Centrosomes must resist microtubule-mediated forces for mitotic chromosome segregation. During mitotic exit, however, centrosomes are deformed and fractured by those same forces, which is a key step in centrosome disassembly. How the functional material properties of centrosomes change throughout the cell cycle, and how they are molecularly tuned, remain unknown. Here, we used optically induced flow perturbations to determine the molecular basis of centrosome strength and ductility in C. elegans embryos. We found that both properties declined sharply at anaphase onset, long before natural disassembly. This mechanical transition required PP2A phosphatase and correlated with inactivation of PLK-1 (Polo kinase) and SPD-2 (Cep192). In vitro, PLK-1 and SPD-2 directly protected centrosome scaffolds from force-induced disassembly. Our results suggest that, before anaphase, PLK-1 and SPD-2 respectively confer strength and ductility to the centrosome scaffold so that it can resist microtubule-pulling forces. In anaphase, centrosomes lose PLK-1 and SPD-2 and transition to a weak, brittle state that enables force-mediated centrosome disassembly.
Centrosomes nucleate and anchor microtubules that make up the mitotic spindle, which segregates chromosomes during somatic cell division. Centrosomes are micrometer-scale, membraneless organelles containing a structured centriole pair surrounded by an amorphous protein mass called pericentriolar material (PCM). PCM carries out most of the functions of a centrosome, including directing cell polarity, cell migration, and chromosomal segregation (Conduit et al., 2015; Woodruff et al., 2014).
For chromosome segregation, centrosomes must bear microtubule-dependent loads that create tensile stresses. Motor proteins anchored at the plasma membrane attach to and walk along astral microtubules extending from centrosomes. These spatially fixed motors thus generate cortically directed pulling forces on centrosomes, and the balance of those forces determines the ultimate position of the mitotic spindle (Colombo et al., 2003; Gönczy et al., 2001; Grill et al., 2001; McNally, 2013; Nguyen-Ngoc et al., 2007). During this time, centrosomes maintain a compact, spherical shape. However, once chromosome segregation is complete and the cell exits mitosis, centrosomes are deformed and fractured by the same microtubule-mediated forces, which is a pronounced event during centrosome disassembly (Megraw et al., 2002; Severson and Bowerman, 2003). How the cell regulates the structural and material integrity of centrosomes is unclear. One possibility is that an increase in cortical forces during mitotic exit induces centrosome disassembly. In Caenorhabditis elegans embryos, the magnitude of microtubule-mediated pulling forces does increase during the metaphase–anaphase transition, yet the same increase in pulling forces also occurs in metaphase-arrested embryos without leading to centrosome deformation or fracture (Labbé et al., 2004). Furthermore, artificially increasing pulling forces via csnk-1 RNAi does not cause premature centrosome disassembly (Magescas et al., 2019; Panbianco et al., 2008). These studies suggest that induction of centrosome deformation and fracture during mitotic exit cannot be sufficiently explained by increased microtubule-mediated forces. An alternative hypothesis is that centrosome mechanical properties significantly change to permit force-driven fracture and dispersal during mitotic exit.
PCM provides most of the mass and microtubule nucleation capacity of a centrosome, and it is widely believed to be responsible for bearing microtubule-mediated forces. PCM is dynamic and expands in size and complexity as cells prepare for mitosis. Self-assembly of coiled-coil proteins, such as Cdk5Rap2 (vertebrates), Centrosomin (Drosophila melanogaster), and SPD-5 (C. elegans), creates the underlying structural scaffold of PCM, which then recruits “client” proteins that nucleate and regulate microtubules (Conduit et al., 2010, 2014a; Fong et al., 2008; Hamill et al., 2002; Woodruff et al., 2015, 2017). Formation of such micrometer-scale scaffolds requires additional regulatory clients such as Polo kinase, Aurora A kinase, and SPD-2/centrosomal protein of 192 kD (Cep192; Conduit et al., 2014a,b; Gomez-Ferreria et al., 2007; Hamill et al., 2002; Hannak et al., 2001; Haren et al., 2009; Lee and Rhee, 2011; Pelletier et al., 2004; Zhu et al., 2008). PCM disassembles at the end of each cell cycle, but the mechanism is not well understood. While this process involves microtubule-mediated PCM fracture and reversal of Polo kinase phosphorylation (Enos et al., 2018; Magescas et al., 2019; Pimenta-Marques et al., 2016), it remains unclear how PCM fracture is initiated, which key molecular targets are dephosphorylated, if these activities are linked, and how dynamic material changes might contribute to the disassembly process.
A material’s load-bearing capacity is determined by its ability to resist permanent deformation and fracture upon stress. In materials science, these properties are described as “strength” and “ductility,” respectively. Strength is achieved through high-affinity bonding and serves to maintain the material’s shape but can sometimes sacrifice flexibility. Ductility is achieved through breakage and reformation of sacrificial bonds or localized neighbor exchange, which dissipates energy over time but sacrifices the material’s shape. For example, glass requires large forces to deform, but it cannot deform much before shattering; thus, glass has high strength and low ductility. On the other hand, chewing gum is easily deformed, and it will stretch to great lengths before breaking; thus, gum has low strength and high ductility. Materials with the highest load-bearing capacity are those that combine strength and ductility, such as rubbers, polyampholyte gels, and high-entropy alloys (George et al., 2019; Sun et al., 2013). Over time, these properties can change via chemical or physical modifications, which is referred to as “material aging.”
For the centrosome, it remains unexplored how molecular-level interactions between PCM proteins generate meso-level mechanical properties such as strength and ductility and how these properties change with time. The noncovalent interactions between PCM scaffold proteins, as well as cross-linking of scaffold molecules by PCM clients, could all contribute. In general, characterizing the mechanical properties of living soft matter, such as cells, organelles, and protein assemblies, has been challenging due to their size (submicrometer scale) and low abundance (submilligram scale). Techniques such as atomic force microscopy and optical trapping can be useful in this respect, but they are limited to easily accessible samples, such as the outer membrane of cultured cells and reconstituted protein complexes. As a complementary method to actively probe mechanical properties in cells with limited accessibility, we previously used focused light-induced cytoplasmic streaming (FLUCS; Mittasch et al., 2018). Specifically, we showed how FLUCS can reveal robust power-law rheology signatures within the cell cytoplasm to distinguish between fluid and gel-like states. Fluids undergo unconstrained motion proportional to stimulus time (i.e., they flow), while solids and gels undergo only limited deformations, which stall after small amounts of time due to their intrinsic elastic constraints. As FLUCS functions via thermoviscous flows, which develop independent of the absolute viscosity of the fluid (Weinert and Braun, 2008; Weinert et al., 2008), FLUCS is particularly suited to distinguish between highly viscous phases and elastic phases. Such a distinction cannot be achieved by passive microrheology, as these two states would exhibit the same fingerprint of reduced motion.
