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The dynamic polymerization and depolymerization of actin filaments is essential for various cellular processes such as cell migration, rotation, cytokinesis, and mammalian oocyte maturation. Tropomodulin 3 (Tmod3) binds to the slow-growing (pointed) ends of the actin filament, thereby protecting the filament from depolymerization. However, the roles of Tmod3 in mammalian oocyte maturation remain elusive. Tmod3 mRNA and protein is present at all stages of mouse oocyte maturation. Tmod3 protein is mainly localized in the cytoplasm and appears enriched near the chromosome during maturation. By knocking down or ectopically overexpressing Tmod3, we confirmed that Tmod3 regulate the level of the intracytoplasmic actin mesh and asymmetric spindle migration. Expression of N-terminal Tmod3 (correspond to 1–155 amino acids), which contains the tropomyosin-binding site, results in decreased density of the actin mesh, thereby demonstrating the importance of the interaction between tropomyosin and tropomodulin for the maintenance of the actin mesh. Taken together, these findings indicate that Tmod3 plays crucial roles in oocyte maturation, presumably by protecting the actin filament from depolymerization and thereby controlling the density of the cytoplasmic actin mesh.
The dynamic reorganization of actin filaments is the main driving force for asymmetric spindle migration and polar body extrusion in mammalian oocytes1,2. The formation of the cortical actin cap near the spindle3 and changes in cytoplasmic actin mesh density4,5 represent two characteristic events occurring during the reorganization of the actin cytoskeleton in maturing oocytes. Various actin-binding proteins (ABPs) play essential roles in facilitating these changes in the actin cytoskeleton, as shown in the other biological systems6,7. For example, actin nucleators, such as formin-2 (FMN2)8,9, Spire10, and the Arp2/3 complex11,12,13, represent a family of proteins that initiate the formation of new actin filaments, thereby playing an important role in oocyte maturation.
In addition to actin nucleators, other ABPs such as the heterodimeric actin capping protein (CP)14 and tropomyosin15 have been recently reported to play roles in oocyte maturation16,17. For example, CP, which binds to the fast growing ends (also known as the barbed ends) of actin filaments to block further elongation, is considered a core protein in the regulation of actin cytoskeleton dynamics18. The roles of CP in oocyte maturation have been recently investigated17. Knockdown of CP expression in mouse oocytes results in significant impairment of spindle migration and asymmetric division of oocytes, as well as a decrease in cytoplasmic actin mesh level. In addition, the expression of the capping protein-binding region of the CARMIL protein which is known to exert decapping activity by reducing the affinity of CP for the barbed ends of actin filaments19,20,21, also decrease in the actin mesh level, indicating that CP is important for the maintenance of cytoplasmic actin mesh level during oocyte maturation. In addition to CP, tropomyosin (nonmuscle isoform Tpm3-1) is also shown to be important for oocyte maturation16. The impairment of Tpm3-1 expression by RNAi has been demonstrated to compromise asymmetric division in oocytes and severely impair oocyte cortical integrity, as evidenced by the formation of blebs during cytokinesis. It has also been shown that the decrease in cortical actin levels due to expression of dominant active cofilin can be rescued by coexpression of Tpm3-1, indicating that tropomyosin binds the sides of actin filaments, protects them from depolymerization by ADF/cofilin15,22 during oocyte maturation.
As demonstrated in these studies, the maintenance of cortical and cytoplasmic actin mesh is crucial for oocyte maturation. In addition to tropomyosin and CP, more than 100 actin binding proteins exist23; however, only a fraction of these proteins have been characterized in terms of their roles in oocyte maturation.
Tropomodulin is a ~40kDa protein known to bind the slow-growing ends (pointed ends) of actin filaments and prevent depolymerization from the pointed ends24,25. Tropomodulin typically consists of an N-terminal tropomyosin-binding helix region, actin-binding region, and C-terminal leucine-rich repeat (LRR) regions26. The recent elucidation of the structure of the tropomodulin-actin complex reveals a detailed mechanistic view of pointed-end capping of tropomodulin27. Two separate actin-binding sites of tropomodulin, located at the N-terminal and C-terminal, bind two actin monomers separately on the pointed end of the actin filament, thereby blocking further elongation of the filament. In addition to interacting with the pointed end of the actin filament, tropomodulins interact with tropomyosin via two tropomyosin-binding sites located at their N-terminal regions28.
