18, 19, 20, 21].
Several members of the dynamin superfamily are initially produced with an N-terminal leader sequences targeting them to mitochondria . Members of this family localize to the space between the outer and inner mitochondrial membranes and play a role in fission or fusion of mitochondria, remodeling of the mitochondrial inner membrane, and cristae formation [22, 23]. The yeast dynamin-related protein Mgm1p, which is involved in mitochondrial fusion [24, 25], is an integral inner membrane protein facing the intermembrane space. Mgm1p is released into the intermembrane space after limited proteolysis by the mitochondrial rhomboid protease [26, 27]. Similarly, the human orthologue of Mgm1p, OPA1, was demonstrated to be tightly bound to the outer surface of the inner membrane [23, 28]. Downregulation of OPA1 in cultured cells leads to mitochondrial fragmentation, disruption of cristae structure, and consequent apoptosis.
Five members of the dynamin family were found in the social amoeba Dictyostelium discoideum: dynamin A (dymA), dynamin B (dymB), dynamin-like protein A (dlpA), dynamin-like protein B (dlpB), and dynamin-like protein C (dlpC). Dynamin A acts in membrane trafficking along the endo-lysosomal pathway, similar to the function of classical dynamins in higher eukaryotic cells . The structure of dynamin A was studied in detail, leading to an atomic resolution model of its GTPase domain  and lower resolution EM-structures of the dynamin A ring complex in the presence and absence of nucleotide . Dynamin-like proteins A, B, and C are closely related to one another, and resemble plant proteins with a role in cytokinesis and chloroplast division. The disruption of each individual gene results in abnormal cytokinesis .
Here we describe the post-translational processing of dynamin B and the cellular localization and function of the protein. Studies with cells producing altered amounts of dynamin B indicate a role in peroxisome biogenesis, maturation, and fission. Additionally, dynamin B is shown to have a modulating effect on cell adhesion, the dynamics of actin-rich structures in the cell periphery, and contractile vacuole function.
Materials and methods
Plasmids generated and used in this study are described below. The dynamin B gene contains no introns (GenBank accession no. XP_642447), and was amplified directly from genomic DNA and cloned between the SacI and XhoI sites of vector pDXA-HY and pDXA-3H . The resulting plasmids pDXA-dynamin B and pC-dynamin B encode the full-length protein with N-terminal and C-terminal histidine tags, respectively. pΔNTS-dynamin B was constructed in the same way as pC-dynamin B, but using a dynamin B gene fragment lacking the first 408 base pairs.
We generated fusions with a C-terminal YFP by cloning gene fragments encoding full-length dynamin B, ΔNTS-dynamin B, and the 136 residues presequence (NTS) between the SacI and XbaI sites of pDXAmcsYFP . The resulting plasmids are pDynamin B-YFP, pΔNTS-dynamin B-YFP, and pDXA/NTSYFP. Plasmid pDNeoGFP-PTS1, encoding a GFP construct with a C-terminal PTS1 tag that specifically targets GFP to peroxisomes, was a kind gift from Dr. M. Maniak.
The generation of dymB knock-out construct pE1-ΔdymB required several steps. A genomic fragment released upon digestion with EcoRI containing the first 1,466 base pairs of dynamin B coding sequence and around 1,500 base pairs of 5′UTR was cloned in pBluescript (Stratagene) giving plasmid pE1. pE1 was cut with Pst I/Xba I and religated to remove the Spe I site within the MCS (multiple cloning site). A 0.4-kb fragment, corresponding to the central part of the GTPase domain, was excised from the resulting plasmid pE1-ΔSpe I by Spe I/Nsi I digestion. The Spe I/Nsi I fragment (base pairs 613–1,020) was replaced by the 1.4-kb blasticidin S resistance cassette that had been excised by HindIII/XbaI digestion from vector pBsr2 . The linearized replacement construct was transformed into AX2 cells. Transformations of D. discoideum cells with gene replacement constructs were carried out as described .