The C. elegans embryo is an ideal system to dissect the molecular determinants of PCM load-bearing capacity. First, C. elegans has a limited core set of proteins needed for rapid PCM assembly and disassembly, most of which are conserved across eukaryotes: PLK-1 (Polo kinase homologue), SPD-2 (Cep192 homologue), SPD-5 (functional homologue of Centrosomin and Cdk5Rap2), and LET-92SUR-6 (protein phosphatase 2AB55α [PP2AB55α] homologue; Decker et al., 2011; Enos et al., 2018; Hamill et al., 2002; Kemp et al., 2004; Magescas et al., 2019; Pelletier et al., 2004; Schlaitz et al., 2007). Second, it is possible to reconstitute PCM assembly and microtubule nucleation in vitro using purified C. elegans proteins (Woodruff et al., 2015, 2017). These experiments previously revealed that PCM forms via self-assembly of SPD-5 into spherical, micrometer-scale scaffolds that recruit PCM client proteins. SPD-2 and PLK-1 enhance SPD-5 self-assembly, while PP2ASUR-6 removes PLK-1–derived phosphates and promotes PCM disassembly. However, these experiments did not reveal the mechanical properties of the SPD-5 scaffold or how they are tuned in a cell cycle–dependent manner.
Here, we ask (a) how centrosomes undergo dynamic structural changes to withstand high tensile stresses in mitosis but not during mitotic exit; (b) which mechanical properties are associated with these distinct functional states; and (c) which molecular players and logics regulate the transient existence of centrosomes. To answer these questions, we combined genetics and pharmacologic intervention with FLUCS to study the mechanical properties of PCM in C. elegans embryos. Our results revealed that PCM transitions from a strong, ductile state in metaphase to a weak, brittle state in anaphase. This mechanical transition is promoted by PP2ASUR-6 and opposed by PLK-1 and SPD-2. Our data suggest that mitotic PCM is a composite of a stable SPD-5 scaffold and proteins that dynamically reinforce the scaffold, such as PLK-1 and SPD-2. During spindle assembly, accumulation of PLK-1 and SPD-2 render the PCM tough enough to resist microtubule-pulling forces. During mitotic exit, departure of PLK-1 and SPD-2 weakens the PCM scaffold to allow microtubule-mediated fracture and disassembly. Thus, PCM undergoes cell cycle–regulated material aging that functions to promote its disassembly.
FLUCS reveals weakening of the PCM scaffold at anaphase onset in
C. elegans embryos
To study the molecular determinants of PCM load-bearing capacity, we studied C. elegans one-cell embryos, in which growth and disassembly of the PCM scaffold are easily visualized using fluorescently labeled SPD-5 (mMaple::SPD-5; Fig. 1 A). During spindle assembly, the C. elegans PCM scaffold is subject to microtubule-mediated pulling forces, but it maintains its spherical shape and structural integrity. However, during telophase, those same pulling forces deform and fracture the PCM scaffold (Fig. 1 A; Enos et al., 2018; Severson and Bowerman, 2003). We hypothesized that PCM undergoes an intrinsic mechanical transition from a strong, tough state in metaphase to a weak state in telophase.
We probed PCM mechanical properties using FLUCS-generated flows complemented with fluorescent imaging. Specifically, we equipped a spinning disk confocal microscope with a laser control unit (wavelength = 1,455 nm) that creates precise, submillisecond thermal manipulations (Fig. 1 B). Unidirectional scans with this laser at 1,500 Hz create traveling temperature fields that are sufficient to induce flows in a viscous medium, including embryonic cytoplasm (Mittasch et al., 2018; see Materials and methods). A Peltier-cooled stage insert dissipates excess heat to keep the sample within its physiological temperature range.
We applied FLUCS to C. elegans embryos expressing mMaple::SPD-5 and mCherry-labeled histones (mCherry::H2B). For each experiment, we induced flows crossing the cytoplasm and continuing through the middle of a centrosome, which should apply stress to the PCM scaffold orthogonal to microtubule-derived tensile stresses (Fig. 1 C). Based on previous experiments (Mittasch et al., 2018), we predicted that cytoplasmic shear flows should weaken the PCM by the relative displacement of scaffold proteins and create a virtual “notch” in the flow path. We used three different amplitudes for the scanning infrared laser (25, 32, and 40 mW) to generate cytoplasmic flow velocities ranging from 5 to 20 µm/min (Fig. 1 D and Video 1); these flows scaled quadratically with laser power (R2 = 0.97), as one would expect for a predominantly viscous medium (Fig. S1 A). Simultaneously, we cooled embryos to 17°C, such that the embryo cytoplasm never exceeded 23°C during laser scanning (C. elegans embryos develop properly at any temperature between 16°C and 25°C; Begasse et al., 2015).
As shown in Fig. 1 E, FLUCS deformed and fractured mature PCM in anaphase embryos. We also detected a slight increase in cytoplasmic fluorescence surrounding the PCM during FLUCS, indicating that flows can dislodge SPD-5 from the PCM, as predicted (Fig. S1 B). FLUCS-induced PCM deformation differed starkly between cell cycle stages. FLUCS was not able to visibly deform PCM during metaphase or before, even though flows were strong enough to detach the centrosome from the spindle and move it toward the cell cortex or out of the focal plane (Figs. 1 D and S1 C and Videos 2 and 3). In contrast, FLUCS deformed and eventually fractured PCM during anaphase and telophase (Fig. 1, E and F; and Videos 4 and 5); in these experiments, the untreated centrosome remained intact.
We then quantified (a) the deformation rate, defined by the rate of PCM length change orthogonal to the flow direction, and (b) the fracture probability, defined by the chance that PCM segments detach completely after FLUCS (Fig. 1 G; see Materials and methods). The PCM deformation rate and fracture probability increased with increasing flow velocity and progression through mitosis (Fig. 1, H and I). To pinpoint when PCM becomes susceptible to FLUCS-induced deformation, we continuously applied FLUCS to centrosomes starting in metaphase and continuing into anaphase. PCM remained spherical and intact during metaphase, but then fractured immediately after anaphase onset, as marked by chromosome segregation (Fig. S1 D and Video 6). Our results suggest that PCM resistance to deformation and fracture is high during metaphase and then declines at anaphase onset, ∼150 s before full PCM disassembly in telophase. We refer to this change in PCM mechanical properties hereon as the “PCM weakening transition.”
Since the generation of FLUCS is accompanied by local temperature gradients, we tested if temperature alone affects PCM structure. Bidirectional scanning at 10 kHz creates local temperature gradients without flow, and these conditions did not cause significant PCM deformation or fracture (Fig. 1, H and I; and Fig. S1 E). Thus, centrosome perturbation during FLUCS is primarily due to the flows and not temperature gradients per se. Furthermore, embryos developed properly after cessation of FLUCS (Fig. S1 F; Mittasch et al., 2018). We conclude that this established method can be used to study organelles inside a living cell.
PCM weakens in anaphase independent of cortical force generation
We next wondered if our FLUCS results could be explained by cell cycle–dependent changes in PCM mechanical properties or changes in cortical force generation. During the metaphase–anaphase transition in early C. elegans embryos, cortical pulling forces increase to induce transverse oscillations and posterior positioning of the mitotic spindle (Pecreaux et al., 2006). Depleting G protein regulator 1 (GPR-1) and GPR-2 (gpr-1/2(RNAi)) significantly reduces cortical microtubule-pulling forces and prevents spindle displacement, spindle oscillation, and PCM deformation and fracture (Colombo et al., 2003; Enos et al., 2018; Grill et al., 2003; Magescas et al., 2019; Pecreaux et al., 2006). Thus, we performed FLUCS in gpr-1/2(RNAi) embryos, where we expect only residual cortical forces that remain relatively constant throughout mitosis.