Four isoforms of tropomodulin, Tmod1, Tmod2, Tmod3, and Tmod4, exist in the genomes of mice and humans25. Several cellular and physiological functions of tropomodulins have been reported recently. For example, red blood cells from tropomodulin 1 (Tmod1)-null mice exhibit an abnormal sphero-elliptocytic shape, with reduced deformability and increased osmotic fragility29, demonstrating the role of Tmod1 in maintain membrane integrity. Depletion of tropomodulin (Tmod3) by siRNA in human microvascular epithelial cells enhances the rate of cell migration30, whereas the overexpression of Tmod3 is associated with impairment of cell migration. Tmod1-null skeletal muscle cells exhibit misaligned myofibrils and swelling of the sarcoplasmic reticulum31,32. In addition, Tmod1 plays an important role in the maintenance of hexagonal geometry in the fiber cells of the eye lens33,34. In the case of Tmod3 knockout mouse, deletion of Tmod3 caused the embryonic lethality at E14.5-E18.5, presumably by anemia caused by impairment of erythroid development35.
Cytoplasmic actin mesh formation is necessary for spindle migration and asymmetric cell division during maturation in mouse oocytes5,36,37. The formation of the actin mesh is mediated by formin2 and spire5,10. In contrast to Arp2/3 complex, which binds to the pointed ends of actin filaments, actin nucleators of the formin family bind to the fast-growing end of actin filaments38,39. Therefore, the pointed ends of actin filaments must be capped by pointed-end binding protein, in order to prevent depolymerization. Tropomodulin is the only known protein capable of capping the pointed ends of the actin filament. Previously, we have shown that knockdown of CP or partial abrogation of expression of CARMIL decreases cytoplasmic actin mesh levels in maturing oocytes17, indicating that actin capping is required for the maintenance of actin mesh filaments in oocytes. We investigated the functional roles of Tmod3 during oocyte maturation, and discovered that this protein is necessary for asymmetric division in oocytes via maintenance of the cytoplasmic actin mesh.
Based on our previous finding that barbed-end actin-capping protein is essential for oocyte maturation17, we investigated the roles of the pointed-end capping protein Tmod3, an ubiquitous isoform of tropomodulin40, in mouse oocyte maturation. To date, there have been no reports on Tmod3 expression in mammalian gametes, including oocytes. Therefore, we examined the expression of Tmod3 at the mRNA and protein level using quantitative reverse-transcription PCR and western blotting. As shown in Supplementary Figure 1A, Tmod3 mRNAs are present at all stages of immature (germinal-vesicle stage; GV) oocytes, germinal vesicle breakdown (GVBD), and metaphase I (MI) and metaphase II (MII) oocytes (Supplementary Figure 1A). Then, we investigated the presence of Tmod3 protein in oocytes by western blotting (Fig. 1A). Tmod3 proteins, around 40kDa in size, were detected at all stages of oocyte maturation. Moreover, their levels remained constant throughout maturation. Next, we investigated the localization of Tmod3 in the oocyte at various stages of maturation using immunostaining with Tmod3 antibody. At all developmental stages, Tmod3 was dispersed throughout the entire cytoplasm of the oocyte in speckle form (Fig. 1B,C). To confirm Tmod3 localizations, we expressed GFP-Tmod3 in oocytes. As similar with immunostaining results, GFP-Tmod3 is dispersed in cytoplasm (Fig. 1D and Supplementary Figure 1B,C). While Tmod3 localizations are not observed in immunostaining results, faint localizations of GFP-Tmod3 is also observed at the cortex. Taken together, these results confirm the expression of Tmod3 in maturing mouse oocytes and localized mainly in the cytoplasm.
