Rocket Launcher Mechanism of Collaborative Actin Assembly Defined by Single-Molecule Imaging

See allHide authors and affiliations

Science  01 Jun 2012:
Vol. 336, Issue 6085, pp. 1164-1168
DOI: 10.1126/science.1218062


Interacting sets of actin assembly factors work together in cells, but the underlying mechanisms have remained obscure. We used triple-color single-molecule fluorescence microscopy to image the tumor suppressor adenomatous polyposis coli (APC) and the formin mDia1 during filament assembly. Complexes consisting of APC, mDia1, and actin monomers initiated actin filament formation, overcoming inhibition by capping protein and profilin. Upon filament polymerization, the complexes separated, with mDia1 moving processively on growing barbed ends while APC remained at the site of nucleation. Thus, the two assembly factors directly interact to initiate filament assembly and then separate but retain independent associations with either end of the growing filament.

Regulation of actin assembly is a fundamental requirement in all eukaryotic cells, and a growing number of factors have been identified that either inhibit or promote this process. For example, the combined presence of the actin monomer–binding protein profilin and the filament end–binding capping protein (CapZ) strongly suppresses both spontaneous filament nucleation and elongation. Thus, filament assembly in vivo requires nucleation and elongation factors to overcome these barriers to assembly (13). The formation of most cellular actin structures depends on two or more such factors, which often interact directly. A formin is a component of many actin assembly–promoting factor (APF) pairs that likely function together in vivo: the formins FMN/Cappucino (Capu) and Spire (4), the formin Bni1 and Bud6 (5), the formin mDia1 and adenomatous polyposis coli (APC) (6), and the formin dDia2 and Dictyostelium vasodilator-stimulated phosphoprotein (DdVASP) (7).

The dimeric formin–homology 2 (FH2) domain of formins processively tracks the growing barbed end of the actin filament, protecting it from capping proteins (810). Adjacent FH1 domains recruit profilin-actin complexes and can increase the rate of elongation at barbed ends (11). Whereas profilin enhances formin-mediated filament elongation, its presence also strongly suppresses filament nucleation by formins (12). Collaboration of formins with other APFs that bind multiple actin monomers (46, 13) may be required to overcome the inhibitory effects of profilin and capping protein. However, direct evidence for this hypothesis has been lacking. To address this, we reconstituted mDia1-APC–mediated actin assembly with purified, fluorescently tagged proteins and used multiwavelength single-molecule TIRFM (total internal reflection fluorescence microscopy) to directly visualize and define the mechanisms promoting collaborative filament assembly.

For single-molecule imaging, we purified a soluble, modified O6-alkylguanine-DNA alkyltransferase (AGT)-tagged (also known as SNAP–tag) C-terminal fragment of APC (APC-C): residues 2130–2843, encompassing its “Basic” domain, which is sufficient to mediate actin nucleation, and the domain that binds EB1 (a microtubule end–binding protein) (6, 14). SNAP–APC-C labeled with SNAP-surface-647 (herein named SNAP-647-APC-C) displayed activities identical to those of APC-C in pyrene-actin assembly assays (fig. S1A). Photobleaching data suggested that most SNAP-647-APC-C molecules are dimeric (fig. S1, B and C; and movie S1), consistent with hydrodynamic studies on maltose-binding protein–tagged APC-C (6).

APC, like Spire and Bud6, has been proposed to catalyze actin nucleation by binding actin monomers to form an F-actin seed (46). We used dual-color TIRFM to directly visualize surface-adsorbed SNAP-647-APC-C molecules, appearing as discrete spots, during the assembly of Oregon Green (OG)–actin filaments (Fig. 1A and movie S2). From some of these spots, we observed actin filaments emerge and grow primarily from their barbed ends, and APC did not alter the growth rate in the presence or absence of profilin (fig. S2A). Further, APC-C did not block polymerization at pointed ends (fig. S2B), which suggests that it stays bound to the filament at the site of nucleation.