Antibody production and immunoblot analysis
A peptide of dynamin B containing amino acid residues from 369 to 523 was produced as hexa-histidine tagged protein in E. coli and purified by Ni–NTA chromatography (Qiagen). The peptide was used to generate polyclonal rabbit antisera against dynamin B. Antibodies were affinity purified using the purified dynamin B fragment coupled to Affi-Gel 10 (BioRad). The antiserum was diluted with TBS (PBS containing 0.05% TWEEN 20) and incubated under agitation with gel matrix overnight. The gel was washed with TBS, and antibodies were eluted with 100 mM glycine pH 2.5. The eluate was immediately neutralized with 1M Tris-HCl pH 8.0, BSA was added as stabilizer, and the solution was concentrated using Centricon 50 spin columns (Amicon).
For immunoblotting, D. discoideum proteins from wild-type and mutant strains were separated on 8% SDS-PAGE gels and transferred to a nitrocellulose membrane (Schleicher and Schuell). Membranes were blocked in TBS containing 5% non-fat dry milk powder for 1 h and incubated with 1:1,000 dilution of affinity purified anti-dynamin B antibody in the same buffer for either 1 h at room temperature or overnight at 4°C, followed by detection with an HRP-conjugated secondary antibody and ECL performed according to the manufacturer’s instructions (Pierce).
Cell culture of D. discoideum
D. discoideum AX2 cells were used throughout this work, unless otherwise indicated. Cells were grown on plates or in culture flasks stirred at 180 rpm at 21°C in HL5C media (ForMedium). Fatty acids (Sigma-Aldrich) were added to the media from ethanol stocks and mixed by vortexing followed by ultrasonication for 5 min in warm water. Identical concentrations of ethanol (usually less than 0.5%) were added as controls.
D. discoideum cells were transformed with expression constructs by electroporation, and transformants were selected in the presence of appropriate antibiotics as described . Selection was performed using 5 μg/ml Blasticidin S (ICN Biomedical) or 10 μg/ml G-418 (ForMedium). In addition, dynamin B-depleted cells (dymB−) were subcloned on bacterial lawns. Deletion of dymB was verified by PCR and Southern blotting. For growth on bacterial lawns 50–100 D. discoideum cells were mixed with 0.5 ml bacterial suspension in MES-buffer (20 mM MES-NaOH pH 6.8, 2 mM MgCl2, 0.2 mM CaCl2), plated on SM agar and incubated at 21°C.
Viability of D. discoideum in HL5C (isotonic condition), 350 mM sorbitol in MES buffer (hypertonic condition), or distilled water (hypotonic condition) was determined after 1 h incubation in the respective medium with shaking at 180 rpm at 21°C. Approximately 100 cells per incubation were plated on bacterial lawns. The number of survivors was determined by colony counting after 5 days.
A total of 2–4 × 106 cells were placed on 22 × 22 mm cover slips in media and allowed to attach for 30 min. Cells were washed twice with 10 mM MES-NaOH, pH 6.5, fixed with 3% paraformaldehyde in 10 mM PIPES buffer pH 6.0 for 30 min, and washed with PBS. Unreacted paraformaldehyde was quenched with 100 mM glycine in PBS for 5 min and permeabilized by washing with 70% ethanol or in case of tubulin staining by incubation with 0.02% Triton X-100 for 5 min followed by three washes with PBS. Cells were blocked with 0.045% fish gelatin (Sigma-Aldrich) and 0.5% BSA in PBS (PBG) for 1 h at room temperature followed by incubation in primary antibody diluted in PBG overnight at 4°C unless otherwise stated. Mitochondria were stained with 1:100 diluted mouse monoclonal anti-mitoporin antibody 70-100-1 , tubulin with 1:150 diluted bovine α-tubulin antiserum T9026 (Sigma–Aldrich), and all dynamin B-YFP fusions for 3 h at room temperature with 1:200 diluted rabbit polyclonal anti-GFP antibody (AB3080 Millipore). For myosin 2 and α-actinin staining mouse monoclonal myosin 2 56-396-5  and mouse monoclonal α-actinin 47-60-8  were used in 1:150 dilutions. After extensive washing with PBS, cells were labeled for 1 h at room temperature with 1:250 dilutions of the appropriate secondary antibodies conjugated with Alexa Fluor 488 or Alexa Fluor 555 or Alexa Fluor 594 (Invitrogen). The F-actin cytoskeleton was stained with Alexa Fluor 633-phalloidin (Invitrogen) for 30 min at room temperature. After extensive washing with PBS, cover slips were mounted on glass slides with SlowFade Gold antifade reagent (Invitrogen). Images were recorded using a Leica TCS SP2 inverted confocal microscope, 63 × 1.4 NA oil immersion objective; identical laser intensity and photo-detector gain were applied for all image acquisition. 3D reconstitutions were obtained by the superimposition of 30 overlapping Z-sections using the Leica software. Images from all focal planes were rendered as a single maximum-intensity projection using Leica software. Peroxisome numbers were counted for 110 cells from three independent experiments. Statistical significance was calculated by paired t test (N = 110, P < 0.0001). Peroxisome velocity was tracked by live time-lapse epi-fluorescence imaging, and DiaTrack 3.01 (Semasopht) was used for image analysis.
