Ciliates, although single-celled organisms, contain numerous subcellular structures and pathways usually associated with metazoans. How this cell biological complexity relates to the evolution of molecular elements is unclear, because features in these cells have been defined mainly at the morphological level. Among these ciliate features are structures resembling clathrin-coated, endocytic pits associated with plasma membrane invaginations called parasomal sacs. The combination of genome-wide sequencing in Tetrahymena thermophila with tools for gene expression and replacement has allowed us to examine this pathway in detail. Here we demonstrate that parasomal sacs are sites of clathrin-dependent endocytosis and that AP-2 localizes to these sites. Unexpectedly, endocytosis in Tetrahymena also involves a protein in the dynamin family, Drp1p (Dynamin-related protein 1). While phylogenetic analysis of AP subunits indicates a primitive origin for clathrin-mediated endocytosis, similar analysis of dynamin-related proteins suggests, strikingly, that the recruitment of dynamin-family proteins to the endocytic pathway occurred independently during the course of the ciliate and metazoan radiations. Consistent with this, our functional analysis suggests that the precise roles of dynamins in endocytosis, as well as the mechanisms of targeting, differ in metazoans and ciliates.
The wings of bats and of birds are similar structures with similar functions but nonetheless evolved independently within these two different branches of animals. Many examples of this phenomenon, called convergent evolution, are known at the level of whole organisms. Here, the authors demonstrate that convergent evolution has also occurred at the level of individual cells, in a pathway responsible for taking up membrane from the cell surface. The authors took advantage of the recent genomic sequencing of distantly related organisms, and in particular of the single-celled ciliate Tetrahymena thermophila. In animal cells, one of the proteins required for membrane uptake is called dynamin. Dynamin is not required for this function in most nonanimal cells, but the authors discovered that Tetrahymena is an exception and that it uses a close relative of dynamin for particle uptake. After reconstructing the history of dynamin proteins, the authors found that the specific role in membrane uptake evolved independently in Tetrahymena and in animals.
Citation: Elde NC, Morgan G, Winey M, Sperling L, Turkewitz AP (2005) Elucidation of Clathrin-Mediated Endocytosis in Tetrahymena Reveals an Evolutionarily Convergent Recruitment of Dynamin. PLoS Genet 1(5): e52. doi:10.1371/journal.pgen.0010052
Editor: Susan Dutcher, Washington University, United States of America
Received: July 1, 2005; Accepted: September 22, 2005; Published: November 4, 2005
Copyright: © 2005 Elde et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Competing interests: The authors have declared that no competing interests exist.
Abbreviations: μ subunit, adaptor protein medium subunit; AP, adaptor protein; CHC, clathrin heavy chain; CME, clathrin-mediated endocytosis; cytB, cytochalasin B; DRP, dynamin-related protein; DTD, Drp1 targeting determinant; GED, GTPase effector domain; GFP, green fluorescent protein; PH, pleckstrin homology; PRD, proline-rich domain
Endocytosis is conserved in eukaryotes, but the molecular machinery deployed by cells to internalize plasma membrane varies according to task, which can range from nutrient absorption to cell signaling . The best understood mechanism of endocytosis involves clathrin-induced membrane deformation to form nascent vesicles (Figure 1A) . Clathrin can also recruit membrane proteins for internalization, often via a multimeric adaptor protein (AP) complex, AP-2 . In metazoans, clathrin-mediated endocytosis (CME) requires classical dynamin, a member of a family of self-assembling GTPases. During endocytosis, the GTP-dependent constriction of an oligomeric dynamin “collar” may induce fission of vesicles from plasma membrane [4,5]. Additionally, dynamin recruits effectors, including actin-binding proteins, which could mediate aspects of vesiculation [6,7].
Figure 1. Overview of Endocytosis
(A) Schematic diagram of clathrin-coated vesicle formation in metazoans. AP-2 (red) serves as an adapter. It can interact with receptors destined for internalization while also recruiting clathrin (green) to the plasma membrane. Clathrin assembly at those sites drives or facilitates membrane invagination. Dynamin (blue) assembles at the neck of a nascent vesicle to promote membrane fission.
(B) Domains of classical dynamin and of DRPs.doi:10.1371/journal.pgen.0010052.g001
Processes closely resembling CME have been described in a small number of eukaryotes outside Metazoa, but it is not clear that any depend on proteins in the dynamin family (dynamin-related proteins [DRPs]). In Saccharomyces cerevisiae, endocytic vesicle formation involves some proteins associated with CME [8,9], but no endocytic role has been discovered for AP-2 or any DRP [10,11]. A wide survey of eukaryotes suggests that the most conserved role for DRPs is in mitochondrial inheritance, while other family members mediate membrane remodeling events distinct from endocytosis [12,13]. For example, while Trypanosoma brucei uses CME for turnover of surface glycoproteins , its single DRP is dedicated to mitochondrial fission . Another eukaryote deeply divergent from metazoans, the red alga Cyanidioschyzon merolae, has two DRPs, one acting in mitochondrial fission and the other in chloroplast division [16,17].
Classical dynamins are composed of five domains (see Figure 1B). Three of these are found in all DRPs: a large N-terminal GTPase domain, a middle domain, and a GTPase effector domain (GED) . The remaining two domains in classical dynamin, pleckstrin homology (PH) and proline-rich domain (PRD), are implicated in targeting to endocytic pits and in the recruitment of SH3 domain-containing proteins, respectively, which in turn regulate actin assembly at these sites [18,19]. These observations are consistent with a recent expansion of the role of DRPs to include CME, in an evolutionary step involving the acquisition of PH domains and PRDs. Classical dynamins are exclusive to Metazoa with two known exceptions, DRP2A and DRP2B, in Arabidopsis thaliana. These nearly identical genes are highly diverged from other dynamins and may be involved in vesiculation of the trans-Golgi network [20,21].
These observations support the view that the founding member of the dynamin family was a DRP required for maintenance of a mitochondrial endosymbiont . Subsequently, gene duplication and differentiation led to the acquisition of new functions. We examined the large radiation of DRPs within ciliates and found that these proteins encompass a surprising variety of roles. In conjunction, we performed molecular characterization of CME in Tetrahymena, along with phylogenetic analysis of components in this pathway. This combination provided insight into the evolution of both endocytosis and dynamin that would not have been evident by taking either approach alone.
Coat-Mediated Endocytosis Visualized with FM1–43 in Tetrahymena
As previously noted, electron microscopy of Tetrahymena and Paramecium thin sections reveals structures, situated near ciliary basal bodies, that resemble coated pits in mammalian cells (Figure 2A) [22,23]. We set out to observe the activity of these structures in live cells. No endocytic cargo molecules in Tetrahymena are known, but endocytic vesicles in a variety of species have been vitally stained using the styryl dye FM1–43 . To preclude FM1–43 uptake via phagocytosis at the oral apparatus, we starved cells for 2 h prior to FM1–43 labeling, a treatment that temporarily eliminates phagosome formation via the regression and eventual replacement of the preexisting oral apparatus . Exposing such starved cultures to FM1–43 led to the immediate appearance of fluorescent puncta, aligned in rows, near the cell surface (Figure 2, 0 min). This pattern recalled the known arrangement of ciliary basal bodies (Figure 3, centrin), with their associated coated pits (see Figure 2A). To observe the itinerary of the putative endocytic vesicles, cultures were exposed to dye for 5 min, and individual cells were observed over time. Ten minutes after exposure to dye, the putative vesicles appeared highly mobile throughout the cytoplasm (Figure 2, 10 min). Over the next 20 min, they appeared to coalesce and accumulate in the posterior of the cell (Figure 2, 14 and 18 min). At the end of this period, the majority of puncta appeared to have coalesced (Figure 2, 22 min and brightfield). Therefore, kinetic analysis of FM1–43 uptake resembled the expected pattern of an endocytic pathway originating from coated pits observed near basal bodies and suggested the existence of a localized endosomal compartment.
Figure 2. Visualizing Sites of Endocytosis
(A) In Tetrahymena, coated pits (cp) are found near the base of cilia, as shown in tangential (left) and cross (right) sections. bb, ciliary basal body; ci, cilia; cv, coated vesicle; mt, mitochondrion; dcv, dense core vesicle. Bars = 200 nm.