Previously, we showed that knockdown of barbed ends binding CP or overexpression of CP-binding region (CBR) in CARMIL lowers cytoplasmic actin mesh levels, thereby impairing spindle migration and asymmetric division in mouse oocytes17. We tested whether the ablation of Tmod3, which is known to cap the pointed ends of actin filaments, affects polar body extrusion or cytoplasmic actin mesh density during oocyte maturation, as observed for CP.
Knockdown of RNA expression levels to 13% of that of negative control-injected oocytes was achieved by injecting double-strand RNA (dsRNA) against the Tmod3 gene (Fig. 2A). We confirmed that the injection of Tmod3 dsRNA results in a depletion of Tmod3 protein using by western blot and immunostaining, as shown in Fig. 2B and Supplementary Figure 1D,E. Next, we examined the effect of Tmod3 knockdown on oocyte maturation. The percentage of oocytes that reached MII stage did not significantly differ between the control and Tmod3 knockdown groups (Supplementary Figure 1F). However, oocytes with knockdown of Tmod3 frequently exhibited an abnormally large polar body, or underwent symmetric division. It was found that the co-injection of RNAi-resistant human Tmod3 rescued these defects (Fig. 2C). On examining the ratio of the size of the polar body to that of the oocyte, we found a significant increase in the ratio of polar body diameter to oocyte diameter. However, in oocytes in which Tmod3 knockdown had been rescued, no significant difference was observed relative to the control group (Fig. 2D), confirming that the failure of spindle migration was caused by Tmod3 knockdown.
In order to elucidate the mechanisms underlying the failure of asymmetric division in Tmod3 knockdown oocytes, we investigated the effect of Tmod3 knockdown on cytoplasmic actin mesh levels, which are crucial for spindle migration and oocyte maturation5,10,36. Following microinjection of Tmod3 dsRNA, oocytes at MI stage were stained with phalloidin and the cytoplasmic actin mesh level was measured (Fig. 2E). Tmod3 dsRNA injections resulted in significantly lower cytosplasmic actin mesh level than that observed in the control dsRNA-injected group, whereas co-injection with dsRNA-resistant human Tmod3 cRNA rescued the actin mesh level (Fig. 2F). We also measured the effect of Tmod3 knockdown on cortical actin stability using fluorescence recovery after photobleaching (FRAP), using mCherry-UtrCH as probe for actin. As shown in the Supplementary Figure 2A–C there is no significant difference in fluorescence recovery between Tmod3 knockdown and negative control control injected groups (See also Supplementary movie 1 and 2). Collectively, these data indicate that the knockdown of Tmod3 impairs asymmetric division and decreases cytoplasmic actin mesh and cortical actin thickness. These phenotypes are very similar to those observed in oocytes knocked down for CP expression17.
In order to further characterize phenotypes mediated by Tmod3, we measured dynamic changes in cytoplasmic actin filaments by microinjecting oocytes with the actin probe GFP-UtrCH141. In control oocytes injected with only GFP-UtrCH, fluorescence levels steadily increased during maturation (n=14), as shown in Fig. 3A,C and Supplementary Movie 3. This finding is consistent with previous reports5. Tmod3 knockdown was associated with a much slower increase in fluorescence intensity (n=29), which is in agreement with actin mesh quantification by phalloidin staining (Fig. 3B,C and Supplementary Movie 4). In addition, we tracked spindle movement by time-lapse imaging of chromatin, as visualized by H2B-mCherry fluorescence. As shown in Fig. 3D and Supplementary Movie 5, the spindle moved from the center of the oocyte to near the cortex in control oocytes; however, the movement of the spindle in Tmod3-knocked down oocytes is far smaller than those of control (Fig. 3E and Supplementary Movie 6). Based on the average movement of chromatin in control oocytes (n=15) and oocytes knocked down for Tmod3 (n=23), it is evident that spindle migration speeds increase after 6h in control oocytes, whereas this rapid migration of spindles is not observed in the Tmod3-knockdown group (Fig. 3F).
Actin-rich membrane blebs are usually associated with actin cytoskeleton collapse in cell cortex42. Previously we reported that knockdown of Tpm3.1 in mouse oocytes caused blebs formations during maturation16. In the case of Tmod3-knockdown group, several oocytes formed membrane blebs during maturation (8/38 of oocyte), while control oocytes did not (0/37) (Supplementary Figure 3). Collectively, these results show that the knockdown of Tmod3 causes impairment of cytoplasmic actin mesh and impairs spindle migration.