In both wild-type and gpr-1/2(RNAi) embryos, FLUCS deformed PCM in anaphase and telophase, but not in metaphase. However, in gpr-1/2(RNAi) embryos, FLUCS-induced PCM deformation rates were slower (Fig. 2, A and B; and Fig. S2 A), and FLUCS caused fracturing only in telophase (Fig. 2 C). These results suggest that PCM mechanical properties change during mitotic exit, but that cortical pulling forces are required to disperse and fracture the preweakened PCM scaffold. To further test this idea, we applied 10 µg/ml nocodazole to depolymerize microtubules and performed high-flow FLUCS. Under these conditions, FLUCS did not visibly affect PCM during metaphase but did dislodge SPD-5 protein from the PCM during telophase (Fig. 2 D); we did not observe stretching or clean fracture of the PCM during any cell cycle stage. These results indicate that (a) the interactions between SPD-5 scaffold molecules weaken independently of microtubule-pulling forces during mitotic exit, and (b) microtubule-pulling forces are required for stretching and fracture of the PCM during mitotic exit. To test if microtubule-mediated pulling forces could be sufficient to deform PCM already in metaphase, we depleted a negative regulator of GPR-1/2, casein kinase 1 gamma (csnk-1(RNAi)), which is reported to increase cortical pulling forces ∼1.5-fold (Panbianco et al., 2008). We did not observe premature deformation or fracture of PCM under these conditions, even though the spindle rocked violently in metaphase (Fig. S2 B). We conclude that an intrinsic mechanical change in the SPD-5 scaffold is the main driver of PCM weakening during anaphase entry.
We next examined the viscoelastic properties of PCM during anaphase by measuring the time-dependent deformation of PCM during FLUCS and relaxation after FLUCS was turned off. We used gpr-1/2(RNAi) embryos to allow residual pulling forces but prevent spindle oscillations, which could complicate our analysis. We observed that continuous application of medium- and high-flow FLUCS in gpr-1/2(RNAi) embryos caused time-dependent strain of the PCM scaffold (Fig. 2 E). Thus, anaphase PCM is ductile and can experience micrometer-scale structural rearrangements without complete fracture during stress. Such behavior is seen in viscous materials. When we turned off FLUCS, PCM remained in its strained, elongated state, indicating the absence of a dominant elastic element strong enough to return the PCM to its original shape (Fig. 2, E and F).
Overall, our FLUCS experiments suggest that the PCM structurally weakens after metaphase. This weakening transition would presumably facilitate PCM disassembly by enabling microtubule-dependent pulling forces to fracture and disperse the PCM scaffold in telophase.
PCM undergoes stepwise compositional changes following anaphase onset
We next investigated the molecular mechanism underlying the PCM weakening transition, in particular, identifying the specific players that determine the dynamic regulation of PCM strength and ductility. PCM is a heterogeneous assembly of proteins required for its assembly and function (Fig. 3 A). In particular, two critical regulatory proteins, PLK-1 and SPD-2, interact with the scaffold protein SPD-5 and enhance its self-assembly into supramolecular structures (Cabral et al., 2019; Decker et al., 2011; Woodruff et al., 2015, 2017). PLK-1 and SPD-2, as well as other PCM-localized client proteins, might also reinforce the mature SPD-5 scaffold. On the other hand, loss or inactivation of these proteins could weaken the PCM scaffold.
To analyze PCM composition changes during anaphase, we visualized nine different GFP-labeled PCM proteins relative to a standard PCM marker, mCherry::γ-tubulin. We then measured the integrated density of PCM-localized mCherry and GFP signals during mitosis (Fig. 3 B). The curves in Fig. 3 D and,Fig. S3 represent averages for >10 experiments (mean ± 95% confidence interval [CI]). mCherry::γ-tubulin signal peaked ∼75–100 s after anaphase onset and then declined, indicating its departure from PCM. GFP::γ-tubulin behaved similarly, as expected (Fig. 3, C and D; and Fig. S3). PLK-1 signal decreased immediately after anaphase onset and was no longer detectable ∼100 s later. SPD-2 also departed from the PCM before γ-tubulin. However, the main scaffold protein SPD-5 departed afterward. All other proteins departed coincidentally with γ-tubulin or soon afterward. The C. elegans homologue of TPX2 (TPXL-1) and Aurora A Kinase (AIR-1) departed in a biphasic manner: an initial loss of signal occurred before γ-tubulin departure, then a second phase occurred after γ-tubulin departure. To compare departure kinetics across all experiments, we determined the halfway point of disassembly for each individual GFP and mCherry curve per experiment and then calculated the time differential between halfway points (ΔtEXIT; Fig. 3 E). The results for anterior and posterior PCM proteins are summarized in Fig. 3, F and G, respectively; statistical analyses are shown in Table S3 and Table S4. A negative ΔtEXIT value indicates GFP::PCM protein departure before γ-tubulin, and a positive value indicates departure after γ-tubulin. Our results reveal that PCM composition changes in a stepwise manner during anaphase: PLK-1 departs first, followed by SPD-2, γ-tubulin, transforming acid coiled coil protein 1 (TAC-1), and finally SPD-5 and proteins that form tight complexes with SPD-5 (regulator of spindle assembly 1 [RSA-1] and RSA-2). TPXL-1 and AIR-1 were more variable in their departure, possibly because they localize to both PCM and microtubules that remain after disassembly of the PCM scaffold (Hannak et al., 2001; Ozlü et al., 2005).
Polo kinase and SPD-2 reinforce the PCM scaffold by increasing its strength and ductility
PLK-1 and SPD-2 are the first proteins to depart the PCM during anaphase, when the PCM begins to weaken. Thus, we hypothesized that PLK-1 and SPD-2 normally reinforce the PCM to achieve full strength and stability in metaphase. If this idea is correct, then acute inhibition of PLK-1 phosphorylation or SPD-2 in metaphase might prematurely weaken the PCM, accelerate its disassembly, or reveal hidden material states not previously visible.
For acute inhibition of PLK-1, we treated semipermeable embryos (via perm-1(RNAi)) with 10 µM Polo kinase inhibitor BI-2536 in prometaphase (Carvalho et al., 2011). After 2 min in drug solution, we applied low-, medium-, and high-flow FLUCS to centrosomes (Fig. 4, A–C). Under these conditions, low- and medium-flow FLUCS deformed metaphase PCM in BI-2536–treated embryos, in contrast to wild-type embryos (Fig. 4 B); in both cases, PCM fracture did not occur. Under high-flow FLUCS, BI-2536 treatment increased the PCM deformation rate as much as ∼11-fold, with fracture occurring only in a minority of the cases (30%; Fig. 4, A and C). The fact that PLK-1 inhibition enabled PCM to be deformed easily without necessarily fracturing suggests that PLK-1 mostly determines PCM strength. This experiment also reveals that wild-type PCM is ductile during metaphase; this could not be observed previously because the deformation resistance of wild-type PCM was too high. BI-2536 treatment also caused premature disassembly of the SPD-5 scaffold in metaphase-arrested embryos, consistent with previous findings (Fig. 4 D; Cabral et al., 2019). Our results show that continuous PLK-1 activity is needed for PCM to achieve full strength and maintain integrity until chromosomes are separated.