(B) Time course of FM1–43 dye uptake. A cell shown immediately after treatment with 5 μM FM1–43 (0 min) shows rows of fluorescent puncta at the cell surface. Time-lapse images (10, 14, 18, and 22 min) of a single cell following 5-min exposure to FM1–43. At the later time points (18 and 22 min), the dye accumulates in what appear as vesicles clustered toward the cell posterior. The brightfield image shows the cell at the end of the time course. Bar = 10 μm.doi:10.1371/journal.pgen.0010052.g002
Figure 3. Analysis of CHC
(A) Cartoon of CHC assembly. The location of the C-terminal hub domain is indicated.
(B) Expression of truncated CHC (hub) inhibits endocytosis. Wild-type (DAPI-labeled) and CHC hub-expressing cells were mixed and incubated with FM1–43. Reduced FM1–43 uptake is detected in the hub-expressing cell.
(C) Quantification of FM1–43 uptake. FM1–43 uptake was quantified by analysis of 20 image pairs such as those shown in (B), as described in Materials and Methods. The fluorescence units are arbitrary (a.u.). WT, wild-type.
(D) Cells expressing Chc1p-hub-GFP (from the MTT1 promoter) were fixed, permeabilized, and labeled with anti-centrin antibody. The merged image shows the close proximity of clathrin hub-GFP to basal bodies, comparable to Figure 2.
Bar = 5 μm (B and D).doi:10.1371/journal.pgen.0010052.g003
Clathrin Is Essential for FM1–43 Uptake
To determine whether FM1–43-labeled vesicles specifically reflected CME in this system, we identified a single clathrin heavy chain (CHC) ortholog (CHC1) in the Tetrahymena macronuclear genome. CHC1 encodes a predicted protein of 1,710 residues, 40% identical to bovine clathrin. In mammalian cells, clathrin function can be blocked in a dominant negative fashion by expressing the C-terminal third of the protein, called the hub (see Figure 3A) . We cloned the CHC1 hub, placing it under the control of the cadmium-inducible MTT1 promoter, and used this to transform Tetrahymena . Within 3 h of cadmium addition, FM1–43 uptake was blocked (Figure 3B and 3C). In the absence of cadmium, internalization of FM1–43 by these cells was indistinguishable from that of wild-type. Cadmium addition itself did not block FM1–43 uptake, in either wild-type cells or cells in which the CHC1 hub was replaced with GRL1, a constituent of secretory granules  (data not shown). These results suggest that FM1–43 selectively labels vesicles derived by CME in Tetrahymena.
The Chc1p hub, tagged with green fluorescent protein (GFP), localized at the plasma membrane in an ordered array. Moreover, dual labeling with an antibody against centrin demonstrated that it was targeted near basal bodies of cilia (Figure 3D). This is consistent with the location of coated pits (see Figure 2A). Taken together, the data support the idea that uptake of FM1–43 can be directly blocked by the Chc1p hub acting at coated pits.
A Family of Adaptor Proteins in Tetrahymena
Endocytosis in animal cells involves AP-2, one of a family of heterotetrameric complexes that mediate diverse membrane trafficking events involving clathrin in many eukaryotes (Figure 4A) . In Tetrahymena, we identified four paralogs encoding AP medium subunits (μ subunits). Phylogenetic analysis of μ subunits, including Tetrahymena, several metazoans, and Arabidopsis, produced a topology in which subunits distributed into functional groups across species (Figure 4B). This tree supports an early diversification of μ subunits, consistent with prior analysis [29,30], and specifically suggests an origin of adaptor-mediated functions that predates the split between ancestors of metazoans and ciliates. Of the Tetrahymena μ subunit genes, a single paralog clustered with the AP-2 family, while two paralogs (APM1A and APM1B) clustered in the AP-1 family. Interestingly, this organism has no recognizable subunits of AP-3, a complex found in a variety of eukaryotes, while the genome does appear to include genes for AP-4 subunits, a complex found previously only in a subset of metazoans and plants . Although not shown, the genome contains the expected large and small AP subunits that compose each of three heterotetrameric complexes.
Figure 4. Phylogenetic Analysis and Localization of the AP-2 μ Subunit
(A) Schematic representation and cellular localization of the heterotetrameric AP complexes. Location of the μ subunit is indicated. TGN, trans-Golgi network.
(B) AP complex μ subunit phylogeny. The topology illustrated is the best maximum likelihood (ML) distance for μ subunits from A. thaliana (At), D. melanogaster (Dm), H. sapiens (Hs), and T. thermophila (Tt). Both ML and maximum parsimony (MP) bootstrap support values are shown at each node.
(C) Fixed, permeabilized cells expressing GFP-tagged AP-2 μ subunit (Apm2p-GFP) (from the MTT1 promoter) were labeled with anti-centrin antibody. The distribution of Apm2p-GFP is similar to that of the CHC hub (Figure 3), but the former is additionally present at the contractile vacuole pores. Bar = 5 μm.doi:10.1371/journal.pgen.0010052.g004
To determine if the phylogenetic classification of the Tetrahymena subunits was consistent with their sites of action, we cloned and GFP-tagged APM1A, APM1B, and APM2. Apm2p-GFP localized near sites of endocytosis in a pattern similar to that of clathrin (Figure 4C). Uniquely among the proteins included in this study, Apm2p-GFP labeled two ring structures in the posterior of the cell, the contractile vacuole pores, indicating a possibly novel function for this protein. GFP-tagged Apm1Ap and Apm1Bp both localized to internal structures in the cell (not shown). The presence of Apm2p-GFP at sites of CME reinforces the roles suggested by the molecular conservation in this pathway. We did not investigate potential effects of APM2 knockdown, because the AP-2 complex appears unlikely to be required for the receptor-independent uptake of FM1–43.
A Dynamin-Related Protein Is Required for Clathrin-Mediated Endocytosis
DRPs have not been clearly demonstrated to participate in endocytosis except in metazoans, but the presence of an unusually large number of DRPs in the Tetrahymena genome prompted us to ask if any might contribute to CME. Drp1p lacks both the PH domain and PRD of classical dynamins. The GTPase domain of Drp1p is 47% identical to human dynamin-1, while the middle domain and GED are 30% and 27% identical to dynamin-1, respectively. When DRP1-GFP was expressed in wild-type cells, it nearly co-localized with centrin, consistent with the location of Chc1p hub-GFP just anterior to basal bodies (Figure 5A). Further examination of Drp1p-GFP localization by immunoelectron microscopy of cryofixed cells confirmed a close association of Drp1p-GFP with coated pits (Figure 5B). Gold labeling appears adjacent to the coated pits, but this may not mirror the precise distribution of endogenous Drp1p at these sites, because GFP-tagging itself may interfere with the activity of Drp1p, as it does for other dynamin family proteins in other systems.
Figure 5. Localization of Drp1p
(A) Fixed, permeabilized cells expressing Drp1p-GFP (from the MTT1 promoter) were labeled with anti-centrin antibody. Like CHC and AP-2 μ subunit, Drp1p-GFP localizes to sites near basal bodies. Bars = 5 μm.
(B) Immuno-gold visualization of Drp1p-GFP shows localization to a coated pit (cp) near a basal body (bb). Bar = 200 nm.doi:10.1371/journal.pgen.0010052.g005
To study the effect of depleting Drp1p from cells, we targeted the transcriptionally silent, germline nucleus of Tetrahymena for disruption of DRP1. We thus obtained heterokaryon strains, which still bore intact copies of DRP1 in the transcriptionally active macronucleus. When mated, the progeny of these strains lose all intact copies of DRP1 as a consequence of nuclear remodeling . Such progeny were unable to divide beyond two or three generations, indicating that the gene was essential for growth. To confirm that the defect was due to disruption of DRP1, a strain was derived from the ΔDRP1 cells by rescuing the progeny of heterokaryon matings with full-length DRP1 tagged with the HA epitope. Southern analysis of a strain expressing DRP1-HA confirmed the complete replacement of wild-type DRP1 with the HA-tagged allele (Figure 6). This strain expressed DRP1-HA at wild-type levels (see Figure 6C) and grew normally. Importantly, immunofluorescence using an antibody to the HA epitope confirmed the localization of Drp1p to endocytic sites (Figure 7). Co-expression of Apm2p-GFP in this strain confirmed that Drp1p and Apm2p show close, partially overlapping localization (Figure 7). Drp1p and Apm2p are present either at adjacent zones on the same structure or on two adjacent structures (see Discussion for further comment on the localization of AP-2).