For the imaging of the peripheral actin cytoskeleton by TIRF microscopy, cells were placed in 35-mm glass-bottom petri plates (MatTek), allowed to adhere for 5 min, and fixed. Cells were stained with Alexa Fluor 633 phallodin (Invitrogen) and subsequently kept in antibleach mix containing 0.1 mg/ml glucose oxidase, 0.018 mg/ml catalase, and 3 mg/ml glucose. For live cell TIRF microscopy, cells expressing GFP-actin were used. Cells were washed three times with MES buffer and kept in MES buffer for 1 h prior to imaging.
For dynamin B TIRF microscopy, AX2 cells producing ΔNTS-dynamin B fused to YFP were used. Cells were washed three times with MES buffer prior to image acquisition. All TIRF images were taken with an Olympus 1X81 inverted microscope equipped with a TIRF module, a 60×/1.49 NA oil immersion objective, and a Hamamatsu C10600 ORCA-R2 CCD camera. A 1.6× Optovar lens was used to enlarge the image on the camera chip. Images were processed using Adobe Photoshop, and figures were compiled using Adobe Illustrator.
Cells were prepared for transmission electron microscopy as previously described . Labeling of cells with colloidal gold was done according to Griffiths and Consigili . AX2 cells over-producing dynamin B-YFP were fixed with 4% paraformaldehyde (Merck) and 0.2% glutaraldehyde (Sigma-Aldrich) in 200 mM HEPES-NaOH, pH 7.3, for 1 h at room temperature, followed by 1 h in 4% paraformaldehyde. Fixed cells were washed with PBS, pelleted at low speed, embedded in 2% low melting point agarose in PBS, and chilled. Small blocks were cut and incubated overnight with 2.3 M sucrose in PBS and then frozen in liquid nitrogen. Ultrathin cryo-sections were cut at −105°C with a Leica FCS cryo-microtome using a Drukeer diamond knife and transferred to coated grids. Grids were blocked for 15 min with 0.5% fish gelatin and 20 mM glycine in PBS. Sections were labeled with rabbit polyclonal anti-GFP antibody (Clontech Laboratories, Inc.) 1:10 diluted blocking buffer and detected with protein A-colloidal gold. Grids were then embedded in aqueous 2% methylcellulose (Sigma-Aldrich) supplemented with 0.3% uranyl acetate (SERVA Electrophoresis GmbH). Images were recorded with a Zeiss EM-10 electron microscope.
RIC/DIC double-view microscopy
Live cells were viewed in glass-bottom petri plates (MatTek, Corp.). Cells were washed and kept in MES buffer. Images were taken with an Olympus FV1000 microscope. An UPLSAPO 60× 1.35N.A. objective, a Chroma HQ filter set, and a 635-nm HeNe laser were used for imaging. Double-view microscopy was performed as described earlier . Cell size and adhesion areas detected by DIC and RIC microscopy were quantified using ImageJ software . The RIC/DIC ratio is used as an indicator of the relative size of the adhesion area per cell. Every fifth frame of 50 frames was measured; data from different measurement were pooled and plotted using Origin 7 software. Statistical significance was calculated by paired t test (N = 132, P < 10−15).
