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A Novel Mutation in β Integrin Reveals an Integrin-Mediated Interaction between the Extracellular Matrix and cki-1/p27KIP1

  • Shingo Kihira ,

    Contributed equally to this work with: Shingo Kihira, Eun Jeong Yu

    Affiliation Department of Biology, Baylor University, Waco, Texas, United States of America

  • Eun Jeong Yu ,

    Contributed equally to this work with: Shingo Kihira, Eun Jeong Yu

    Affiliation Department of Biology, Baylor University, Waco, Texas, United States of America

  • Jessica Cunningham,

    Affiliation Department of Biology, Baylor University, Waco, Texas, United States of America

  • Erin J. Cram,

    Affiliation Department of Biology, Northeastern University, Boston, Massachusetts, United States of America

  • Myeongwoo Lee

    myeongwoo_lee@baylor.edu

    Affiliation Department of Biology, Baylor University, Waco, Texas, United States of America

A Novel Mutation in β Integrin Reveals an Integrin-Mediated Interaction between the Extracellular Matrix and cki-1/p27KIP1

  • Shingo Kihira, 
  • Eun Jeong Yu, 
  • Jessica Cunningham, 
  • Erin J. Cram, 
  • Myeongwoo Lee
PLOS
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Abstract

The cell-extracellular matrix (ECM) interaction plays an essential role in maintaining tissue shapes and regulates cell behaviors such as cell adhesion, differentiation and proliferation. The mechanism by which the ECM influences the cell cycle in vivo is poorly understood. Here we demonstrate that the β integrin PAT-3 regulates the localization and expression of CKI-1, a C. elegans homologue of the cyclin dependent kinase inhibitor p27KIP1. In nematodes expressing wild type PAT-3, CKI-1::GFP localizes primarily to nucleoli in hypodermal cells, whereas in animals expressing mutant pat-3 with a defective splice junction, CKI-1::GFP appears clumped and disorganized in nucleoplasm. RNAi analysis links cell adhesion genes to the regulation of CKI-1. RNAi of unc-52/perlecan, ina-1/α integrin, pat-4/ILK, and unc-97/PINCH resulted in abnormal CKI-1::GFP localization. Additional RNAi experiments revealed that the SCF E3 ubiquitin-ligase complex genes, skpt-1/SKP2, cul-1/CUL1 and lin-23/F-box, are required for the proper localization and expression of CKI-1, suggesting that integrin signaling and SCF E3 ligase work together to regulate the cellular distribution of CKI-1. These data also suggest that integrin plays a major role in maintaining proper CKI-1/p27KIP1 levels in the cell. Perturbed integrin signaling may lead to the inhibition of SCF ligase activity, mislocalization and elevation of CKI-1/p27KIP1. These results suggest that adhesion signaling is crucial for cell cycle regulation in vivo.

Introduction

Integrins are αβ heterodimeric receptors that mediate bi-directional interactions between cells and extracelluar matrix (ECM) [1]. In mammals, 13α and 8β chains comprise more than twenty heterodimers and play important roles in controlling cell behaviors such as cell adhesion, migration and proliferation [2]. Among the β subunits, β1 integrin is broadly expressed and has multiple splice variants. For example, four β1 splice variants, β1A, β1B, β1C and β1D differing in their cytoplasmic tails, are expressed in many tissues [3]. β1A is the dominant splice form and is expressed ubiquitously [3]. β1D is produced by alternative splicing and is found in striated muscle cells only [4]. Both β1A and β1D forms are localized to focal adhesions and retain the conserved NPxY phosphorylation motif [5], [6]. However, the β1B variant, expressed in keratinocytes and hepatocytes, fails to localize to focal adhesions and exhibits dominant negative activity to β1A-paired integrins [7], [8]. β1B is the result of mis-splicing of intron 7, and retains intronic sequence in its mRNA [9]. β1C is expressed in normal tissues, such as the prostatic epithelium, and is downregulated in cancer cells [10]. β1C integrin is produced from an alternative splicing event in the cytoplasmic tail of β1 integrin, usually includes exon C and results in a protein 27 amino acids longer than the regular β1A splice form [5], [11].

In many cancerous conditions, integrins lose their connection to the ECM or change their expression patterns [3], [12], [13]. The ECM also undergoes remodeling, resulting in abnormal deposition of proteins or increased ECM stiffness. A change in ECM composition or mechanical properties may upregulate integrin signaling, which promotes cell survival, adhesion and proliferation [14], [15]. For example, cell detachment from the ECM increases the level of cyclin dependent kinase (CDK) inhibitors thereby preventing advancement to S phase of the cell cycle [16].