It is known that Tmod3 has two binding sites for tropomyosin, and that the interaction between tropomodulin and tropomyosin enhances pointed-end binding affinity27,43. Moreover, antibodies specific for the tropomyosin-binding regions of Tmod1 result in unstable pointed ends of actin filaments by dissociating tropomyosin from these ends44, suggesting that the interplay between tropomodulins and tropomyosin is crucial for their roles as actin- binding proteins.
Previously, we reported that knockdown of Tpm3.1 causes a decrease in cortical actin levels16; however, the effect on cytoplasmic actin mesh levels has not been investigated. As the knockdown of Tmod3 decreases actin mesh levels significantly (Fig. 2), we reasoned that Tpm3.1 knockdown might affect the levels of cytoplasmic actin mesh as well as those of cortical actin. We checked the actin mesh levels in oocytes in which Tmod3 and Tpm3.1 had been separately knocked down and compared these with actin mesh levels in the control. First we confirmed Tpm3.1 knockdown by siRNA injections (Supplementary Figure 4). We found that knockdown of Tpm3.1 decreases actin mesh levels significantly, similarly to Tmod3 knockdown (Fig. 4A,B). Knockdown of both Tmod3 and Tpm3.1 was found to elicit a greater decrease in the actin mesh level than separate knockdown of Tmod3 or Tpm3.1 (Fig. 4A,B), indicating that the negative effect of Tmod3 and Tpm3.1 on actin mesh levels is additive and suggesting a synergy between Tmod3 and Tpm3.1 in the maintenance of actin mesh levels.
The domain structures of Tmod3 reveal that this protein consists of an N-terminal region, which binds two tropomyosin molecules, and C-terminal Leucine-Rich-Repeat (LRR) regions, which bind the pointed ends of actin filaments (Fig. 5A).
In order to confirm that Tmod3 protects the pointed ends of actin filaments in the cytoplasmic actin mesh, and to demonstrate direct interactions between tropomyosin and Tmod3, we designed two Tmod3 constructs. The first one corresponded to the full-length Tmod3 protein fused with N-terminal GFP (GFP-Tmod3). The other corresponded to the N-terminal half (amino acids 1–155) of Tmod3, which contained two tropomyosin-binding site (TM1 and TM2) and one actin-binding site (ABS1).
The percentage of oocytes that occurred cytokinesis did not significantly differ between the GFP-control and GFP-Tmod3 overexpression groups (Supplementary Figure 1G). However, Overexpression of the full-length Tmod3 or Tmod31-155 resulted in an abnormally large polar body, or underwent symmetric division, as similar with phenotype observed in Tmod3 knockdown groups (Fig. 5B,C), indicating that overexpression of full-length Tmod3 or Tmod31-155 also impair spindle migrations. We checked the effects of Tmod3 constructs overexpression on cytoplasm actin mesh density. While full-length Tmod3 overexpressed oocytes have significantly higher cytoplasmic actin mesh levels than in the controls (Fig. 5D,E), indicating that overexpression of Tmod3 increases the stability of cytoplasmic actin mesh. In contrast, overexpression of Tmod31-155, which contains tropomyosin-binding sites, but lacks the pointed end-capping LRR domain, resulted in a decreased cytoplasmic actin mesh level compared with control oocytes, indicating that the expression of N-terminal regions of Tmod3 elicits dominant-negative effects on actin mesh levels.