Figure 6. Functional Analysis of DRP1
(A) The DRP1 locus, with strategy for NEO3 disruption and HA epitope tagging, both via homologous recombination.
(B) Southern blot of wild-type (WT) and drp1–1::neo3 lines rescued with DRP1 integrated at the MTT1 locus (DRP1-MTT1) or DRP1 tagged with HA (DRP1-HA).
(C) Northern blots of wild-type (WT) and rescued (DRP1-MTT1) lines. Analysis of DRP1-MTT1 maintained with (+) or without (−) cadmium for 16 h demonstrates that transcript expression is cadmium-dependent. The expression of DRP1-HA, at the endogenous locus, is comparable to wild-type. The band near 1 kb serves as a loading control.
(D) FM1–43 uptake depends on Drp1p. DRP1-MTT1cells were maintained in cadmium-free medium for 16 h and mixed with wild-type (DAPI labeled) as described in text.
(E) Impaired uptake of FM1–43 in cells expressing, from the MTT1 promoter, the K51E allele of DRP1.
(F) Quantitative comparison of FM1–43 uptake, shown in arbitrary fluorescence units (a.u.).
Bar = 10 μm (D and E).doi:10.1371/journal.pgen.0010052.g006
Figure 7. Dual Localization of Drp1p-HA and Apm2p-GFP
Cells expressing Drp1p-HA at the wild-type locus were transformed to express Apm2p-GFP driven by the MTT1 promoter. Fixed, permeabilized cells were immunolabeled with anti-HA antibody. The merged image (bottom) indicates that the two proteins are present in adjacent, partially overlapping puncta. Bar = 5 μm.doi:10.1371/journal.pgen.0010052.g007
To test if DRP1 is specifically required for endocytosis, we rescued the progeny of ΔDRP1 heterokaryons by transforming with an intact DRP1 gene that integrated adjacent to the endogenous MTT1 promoter. The resulting strain, lacking DRP1 at its native locus (labeled as DRP1-MTT1 in Figure 6B), depended on cadmium for DRP1 expression (Figure 6C) and for normal growth, consistent with the ΔDRP1 phenotype. Removing these cells from cadmium for 16 h resulted in a dramatic reduction in the uptake of FM1–43 compared to wild-type cells (Figure 6D and 6F). Importantly, cells could be maintained, although not dividing, without cadmium for 96 h and then restored to normal growth by replenishing the medium with cadmium. This indicates that the endocytosis phenotype was not the result of a nonreversible, ill effect on cells depleted of Drp1p. Additionally, other subcellular features such as mitochondria retained a wild-type appearance in electron micrographs of cells depleted of cadmium for 16 h (not shown). Inhibition of FM1–43 uptake in cadmium-depleted cells supports a specific requirement for DRP1 in CME.
Several alleles with single residue substitutions disrupt GTP turnover and impair dynamin function, in a dominant negative fashion, in mammalian cells . These were used to design similar alleles of DRP1, taking advantage of the conservation of residues in the tripartite GTP-binding motifs. Tetrahymena were very sensitive to the expression of these alleles under the inducible MTT1 promoter, even in the absence of cadmium. We did not obtain transformants with a Drp1p-T72F construct (analogous to T65F) in multiple attempts. However, cells expressing Drp1p-K51E (analogous to K44E) were recovered. In the presence of cadmium, this strain was impaired for uptake of FM1–43 when compared to wild-type cells (Figure 6E and 6F). The dominant negative activity of this allele confirms an endocytic role of Drp1p and is consistent with its activity as a GTPase.
DRP1 Is Not Closely Related to Classical Endocytic Dynamin
Because DRPs have not previously been clearly identified with roles in endocytosis, we included DRP1 in phylogenetic analyses to determine if it would associate with classical endocytic dynamins or instead with other classes of DRPs. Phylogenetic comparisons of dynamin and DRPs have revealed a general distribution of proteins according to function, e.g., mitochondrial fission versus vesicle scission [15,33,34]. To determine if this extended to ciliates, we included seven additional DRPs in the Tetrahymena genome and nine from a second available ciliate genome, that of Paramecium tetraurelia, together with dynamin and DRPs from other eukaryotes. We initially focused our analysis on unambiguously aligned regions in the GTPase domain, middle domain, and GED common to all dynamins and DRPs. (For domain boundary definitions, see Materials and Methods and Figure S1.) The phylogeny generally confirmed a clustering of proteins according to function, as expected (Figure 8). This was especially clear for the classical endocytic dynamins in metazoans and for DRPs implicated in mitochondrial fission across a broad swath of species, including some likely to play this role in ciliates. The localization of T. thermophila Drp7p to subcortical mitochondria is consistent with observations of mitochondrial DRP localization in yeast and mammals, supporting its inclusion in the mitochondrial cluster (Figure S2) . In striking contrast, other DRPs from ciliates did not partition into known functional clades but instead appeared to associate among themselves. In particular, DRP1 is more closely related to other ciliate DRPs than it is to classical metazoan dynamins. Importantly, this conclusion does not depend on the absence of a PRD or PH domain in DRP1, because only universally conserved regions of the protein were included in the analysis, nor does it depend on any assumption about the function of the ancestral DRP. This conclusion was also strongly supported in a phylogeny derived by Bayesian analysis of these proteins (Figure S3) and by both maximum likelihood and parsimony-based phylogenies derived by comparison of the GTPase domain, middle domain, or GED alone (not shown). This strongly argues that Drp1p specialized as an endocytic protein after progenitors of ciliates branched from other eukaryotes. Rather than reflecting shared ancestry, the similarity between the roles of Drp1p and classical dynamins is likely to have arisen via functional convergence within this protein family.
Figure 8. Phylogenetic Analysis of Dynamin and DRPs
Best maximum likelihood topology for dynamin and DRPs. Maximum likelihood (ML) and maximum parsimony (MP) bootstrap values over 50% are indicated. Ciliate DRPs (Tetrahymena and Paramecium) are in italics, DRPs with mitochondrial function are green, nuclear DRPs are in blue, and endocytic dynamins are red. A. nidulans, Aspergillus nidulans; G. intestinalis, Giardia intestinalis; G. maxx, Glycine max; P. falciparum, Plasmodium falciparum; P. yoelii, Plasmodium yoelii.doi:10.1371/journal.pgen.0010052.g008
Unique Features of DRP1-Mediated Endocytosis
Classical dynamin can recruit mediators of actin assembly via its C-terminal PRD, and actin assembly appears to be important for endocytosis in some, but not all, animal cells . Actin assembly also appears to be essential for endocytosis in a variety of unicellular organisms [36,37]. Tetrahymena Drp1p is missing the PRD but could associate with actin via a PRD-independent mechanism . We first asked whether actin assembly was indeed required for endocytosis in this lineage, by measuring FM1–43 uptake following treatment with chemical inhibitors of actin assembly. Tetrahymena treated for 30 min with cytochalasin B (cytB; 25 μM) showed no inhibition of FM1–43 uptake compared to wild-type cells (Figure 9A and 9B). To confirm that this concentration of cytB blocked a bona fide actin-dependent process, we monitored uptake of ink particles via phagosome formation. As previously reported , inhibition of actin assembly by cytB blocked the release of nascent phagosomes from the oral apparatus and prevented the accumulation of phagosomes in the cytoplasm (Figure 9C). Similarly, FM1–43 uptake, but not phagosome formation, appeared normal in cells treated for 5 min with the actin inhibitor latrunculin A (10 μM; data not shown). The results suggest that CME in Tetrahymena is less dependent on actin assembly than is phagocytosis.
Figure 9. Comparison of the Actin-Dependence of Endocytosis versus Phagocytosis
(A) Cells treated with cytB (25 μM, 30 min) were mixed with untreated cells and incubated with FM1–43 (5 min, no cytB). Prior to mixing, cells not treated with cytB were incubated for 10 min with DAPI, to label the nuclei. All cells showed equivalent FM1–43 uptake.