Functional analysis of mitochondria and peroxisomes
The activity of the mitochondrial marker succinate dehydrogenase was measured in whole-cell lysates as described previously . Total catalase was measured using the Amplex catalase kit (Invitrogen) following the manufacturer’s protocol. Whole-cell lysates were used for measurements, and total catalase activity normalized for protein content was determined. Statistical significance was calculated by paired t test (N = 9, P < 0.005).
Protease accessibility assay
Mitochondria from AX2 cells overproducing dynamin B-YFP were prepared as described . Purified mitochondria were incubated on ice for 5 or 30 min in the presence or absence of up to 0.1 mg/ml trypsin. Reactions were stopped by the addition of 10 mM PMSF; equal amounts of protein were separated by SDS-PAGE and analyzed by immunoblotting on nitrocellulose membranes. Dynamin B was detected as described above, and mitochondrial nucleoside diphosphate kinase (mNDP kinase) was detected using the rabbit polyclonal antibody described by Troll and coworkers .
Cell-to-substrate adhesion was analyzed in HL5C media in the presence and absence of 10 mM EDTA; 4 ml cell suspension containing 1 × 106 cells/ml was placed in 50-ml conical flasks and incubated for 45 min without agitation, followed by 3 min incubation on a rotary shaker at 80 rpm. The number of non-adherent cells was determined by counting cells in the supernatant.
For cell-to-cell adhesion, a suspension with a final density of 1 × 105 cells/ml was incubated on a rotary shaker at 180 rpm for 3 days. At intervals, samples were taken, and the number of non-aggregated cells was determined by counting single cells only. The total number of cells was determined after breaking down all aggregates by passing the suspension 20 times through a narrow-bore plastic pipette tip. The fraction of single cells was used as the measure of cell-to-cell adhesion. Measurements were performed each time in triplicate, and the results shown represent several independent experiments.
Pinocytosis and phagocytosis assays
Phagocytosis and pinocytosis were measured as described previously .
Domain organization of D. discoideum dynamin B
Processing and subcellular localization of dynamin B
Dynamin B isolated from wild-type cells migrates on SDS-PAGE with an apparent molecular weight of 92 kDa, which corresponds to the predicted size of dynamin B after truncation of the predicted presequence (Fig. 1c). Over-production of recombinant dynamin B preprotein and amino- or carboxy-terminal histidine tagged versions of the protein result in the appearance of a second band corresponding to the unprocessed preprotein. In addition to a partial overloading of the processing machinery that is apparent when the untagged protein is overproduced, the presence of sequence tags appears to interfere with effective processing. The presence of an amino-terminal histidine tag results in stronger interference with protein processing than C-terminal tagging (Fig. 1d). Amino-terminal YFP-tagging blocks proteolytic processing of the preprotein completely (data not shown).
As it is well established that dynamins play an important role in mitochondrial fusion and fission , we generated dymB deletion mutants by homologous recombination to test for changes in mitochondrial morphology and function. The resulting dymB− cells did not display obvious differences in mitochondrial morphology (Fig. 4b). An apparent reduction in the number of mitochondria correlates with the smaller cell size of dymB− cells. Succinate dehydrogenase activity normalized for protein content is slightly reduced in dymB− cells (−11 ± 6%).
Cellular morphology of dynamin B-depleted cells
We measured cell-spreading areas of 113 ± 27 μm2 and 150 ± 40 μm2 for dymB− and wild-type cells, respectively (N = 200, P value <0.0005). In addition to their smaller size, dymB− cells show a number of subtle changes in their overall morphology. Deletion of the genes encoding dynamin A, DlpA, DlpB, or DlpC was shown to interfere with normal cytokinesis and to induce the formation of large multinucleated cells [8, 31]. In contrast, dymB− cells show no cytokinesis defect. Similarly, development and differentiation are not affected by dynamin B-depletion, and spore viability is normal in dymB− cells.