Next, we analyzed embryos expressing a temperature-sensitive version of SPD-2 (spd-2(or188ts); Kemp et al., 2004). We mounted spd-2(or188ts) gfp::spd-5 embryos in cold medium and maintained the sample at 17°C while imaging until prometaphase, then upshifted the embryos to 25°C for 1 min to inactivate SPD-2or188ts. We then lowered the temperature to 17°C to perform FLUCS in metaphase as usual (Fig. 4 E; note that because of the local heating caused by FLUCS, the treated centrosome remained at ∼23°C throughout the experiments). The absence of fully functional SPD-2 made PCM more susceptible to FLUCS-induced fracture and disintegration at all applied flow velocities (Fig. 4, E–G). Even in PCM that did not fracture into observable pieces, the GFP∷SPD-5 signal decayed after application of FLUCS (Fig. 4 F). We did not observe this phenotype in wild-type PCM or spd-2 mutant PCM not treated with FLUCS (Fig. 4 F). Our interpretation of these data is that SPD-2 is required for PCM ductility and strength. Without SPD-2, PCM becomes brittle and susceptible to fracture and diffusion-driven departure of constituents after modest mechanical agitation. In line with this view, inactivation of SPD-2 caused premature disassembly of the SPD-5 scaffold in early anaphase, even without FLUCS perturbations (Fig. 4 H). Deformation rates were difficult to measure, because rapid fracture and vanishing GFP::SPD-5 signal precluded a flow analysis. We conclude that both Polo kinase and SPD-2 help PCM achieve maximal strength and ductility to prevent disassembly.
We next used a minimal in vitro system to test if PLK-1 and SPD-2 directly affect the mechanical properties of the SPD-5 scaffold. When incubated in a crowded environment (e.g., >4% polyethylene glycol [PEG]), purified recombinant SPD-5 assembles into micrometer-scale condensates that recruit PLK-1, SPD-2, and other PCM proteins (Woodruff et al., 2017). We could not assess SPD-5 condensates using FLUCS because the condensates were propelled quickly away from the flow path (not depicted); thus, our simplified in vitro conditions do not exactly match those found in native cytoplasm. As another way to assess the strength of SPD-5 interactions, we induced disassembly of young RFP-labeled SPD-5 condensates (500 nM SPD-5::RFP; 5 min after formation) through application of pipetting shear forces and dilution, then measured the amount of condensates that survived using fluorescence microscopy (Fig. 5 A; note that dilution is required to prevent SPD-5 reassembly; thus, this assay tests resistance to disassembly only; Enos et al., 2018). This treatment completely disassembled condensates composed solely of SPD-5 (Fig. 5, B and C). Addition of constitutively active PLK-1 (PLK-1CA; T194D T-loop phosphomimic) or SPD-2 prevented SPD-5 condensate disassembly, with the combination of the two yielding the greatest protection (Fig. 5, B and C). Kinase-dead PLK-1 (PLK-1KD; K67M mutant) did not promote SPD-5 condensate survival. These results suggest that PLK-1 phosphorylation of SPD-5, along with direct binding of SPD-2, reinforces the interactions between SPD-5 molecules and thus enhances the ability of PCM to resist disassembly. Our in vitro and in vivo data together suggest that PLK-1 and SPD-2 tune PCM load-bearing capacity by conferring strength and ductility to the SPD-5 scaffold.
Phosphatase PP2ASUR-6 promotes PCM disassembly by compromising scaffold ductility
We next investigated how embryos promote the PCM weakening transition during anaphase. PP2A phosphatase localizes to the PCM and plays multiple roles in centriole biogenesis, spindle assembly, and mitotic exit (Wlodarchak and Xing, 2016). The C. elegans homologue of PP2A (LET-92) complexed with the B55α regulatory subunit SUR-6 (PP2ASUR-6) is required for complete PCM disassembly (Enos et al., 2018; Magescas et al., 2019). We thus tested if PP2ASUR-6 drives PCM disassembly by compromising the mechanical properties of PCM.
We treated semipermeable one-cell embryos with 10 µM PP2A inhibitor (LB-100) in metaphase and then performed high-flow FLUCS in anaphase. Unlike in wild-type embryos, where PCM fractured quickly after high-flow FLUCS, the PCM in LB-100–treated embryos stretched orthogonal to the induced flow but resisted fracture (Fig. 6 A). PCM deformation velocity was approximately twofold higher (0.26 vs. 0.12 µm/min), initially suggesting that PCM is easier to deform when PP2A is inhibited (Fig. 6 B). However, PP2A inhibition also elevated the ductility of PCM 1.5-fold (final length divided by the original length) and lowered the fracture probability more than twofold in all cell cycle stages (Fig. 6, C and D). In 2 of 10 anaphase embryos treated with LB-100, PCM stretched as much as fourfold in length after FLUCS, reaching up to 10 µm while staying connected. PCM was also more resistant to fracture in embryos depleted of the PP2A regulatory subunit SUR-6 (Fig. S4, A–C). These results suggest that, when PP2A is inhibited, the ductile nature of PCM is preserved throughout anaphase, allowing PCM to absorb more energy overall without fracturing. This is likely achieved through “self-healing,” or the breakage and reformation of weak inter-scaffold interactions. The increase in deformation velocity may then result from ductile PCM becoming easier to stretch as it becomes more extended. On the other hand, wild-type PCM is brittle during anaphase and can only be extended short distances before fracturing. We conclude that PP2A normally functions to eliminate “self-healing” PCM scaffold interactions, thus making PCM brittle during anaphase and susceptible to microtubule-mediated fracture in telophase. Consistent with this conclusion, LB-100 inhibition of PP2A or depletion of its regulatory subunit SUR-6 inhibited SPD-5 scaffold disassembly in telophase (Fig. 6 E; Enos et al., 2018). We speculate that PCM may be less porous in this mutant ductile state compared with the wild-type brittle state, which could delay PCM disassembly further by preventing access of additional disassembly machinery and/or delaying the departure of PLK-1 and SPD-2. Consistent with the latter concept, both let-92 RNAi and sur-6 RNAi impaired SPD-2 and PLK-1 departure from PCM during anaphase (Fig. S4, D–G; Magescas et al., 2019).
To determine when and where PP2A might dephosphorylate PCM proteins, we visualized embryos expressing GFP::LET-92 (Schlaitz et al., 2007). GFP::LET-92 localized to the PCM and persisted there until SPD-5 scaffold disassembly, ∼100 s after PLK-1 had departed from the PCM (Fig. 6 F), consistent with previous observations (Magescas et al., 2019). Our results suggest that, during anaphase, Polo kinase activity at the PCM ceases and PP2A removes Polo-delivered phosphates and contributes to SPD-2 departure. This shift in the balance of phosphorylation and dephosphorylation changes the mechanical properties of the PCM, making it more brittle and susceptible to fracture and dissolution.
Mitotic spindle assembly and positioning require that centrosomes bear tensile microtubule-dependent forces without structural failure. As mitosis ends, however, these same forces are sufficient to deform and fracture centrosomes, facilitating their disassembly. Disassembly is essential to release centrioles and avoid accumulation of old centrosomes over successive rounds of cell division. Here, we combined flow-driven mechanical perturbations in vivo with biochemical reconstitution in vitro to determine the molecular mechanisms regulating deformation resistance and fracture resistance of PCM, the outer and most massive layer of a centrosome.