Fig. 1

Single-molecule analysis of the APC-C– and mDia1-C–mediated actin assembly processes. (A) Dual-color TIRFM of OG-actin filaments (1 μM, 10% labeled, green) originating from SNAP-647-APC-C spots (10 nM, red). Green arrowheads mark the growing barbed ends. (B) Fluorescence intensity analysis of number of SNAP-647-APC-C subunits at filament ends. (C) Micrographs of OG-actin accumulation at SNAP-647-APC-C spots in the absence and presence of latB. (D and E) Dual-color TIRFM of OG-actin filaments (1 μM, 10% labeled, green) being elongated by single SNAP-549-mDia1-C molecules (red) without (D) and with (E) profilin. Time is given in seconds. Red arrowheads in (E) mark the formin molecule associated with the barbed end. (F) Average elongation rates of mDia1-C– and SNAP-549-mDia1-C–assembled filaments without and with profilin. Error bars represent SE, n ≥ 12, N = 3.

For the majority of surface-tethered filaments (88 out of 106 observed), APC fluorescence remained visible at the nucleation site 10 min after nucleation, which suggested a thermodynamically stable association. We also observed filaments with APC-C associated at their ends freely diffusing near the surface, which suggested that the stable association is not due to surface tethering. At concentrations ≥10 nM SNAP-647-APC-C, we occasionally observed APC-C accumulating on filament sides, which led to bundling (fig. S3 and movie S3), consistent with previous reports (15).

Quantifying the oligomeric state of APC-C at the onset of nucleation suggested that an APC-C dimer was sufficient to nucleate filament assembly, although a minority of the filaments originated from spots consisting of more than two APC-C subunits (Fig. 1B). When we included latrunculin B (latB), which associates with actin monomers and blocks polymerization, OG-actin still accumulated in some of the SNAP-647-APC-C spots; however, no filaments polymerized (Fig. 1C and movie S4). These observations suggest that nucleation by APC involves monomer recruitment, as opposed to capture of spontaneously formed F-actin intermediates.

We next purified SNAP-tagged mDia1-C—which contains FH1, FH2, and diaphanous autoregulatory (DAD) domains—and fluorescently labeled it (SNAP-549-mDia1-C). Single-molecule photobleaching experiments suggested that the SNAP-549-mDia1-C preparation is predominantly dimeric but also contains higher-order oligomers (fig. S4, A and B). SNAP-549-mDia1-C and unlabeled mDia1-C stimulated indistinguishable rates of pyrene-actin assembly (fig. S4C). Using dual-color TIRFM, we observed single SNAP-549-mDia1-C molecules translocating with the growing barbed ends of filaments both in the presence and absence of profilin (Fig. 1, D and E; fig. S5; and movies S5, S6, and S7). Processive association of the formin was verified by additional lines of evidence (figs. S5 and S6 and movie S7). mDia1-C and SNAP-549-mDia1-C each elongated filaments at equivalent rates in presence and absence of profilin (Fig. 1F). Similar results were obtained with SNAP-549-mDia1-C in the presence of 1 nM CapZ. Our observations directly confirm that individual formin molecules processively track filament barbed ends, with or without profilin, and accelerate elongation in a profilin-dependent manner (11).

APC binds mDia formins in solution (16). Therefore, we used dual-color TIRFM to investigate interactions between SNAP-647-APC-C and SNAP-549-mDia1-C molecules. After mixing the two labeled proteins in solution, we examined the composition of complexes that adsorbed to the surface. We found that 51 ± 2.3% (SEM) of SNAP-549-mDia-C spots colocalized with SNAP-647-APC-C spots (Fig. 2A). Coincidental colocalization was minimal (1.7%) (14). Taking into account the labeling stoichiometries of both proteins, our analysis is consistent with a model in which most of the fluorescent spots contain two SNAP-647-APC-C and two SNAP-549-mDia1-C molecules (Fig. 2, A and B). Similar results were obtained in the presence of latB-sequestered actin monomers [60 ± 3.9% (SEM) colocalization] (Fig. 2, C and D). These data suggest that actin monomers neither interfere with APC-formin interactions nor change the oligomeric state of the complex and may even modestly promote APC-formin interactions. Using triple-color TIRFM, we observed 54.8 ± 6.6% (SEM) of APC/mDia1 complexes stably occupied by latB–OG-actin (Fig. 2, E and F). These assemblies may represent nucleation intermediates that are normally short-lived during filament assembly but can be trapped by latB. In the absence of mDia1, OG-actin accumulation was observed in 40.5 ± 4.6% (SEM) of SNAP-647-APC-C spots, but in the absence of APC-C, OG-actin accumulation was observed in only 4.0 ± 0.7% (SEM) of SNAP-549-mDia1-C spots (Fig. 2F). These observations suggest that APC-C is the primary actin monomer–recruiting factor in the APC-mDia1 complex. Profilin did not change OG-actin accumulation in SNAP-647-APC-C spots but resulted in an increase in OG-actin accumulation to 20.2 ± 1.8% (SEM) in SNAP-549-mDia1 spots, which likely represents profilin-actin recruitment by FH1 domains. Consistent with this view, competition with a 50-fold excess of profilin over OG-actin reduced the number of formin spots, with OG-actin accumulation to 8.5 ± 0.9% (SEM).