(B) Quantitative comparison of FM1–43 uptake, in arbitrary fluorescence units (a.u.). The first set of bars represents pairs (n = 4) of cells as described in (A). The second set of bars represents pairs (n = 20) of cells in which cytB was also included during the 5-min incubation with FM1–43, to rule out potential reversal of inhibition during drug washout. Exposure to cytB for 5 min did not itself inhibit FM1–43 uptake. This is shown in the third set of bars, representing pairs (n = 20) of cells incubated for 5 min in FM1–43 or FM1–43 plus cytB.
(C) Under the same conditions as (A), cytB treatment inhibited india ink uptake via phagocytosis from the oral apparatus. Treated cells show a single ink-containing vacuole (arrow), while untreated cells (DAPI labeled) always contain several.
Bars = 10 μm.doi:10.1371/journal.pgen.0010052.g009
Localization of Drp1p Depends on a Novel Motif
If classical dynamin and Drp1p are independently adapted to roles in endocytosis, the mechanisms of targeting to endocytic sites may be different. That the mechanisms are different is suggested by the sequence differences between the two proteins. The PH domain of classical dynamin binds phosphatidylinositol-4,5-P2 at the plasma membrane, which contributes to its localization [18,40]. At the position of the PH domain, Tetrahymena Drp1p has a short stretch of 28 residues with no recognizable motif. To ask which regions of Drp1p are important for localization, we created full-length chimeras between DRP1 and a paralog whose product showed a different subcellular localization. An ideal partner for chimera construction was found after GFP-tagging one of the seven additional Tetrahymena DRPs. Drp6p-GFP localized at the nuclear envelope in a pattern easily distinguished from Drp1p-GFP (Figure 10A and 10B). These paralogs share 50% and 30% identity between the GTPase and middle domains, respectively, but none between the more C-terminal domains. Only one other dynamin (MxB, in humans) has previously been reported at the nuclear envelope .
Figure 10. Analysis of Drp1p Targeting by Chimera Analysis
(A) Compiled stack of confocal sections through fixed cell expressing Drp6p-GFP (driven by the MTT1 promoter) shows localization at the nuclear envelope. Bar = 10 μm.
(B) Immuno-gold visualization of Drp6p-GFP shows localization in clusters on the cytoplasmic face of the nuclear envelope (ne). Regions of heterochromatin within the macronucleus (mac) are indicated (*). Bar = 200 nm.
(C) Domain comparison of Drp1p and Drp6p and diagrams of Drp-GFP chimeras (expressed under the MTT1 promoter) indicating localization. Numbered images at right show localization patterns observed in cells expressing chimeric proteins. Bar = 10 μm. nd, not detected.
(D) Western blot of total cell lysates from Drp-GFP cells confirms stability of full-length chimeras.doi:10.1371/journal.pgen.0010052.g010
We exchanged the coding sequence for several domains between DRP1 and DRP6 to create a series of chimeras, whose localization is shown in Figure 10C and stability is demonstrated in Figure 10D. Neither GTPase domain altered the localization of the remaining three domains (Figure 10D, 6111 and 1666). Exchanging the domain just C-terminal to the middle domain, in contrast, was highly informative. We named this domain the Drp targeting determinant (DTD). A chimera in which a Drp6p backbone contained the DTD of Drp1p (Figure 10D, 6616) was targeted to endocytic sites. Some of the chimera, however, was diffusely distributed in the cytoplasm, suggesting that targeting determinants also lay in other domains. We therefore tested chimeras in which both the DTD and GED were exchanged. Chimeras containing the DTD and GED of Drp1p strongly localized to coated pits (Figure 10D, 6611). The Drp1p GED was necessary for full targeting, but not sufficient, because exchanging just the GED between Drp1p and Drp6p resulted in only diffuse cytoplasmic localization (Figure 10D, 6661 and 1116). Similarly, although the combined DTD and GED were sufficient to define targeting in the context of the full-length protein, a construct consisting of just the Drp1p DTD and GED, linked to GFP, localized diffusely in the cytoplasm (Figure 10D, xx11). This may be explained if efficient localization requires oligomer assembly, for which at least three dynamin domains are required .
Interestingly, targeting of the reciprocal chimeras (Drp6p determinants in a Drp1p context) was significantly less efficient, and both the Drp6p DTD and GED were required for nuclear targeting (Figure 10D, 1166).
The molecular mechanisms underlying eukaryotic membrane traffic are likely to have an ancient origin because components of these pathways are conserved across multiple lineages. For example, phylogenetic analysis of syntaxins, a family of SNARE proteins involved in vesicle fusion, supported an early origin for the functional diversification of these paralogs, which implies a set of primitively differentiated pathways in membrane traffic [43,44]. Nonetheless, conclusions based on phylogenetics without accompanying functional data are limited, and potentially misleading, because genes within families can evolve new roles in individual lineages. The great majority of functional studies of membrane traffic have been performed in either animal cells or budding yeast. Because the fungal lineage diverged relatively recently from that of animals, when compared to many other eukaryotic lineages, the oft-cited interval “from yeast to humans” represents a surprisingly small sampling of the potential molecular variation among existing organisms . Fortunately, an increasing number of species are associated with extensive genomic data and tools for gene manipulation, allowing functional analysis of genes within highly conserved families. We have used the combination of tools available in Tetrahymena to analyze the molecular machinery at endocytic structures called parasomal sacs.
Clathrin-Mediated Endocytosis in Tetrahymena
Our analysis demonstrates that parasomal sacs are sites of clathrin-dependent membrane internalization. FM1–43 uptake was blocked by inducible expression of a domain of Tetrahymena clathrin, equivalent to the dominant negative hub domain of mammalian clathrin. In animal cells, this domain does not itself localize to coated pits , but the equivalent Tetrahymena domain localized to endocytic sites, suggesting that some mechanisms used for clathrin localization may differ. However, clathrin recruitment in Tetrahymena, as in animal cells, is likely to involve the AP-2 complex, because the μ subunit localized to the region of endocytic sites. Phylogenetic analysis of AP complexes, from Tetrahymena to humans, indicates that gene duplication and pathway-specific differentiation within this family predated the divergence of ciliates from higher eukaryotes.
Surprisingly, CME in Tetrahymena requires a DRP, Drp1p, which also localizes to endocytic sites. The function of dynamin in endocytosis was first recognized in Drosophila , but no comparable direct role has previously been demonstrated in any unicellular organism, nor for any DRP. The discovery of Drp1p's role in endocytosis in Tetrahymena therefore raises both evolutionary and mechanistic questions.
Evolution of Dynamin-Related Proteins
The most widely conserved role for DRPs is in mitochondrial maintenance, and a DRP with that function has therefore been proposed as a possible founder of the dynamin family . The association with endocytosis in metazoans may have involved subsequent gene duplication and neofunctionalization in that lineage. The endocytic function of Drp1p in Tetrahymena raises the possibility that endocytosis was a more ancestral function for dynamins, which was retained in metazoans and ciliates but lost in representatives from at least three other lineages, i.e., Fungi, trypanosomes, and red algae. This scenario was not, however, supported by our extensive phylogenetic analysis. Classical metazoan dynamins associate in a clade distinct from Drp1p. This was true whether the whole proteins, or individual domains, were compared, which argues against the idea that clustering may reflect lineage-specific partial gene conversion. Similarly, Drp1p was more related to a cornucopia of DRPs in both ciliates and Plasmodium, than to any metazoan protein. This clustering according to lineage, rather than according to function, suggests that dynamins independently underwent duplication and neofunctionalization in the Alveolates, a family including ciliates and Plasmodium. We therefore hypothesize that the functional similarity between classical dynamins and Drp1p reflects independent innovations, within the same protein family, in two distant lineages. Many DRPs may be fundamentally similar in their mechanism of action, namely, membrane deformation upon protein self-assembly, so one important class of innovations may be accounted for simply by mutation-induced changes in subcellular targeting.