It is known that the actin mesh in the oocyte cytoplasm is generated by formin-25 and spire10 considering that the actin nucleators of the formin family elongate actin filaments and bind to their fast-growing ends38, capping of the pointed ends of filaments by tropomodulin may be necessary to prevent depolymerization. In order to demonstrate the importance of pointed-end capping in the maintenance of cytoplasmic actin mesh levels, we overexpressed Formin2 (FH1-FH2 domains of FMN2 gene) as a GFP fusion protein and examined its effects on cytoplasmic actin mesh. Consistent with previous results17,36, the expression of GFP-FMN2 (FH1FH2) results in higher actin mesh levels compared with those in the GFP control group. However, when dsRNA against Tmod3 is co-injected with GFP-FMN2 (FH1FH2) cRNAs, the actin mesh level is significantly lower than that in GFP-FMN2 (FH1FH2) as well as in the GFP control (Fig. 6A,B). These results indicate that FMN2, even at high levels, is unable suppress the effect of Tmod3 in decreasing actin mesh levels, highlighting the importance of Tmod3 in the maintenance of actin mesh levels.
In this study, we demonstrated that Tmod3 is required for the maintenance of the cytoplasmic actin mesh and during oocyte maturation and failure of maintenance of proper actin mesh levels impair spindle migration. We additionally showed that the interplay between Tmod3 and Tpm3 is crucial for their activity. Since the importance of dynamic actin reorganization in oocyte maturation became known to the community, several studies have focused on the roles of actin nucleators such as formin-28,9, spire10, the Arp2/3 complex11, and NPFs, which activate the Arp2/3 complex—for example, WAVE245, JMY46, N-WASP47 and WASH48. However, far less attention has been paid to the roles of other actin-binding proteins in oocyte maturation. As in previous studies on the roles of CP17 and tropomyosin16, we showed that the control of post-nucleated actin filaments by actin cytoskeleton remodeling is also important for meiotic maturation, as already shown in other cellular phenomena such as cell migration6 and cytokinesis49.
In this study, we demonstrated the ablation of spindle migration and failure of asymmetric division following the knockdown of Tmod3. These phenotypes may be linked with a decrease in cytoplasmic actin mesh levels observed during oocyte maturation, as shown by the measurement of the levels of phalloidin-stained actin mesh and time-lapse imaging of maturating oocytes/Formin-2/spire are known to be responsible for the generation of actin filaments in the cytoplasmic actin mesh in oocytes8,9,10. Moreover, formin-2 is a member of the formin-family proteins which nucleate and elongate actin filaments by binding to their fast-growing barbed ends38,39,50,51. The opposite site of actin filaments, slow-growing pointed ends need to be protected from depolymerization as the critical concentration of actin polymerization at the pointed end of the filaments is over 10-fold higher than that at the barbed ends52. Our results confirm the importance of pointed-end capping proteins in the maintenance of actin mesh during oocyte maturation. As shown in Fig. 6, even increased formin-2 levels are not sufficient to maintain cytoplasmic actin mesh in oocytes knocked down for Tmod3, indicating that both pointed-end capping and protection by Tmod3, as well as presence of the actin nucleator, are essential for the maintenance of the cytoplasmic actin mesh.
It is well established that tropomodulin binds tropomyosin, and that the presence of tropomyosin significantly enhances pointed-end capping activity of Tropomodulin27,43,53. Therefore, we investigated the functional roles of the interaction between Tmod3 and Tpm3.1, which is also reported to be important for oocyte maturation via maintenance of cortical integrity. The results of the present study indicate that pointed-end capping of Tmod3 and filament protection by Tpm3.1 are tightly coupled due to interaction between the two proteins. In addition to the additive negative effects of Tmod3 and Tpm3.1 knockdown on cytoplasmic actin mesh levels, the expression of the N-terminal region of Tmod3, which contains two tropomyosin-binding sites, exerts dominant-negative effects on the actin mesh level, presumably by sequestering of Tpm3.1 via tropomyosin binding region in N-terminal half of Tmod3. These results show that tropomyosin-tropomodulin interaction is essential for the maintenance of the actin mesh during oocyte maturation.
Based on the results of the present study, we suggested a hypothetical model for the roles of Tpm3 and Tmod3 in the maintenance of the cytoplasmic actin mesh in maturing oocytes (Fig. 7). The pointed ends of actin filaments are capped by Tmod3, whose binding is facilitated by the binding of Tpm3 to the actin filament. Tpm3 binding also protects actin filaments from depolymerization by ADF/cofilin. CP binds to the barbed ends of actin filaments, thereby preventing further elongation of filaments or depolymerization17. A decrease in, or abrogation of, Tmod3 levels results in depolymerization of pointed ends, thereby decreasing actin mesh levels.