In some cases, integrin signaling can promote cell cycle arrest [17]. For example, the expression of integrin β1C in mammalian cells increases the level of p27KIP1, a CDK inhibitor [18]. In contrast, lowering the level of p27KIP1 allows activation of the CDK/cyclin complex and promotes the cell cycle transition from G1 to S [19][22]. In these cells, adhesion to the ECM activates an E3 ubiquitin ligase that is essential for the degradation of p27KIP1. The expression of SKP2, an important component of the SCF ubiquitin ligase (E3) complex, is also dependent on cell adhesion at the G1 to S transition [23]. However, there is little information available about how integrin signaling regulates the level of cell cycle inhibitors like p27KIP1 in vivo.

The nematode Caenorhabditis elegans expresses only two integrins, PAT-3/INA-1 [24] and PAT-3/PAT-2 [25], which simplifies the analysis of genetic interactions between integrin and cell cycle control genes. Overexpression of C. elegans p27KIP1/CKI-1 has been found to induce growth arrest and the cki-1 null mutation results in hyperplasia of tissues such as the hypodermis, the vulva and the intestine [26][28]. The disruption of cki-1 also results in the production of extra distal tip cells from the somatic gonad lineage [29], [30]. The activity of cki-1 is regulated by the coordination of stage-specific cellular events such as binding to the CDK/cyclin complex and a sharp increase in expression at the late larval and young adult stages [26], [31][33].

This study the role of pat-3(sp) (previously known as pat-3(β1C)) builds on our previous work on the function of PAT-3 signaling in C. elegans [34]. pat-3(sp) is a frameshift mutation in the splice acceptor region (ag to aa) that abolishes conserved interaction domains such as the NPxY motifs and creates a splice variant with an extra 19 amino acids. The pat-3(sp) animals not only produce mutant pat-3, but also express the regular splice form due to utilization of an unusual splice acceptor [34]. pat-3(sp) has similarities to the human β1B and β1C integrins. The pat-3(sp) mutant is similar to β1B because it retains intron sequence in the mRNA and the transgenic line expresses mutant and normal splice forms simultaneously. The mutant is similar to the β1C variant in that it is expected to produce a longer PAT-3 lacking the NPxY motifs [34].

In this study, we assessed the role of pat-3(sp) in cell cycle regulation. Briefly, in transgenic pat-3 rescued lines carrying pat-3(sp) [34], cki-1::GFP [26] was upregulated and exhibited a distinct sub-nuclear localization compared to wild type animals. RNA interference analyses revealed that the localization and level of CKI-1 are mediated by focal adhesion molecules and the SCF E3 ubiquitin ligase complex [35], [36]. Taken together, our findings suggest that integrin signaling, in conjunction with SCF E3 ligase complex activity, plays a crucial role in the localization and level of CKI-1 in vivo.

Results

βpat-3(sp) Increases CKI-1 Levels and Exhibits a Distinct Localization in Nuclei

PAT-3 β integrin is expressed in virtually all tissues in the nematode C. elegans [37], and is required for muscle development and function. Null mutations in pat-3 cause a fully penetrant embryonic arrest due to defective muscle elongation [25], [38]. Previously, we created a mutation at the intron 7 splice junction in the cytoplasmic tail of PAT-3 integrin (Figure 1) [3], [34]. The transgenic rescued line, pat-3(sp), is viable but exhibits cold-sensitive larval arrest with gonad and muscle defects. We found that pat-3(sp) expresses the non-spliced as well as the spliced pat-3 mRNA, suggesting that mutant pat-3 might inhibit the function of wild type pat-3. In this study, we have expanded our analysis to investigate the molecular function of pat-3(sp) [34].

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Figure 1. Sequences of the PAT-3 cytoplasmic tails.

Wild type and mutant PAT-3 tails are compared to human β1A, β1B, and β1C cytoplasmic tails. Location of intron 7 is indicated by the red arrow.

https://doi.org/10.1371/journal.pone.0042425.g001

Studies of the mammalian β1B and β1C integrins in mammalian cells revealed that expression of these integrins suppresses cell adhesion and proliferation [5] and upregulates the expression of p27KIP1 [39]. To investigate a potential linkage between PAT-3 and CKI-1, the C. elegans homolog of mammalian p27KIP1 [26], [29], [40], we created rescued transgenic lines containing pat-3(+) or pat-3(sp) genomic DNA by co-injecting with DNA encoding a CKI-1::GFP fusion protein [26], [34]. As previously described [26], [29], CKI-1::GFP is expressed in hypodermal cells of late L4 and young adult animals. Nuclear expression is observed within an ER meshwork, typical of the hypodermal syncytium (hyp 7) (Figure 2A and 2B) [41]. In pat-3(+) rescued animals, the appearance of CKI-1::GFP is a distinct fluorescent spot within a round green nucleus, suggesting nuclear and nucleolar localization (Figures 2A and 2C). To substantiate our interpretation that CKI-1::GFP localizes to the nucleolus, the ncl-1 gene, disruption of which results in enlarged nucleoli, was depleted using RNAi [42], [43]. In the pat-3(+) background, ncl-1 (RNAi) significantly increased the size of the CKI-1::GFP spot. ImageJ analysis showed that the size of the green spot was increased by 2.4 fold when compared to that of control RNAi animals (Figure S1, Table S1). Therefore, we conclude that the observed spots on the nuclei are likely to represent nucleolar localization.