Our discovery may not represent a unique example in the evolution of the dynamin family. Both T. thermophila Drp6p and Homo sapiens MxB are targeted to nuclear pores, but the functional relationship between the two proteins remains to be investigated. Moreover, the phylogenetic relationship is also ambiguous, because both are at the ends of long branches in a relatively bare region of the tree where some important branch nodes have intermediate bootstrap values. However, the phylogeny may become more robust as more protist genomes are sequenced. Future analysis may therefore reveal that Drp6p and MxB were independently recruited to play similar roles. Another potential example comes from VPS1, a S. cerevisiae DRP involved in vacuolar protein sorting, which is phylogenetically linked with mitochondrial DRPs (see Figure 8). However, interpreting the phylogeny of VPS1 is complicated because both it and mammalian DLP1, a “mitochondrial” DRP, also function in peroxisomal division [48–50]. Additionally, no mammalian dynamin or DRP has been clearly demonstrated to be functionally equivalent to VPS1. In this case, therefore, the issue of functional convergence is unresolved.
An unresolved issue, not accounted for in the phylogenetic analysis, is the existence of classical dynamins with PRDs and PH domains in Arabidopsis. However, their relationship to metazoan dynamins is currently ambiguous, because the plant proteins are strikingly diverged in sequence, including within the otherwise strictly conserved catalytic GTPase motifs, and their roles are not yet clear . Another informative lineage may be that of Dictyostelium discoideum, where disruption of a DRP gene resulted in pleiotropic defects in organelle morphology, cytokinesis, and endocytosis .
Mechanism of Dynamin Function in Endocytosis
The role of Drp1p in endocytosis was also unexpected because the Tetrahymena protein lacks two domains important for the activity of classical dynamin. The absence of a PRD in Drp1p suggested that Drp1p's function does not depend upon actin recruitment. While essential for endocytosis in S. cerevisiae, actin appears to have a less critical role in animal cells , although recent work suggests some role for actin at several stages of vesicle formation . In Tetrahymena, neither cytB nor latrunculin A, at levels that completely blocked phagocytosis, had a discernible effect upon FM1–43 internalization. We note, however, that this organism appears to encode at least four actin genes, whose sequences are highly divergent for such an otherwise highly conserved protein (unpublished data). Therefore, we cannot rule out that some actin isoforms, resistant to these agents, may be involved.
Also missing in Drp1p, but present in classical dynamins, is the PH domain. To determine how Drp1p is targeted in its absence, we characterized additional Tetrahymena DRP family members to identify a paralog suitable for constructing informative chimeras. The Tetrahymena genome contains eight DRP genes, an unusually large number when compared to other unicellular organisms. Similarly, the genome of Paramecium appears to contain nine DRP genes. The apparent lineage-specific expansion of this gene family may reflect the elaborate endomembrane system of ciliates . To our surprise, a GFP-tagged DRP in Tetrahymena, Drp6p, targeted to the nuclear envelope. This distinct localization combined with structural similarity provided us with a partner for chimera analysis.
Analysis of a set of DRP1-DRP6 chimeras demonstrated that localization depended on the two C-terminal domains of the protein. The more important was the DTD, because this domain by itself gave partial localization. Based on its location in the primary sequence, the DTD is likely to occupy the same position as the PH domain in classical dynamin, also involved in localization. The DTD shows no sequence similarity to a PH domain, however. It is unlikely to represent a functional PH domain diverged to the point of being unrecognizable, because highly conserved PH domains are easily recognized in other Tetrahymena genes (unpublished data). These observations are consistent with the hypothesis of independent innovation of ciliate and metazoan endocytic dynamins but are challenging to reconcile with a model based on shared derivation and multiple losses in other lineages.
Our results on targeting determinants are similar, but not identical, to those from a similar domain-swapping approach in a study of dynamin-2 and a mitochondrial DRP, DLP1, in mammalian cells . In that study, DLP1 targeting required determinants in the C-terminal domains but also in the middle domain. Because the middle domain is involved in self-assembly, this requirement suggested that localization involves motifs whose affinity is too low, in the monomeric state, for effective targeting. Consistent with this idea, we found that the DTDs and GEDs of Drp1p were targeted to endocytic sites only in the context of the holo-protein. However, and unlike DLP1, targeting was efficient even if the middle domain came from Drp6p. One possibility is that the chimera containing the Drp6p middle domain in a Drp1p backbone undergoes efficient self-assembly, in a way that is not possible for the corresponding domains in DLP1 and dynamin-2. This difference in interchangeability is not, however, supported by the sequences themselves, because Drp1p and Drp6p appear more unrelated than DLP1 and dynamin-2. A second possibility is that Drp1p targeting does not require self-assembly. This issue, as well as the mechanism of targeting, will be clarified in future studies.
Parasomal Sacs and Ciliate Physiology
Our results suggest that CME in Tetrahymena is essential, and future work may identify the physiological cargoes in this pathway. The proximity of parasomal sacs to basal bodies, and the presence of AP-2, suggests the possibility that these sites are adapted for uptake of sensory receptors on cilia, either for turnover or for signaling from endosomes . Complete inhibition of visible FM1–43 uptake, in cells expressing clathrin dominant negative constructs, is consistent with the idea that no compensatory pathways of clathrin-independent internalization exist at these sites or elsewhere on the cell surface, although we cannot rule out the possibility of dominant negative inhibition of a parallel pathway that utilizes some common machinery.
In conclusion, our study reveals unexpected relationships, both molecular and evolutionary, between endocytosis in ciliates and animals. This includes the sharing of some features that are absent in fungi, even though the fungal and animal lineages are much more closely related than either is to ciliates . The tools available in Tetrahymena  should facilitate the discovery and analysis of regulatory features of the endocytic pathway mediated by clathrin and Drp1p. Whether convergent evolution of function has occurred within the dynamin family, and how frequently, may be further illuminated by analysis of the large family of DRPs in ciliates.
Materials and Methods
Tetrahymena strains and culture conditions.
Wild-type B2086, CU427, and CU428.1 strains of T. thermophila were provided by Peter Bruns (Cornell University). Strain B*VI was provided by Sally Allen (University of Michigan). Unless stated otherwise, cells were grown at 30 °C in SPP medium (1% proteose peptone, 0.2% dextrose, 0.1% yeast extract, 0.009% ferric EDTA). For conjugation, cells of different mating types growing in log-phase were washed, starved (16–20 h at 30 °C), and mixed in DMC, a one-tenth dilution of Dryl's (1.7 mM sodium citrate, 1 mM NaH2PO4, 1 mM Na2HPO4, 1.5 mM CaCl2) supplemented with an additional 0.1 mM MgCl2 and 0.5 mM CaCl2.
CHC hub, AP μ subunits, and dynamin-related genes.
A single, CHC homolog (CHC1) was identified from whole genome sequence of Tetrahymena macronuclear DNA (preliminary sequence data were obtained from The Institute for Genomic Research Web site at http://www.tigr.org). Using primers designed from genomic sequence, the 3′ portion of the gene encoding the hub fragment was amplified by PCR using a cDNA library from growing Tetrahymena . AP-1 μ subunit (APM1A), AP-2 μ subunit (APM2), and a dynamin-related (DRP1) homolog were identified from ESTs (unpublished data) and full-length clones were amplified by PCR. An additional AP-1 μ subunit gene (APM1B), a putative AP-4 μ subunit homolog (APM4), and seven additional DRP genes (DRP2 through DRP8) were identified from genome sequence. Full-length DRP6 was amplified from genomic DNA. All PCRs were performed with Pfu-Ultra Taq polymerase (Stratagene, La Jolla, California, United States). Products were cloned into pCRII (Invitrogen, Carlsbad, California, United States) and sequenced to confirm accuracy.
Dynamin domains were defined using the NCBI Conserved Domains database (http://www.ncbi.nlm.nih.gov/Structure/cdd/cdd.shtml) and were aligned using ClustalW (http://www.ebi.ac.uk/clustalw/), as were AP μ subunit sequences. Unambiguously aligned regions of sequence were identified by eye and used for analysis. Protein maximum likelihood analysis was done using PROML (Phylip 3.6; Joe Felsenstein, University of Washington). The topology shown is the best tree generated by PROML. Bootstrapping analysis by maximum likelihood and maximum parsimony using PROTPARS was performed with 100 datasets. All alignments are available upon request.
Construction of DRP1 germline knockout strains.