Fig. 2

Association of APC-C and mDia1-C and formation of tripartite complexes with G-actin. (A) Colocalization of SNAP-647-APC-C and SNAP-549-mDia1-C in surface-adsorbed complexes. The proteins (200 nM each) were preincubated for 10 min, diluted 200-fold, and visualized by TIRFM. Spots emitting fluorescence from SNAP-549, SNAP-647, or both were counted. (B) Oligomeric state of APC-C–mDia1-C complexes (n = 91) determined by fluorescence intensity analysis for mDia1-C and photobleaching step analysis for APC-C (see methods). (C and D) Same as (A) and (B), except that 20 μM latB-sequestered actin monomers were included during preincubation (100 nM in final reaction). In (D), n = 43. Error bars represent SE. (E) Tripartite complexes formed by preincubating 200 nM SNAP-647-APC-C, 200 nM SNAP-549-mDia1-C, or 8 μM latB–OG-actin and then diluting 200-fold before surface adsorption. Field-of-view (top) and time-lapse record of a single spot containing all three proteins (bottom). (F) Fraction of APC-mDia1 spots that contain detectable OG-actin in the presence or absence of profilin (see the supplementary materials).

Next, we used triple-color TIRFM to define the sequence of events and spatial locations of SNAP-549-mDia1-C and SNAP-647-APC-C during collaborative filament assembly. We included CapZ and profilin to reconstitute cellular barriers to actin assembly. Tripartite complexes consisting of SNAP-549-mDia1-C, SNAP-647-APC-C, and OG-actin were observed (asterisk in Fig. 3A). Filaments grew from some of these spots. Concomitant with filament growth, APC and mDia1 invariably separated (n > 100), which left SNAP-647-APC-C at the pointed end and SNAP-549-mDia1-C translocating on the growing barbed end (Fig. 3A, fig. S8, and movie S8). The same was observed in the absence of profilin (fig. S9 and movie S9). Most nucleation complexes had already separated by the start of imaging, as indicated by the presence of many short filaments carrying SNAP-549-mDia1-C at their barbed ends and SNAP-647-APC-C at their pointed ends (fig. S10). Note that SNAP-647-APC-C molecules were never seen bound to processively moving formins (n > 100), which suggested that mDia1 molecules in the process of catalyzing barbed-end polymerization may not be capable of interacting with APC-C. Filaments bearing APC-C on one end and mDia1 on the other end showed rates of elongation indistinguishable from rates observed for mDia1-C without APC-C (fig. S11). Thus, elongation of filaments is likely to be purely mDia1-catalyzed with no contribution from APC.