PCM mechanical properties, function, and renewal can be achieved through transient reinforcement of the PCM scaffold
Using C. elegans embryos as a model system, we found that PCM deformation resistance, fracture resistance, and composition are tuned in a cell cycle–dependent manner (Fig. 7, A and B). During metaphase, PCM resists both microtubule-mediated forces and induced flow perturbations without deforming or fracturing. In this state, PCM is structured as a reinforced composite, comprising a nondynamic scaffold of SPD-5 molecules filled with a dynamic phase of regulatory molecules such as SPD-2 and PLK-1, which frequently bind and unbind the scaffold (Fig. 7 B). During anaphase, PCM loses PLK-1 and SPD-2 and then becomes susceptible to deformation and fracture. During telophase, PCM is at its weakest and is easily fractured and dispersed by microtubule-mediated forces, a hallmark step in the PCM disassembly process.
Our implementation of flow perturbations in vivo using FLUCS reveals how PLK-1, SPD-2, and PP2A contribute to the dynamic mechanical properties of the PCM. We interpret deformation resistance as an indicator of strength and fracture resistance and strain as indicators of ductility. Wild-type metaphase PCM is highly resistant to flow perturbations, but underlying features appear in different mutant states (Fig. 7 C). When PLK-1 is inhibited, the PCM scaffold is easily deformed by FLUCS and stretches without fracturing. Thus, PLK-1 normally maintains PCM strength. On the other hand, when SPD-2 is inhibited, the PCM scaffold is easily fractured and dissolved by FLUCS but does not stretch. Thus, SPD-2 normally maintains PCM ductility and strength. Elimination of either PLK-1 or SPD-2 causes premature PCM disassembly, suggesting that the combination of strength and ductility is necessary for PCM function and maintenance during spindle assembly in metaphase. In anaphase, wild-type PCM is more easily deformed and fractured by FLUCS. Yet, when PP2A is inhibited, PCM is difficult to fracture by FLUCS and instead stretches up to four times its original length, revealing that the high ductility of the PCM, which was established before metaphase, is preserved. Thus, PP2A normally functions to drive PCM disassembly by reducing PCM ductility.
We propose that that the balance of PLK-1, SPD-2, and PP2A activities determines the mechanical properties and assembly/disassembly state of the PCM (Fig. 7 D). In metaphase, PLK-1 phosphorylation of SPD-5 and direct binding of SPD-2 reinforce the SPD-5 scaffold, conferring strength and ductility. During anaphase, PLK-1 and SPD-2 depart from the PCM, while PP2A phosphatase remains and removes PLK-1–derived phosphates. As a result, PCM becomes progressively brittle and weak, allowing microtubule-dependent forces to deform and fracture it in telophase. Since PLK-1 and SPD-2 stabilize the SPD-5 scaffold, but are themselves dynamic, we call this mode of PCM regulation “transient reinforcement.”
Transient reinforcement of the PCM scaffold, in theory, could enable cell cycle–regulated PCM assembly, function, and renewal. In preparation for mitosis, PCM must rapidly assemble and provide a solid foundation for nucleating and anchoring microtubules. If PCM assembly fails, then mitotic spindle assembly and chromosome segregation are severely impaired (Doxsey et al., 1994; Hamill et al., 2002; Sunkel and Glover, 1988). PLK-1 and SPD-2 thus play dual roles in PCM functionality: (a) catalyzing assembly of the PCM scaffold and (b) strengthening it to withstand microtubule-dependent pulling forces (shown here). While PCM is stable during spindle assembly, PCM disassembles in telophase, only to be rebuilt in the next cell cycle. PCM disassembly is essential for entry into various postmitotic states, including the formation of acentriolar oocytes and heart tissue (Pimenta-Marques et al., 2016; Zebrowski et al., 2015). How might transient reinforcement enable PCM disassembly and renewal? Based on in vivo and in vitro FRAP data, PLK-1 and SPD-2 are mobile within the PCM, suggesting that they frequently bind and unbind the SPD-5 scaffold (Laos et al., 2015; Woodruff et al., 2017). Either decreasing their association or increasing their dissociation rates with the SPD-5 scaffold would reduce SPD-2 and PLK-1 levels at the PCM. One potential mechanism is through localized ubiquitination and degradation, which controls Polo kinase levels at centrosomes in human tissue culture cells during anaphase (Lindon and Pines, 2004). It is currently unknown how PCM levels of SPD-2 or its homologue Cep192 are tuned. The completeness and speed of SPD-2 and PLK-1 removal during anaphase are also suggestive of feedback. Thus, the system could be set up such that minor changes to SPD-2 and PLK-1 affinity elicit large, switch-like changes in PCM structure and mechanical properties. Further experiments are needed to define how the other numerous PCM proteins and centriole tethers contribute to PCM mechanical properties. One possible control point is linkage of the SPD-5 scaffold to the centriole via pericentriolar matrix deficient 1 (PCMD-1); inactivation of PCMD-1 or laser ablation of centrioles leads to aberrant PCM deformation, presumably because PCM can no longer fully resist microtubule-pulling forces (Cabral et al., 2019; Erpf et al., 2019).
PCM mechanical properties in other eukaryotes
The mechanical properties of PCM in other species have yet to be determined. We speculate that our transient reinforcement model for tuning PCM load-bearing capacity may be conserved for three reasons. First, diverse eukaryotic species (nematodes, frogs, flies, and human cells) use both Polo kinase and SPD-2/Cep192 to enhance assembly of the PCM scaffold (Conduit et al., 2014b; Decker et al., 2011; Haren et al., 2009; Joukov et al., 2014; Kemp et al., 2004; Pelletier et al., 2004; Woodruff et al., 2015). Second, PP2A is highly conserved in eukaryotes and is required for mitotic exit in these species (Wlodarchak and Xing, 2016). Third, in Drosophila embryos, PCM undergoes cell cycle–regulated deformation and fracture, termed “flaring,” which appears similar to disassembling PCM in C. elegans (Megraw et al., 2002). PCM flares are visible during interphase, cease during metaphase and anaphase, and then escalate during telophase. Flares also require dynamic microtubules. Thus, Drosophila PCM flaring may be due to decreasing PCM strength and ductility during telophase, such that PCM can no longer resist microtubule-mediated forces.
Parallels between PCM and common soft materials in engineering
The mechanical properties and structure of mature PCM are analogous to common composite materials such as flexible plastics and hydrogels. Most modern plastics comprise cross-linked polymer chains embedded with plasticizers, chemicals that make the plastic more flexible and ductile. Over time, these plasticizers exit by diffusion, making the remaining plastic brittle and weak, which is a form of material aging. The rubber sole on a shoe will crack with age; flexibility of the old sole can be restored by impregnating the rubber with a plasticizer such as silicone. For PCM, the SPD-5 scaffold is most similar to the polymer chains, whereas PLK-1 and SPD-2 could act as plasticizers. Similar to aging rubber losing its plasticizers, our results show that the PCM scaffold becomes brittle and weak during anaphase, coincident with both PLK-1 and SPD-2 leaving the PCM.