The neo3 cassette  was ligated into a genomic clone of DRP1 at EcoRI sites to generate the drp1::neo3 construct (see Figure 5A). B2086 and CU428 cells were mixed for 2.5 h and transformed with linearized drp1::neo3 by biolistic particle bombardment to target DRP1 in the micronucleus by homologous recombination. Knockout heterokaryon strains with disrupted DRP1 in the micronucleus and wild-type copies of DRP1 in the somatic macronucleus were isolated as described . Subsequent matings of the germline knockout strains resulted in drug-resistant progeny with disrupted DRP1 in both nuclei.
Construction and expression of transgenes.
Two constructs were designed to rescue the progeny of DRP1 germline knockout matings. A DRP1-HA construct was built by ligating the HA epitope sequence into PmeI and XhoI sites upstream of a modified DRP1 genomic clone. The DRP1-MTT1 construct was built by replacing the MTT1 gene with a cDNA clone of DRP1 in a plasmid containing the MTT1 locus . Knockout heterokaryons were mixed for 24 h and transformed with these linearized constructs by biolistic bombardment. Drug-resistant clones were recovered and, in the case of the DRP1-MTT1-expressing cells, maintained in 1 μg/ml cadmium. An additional strain was derived from the DRP1-HA line, by transforming it biolistically with the APM2-GFP fusion. For this transformation, the APM2-GFP fusion was engineered into a vector (nCV-B) that permits selection with Blasticidin (60 μg/ml) .
Other monomeric eGFP (GFP) fusions and dominant negative DRP1 alleles resided in a modified version of the rDNA expression vector pVGF (Meng-Chao Yao, FHCRC, Seattle, Washington, United States). Genes were inserted downstream of the inducible MTT1 promoter and GFP with a ligation into XhoI and ApaI sites. APM1A, APM1B, APM2, DRP1, DRP6, and the hub portion of CHC1 were each amplified by PCR with flanking XhoI and ApaI sites. Chimeras between DRP1 and DRP6 were assembled by an overlap PCR strategy  with domain borders defined by the NCBI Conserved Domains database and refined by eye to match between DRP1 and DRP6. The dominant negative alleles DRP1-K51E and DRP1-T72F were generated by site-directed mutagenesis PCR (Stratagene) and ligated into pVGF via PmeI and ApaI sites that excluded GFP from the constructs. B2086 and CU428 cells were mixed for 10 h and transformed with plasmid by electroporation . To bring transgenes into expression, cells were treated with 1 μg/ml cadmium for 12 to 16 h, unless otherwise noted. A complete description of the strains used in this study is found in Table S1.
All assays were performed with log-phase growing cells starved for 2 h in DMC. Cells were treated with 5 μM FM1–43 (Molecular Probes, Eugene, Oregon, United States) and placed under coverslips for immediate viewing. For time-course assays, cells were treated with FM1–43 for 5 min, washed three times in DMC, and immobilized using a rotocompressor (made by Warren Ringlien, Carleton College, Northfield, Minnesota, United States) for observation over a time course.
FM1–43 uptake comparisons between strains were performed by treating CU428 with 200 ng/ml DAPI in DMC for 5 min. Cells were washed and mixed with an equal number of cells expressing either the CHC1 hub fragment or the K51E allele of DRP1 after 3 h in 1 μg/ml cadmium. The same mixing protocol was used for cells treated with 25 μM cytB for 30 min or 10 μM latrunculin A for 5 min, or DRP1-MTT1 cells maintained without cadmium for 16 h. All cell mixtures were treated with 10 μM FM1–43 for 5 min, washed three times, and photographed after 10 min. For experiments with cytB, the drug was also included during the FM1–43 incubation in some trials.
To quantify uptake, 20 representative images per experiment were analyzed on a Macintosh computer using NIH Image 1.63 (http://rsb.info.nih.gov/nih-image/). The images chosen were those in which both a control cell and an experimental cell were captured in a single frame. Mean density measurements from each set of cells were averaged for comparison. To assess phagocytic uptake in cytB-treated cells, 0.1% India ink was substituted for FM1–43.
Immunocytochemistry and fluorescence microscopy.
Cells were fixed and prepared as described previously  but with incubations performed at room temperature. Basal bodies were visualized using a 1:1,000 dilution of monoclonal antibody 20H5, recognizing centrin (provided by Jeff Salisbury, Mayo Clinic, Rochester, Minnesota, United States), followed by 1% (v/v) Texas red-conjugated goat anti-mouse antibody (Jackson ImmunoResearch, West Grove, Pennsylvania, United States). Similarly, Drp1p-HA was visualized using a 1:1,000 dilution of monoclonal HA.11 (Covance, Princeton, New Jersey, United States). For two-color labeling, GFP fluorescence was enhanced by including 0.5% (v/v) rabbit anti-GFP primary antibodies (Molecular Probes), followed by 1% (v/v) fluorescein-conjugated anti-rabbit antibody (Jackson ImmunoResearch). This also guaranteed detection of the entire pool of GFP-labeled protein. Samples were viewed under a Zeiss (Thornwood, New York, United States) Axiovert microscope interfaced with a Zeiss LSM 510 confocal laser system and software. Endocytic uptake assays were observed using a Zeiss Axioplan 2 microscope interfaced with a Zeiss Axiocam and Axiovision software.
Cryofixation and immunoelectron microscopy.
Cells were grown in SPP with 150 mM mannitol and 2 μg/ml CdCl2. After cells were collected via centrifugation, they were washed with SPP and mannitol, and a few microliters of the cell pellet/slurry were transferred to an aluminum planchette (Type A) with a 100-μm-deep well (engineering office of M. Wohlwend, Senwald, Switzerland) and sandwiched with the flat side of a Type B aluminum planchette, coated with hexadecene . Cells were cryofixed in a BAL-TEC (Balzers, Switzerland) HPM-010 high-pressure freezer and then freeze-substituted in 0.25% glutaraldehyde and 0.1% uranyl acetate in acetone. Embedding was as described by Giddings  except that isopropyl alcohol was used in place of methanol to maintain the sample at −45 °C for polymerization of the HM20.
Embedded cells were serially sectioned (50–60 nm) and put on formvar-coated nickel grids. Some sections were immunolabeled with a polyclonal anti-GFP antibody diluted 1:200 in a blocking solution of 1% nonfat dry milk in PBST and 15 nm of colloidal gold-conjugated secondary antibodies (Ted Pella, Redding, California, United States). Samples were stained with 2% uranyl acetate in 70% methanol/30% water for 5 min and lead citrate for 4 min. The sections were viewed on a Philips (Eindhoven, Netherlands) CM10 electron microscope operating at 80 kV. Images were captured with a Gatan (Pleasanton, California, United States) digital camera and viewed with the Digital Micrograph Software package (Gatan).
For Southern analysis, genomic DNA was prepared from CU428-, DRP1-MTT1-, and DRP1-HA-expressing cells and detected with a probe corresponding to the 5′ EcoRI restriction fragment of DRP1. Northern blotting of total RNA extracted from CU428- and DRP1-MTT1-expressing cells maintained with and without cadmium, and DRP1-HA- expressing cells was performed following standard techniques  using a DRP1 riboprobe. A cross-reactive band near 1 kb serves as a loading control. For Western analysis, whole-cell lysates were prepared as described previously . GFP-tagged chimeras of Drp1p and Drp6p were detected using 0.125% (v/v) rabbit anti-GFP primary antibodies (Molecular Probes), followed by 0.1% (v/v) AP-conjugated anti-rabbit antibody (Jackson ImmunoResearch).
Figure S1. Alignment of DRPs from Tetrahymena with Dynamin-1 (H. sapiens)
The peptide sequence alignment was generated using ClustalX and highlights residues that are completely conserved (*), strongly conserved (:), and weakly conserved (.). The color coding indicates which residues are small/hydrophobic (blue), acidic (purple), basic (red), hydroxyl/amine (green), glycines (brown), and prolines (yellow). Also indicated are domain boundaries defined using the NCBI Conserved Domains database, the strictly conserved catalytic motifs in the GTPase domain, and the residues where substitutions generated dominant negative alleles of DRP1 (arrowheads).