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Figure 2. CKI-1::GFP is localized to the nucleus and nucleolus in pat-3 transgenic rescued animals.

CKI-1::GFP transgenic animals were examined using fluorescence microscopy. Panels A and B show mid-body regions of pat-3(+) and pat-3(sp) rescued animals, respectively. Arrows indicate the nuclei of hypodermal cells at early adult stages. Panels C and D depict a hypodermal nucleus in pat-3(+) and pat-3(sp) worms, respectively. CKI-1::GFP appeared to be nucleolar (arrow heads) in pat-3(+), while the CKI-1::GFP appeared clumped in pat-3(sp) nuclei (arrows). Scale bar = 50 µm.

https://doi.org/10.1371/journal.pone.0042425.g002

In the pat-3(sp) rescued animals, CKI-1::GFP localization was visibly different from that seen in pat-3(+) animals. In contrast to the compact, nucleolar staining seen in pat-3(+) animals, CKI-1::GFP in pat-3(sp) was clumped and accumulated in a ring around a dark center in the nucleus (Figures 2B and 2D), suggesting mislocalization and possible exclusion from the nucleolus. In addition, the intensity of green fluorescence in pat-3(sp) was increased compared to pat-3(+). In order to test for a possible correlation between the level of CKI-1::GFP and the integrin (pat-3(+) or pat-3(sp)) expressed, we first analyzed the amount of CKI-1::GFP in the pat-3 rescued lines. Protein lysates were prepared from an equal number of L4/young adult transgenic animals and tested for CKI-1::GFP protein levels. CKI-1::GFP level in pat-3(sp) was ten fold more intense than that seen in pat-3(+) lysates (Figure 3A), suggesting that PAT-3 signaling may control CKI-1 levels.

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Figure 3. Immunoblot analysis of CKI-1::GFP protein in transgenic animals.

Panel A: CKI-1::GFP expression levels were assessed in the transgenic rescued lines. Top bands in lanes 1 and 2 show the relative level of UNC-54/myosin B in each sample. Bottom bands indicate the level of CKI-1::GFP. Lanes 1 and 2 represent pat-3(+) and pat-3(sp), respectively. Quantification (Table S1) using ImageJ software revealed that CKI-1::GFP level was 10-fold increased in pat-3(sp) animals compared to pat-3(+) animals. Panel B: CKI-1::GFP expression levels were assessed in pat-3(+) animals treated with RNAi directed against focal adhesion genes. Top bands represent the amount of CKI-1::GFP in extracts prepared from each RNAi condition. L4440 is a negative RNAi control. The pat-3, ina-1, unc-97, unc-52, pat-6 and let-2 RNAi caused upregulation of CKI-1::GFP, while unc-112 RNAi had no effect. Bottom bands indicate MH33 [90] levels in each lane as a loading control. Quantification (Table S1) using ImageJ software revealed that CKI-1::GFP level was increased by RNAi of pat-3, ina-1, unc-97, unc-52, pat-6, and let-2. Panel C: CKI-1::GFP expression levels were also measured in pat-3(+) animals treated with E3 ligase gene RNAi. Top bands represent the amount of CKI-1::GFP in the extracts prepared from each RNAi condition. L4440 is a negative RNAi control. The skpt-1, lin-23 and cul-1 RNAi depletions caused upregulation of CKI-1::GFP, while rbx-1 and cul-4 RNAi had no effect. Bottom bands indicate MH33 [90] levels in each lane as a loading control. Quantification (Table S1) using ImageJ software revealed that the CKI-1::GFP level was increased by RNAi of skpt-1, lin-23 and cul-1.

https://doi.org/10.1371/journal.pone.0042425.g003

Because the immunoblot results revealed that pat-3(sp) animals produced more CKI-1::GFP protein than pat-3(+), we next assessed the effect on cki-1 transcription. RNA from each rescued line was isolated and analyzed for the amount of pat-3 or cki-1 mRNA using RT-PCR (Figure 4A). We also measured the cki-1 mRNA level in BU7221, a pat-3(sp) rescued line without cki-1::GFP [34]. No significant differences were seen in any of the experiments, suggesting that pat-3(sp) does not significantly increase the level of cki-1 mRNA compared to controls (Figure 4B).