PCM is also similar to physical composites such as polyampholyte hydrogels, which exhibit a unique combination of high tensile strength and flexibility. Polyampholyte gels comprise polymers cross-linked with a combination of high- and low-affinity noncovalent bonds. Upon stress, the low-affinity bonds break and dissipate energy, while the high-affinity bonds maintain the overall supramolecular structure. The low-affinity bonds then quickly reform, resulting in self-healing that prevents structural fatigue from repeated stresses (Sun et al., 2013). These bonds also make the material more ductile, such that it will undergo plastic deformation instead of fracturing. For PCM, it is possible that PLK-1, SPD-2, and other PCM-resident proteins dissipate stress by unbinding from the PCM scaffold and then rebinding to achieve self-healing. Eliminating these weak interactions would make the PCM weaker and more brittle. This would naturally occur in anaphase as PLK-1 and SPD-2 depart from the PCM. This concept could also explain why FLUCS induces PCM fracture and deformation in metaphase when we acutely inhibit PLK-1 and SPD-2. Alternatively, in PP2A-inhibited embryos, PCM is ductile due to the preservation of low-affinity, self-healing bonds. Although stronger and more ductile than normal, this mutant PCM still weakens and disassembles in telophase, suggesting that another as-yet-unknown process disrupts the strong interactions between SPD-5 molecules.
This work establishes that PCM, the most substantial layer of the centrosome, transitions from a strong, ductile state in metaphase to a weak, brittle state in telophase. This transition is driven by PP2A phosphatase and inactivation of Polo kinase and SPD-2/Cep-192, which are essential for centrosome assembly and reinforce the PCM scaffold during metaphase. This mode of mechanical regulation, which we term transient reinforcement, is a functional form of material aging that allows PCM to resist microtubule-mediated tensile stresses during spindle assembly and then to be fractured and disassembled by similar forces during mitotic exit. Implicitly, our work demonstrates how flow perturbations can reveal functional mechanical states of membraneless organelles in vivo.
Materials and methods
Contact for reagent and resource sharing
Further requests and information for resources and reagents should be directed to and will be fulfilled by the lead contact, Jeffrey Woodruff.
Experimental model and subject details
C. elegans worm strains were grown on nematode growth medium (NGM) plates at 16°C–23°C, following standard protocols (http://www.wormbook.org). Worm strains used in this study are listed in Table S1 and were created using CRISPR (Paix et al., 2015, 2017), MosSCI (Frøkjaer-Jensen et al., 2008), or microparticle bombardment. Cas9 enzyme was purified by the Protein Expression Facility at Max Planck Institute of Molecular Cell Biology and Genetics. The mMaple plasmid (pCFJ350) was provided by Abby Dernburg (University of California, Berkeley, Berkeley, CA). Protein expression plasmids are listed in Table S2. Statistical analyses for Fig. 3 are shown in Table S3 and Table S4. Oligonucleotides for creating the mMaple::SPD-5 CRISPR repair template are listed in Table S5. For expression of recombinant proteins, we used suspended SF9-ESF Spodoptera frugiperda insect cells grown at 27°C in ESF 921 Insect Cell Culture Medium, Protein-Free (Expression Systems), supplemented with FBS (2% final concentration; Lemaitre et al., 2019).
RNAi was done by feeding using sur-6, gpr-2, csnk-1, and perm-1 feeding clones from the Ahringer and Vidal collections (Source BioScience; Rual et al., 2004). The spd-5 feeding clone targets a region that is reencoded in our MosSCI transgenes (Woodruff et al., 2015). Bacteria were seeded onto NGM supplemented with 1 mM IPTG and 100 µg ml−1 ampicillin. For perm-1 feeding plates, 0.1 mM IPTG was used. L4 hermaphrodites were grown at 23°C for 24–28 h for all conditions except perm-1, which was at 20°C for 18–19 h.
Drug treatment of semipermeable embryos
For all drug treatments, C. elegans embryos were permeabilized using perm-1 RNAi (Carvalho et al., 2011) and dissected into a 62% solution of ESF-921 Media (Expression Systems). To arrest the embryos at metaphase, MG-132 (EMD Millipore) was used at 10 µM in 62% ESF, diluted from a 10-mM stock concentration in EtOH. To inhibit PLK-1, BI-2536 (Advanced ChemBlocks) was used at 10 µM, diluted from a 10-mM stock in ethanol. To inhibit PP2A, LB-100 (SelleckChem) was used at 10 µM, diluted from a 10-mM stock in dH2O. Nocodazole (Sigma-Aldrich) was diluted from a 5-mg/ml stock concentration in DMSO. Samples were flushed with water or M9 after each experiment to test for permeability (water will cause swelling and M9 will cause shrinking).
Construction of the FLUCS microscope
To measure the physical material state of centrosomes inside living C. elegans embryos, we performed intracellular flow perturbations by using the previously published technology FLUCS (Mittasch et al., 2018). The FLUCS setup consists of three major modules: (a) an infrared laser scanning unit for thermal manipulations; (b) a microscope allowing simultaneous induction of thermal patterns and performance of high-sensitivity fluorescence imaging; and (c) a heat management stage.
The infrared laser scanning unit consists of a fiber-based infrared Raman laser (CRFL-20-1455-OM1, 20 W, near TEM00 mode profile, Keopsys) with a wavelength of 1,455 nm, operated in continuous-wave mode and linearly polarized using a polarizing beam splitter cube (CCM1-PBS254, Thorlabs). To precisely correct for the divergence of the laser beam, a telescope was used, composed of two telescope lenses with focal lengths of FL1 = 100 mm and FL2 = 150 mm (AC254-C series, Thorlabs). A lambda-half plate (waveplate, 1/2 1550, Edmund Optics) was used to rotate the linearly polarized laser light to match the optical axis of the acoustic-optical deflector (AOD). A variable optical beam expander (4× expander, 36100, Edmund Optics) allows control of the beam diameter (∼1.5-mm beam diameter at back-focal-plane was used) without changing the size of the scan pattern. Rapid (≤1-MHz update rate) and precise (≥100 nm) infrared laser scanning was achieved by using 2D AOD (AA.DTSXY-A6-145, Pegasus Optik), electronic oscillators (AA.DRFAI0Y-B-0-x, Pegasus Optik), and electronic amplifiers of 2.5 W (AA.AMPA-B-34-20.4, Pegasus Optik). The AOD was controlled by generating analogue signals using custom software in LabVIEW (National Instruments) in combination with a PCI (peripheral component interconnect) controller card (PCIe 6369, National Instruments). To precisely translate the AOD-induced beam scanning into the back-focal-plane of the microscope objective lens, a telescope composed of two telescope lenses with focal lengths of FL3 = 300 mm and FL4 = 300 mm (AC254-C series, Thorlabs) was used. A dichroic mirror (F73-705, AHF) was used to couple the infrared laser beam into the light path of the microscope (IX83, Olympus) by selectively reflecting the infrared light but transmitting visible wavelengths that were used for fluorescence imaging.