(1.4 MB DOC)
Figure S2. Expression of DRP4-GFP and DRP7-GFP
(A) Confocal sections of a live cell expressing DRP7-GFP (under the MTT1 promoter) are shown at the cortex, i.e., just beneath the cell surface (left), and at the middle of the cell (middle). Most GFP signal is at the cortex.
(B) A confocal section from the middle of a live cell expressing DRP4-GFP (under the MTT1 promoter) showing that punctate GFP fluorescence is distributed throughout the cytoplasm (right). Bar = 5μm.
(C) DRP7-GFP-expressing cells were incubated for 60 min in 50 nM MitoTracker Red CMXRos (Molecular Probes). Shown is a cortical confocal section of a living cell, revealing association of Drp7p-GFP with mitochondria. Bars = 5 μm.
(21.3 MB EPS)
Figure S3. Phylogenetic Tree of Dynamin and DRPs from a Bayesian Approach
The alignment used for maximum likelihood and maximum parsimony analysis in Figure 6 was subjected to Bayesian-based tree construction using MrBayes v3.0 . After the burn-in phase, every 100th sample of 1 × 106 generations was considered. The resulting 50% majority rule consensus tree is shown with percent posterior probabilities indicated at each node.
(168 KB EPS)
Table S1. Strains Used in This Study
(32 KB DOC)
The Tetrahymena and Paramecium genes discussed in this paper have been submitted to GenBank (http://www.ncbi.nlm.nih.gov/Genbank/) under the following accession numbers: Tetrahymena APM1A (DQ219841), APM1B (DQ219842), APM2 (DQ219843), CHC1_hub (DQ219844), DRP1 (DQ219845), DRP4 (DQ219846), DRP6 (DQ219847), and DRP7 (DQ219848); and Paramecium DRPA1 (CR856028), DRPA2 (CR856027), DRPB1 (CR856026), DRPB2 (CR856025), DRPC1 (CR856024), DRPC2 (CR856023), DRPD (CR856022), DRPE (CR856021), and DRPF (CR856020).
We wish to thank Manyuan Long, J. J. Emerson, Nate Pearson, Steve Dorus, and David Witonsky (University of Chicago) for assistance and advice on phylogenetic analysis. We acknowledge Rohan Purvanik for his contributions to the construction of DRP chimeras. Alex Stemm-Wolf (University of Colorado, Boulder) provided assistance with immunoelectron microscopy, while Joe Frankel (University of Iowa), Grant Bowman, Andy Cowan, Kyle Edwards, Adam Linstedt, Harmit Malik, Clive Palfrey, and M. Nasone provided valuable comments and advice. LS gratefully acknowledges support from the Ministere de l'Education Nationale de la Recherche et de la Technologie, programs “Centre de Ressources Biologiques” and ACI IMPbio (contract 2004 14). NCE was supported by National Institutes of Health (NIH) National Institute of General Medicine Sciences Training Grant GM-07197. APT acknowledges funding from NIH grant GM-592688 and National Science Foundation grant MCB-0422011. MW was supported by NIH grant GM-067898.
NCE and APT conceived and designed the experiments. NCE and GM performed the experiments. NCE, GM, MW, and APT analyzed the data. MW, LS, and APT contributed reagents/materials/analysis tools. NCE and APT wrote the paper.
- 1. Conner SD, Schmid SL (2003) Regulated portals of entry into the cell. Nature 422: 37–44.
- 2. Brodsky FM, Chen CY, Knuehl C, Towler MC, Wakeham DE (2001) Biological basket weaving: Formation and function of clathrin-coated vesicles. Annu Rev Cell Dev Biol 17: 517–568.
- 3. Kirchhausen T (1999) Adaptors for clathrin-mediated traffic. Annu Rev Cell Dev Biol 15: 705–732.
- 4. Marks B, Stowell MH, Vallis Y, Mills IG, Gibson A, et al. (2001) GTPase activity of dynamin and resulting conformation change are essential for endocytosis. Nature 410: 231–235.
- 5. Chen YJ, Zhang P, Egelman EH, Hinshaw JE (2004) The stalk region of dynamin drives the constriction of dynamin tubes. Nat Struct Mol Biol 11: 574–575.
- 6. Sever S, Muhlberg AB, Schmid SL (1999) Impairment of dynamin's GAP domain stimulates receptor-mediated endocytosis. Nature 398: 481–486.
- 7. Song BD, Schmid SL (2003) A molecular motor or a regulator? Dynamin's in a class of its own. Biochemistry 42: 1369–1376.
- 8. Kaksonen M, Sun Y, Drubin DG (2003) A pathway for association of receptors, adaptors, and actin during endocytic internalization. Cell 115: 475–487.
- 9. Newpher TM, Smith RP, Lemmon V, Lemmon SK (2005) In vivo dynamics of clathrin and its adaptor-dependent recruitment to the actin-based endocytic machinery in yeast. Dev Cell 9: 87–98.
- 10. Yeung BG, Phan HL, Payne GS (1999) Adaptor complex-independent clathrin function in yeast. Mol Biol Cell 10: 3643–3659.
- 11. Geli MI, Riezman H (1998) Endocytic internalization in yeast and animal cells: Similar and different. J Cell Sci 111: 1031–1037.
- 12. Osteryoung KW, Nunnari J (2003) The division of endosymbiotic organelles. Science 302: 1698–1704.
- 13. Praefcke GJ, McMahon HT (2004) The dynamin superfamily: Universal membrane tubulation and fission molecules? Nat Rev Mol Cell Biol 5: 133–147.
- 14. Grunfelder CG, Engstler M, Weise F, Schwarz H, Stierhof YD, et al. (2003) Endocytosis of a glycosylphosphatidylinositol-anchored protein via clathrin-coated vesicles, sorting by default in endosomes, and exocytosis via RAB11-positive carriers. Mol Biol Cell 14: 2029–2040.
- 15. Morgan GW, Goulding D, Field MC (2004) The single dynamin-like protein of Trypanosoma brucei regulates mitochondrial division and is not required for endocytosis. J Biol Chem 279: 10692–10701.
- 16. Nishida K, Takahara M, Miyagishima SY, Kuroiwa H, Matsuzaki M, et al. (2003) Dynamic recruitment of dynamin for final mitochondrial severance in a primitive red alga. Proc Natl Acad Sci U S A 100: 2146–2151.
- 17. Miyagishima SY, Nishida K, Mori T, Matsuzaki M, Higashiyama T, et al. (2003) A plant-specific dynamin-related protein forms a ring at the chloroplast division site. Plant Cell 15: 655–665.
- 18. Vallis Y, Wigge P, Marks B, Evans PR, McMahon HT (1999) Importance of the pleckstrin homology domain of dynamin in clathrin-mediated endocytosis. Curr Biol 9: 257–260.
- 19. Orth JD, McNiven MA (2003) Dynamin at the actin-membrane interface. Curr Opin Cell Biol 15: 31–39.
- 20. Jin JB, Kim YA, Kim SJ, Lee SH, Kim DH, et al. (2001) A new dynamin-like protein, ADL6, is involved in trafficking from the trans-Golgi network to the central vacuole in Arabidopsis. Plant Cell 13: 1511–1526.
- 21. Hong Z, Bednarek SY, Blumwald E, Hwang I, Jurgens G, et al. (2003) A unified nomenclature for Arabidopsis dynamin-related large GTPases based on homology and possible functions. Plant Mol Biol 53: 261–265.
- 22. Nilsson JR, van Deurs B (1983) Coated pits with pinocytosis in Tetrahymena. J Cell Sci 63: 209–222.
- 23. Allen RD, Schroeder CC, Fok AK (1992) Endosomal system of Paramecium: Coated pits to early endosomes. J Cell Sci 101: 449–461.
- 24. Cochilla AJ, Angleson JK, Betz WJ (1999) Monitoring secretory membrane with FM1–43 fluorescence. Annu Rev Neurosci 22: 1–10.
- 25. Nelsen EM (1978) Transformation in Tetrahymena thermophila. Development of an inducible phenotype. Dev Biol 66: 17–31.
- 26. Liu SH, Wong ML, Craik CS, Brodsky FM (1995) Regulation of clathrin assembly and trimerization defined using recombinant triskelion hubs. Cell 83: 257–267.