Dynamin B-depletion affects peroxisome morphology and function
Mitochondria and peroxisomes are metabolically linked organelles, with the β-oxidation of very long chain fatty acid being restricted to peroxisomes [52, 53]. To test the functional competence of peroxisomes in dymB− cells, we grew cells in media supplemented with different concentrations of oleic, linoleic, and cis-4,7,10,13,16,19-docosahexanoic acid. Unsaturated long-chain fatty acids have no effect on cell growth at concentrations below 10 μM. However, the reduced tolerances of dymB− cells to media supplementation with fatty acids concentrations above 10 μM suggest that dynamin B-depletion affects the metabolic competence of peroxisomes (Fig. 6b, c).
Peroxisomes play a key role in governing H2O2 metabolism . To examine the extent to which the reduced number and altered morphology of peroxisomes in dymB− cells affect their function, we compared catalase activity levels in total cell lysates from AX2 and dymB− cells. Normalized for protein content, dymB− cells displayed a 20% reduction in catalase activity (Fig. 6d). Therefore, our results indicate that peroxisome morphology and function are compromised in dymB− cells.
Dynamin B affects cell adhesion, cytoskeletal structures, and osmo-regulation
Compared to wild-type cells, dymB− cells display a stronger tendency to form cellular aggregates. We observed large cell aggregates when dymB− cells were cultivated in suspension. A suspension of dymB− cells with a final density of 1 × 105 cells/ml was grown for 3 days on a rotary shaker. At intervals, samples were taken, and the number of non-aggregating single cells was counted. In parallel a second sample was taken, and aggregates were disrupted by repeated pipetting before counting. The number of cells in aggregates, calculated as the difference in cell counts of both samples, was significantly higher for the dymB null cells 66% (±6%) in comparison to the wild-type cells 27% (±5%). This means that under these conditions, the apparent cell-cell adhesion of dymB null cells is on average 2.4-fold greater than for wild-type cells. Cells over-producing dynamin B sixfold form significantly fewer aggregates. The number of cells in aggregates was 18% (±6%) corresponding to a 1.5-fold reduction in their case (Fig. 7b). These results indicate that dynamin B negatively regulates bivalent cation-sensitive cell-to-cell and cell-to-surface adhesion.
Relative to their size, dynamin B null cells form larger contact areas with the glass surface than control cells (Fig. 7c). This can be visualized by reflection interference contrast microscopy (RICM) when applied in combination with differential interference contrast microscopy (DICM) . Compared to wild-type cells, migrating dymB− cells display similar activity in the extension and retraction of pseudopodial structures, but form more stable contact areas and display slower and less directed movements of the cell centroid (Supplementary movie 5 and 6). The ratio of the RICM-to-DICM areas gives the normalized attachment area. Our results show that the deletion of dynamin B significantly (P < 10−15) changes cell attachment; dymB− cells are more adherent with a mean ratio of 0.82 ± 0.1 compared to 0.70 ± 0.1 for AX2 (Fig. 7d).
In addition to revealing the surface areas that are in close contact with the substratum, RIC microscopy is ideally suited for imaging membranous organelles that are in very close proximity to the plasma membrane and near to the cover glass surface. The contractile vacuole system of D. discoideum is an osmoregulatory organelle formed by a circumferential network that directly underlies the plasma membrane [56, 57]. The activity of the organelle allows D. discoideum to survive under hypotonic stress by accumulating and expelling excess water out of the cell. An association of dynamin B with the contractile vacuole system was first suggested by a partial co-localization in immunogold-labeled electron micrographs (Fig. 3a). A role of dynamin B in the regulation or maintenance of this organelle was further indicated by the twofold increase in viability of dymB− cells following exposure to hypotonic conditions (Supplementary Fig. 1C). The cisternae and interconnecting ducts of the contractile vacuole system are well visible in RIC images as dark vesiculotubular structures. Movie sequences assembled from RIC images show that the morphology and dynamics of the contractile vacuole system is altered in dymB− cells in favor of increased tubulation and decreased contractile activity of large cisternae (Supplementary movie 5 and 6).