The microscope was equipped with bright-field and fluorescent imaging optics. For simultaneous high-resolution fluorescence imaging and precise infrared laser scanning, an infrared-coated microscope objective lens (60× UPLSAPO, NA = 1.2, W-IR coating, Olympus) was used, which was operated with heavy water (D2O) as immersion liquid to reduce undesired infrared laser light absorption in the immersion layer. For bright-field illumination, a high-power light-emitting diode (LED; M565L3, Thorlabs) in combination with dedicated LED driver (LEDD1B, Thorlabs) was used. For confocal fluorescence imaging, a VisiScope confocal imaging system (Visitron) coupled to a Yokogawa CSU-X1-A12 scan head and an iXON Ultra electron-multiplying charge-coupled device camera (EMCCD; Andor) were used.
The heat management unit consisted of a thin sample mounting chamber based on a standard coverslip (18 × 18 × 0.17 mm; Menzel) facing the objective lens and a high-thermal-conductive sapphire cover slide (thermal conductivity of 27.1 W/m ⋅ K, SMS-7521, UQG Optics) closing the sandwich-like chamber from the top. To efficiently remove the induced heat from the samples, e.g., C. elegans embryos, the sapphire slide was actively cooled from room temperature to 17°C. This active cooling was performed by using Peltier elements (TES1-127021, TEC, Conrad) glued to the sapphire slides. The cooling power of the Peltier elements was controlled by a proportional–integral–derivative hardware controller (TEC-1089-SV, Meerstetter Engineering). A custom-built water-cooling stage was used to dissipate the heat produced by the Peltier elements. The height of the buffer-filled chamber was defined using polystyrene beads (Polybead, Polysciences) with a diameter of 15 µm. The height of the resulting chamber was measured by locating the upper and lower chamber surface using a piezo stage.
Application of FLUCS within embryos
Late L4 hermaphrodites were grown for 18–19 h on standard NGM or perm-1 feeding plates. Worms were then dissected on an 18 × 18–mm coverslip (0.17-mm thickness) in 6 µl of M9 buffer or 62% ESF 921 (for permeabilized embryos) with 15-µm polystyrene beads. The sample was placed onto a sapphire microscope slide equipped with Peltier cooling elements, and the coverslip was sealed with dental silicone (Twinsil, Picodent). The cooling stage and sample were then mounted on the FLUCS microscope stage. Embryos were identified and staged using a 10× air objective and imaged with a 60× 1.2-NA Plan Apochromat water immersion objective (Olympus) using 488- and 561-nm laser illumination, 1 × 1 binning, and 2-s intervals.
Hydrodynamic flows were generated by scanning the 1,455-nm laser through either (a) center of centrosome or (b) cytoplasm for velocity calibration. Custom-written LabVIEW software superimposes the scan path of the infrared laser with the high-resolution image of the camera. The subpixel alignment of the induced flow field and the camera image was verified routinely before the embryo experiments by using fluorescent tracer particles immersed in a highly viscous sucrose solution. FLUCS experiments used unidirectional but repeated laser scans with 1.5-kHz scan frequency, a scan length of 30 µm, and three different laser powers (25, 32, and 40 mW).
Centrosomes were targeted for FLUCS at metaphase, anaphase, or telophase. Centrosomes were affected by FLUCS between 30 and 60 s. For experiments requiring drug treatment, worms were dissected in 6 µl of the specific drug solution and quickly placed on the microscope within 1–2 min. To maintain consistency of drug treatment duration, only embryos found exactly at prometaphase (for metaphase experiments) and metaphase (for anaphase experiments) were then targeted for FLUCS. Temperature-sensitive worms were dissected in cold 62% ESF-921 medium on a cooled dissecting scope and quickly mounted onto the cooling stage, which was maintained at 17°C. At prometaphase, temperature was upshifted to 25°C for 1 min, then decreased to 17°C. Centrosomes were then targeted for FLUCS at metaphase.
Confocal microscopy and live-cell imaging
Adult worms were dissected in M9 before being mounted on a 5% agar pad for imaging. For live-cell imaging with drug treatments, perm-1 adult worms were dissected in 8–10 µl of 62% ESF 921 with 15-µm polystyrene beads (Sigma-Aldrich) on a 22 × 50–mm coverslip. Samples were mounted on a 1-mm-thick glass slide with 2 × 6–mm laser-cut holes 30 mm apart (Potomac) to produce a flow chamber. In one open chamber, 40 µl of the drug solution in 62% ESF was added during prometaphase. Liquid was wicked from the opposite chamber using a Kimwipe to then allow more of the drug solution to be added to the sample. To arrest embryos in metaphase, perm-1 adult worms were dissected in 10 µM MG-132 solution. Cell cycle stage was indicated based on mCherry::HIS-58 fluorescence and cell morphology (metaphase, aligned chromosomes; anaphase, chromosomes separate; telophase, chromosomes decondense and cytokinetic furrow ingresses).
Time-lapse images were taken using an inverted Nikon Eclipse Ti microscope with a Yokogawa spinning disk confocal head (CSU-X1), piezo Z stage, and an iXon Ultra EMCCD camera (Andor) controlled by Metamorph software. On this system, the 60× 1.4-NA Apochromat oil objective was used to acquire 36 × 0.5-µm Z-stacks every 10 s, with 100-ms exposures and 2 × 2 binning. For PCM localization in csnk-1(RNAi) embryos and PP2A localization, time-lapse images were acquired with an inverted Nikon Eclipse Ti2-E microscope with a Yokogawa confocal scanner unit (CSU-W1), piezo Z stage, and an iXon Ultra 888 EMCCD camera (Andor), controlled by Nikon Elements software. For most experiments, we used a 60× 1.2-NA Plan Apochromat water-immersion objective to acquire 35 × 0.5-µm Z-stacks every 10 s, with 100-ms exposures and 2 × 2 binning. Simultaneous imaging with the 488- and 561-nm lasers was achieved using an OptoSplit II beam splitter (Cairn). For LET-92::GFP imaging, a 100× 1.35-NA Plan Apochromat silicone oil objective was used to acquire 11 × 0.5-µm Z-stacks in 20 s intervals, with 100-ms exposures and 2 × 2 binning. Images in Fig. 3 were taken using an inverted Olympus IX81 microscope with a Yokogawa spinning-disk confocal head (CSU-X1), a 60× 1.2-NA Plan Apochromat water objective, and an iXon EM + DU-897 BV back illuminated EMCCD (Andor).
spd-2(or188ts) temperature shift assay
JWW69 (control) and JWW89 (spd-2(or188ts)) strains were used for imaging. Sequencing of JWW89 confirmed a single point mutation in spd-2 resulting in a glycine-to-glutamic-acid amino acid substitution (G615E) as described in Kemp et al. (2004). Both worm strains propagated at 16°C, which is the permissive temperature for spd-2(or188ts). To prepare the embryos for imaging, a metal block was buried halfway in wet ice. A 24 × 60-mm glass coverslip (thickness of 1.5) and a flow chamber slide were placed over the cold block. To prevent sticking of the glass to the cold block due to water condensation, two Kimwipes were placed between the glass and the cold block. To minimize exposure to elevated temperatures during embryo dissection, the glass stage on the dissecting microscope stand was placed in a 4°C refrigerator and left to cool for ∼10 min. Once everything was cold, 10 µl of cold M9 plus 15 µm polystyrene beads (Sigma-Aldrich) was pipetted to the middle of the 24 × 60-mm coverslip.