Fig. 3

Single-molecule visualization of APC-C and mDia1-C collaborating to assemble actin filaments. (A) Triple-color TIRFM of the assembly of 1 μM OG-actin (green) in the presence of 50 pM SNAP-549-mDia1-C (red), 5 nM SNAP-647-APC-C (blue), 1 nM CapZ, and 5 μM profilin. Asterisk indicates APC-mDia1-actin nucleation complex. Images (left; time in seconds) and corresponding profiles of fluorescence intensity along the length of the filament (right). Arrowheads mark the barbed end (green), mDia1 (red), and APC (blue). (B) (Left) Density of formin-elongated filaments per 100- × 100-μm area for reactions containing 80 pM SNAP-549-mDia1-C, 1 nM CapZ, or variable concentrations of SNAP-APC-C, ±5 μM profilin. Error bars represent SD, N = 3. (Right) APC-C–dependent fold increase in density of formin-elongated filaments in the presence (black) and absence (gray) of profilin. (C) Same as (B), except using non–SNAP-tagged APC-C, mDia1-C and tail-less mDia1 FH1FH2. (D) Western blot with antibody against the six-histidine tag (6His) showing levels of mDia1-C and mDia1 FH1FH2 (both tagged with 6His) in supernatants after depletion by glutathione S-transferase (GST)–tagged (control) or GST–APC-C beads. Error bars represent SD, N = 2. (E) Proposed “rocket launcher” model for mDia1-APC collaboration during actin filament assembly (details in text).

Increasing concentrations of APC-C produced increasing numbers of SNAP-549-mDia1-C–elongated filaments in the presence of profilin and CapZ (Fig. 3B and fig. S12A). Quantitatively similar results were obtained using unlabeled APC-C and mDia1-C (Fig. 3C). Moreover, longer preincubation of mDia1-C and APC-C increased the number of mDia1-C–elongated filaments by about another twofold (fig. S12B). These effects of APC-C were less pronounced in the absence of profilin (Fig. 3B), which suggested that APC-C plays a key role in overcoming the nucleation barrier imposed by profilin.

Two other APFs (Spire and Bud6) were recently shown to bind to formin C-terminal tail sequences (4, 5, 13, 17). Similarly, we found that APC-C–coated beads depleted soluble mDia1-C but not mDia1-FH1FH2 (which lacks tail sequences) from supernatants (Fig. 3D), which suggests that APC binds mDia1 tail sequences. Moreover, APC-C failed to increase actin assembly activity in combination with mDia1-FH1FH2 (red bars, Fig. 3C and fig. S13). These observations strongly suggest that direct interactions between APC and mDia1 tail sequences are required for their collaborative effects in actin assembly.

Taken together, our results suggest a mechanism (Fig. 3E) in which APC-C dimers recruit actin monomers and bind the tail region of mDia1-C to form a tripartite nucleation complex. At the onset of actin polymerization, the complex separates, leaving APC-C stably associated near the pointed end, while mDia1-C is propelled away on the rapidly growing barbed end (Fig. 3E). By this mechanism, APC plays the central role in assembling the nucleation seed, and the formin then detaches and serves as the elongation catalyst. It remains to be seen whether the same mechanism applies to other pairs of APFs that are known to interact, e.g., Spire with Capu and Bud6 with Bni1 (4, 5). This work may have important implications for APC biological function. Full-length APC is a large protein that binds to numerous other cellular factors and functions in a wide variety of regulatory pathways (18). Thus, the mechanism for APC-mDia1 collaboration described here may result in site-specific actin assembly and, possibly, tethering of polymerizing actin filaments at their pointed ends to APC-binding partners (e.g., IQGAP1, microtubule plus ends) (19, 20). These phenomena may serve to promote directed cell migration or other functions that require coordinated reorganization of the actin cytoskeleton with respect to other cellular structures.

Supplementary Materials

Materials and Methods

Figs. S1 to S13

References (2131)

Movies S1 to S9

References and Notes

  1. Materials and methods are available as supplementary materials on Science Online.
  2. Acknowledgments: We thank B. McCartney, H. Higgs, J. Moseley, S. Reck-Petersen, and B. Smith for helpful comments on the manuscript; K. Okada and A. Deaconescu for purifying CapZ and generating the SNAP-APC-C plasmid; and B. Smith for advice on single-molecule imaging. The project was supported by grants from Deutsche Forschungsgemeinschaft (BR 4116/1-1 to D.B.), NSF (DMR-MRSEC-0820492 to J.G and B.G), and NIH (GM43369 and GM81648 to J.G., GM083137 to B.G.).

Stay Connected to Science

Navigate This Article