Here we describe the post-translational processing and the cellular functions of D. discoideum dynamin B. Dynamin B is a nuclear-encoded protein, which is synthesized as preprotein in the cytosol, shuttled for processing to mitochondria, and returned in mature form to the cytosol, where it interacts with a distinct subset of organelle membranes, the plasma membrane, and cytoskeletal structures. Dynamin B contains a QPS-rich domain that appears to mediate many of the interactions involved. The presence of one or more regions that are enriched for glutamine, proline, serine, and asparagine residues or contain repeats of these residues is a frequent feature of Dictyostelium proteins. These regions are thought to mediate protein-protein interactions , and they are frequently found at positions where protein interaction domains are present in the metazoan orthologs. In the case of dynamin A, which contains a QNS-rich domain but lacks a PH domain, we were able to show direct binding to lipid membranes containing phosphatidic acid or phosphatidylinositol phosphates .
Cellular localization studies with YFP fused to the dynamin B presequence and YFP-tagged dynamin B preprotein show that the 136-residue preprotein acts as an efficient mitochondrial targeting sequence. The protease accessibility assay indicates that the protein remains mostly exposed at the outside of mitochondria while processing occurs. Therefore, the unusually long presequence appears to enter the mitochondrial intermembrane space and the matrix, where a yet unidentified protease converts the 105-kDa preprotein into the mature 92-kDa form. The processing of dynamin B thus differs from that of Mgm1p, the yeast homologue of the mammalian protein OPA1. Mgm1p functions specifically in membrane fusion. It is the only one of the three dynamin family GTPases regulating mitochondrial membrane dynamics in yeast that has an amino-terminal signal peptide. Mgm1p is found in the full-length and rhomboid (Rbd1p) processed forms, and both forms are required for efficient fusion . Dynamin B lacks transmembrane domains, but contains an R-2 sequence motif that can be recognized by matrix processing proteases involved in preprotein processing . This suggests that matrix processing proteases are responsible for the cleavage of dynamin B. The mature protein is released into the cytosol. A transient association of the preprotein with mitochondria is supported by the protease accessibility assay, whereas the fluorescence pattern of the YFP-tagged preprotein appears to indicate a more stable association of dynamin B with mitochondria. However, this can be explained by the combined effects of the YFP-tag interfering with effective processing and the high level production of the recombinant protein overloading the mitochondrial processing machinery. Dynamin B is produced in low abundance in vegetatively growing cells (data not shown). The processing and stable mitochondrial association of the presequence-tagged YFP construct demonstrates that the dynamin B presequence is sufficient to direct proteins to mitochondria.
Despite being targeted to and processed in association with mitochondria, dynamin B plays no obvious role in the division and maintenance of mitochondria. The mitochondrial fission mechanism employed by D. discoideum involves the extra-mitochondrial dynamin-based system used in plants and fungi and the ancient FtsZ-based intra-mitochondrial fission process inherited from the bacterial ancestor . Deletion of D. discoideum dynamin A or the FtsZ orthologues FszA and FszB was shown to result in the formation of large tubular mitochondria [8, 60]. FtsZ proteins were functionally replaced by dynamin-like proteins in most eukaryotes, but they still retain this function in some lower eukaryotic organisms . Experiments designed to knock out the genes encoding dynamin A, FszA, or FszB in a dymB− background produced no viable transformants (Nöthe, Rai, Manstein, unpublished results).
Several dynamin family members were shown to represent evolutionarily conserved components of the peroxisomes division/proliferation machinery. Consistent with the close relationship of dynamin B and yeast Vps1p indicated by phylogenetic analysis , the phenotypic changes displayed by dynamin B-depleted cells indicate a role of the protein in peroxisome biogenesis, maturation, and fission. In particular, a cargo-selected vesicular transport pathway from mitochondria to peroxisomes has been reported . Some dynamin family members, such as plant DRP3A and DRP3B, yeast Dnm1p, and mammalian Drp1, participate in the division of peroxisomes and mitochondria, possibly coordinating the division of these metabolically linked organelles [13, 19, 63]. Our results show that similar to the situation following depletion of the dynamin-like GTPases Vps1p and Dnm1p in yeast and Drp1 in mammalian cells [13, 21, 51], depletion of dynamin B severely affects peroxisome morphology and abundance. The increased sensitivity to media supplementation with long chain fatty acids and decreased amount of catalase indicates that peroxisome function is affected by the depletion of dynamin B.