For each worm strain, plates were transported inside the ice bucket directly contacting ice to the dissecting microscope area. The microscope glass stage was taken out of the refrigerator and assembled into its place. Three to four adult worms containing a single row of eggs were transferred to the M9 plus beads on the coverslip still located on top of the cold block. The coverslip was transferred to the dissecting scope, and the worms were cut open using 22-gauge needles. The coverslip was mounted on the flow chamber slide, and the edges of the coverslip were sealed using clear nail polish. The sample was moved to the imaging room on the cold block.
The Nikon Eclipse Ti2 microscope described above was used for imaging. Embryos were staged using a 10× air objective, then imaged with a 60× 1.2-NA water objective. To rapidly raise the temperature of the sample (up-shift), 40 µl of 25°C M9 was pipetted into the flow chamber well. 30 × 0.5-µm Z stacks were collected every 10 s using simultaneous illumination with 488- and 561-nm lasers (14.7% and 17.7% intensity, respectively), 2 × 2 binning, and 100-ms exposures.
Protein expression and purification
All expression plasmids are listed in Table S2. SPD-5, SPD-2, and PLK-1 proteins were expressed using the FlexiBAC baculovirus system (Lemaitre et al., 2019) and purified as previously described (Woodruff and Hyman, 2015; Woodruff et al., 2015), with the following exception: SPD-2 was stored in its uncleaved form (MBP-TEV-SPD-2).
In vitro SPD-5 condensate disassembly assay
SPD-5 condensates were formed by diluting 10 µM SPD-5 (1:10 mixture of SPD-5 and SPD-5::TagRFP) in condensate buffer (25 mM Hepes, pH 7.4, and 150 mM KCl) containing PEG 3350 (Sigma-Aldrich) and fresh 0.5 mM DTT. Before use, the SPD-5 stock solution was centrifuged for 5 min at 80,000 rpm to remove residual aggregates. 5 min after formation, SPD-5 condensates were placed in glass-bottom 96-well dishes (Corning, 4850, high content imaging dish) precleaned with 2% Hellmanex and washed in water. For each sample, half was placed in the well undisturbed (control), and the other half was diluted 10-fold, pipetted five times, and placed in a well (induced disassembly). 96-well plates were imaged on an inverted Nikon Ti-E microscope using a 60× 1.4-NA Plan Apochromat oil objective, a Zyla cMOS camera (Andor), and MicroManager control software. For each image, SPD-5 condensates were identified through applying a threshold then using the particle analyzer function in Fiji. When analyzing condensate formation, we report the sum of the integrated intensities of each condensate per image (total condensate mass). Survival percentage plotted in Fig. 5 assumes a 10-fold loss in total condensate mass due to dilution.
Quantification and statistical analysis
Images were analyzed with Fiji (https://fiji.sc/), R (https://www.r-project.org/), and GraphPad Prism (https://www.graphpad.com). For FLUCS experiments, centrosome deformation was calculated by measuring the long axis (orthogonal to the flow direction) of PCM-localized SPD-5 at the initial and final time points of PCM deformation, before fracture (defined below). The deformation rate equaled the difference in PCM lengths divided by the time interval. Centrosome fracture was measured using line scans across the long axis of PCM-localized SPD-5. Fracture was scored if signal dropped to cytoplasmic levels over three consecutive pixels on the long axis across the entire flow path, and if this signal gap persisted for the rest of the images. For all other experiments, centrosome tracking and measurement was conducted using maximum-intensity projections and correction for photobleaching, followed by thresholding and particle analysis. Thresholds were determined using mean background intensity of the cytoplasm + b × (SD of background), where b represents an integer value that is identical for all samples within an experiment. The integrated fluorescence density for the centrosome-localized signals were normalized to either the first intensity value or maximum-intensity value (Fig. 3) and plotted over time.
All data are expressed as the mean ± 95% CIs as stated in the figure legends and results. The value of n and what n represents (e.g., number of images, condensates, or experimental replicates) is stated in figure legends and results. Normality tests were first performed before applying statistical tests. Statistical tests were performed with GraphPad Prism.
Online supplemental material
Fig. S1 shows controls for the FLUCS experiments. Fig. S2 shows contributions of microtubule-pulling forces to PCM deformation. Fig. S3 shows the disassembly profiles of posterior-localized PCM proteins. Fig. S4 shows FLUCS and localization experiments in sur-6(RNAi) embryos. Video 1 shows FLUCS flow control using 25-, 32-, and 40-mW laser scans at 1.5 kHz. Videos 2, 3, 4, 5, and 6 show high-flow FLUCS targeting the centrosome in a one-cell embryo during prometaphase, metaphase, anaphase, telophase, and metaphase-anaphase transition, respectively. Table S1 lists the strain used in this study. Table S2 lists the protein expression plasmids used in this study. Table S3 and Table S4 show statistical analyses for Fig. 3, F and G. Table S5 shows the oligonucleotides used for CRISPR tagging of SPD-5.
We thank Karen Oegema (University of California, San Diego, San Diego, CA), Arshad Desai (University of California, San Diego, San Diego, CA), Anthony Hyman (Max Planck Institute, Dresden, Germany), Alexander Dammermann (Max Perutz Labs, Vienna, Austria), and Bruce Bowerman (University of Oregon, Eugene, OR) for providing strains; Andrea Zinke, Anne Schwager, and Susanne Ernst (Max Planck Institute, Dresden, Germany) for help with worm maintenance; Abby Dernburg (University of California, Berkeley, Berkeley, CA), Carsten Hoege (Max Planck Institute, Dresden, Germany), and David Drechsel (IMP Vienna, Vienna, Austria) for providing CRISPR reagents; Stephan Daetwyler (University of Texas Southwestern, Dallas, TX), Lena Hersemann, and Robert Ernst (Max Planck Institute, Dresden, Germany) for help with image analysis and script writing; the Live Cell Imaging Facility at UT Southwestern and Light Microscopy Facility at the Max Planck Institute of Molecular Cell Biology and Genetics for help with microscopy; and the Protein Expression Facility at Max Planck Institute of Molecular Cell Biology and Genetics for help with protein expression.
J.B. Woodruff is supported by a Cancer Prevention and Research Institute of Texas grant (RR170063) and the Endowed Scholars program at University of Texas Southwestern Medical Center. M. Kreysing is supported by the Max Planck Society and European Research Council (grant 853619), and we acknowledge a Deutsche Forschungsgemeinschaft–financed Dresden International PhD Program fellowship for M. Mittasch.
The authors declare no competing financial interests.
Author contributions: M. Mittasch, A.W. Fritsch, and M. Kreysing built the FLUCS microscope. M. Mittasch and V.M. Tran performed and analyzed the FLUCS experiments on C. elegans embryos. M.U. Rios performed the spd-2 temperature-sensitive experiments. B. Ferreira Gomes and S.J. Enos performed two-color imaging of PCM proteins during anaphase and wrote the image analysis scripts. A. Bond performed imaging of sur-6(RNAi) mutants. J.B. Woodruff purified proteins and performed the in vitro assays. V.M. Tran performed all other in vivo experiments and analysis. J.B. Woodruff and M. Kreysing analyzed data and wrote the manuscript.
M. Mittasch and V.M. Tran contributed equally to this paper.