Considering the roles of Tmod3 and Tpm3 in the maintenance of the cytoplasmic actin mesh, the modulation of the actin-capping activity of Tmod3 may represent a potential regulatory mechanism controlling the amounts of actin mesh in the cell. However, it is not clear as to how Tmod3 activity is regulated. A recent report shows that Tmod3 is an effector of Akt2, and that phosphorylation of Tmod3 at Ser71 in its first actin-binding region regulates GLUT4 exocytosis via actin remodeling54. This suggests the possibility of a regulatory pathway of Tmod3 involving Akt in mammalian oocytes. Akt has been reported to be involved in mammalian oocyte maturation53,55,56,57,58. Additionally, the inhibition of Akt activity impairs meiotic maturation or spindle formation59. However, its effect on the actin cytoskeleton and possible links with tmod3 Tmod3 remained to be investigated.
Previously, various functional roles of tropomodulins have been reported. For example, it has been shown that the knockdown of Tmod3 in epithelial cells causes altered cell morphology, presumably due to decreased F-actin content in lateral membranes60. Additionally, it has been shown mouse lens fiber cells in Tmod1- knockout mice show disruption of spectrin-actin links and abnormal morphology34. The present study is the first demonstration describing the roles of Tropomodulin in gamete formation. Collectively, our data demonstrate the importance of pointed-end capping protein for maintenance of proper asymmetric division in mammalian oocytes. Further studies are required to elucidate the potential roles of these actin-binding proteins in early embryogenesis.
Goat polyclonal antibody against human Tmod3 (G-16, sc-19205) was acquired from Santa Cruz Biotech (Santa Cruz, CA, USA). A mouse monoclonal antibody against Tpm3 (CG3)61 was obtained from the Developmental Study Hybridoma Bank at the University of Iowa. An Alexa-Fluor-488-conjugated rabbit anti-goat-IgG antibody was purchased from Invitrogen (Carlsbad, CA, USA), and a mouse monoclonal anti-α-tubulin–FITC antibody was obtained from Sigma (St Louis, MO, USA).
All animal manipulations were approved and conducted according to the guidelines of the Animal Research Committee of Chungbuk National University (approval no. CBNUR-889-15-02). Germinal vesicle (GV)-intact oocytes were collected from the ovaries of 6–8-week-old imprinting control region (ICR) mice and cultured in M16 medium (Sigma) under paraffin oil at 37°C in 5% CO2. Oocytes were collected for immunostaining and microinjection after culturing for various amounts of time.
Tmod3 expression was analyzed by real-time quantitative PCR (qRT-PCR) and the ΔΔCT method62. Total RNA was extracted from 30 oocytes using a Dynabead mRNA DIRECT Kit (Life Technologies, Foster City, CA). First-strand cDNA was generated using a cDNA Synthesis Kit (Takara, Kyoto, Japan) and Oligo (dT)12–18 primers. The PCR primers used to amplify Tmod3 are listed in Table 1. qRT-PCR was performed with SYBR Green in a final reaction volume of 20μl (qPCR kit, Finnzymes, Vantaa, Finland). PCR conditions were as follows: 94°C for 10min, followed by 39 cycles of 95°C for 15s, 60°C for 15s, and 72°C for 45s, with a final extension step at 72°C for 5min. Finally, relative gene expression was quantified by normalization to the level of GAPDH mRNA. Experiments were conducted in triplicate.
Tmod3 dsRNA was generated as described previously17. Briefly, a 604bp fragment of the TMOD3 gene (corresponding to 644–1248bp of NM_016963.2) was amplified from first-strand cDNA, which was generated from RNA extracted from MII oocytes using gene-specific primers containing the T7 promoter sequence (Supplementary Table S1). In vitro transcription was performed using a Megashortscript T7 Kit (Life Technologies). For overexpression of the TMOD3 gene, synthetic DNA fragments corresponding to the ORF of the mouse TMOD3 sequence were synthesized by Bioneer Co (Daejun, Korea) and subcloned as a GFP fusion into the pCS2+ vector63. For the expression of the N-terminal region (corresponding to amino acids 1–155 of Tmod3), the corresponding sequence of the TMOD3 gene was amplified by PCR and subcloned as an N-terminal GFP fusion.