Mitochondria and peroxisomes are metabolically linked organelles. They cooperate in the β-oxidation of fatty acids and metabolism of reactive oxygen species (ROS). The preferred initial substrates for peroxisomal β-oxidation are the CoA esters of long chain fatty acids including (poly-) unsaturated fatty acids. Peroxisomal β-oxidative chain shortening generates H2O2 and ceases at the stage of octanyl CoA . The observed correlation between the chain length of the supplemented fatty acids and the reduction in cell growth in combination with reduced levels of catalase activity suggests that dynamin B-depleted cells are less efficient in degrading ROS or less able to cope with ROS-induced damage. Moreover, reduced peroxisomal β-oxidation can increase the intracellular concentrations of free unsaturated long chain fatty acids. This may further contribute to the observed phenotype because of interference with calcineurin signaling pathways .
Our analysis of dynamin B-depleted cells indicates extensive changes in the morphology and function of the contractile vacuole system, a highly specialized osmoregulatory organelle, which is driven by actomyosin in cooperation with microtubule-associated motors. Increased tubulation of the contractile vacuole system observed in dynamin B-deficient cells correlates with F-actin enrichment at the cell periphery and can be a secondary effect resulting from changes in actin organization. However, the observed association of dynamin B with contractile vacuole membranes suggests a more direct involvement of the protein in the dynamics of the contractile vacuole system.
Our results indicate that dynamin B plays yet another role as a modulator of cell-surface interactions and cytoskeletal dynamics. The observed increase in capacity for the uptake of particles and the faster growth rate displayed by dymB− cells on bacterial lawns appears to be directly related to the formation of stronger cell-surface contacts. Similarly, classical dynamins have been implicated in controlling cell adhesion in cells forming focal contacts; planar assemblies of proteins formed at the sites where clustered integrins interact with immobilized extracellular matrix . The dominant negative K44A mutation of mammalian dynamin 1 affects adhesion and associated changes in the organization of the actin cytoskeleton . Dynamin 2-depleted U2-OS cells display increased levels of α-actinin-induced actin crosslinking, while depletion of dynamin 2 in fibroblasts inhibits migration of adherent cells . These findings link the function of dynamin B to the regulation of cell adhesion and actin-dependent processes. Thus, they strengthen the functional parallel between focal adhesion sites of mammalian cells and actin foci in D. discoideum. Actin foci, which are formed in migrating D. discoideum cells at the sites where the ventral cell membrane is closely opposed to the substratum, are considered to be functionally similar to the focal adhesions or podosomes of higher eukaryotes [69, 70].
In summary, our data show that the low abundance protein dynamin B interacts with multiple target structures and plays a critical role in a wide range of cellular processes, which require the action of distinct classical and non-classical dynamin family members in other organisms. Dynamin B is initially produced as a preprotein with an unusually long 136-residue presequence that is efficiently targeted to mitochondria for processing. Processing involves a transient association with the outer mitochondrial membrane and goes to completion. The mature 92-kDa form of the protein functions in the context of actin-rich structures and multiple target membranes, including peroxisomes, the osmoregulatory contractile vacuole system, phagosomes, and the plasma membrane.
We thank S. Eschenburg, T.F. Reubold, G. Griffiths, and H. Horstmann for their help and discussions; M. Maniak for providing GFP-PTS1. The monoclonal anti-mitoporin 70-100-1, monoclonal anti-myosin 2 56-396-5, and α-actinin antibody developed by G. Gerisch and co-workers were obtained from the Developmental Studies Hybridoma Bank developed under the auspices of the NICHD and maintained by The University of Iowa, Department of Biology, Iowa City, IA, 52242. The work was supported by Deutsche Forschungsgemeinschaft Grant MA 1081/7-2 to D.J.M.
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