- 27. Shang Y, Song X, Bowen J, Corstanje R, Gao Y, et al. (2002) A robust inducible-repressible promoter greatly facilitates gene knockouts, conditional expression, and overexpression of homologous and heterologous genes in Tetrahymena thermophila. Proc Natl Acad Sci U S A 99: 3734–3739.
- 28. Chilcoat ND, Melia SM, Haddad A, Turkewitz AP (1996) Granule lattice protein 1 (Grl1p), an acidic, calcium-binding protein in Tetrahymena thermophila dense-core secretory granules, influences granule size, shape, content organization, and release but not protein sorting or condensation. J Cell Biol 135: 1775–1787.
- 29. Boehm M, Bonifacino JS (2001) Adaptins: The final recount. Mol Biol Cell 12: 2907–2920.
- 30. Morgan GW, Hall BS, Denny PW, Field MC, Carrington M (2002) The endocytic apparatus of the kinetoplastida. Part II: Machinery and components of the system. Trends Parasitol 18: 540–546.
- 31. Karrer KM (2000) Tetrahymena genetics: Two nuclei are better than one. Methods Cell Biol 62: 127–186.
- 32. Damke H, Binns DD, Ueda H, Schmid SL, Baba T (2001) Dynamin GTPase domain mutants block endocytic vesicle formation at morphologically distinct stages. Mol Biol Cell 12: 2578–2589.
- 33. van der Bliek AM (1999) Functional diversity in the dynamin family. Trends Cell Biol 9: 96–102.
- 34. Miyagishima SY, Nishida K, Kuroiwa T (2003) An evolutionary puzzle: Chloroplast and mitochondrial division rings. Trends Plant Sci 8: 432–438.
- 35. Fujimoto LM, Roth R, Heuser JE, Schmid SL (2000) Actin assembly plays a variable, but not obligatory role in receptor-mediated endocytosis in mammalian cells. Traffic 1: 161–171.
- 36. Engqvist-Goldstein AE, Drubin DG (2003) Actin assembly and endocytosis: From yeast to mammals. Annu Rev Cell Dev Biol 19: 287–332.
- 37. Garcia-Salcedo JA, Perez-Morga D, Gijon P, Dilbeck V, Pays E, et al. (2004) A differential role for actin during the life cycle of Trypanosoma brucei. EMBO J 23: 780–789.
- 38. Yu X, Cai M (2004) The yeast dynamin-related GTPase Vps1p functions in the organization of the actin cytoskeleton via interaction with Sla1p. J Cell Sci 117: 3839–3853.
- 39. Nilsson JR (1977) Fine structure and RNA synthesis of Tetrahymena during cytochalasin B inhibition of phagocytosis. J Cell Sci 27: 115–126.
- 40. Achiriloaie M, Barylko B, Albanesi JP (1999) Essential role of the dynamin pleckstrin homology domain in receptor-mediated endocytosis. Mol Cell Biol 19: 1410–1415.
- 41. King MC, Raposo G, Lemmon MA (2004) Inhibition of nuclear import and cell-cycle progression by mutated forms of the dynamin-like GTPase MxB. Proc Natl Acad Sci U S A 101: 8957–8962.
- 42. Smirnova E, Shurland DL, Newman-Smith ED, Pishvaee B, van der Bliek AM (1999) A model for dynamin self-assembly based on binding between three different protein domains. J Biol Chem 274: 14942–14947.
- 43. Dacks JB, Doolittle WF (2002) Novel syntaxin gene sequences from Giardia, Trypanosoma and algae: Implications for the ancient evolution of the eukaryotic endomembrane system. J Cell Sci 115: 1635–1642.
- 44. Dacks JB, Doolittle WF (2004) Molecular and phylogenetic characterization of syntaxin genes from parasitic protozoa. Mol Biochem Parasitol 136: 123–136.
- 45. Baldauf SL, Roger AJ, Wenk-Siefert I, Doolittle WF (2000) A kingdom-level phylogeny of eukaryotes based on combined protein data. Science 290: 972–977.
- 46. Liu SH, Marks MS, Brodsky FM (1998) A dominant-negative clathrin mutant differentially affects trafficking of molecules with distinct sorting motifs in the class II major histocompatibility complex (MHC) pathway. J Cell Biol 140: 1023–1037.
- 47. van der Bliek AM, Meyerowitz EM (1991) Dynamin-like protein encoded by the Drosophila shibire gene associated with vesicular traffic. Nature 351: 411–414.
- 48. Smirnova E, Griparic L, Shurland DL, van der Bliek AM (2001) Dynamin-related protein Drp1 is required for mitochondrial division in mammalian cells. Mol Biol Cell 12: 2245–2256.
- 49. Li X, Gould SJ (2003) The dynamin-like GTPase DLP1 is essential for peroxisome division and is recruited to peroxisomes in part by PEX11. J Biol Chem 278: 17012–17020.
- 50. Hoepfner D, van den Berg M, Philippsen P, Tabak HF, Hettema EH (2001) A role for Vps1p, actin, and the Myo2p motor in peroxisome abundance and inheritance in Saccharomyces cerevisiae. J Cell Biol 155: 979–990.
- 51. Wienke DC, Knetsch ML, Neuhaus EM, Reedy MC, Manstein DJ (1999) Disruption of a dynamin homologue affects endocytosis, organelle morphology, and cytokinesis in Dictyostelium discoideum. Mol Biol Cell 10: 225–243.
- 52. Yarar D, Waterman-Storer CM, Schmid SL (2005) A dynamic actin cytoskeleton functions at multiple stages of clathrin-mediated endocytosis. Mol Biol Cell 16: 964–975.
- 53. Frankel J (2000) Cell biology of Tetrahymena thermophila. Methods Cell Biol 62: 27–125.
- 54. Pitts KR, McNiven MA, Yoon Y (2004) Mitochondria-specific function of the dynamin family of protein DLP1 is mediated by its C-terminal domains. J Biol Chem 279: 50286–50294.
- 55. Vallesi A, Ballarini P, Di Pretoro B, Alimenti C, Miceli C, et al. (2005) Autocrine, mitogenic pheromone receptor loop of the ciliate Euplotes raikovi: Pheromone-induced receptor internalization. Eukaryot Cell 4: 1221–1227.
- 56. Turkewitz AP, Orias E, Kapler G (2002) Functional genomics: The coming of age for Tetrahymena thermophila. Trends Genet 18: 35–40.
- 57. Chilcoat ND, Elde NC, Turkewitz AP (2001) An antisense approach to phenotype-based gene cloning in Tetrahymena. Proc Natl Acad Sci U S A 98: 8709–8713.
- 58. Hai B, Gorovsky MA (1997) Germ-line knockout heterokaryons of an essential alpha-tubulin gene enable high-frequency gene replacement and a test of gene transfer from somatic to germ-line nuclei in Tetrahymena thermophila. Proc Natl Acad Sci U S A 94: 1310–1315.
- 59. Bowman GR, Elde NC, Morgan G, Winey M, Turkewitz AP (2005) Core formation and the acquisition of fusion competence are linked during secretory granule maturation in Tetrahymena. Traffic 6: 303–323.
- 60. Horton RM, Ho SN, Pullen JK, Hunt HD, Cai Z, et al. (1993) Gene splicing by overlap extension. Methods Enzymol 217: 270–279.
- 61. Gaertig J, Gu L, Hai B, Gorovsky MA (1994) High frequency vector-mediated transformation and gene replacement in Tetrahymena. Nucleic Acids Res 22: 5391–5398.
- 62. Bowman GR, Turkewitz AP (2001) Analysis of a mutant exhibiting conditional sorting to dense core secretory granules in Tetrahymena thermophila. Genetics 159: 1605–1616.
- 63. Giddings TH (2003) Freeze-substitution protocols for improved visualization of membranes in high-pressure frozen samples. J Microsc 212: 53–61.
- 64. Sambrook J, Fritsch EJ, Maniatis T (1989) Molecular cloning: A laboratory manual, 2nd ed. Plainview (New York): Cold Spring Harbor Laboratory Press. 1 v.
- 65. Huelsenbeck JP, Ronquist F (2001) MRBAYES: Bayesian inference of phylogeny. Bioinformatics 17: 754–755.