For the expression of the FH1-FH2 domains of FMN2, cDNA spanning 811–1579aa of FMN2 proteins were amplified from mouse FMN2 cDNA clone (Obtained from GE Dharmacon), then subcloned into pRN3 vector64 as C-terminal GFP fusion. The pRN3-H2B-mCherry plasmids65 were kindly provided by Dr. JungSoo Oh (Sung Kyun Kwan University, Suwon, Korea). For in vitro transcription, a mMessage mMachine SP6 or T3 Kit (Life Technologies) was employed. In some cases, poly-A tails were added using a poly-A Tailing Kit (Life Technologies).
siRNA, dsRNAs and cRNAs were microinjected into GV-stage mouse oocytes, as described previously17. TMOD3 knockdown was achieved by diluting TMOD3 dsRNA to obtain a final concentration of 1mg/ml and microinjecting it into the cytoplasm of a fully grown GV-stage oocyte using an Eppendorf Femto Jet (Eppendorf AG, Hamburg, Germany) and a Nikon Diaphot ECLIPSE TE300 inverted microscope (Nikon UK Ltd, Kingston upon Thames, Surrey, UK) equipped with a Narishige MM0-202N hydraulic three-dimensional micromanipulator (Narishige Inc., Sea Cliff, NY). After injection, oocytes were incubated in M16 medium containing 5mM milrinone for 20hr to ensure knockdown. The oocytes were then transferred into fresh M16 medium and cultured for a further 12h. The developmental stages of the oocytes were visualized by DAPI staining. Control oocytes were microinjected with 5–10pl of dsRNA against GFP. In the case of TPM3.1 knockdown, Approximately 5–10pl of 50μM TPM3.1-targeting siRNA (5′-CAGCUUUGGU GUCUUUGAA (dTdT)-3′) corresponding to 1499–1517bp of NM_001253738.1, Bioneer) was used as described previously16.
Polar body extrusion and cytokinesis were observed using a stereomicroscope. For rescue experiments, cRNAs encoding dsRNA-resistant human Tmod3 were added to the dsRNA at a concentration of 0.1mg/ml. In order to microinject FMN2-GFP cRNAs, the concentrations of cRNA were adjusted to 1mg/ml. Approximately 5–10pl of cRNA was microinjected into the cytoplasm of a fully-grown GV-stage oocyte. After injection, oocytes were cultured in M16 medium containing 5mM milrinone for 3hr, then oocytes were washed five times in milrinone-free M16 medium for 2min each time. The oocytes were then transferred into fresh M16 medium and cultured under paraffin oil at 37°C in an atmosphere of 5% CO2 in air. Control oocytes were microinjected with 5–10pl of GFP cRNA. For the quantification of oocyte and polar body diameter, image of oocytes after in vitro maturation were acquired using Nikon Diaphot ECLIPSE TE300 inverted microscope. The longest diameters of oocytes and polar bodies were measured using ImageJ.
For immunostaining of Tmod3 or Tpm3-1, oocytes were fixed in 4% paraformaldehyde dissolved in phosphate-buffered saline (PBS) for 30min at 20°C, and then transferred into a membrane permeabilization solution (0.5% Triton X-100 in 0.1% polyvinylalcohol in phosphate-buffered saline, PVA-PBS) and incubated for 1h. For the quantitative measurement of cortical and cytoplasmic actin mesh, membrane permeabilization step was skipped to preserve actin density. After 1h in blocking buffer (PBS containing 1% BSA), the oocytes were incubated overnight at 4°C with a goat anti-Tmod3 antibody at a 1:200 dilution. After three washes in washing buffer (PBS containing 0.1% Tween 20 and 0.01% Triton X- 100), the oocytes were labeled with Alexa-Fluor-488-conjugated goat anti-mouse-IgG (1:100) for 1–2h at room temperature. In order to stain cytoplasmic actin mesh or cortical actin, oocytes were fixed and stained with phalloidin–TRITC (10mg/ml), which labels F-actin. For anti-α-tubulin–FITC (1:200) antibody staining, oocytes were incubated for 1h, washed three times in washing buffer for 2min each time, then incubated with Hoechst 33342 (10mg/ml in PBS) for 15min. Samples were examined using a confocal laser-scanning microscope (Zeiss LSM 710 META, Jena, Germany) with a 40x water-immersion objective lens for fixed oocytes. Quantification of actin mesh density was carried out using a single section in the center of the oocyte image acquired by a 63x oil-immersion objective lens. Cytoplasmic regions devoid of cortical actin and actin-rich spindle were selected as square (10μm×10μm), then average greyscale of phalloidin channel in the selected region were measured using imageJ. To normalize variations in phalloidin intensity between experimental repeats (n=3), intensity values of each oocyte were normalized as percent of mean values of control group of each experimental repeat.
A total of 100 mouse oocytes were placed in SDS sample buffer and heated at 100°C for 5min. Proteins were separated by SDS-PAGE and transferred to polyvinylidene fluoride membranes and probed with a goat anti-Tmod3 antibody and anti-actin antibody. As secondary antibody, HRP-conjugated goat anti-goat-IgG (1:1000; Santa Cruz Biotech, Santa Cruz Biotechnology, CA) was used. Signals were detected using Pierce ECL western blotting substrate (Thermo Fisher Scientific, Rockford, IL).
Time-lapse imaging was performed on oocytes in which Tmod3 was knocked down or overexpressed. dsRNA or cRNA was microinjected into GV-stage oocytes, as described above. For visualization of chromosomes, H2B–mCherry mRNA was also injected. Images were captured at 300s intervals, for 7–8h, using Lumascope 620 (Etaluma Inc, Carlsbard, CA) inverted microscope installed inside an incubator maintained at 37°C and 5% CO2.
To track the spindle, single multicolor z slices were aligned based on the differential interference contrast channel for removal of sample drift, using a modified version of the StackRegJ plugin66 for ImageJ67. The position of chromatin was tracked using the MTrackJ plugin68 for ImageJ, using the RFP channels of images processed by segmented thresholding. The distances between the positions of chromatin at the starting point and at subsequent time points were recorded.
Fluorescence recovery after photobleaching (FRAP) was done by a confocal laser-scanning microscope (Zeiss LSM 710 META, Jena, Germany) with a 4X zoom of 63x/1.40 oil-immersion objective lens. For FRAP measurements, UtrCH-mCherry mRNA was injected at GV stage and incubated for 9hr, and FRAP measurement was performed at MI stage. FRAP was carried out with 2 pre-bleach scans followed by a laser power of 100% of the 543nm laser line, point-bleach function with full power for 5.508s and 48 post-bleach scans. Images were taken in 512*512 format and frames were acquired at 0.97sec/frame speed. The fluorescence intensity was measured directly acquisitions in the photo-bleached region. In order to minimize error, each oocyte measured different 3 points and then averaged. Intensity of measurement was normalized based on the pre-bleach point intensity.
At least three replicate experiments were performed for each treatment. Statistical analyses were conducted using Welch’s t-test, Pearson’s chi-square test, Fisher’s exact test, or an analysis of variance (ANOVA), followed by Tukey’s multiple comparisons of means by R (R Development Core Team, Vienna, Austria). Data are expressed as the mean±S.E.M., and P<0.05 was considered significant.
How to cite this article: Jo, Y.-J. et al. Tropomodulin-3 is essential in asymmetric division during mouse oocyte maturation. Sci. Rep. 6, 29204; doi: 10.1038/srep29204 (2016).
This study was supported by a grant from the Next Generation Biogreen 21 Program to S.N. (PJ011206) and N.-H.K. (PJ011126), Rural Developmental Adminstration, Republic of Korea.
Author Contributions S.N. and N.-H.K. conceived the project. Y.-J.J., W.-I.J. and S.N. conducted experiments. S.N. and Y.-J.J. wrote and revised the manuscript. All authors reviewed the manuscript.