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Figure 4. RT-PCR analysis of cki-1 mRNA in cki-1::GFP transgenic and βpat-3 rescued lines lacking cki-1::GFP.

Panel A: Lanes 1 and 2 display the level of mRNA in pat-3(+) and pat-3(sp) animals, respectively. The GAPDH (glyceraldehyde-3-phosphate dehydrogenase) gene, gpd-1, was used as an mRNA loading control. The level of each transcript was measured using ImageJ software. Quantification of cDNA using ImageJ software revealed that cki-1 mRNA levels were similar in all lines compared (Table S1). Panel B: cki-1 mRNA was measured in βpat-3 rescued lines lacking the CKI-1::GFP construct. Lanes 1–3 are N2, JE443 pat-3(+), and BU7221 pat-3(sp). The GAPDH gene, gpd-1, was used as an mRNA loading control. Quantification of cDNA levels using ImageJ software revealed that cki-1 mRNA levels were similar in all lines compared (Table S1).

https://doi.org/10.1371/journal.pone.0042425.g004

Integrin Signaling Regulates CKI-1 Localization

In order to define genetic pathways that link PAT-3 integrin to CKI-1, a series of RNAi experiments were performed. We hypothesized that the integrin effect on the localization of CKI-1::GFP in pat-3(sp) would be mediated by genes that interact with the cytoplasmic domain of β integrin. Thus, candidate genes were selected from known focal adhesion components [44]. Previous analysis of embryonic muscle development identified 20 essential genes, mostly encoding components of dense bodies and M-lines, which are analogous to focal adhesions [44][45]. Integrins are located in the base of these structures and anchor the sarcomeres to the basement membrane. Data from the SAGE database [37] indicated ten of the integrin signaling genes were expressed in the hypodermis. To screen for the genes involved in CKI-1 localization, we tested if RNAi depletion of these integrin signaling components [44] in pat-3(+) would result in mislocalization of CKI-1::GFP in the nucleoplasm, similar to that seen in pat-3(sp) animals (Results summarized in Table 1).

In pat-3(+) animals, pat-3(RNAi) resulted in CKI-1::GFP accumulation in the nucleoplasm similar to that seen in pat-3(sp) (Figures 5B and 2D). Next, integrin α subunits were depleted. Depletion of ina-1 in the pat-3(+) animals also resulted in abnormally clumped CKI-1::GFP (Figures 5C), suggesting that the CKI-1 localization is integrin dependent. Among the focal adhesion genes, pat-4/ILK [46], unc-97/PINCH [47] and pat-6/parvin [48] together form an IPP complex, which is implicated in the control of signaling pathways by the phosphorylation of downstream targets [49]. RNAi of pat-4/ILK or unc-97/PINCH in pat-3(+) resulted in the expected uncoordinated phenotypes (Figure S2) and CKI-1 mislocalization in hypodermal nuclei (Figure 5D and 5E). However, in pat-6/parvin RNAi animals, CKI-1 maintained its wild-type localization, possibly suggesting that the CKI-1 localization is independent of parvin (Figure 5F). Because pat-6 RNAi did not result in a strong uncoordinated phenotype (Figure S2), it is possible that the pat-6 RNAi is not as effective as the RNAi to pat-4 and unc-97. However, our data is consistent with the interpretation that ILK and PINCH are mediating integrin signals to control CKI-1 localization in the nucleus.

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Figure 5. RNAi analysis showed that some focal adhesion and E3 ligase genes are required for CKI-1::GFP localization.

Panels depict the results of RNAi of focal adhesion genes, dense body or M-line components, on the localization of CKI-1::GFP. Panels A: the negative control L4440 plasmid, B: pat-3 RNAi, C: ina-1 RNAi, D: pat-4 RNAi, E: unc-97 RNAi, F: pat-6 RNAi, G: unc-52 RNAi, H: let-2, I: skpt-1 RNAi, J: lin-23 RNAi and K: cul-1 RNAi.

https://doi.org/10.1371/journal.pone.0042425.g005

Our RNAi screen also found that unc-52/perlecan, a basement membrane component and presumptive integrin ligand [50][52], is required for the proper localization of CKI-1. RNAi of unc-52 in pat-3(+) affected the CKI-1 localization pattern (Figure 5G). In contrast, depletion of other basement membrane components, such as let-2/collagen IV [53], failed to affect the localization (Figure 5H), suggesting that a subset of ECM components is required for CKI-1 localization.

Ubiquitin-mediated Protein Degradation Regulates Localization of CKI-1::GFP

Next, we investigated the mechanism by which integrin regulates CKI-1 protein levels without affecting RNA levels. One plausible explanation is that integrin signaling leads to the degradation of CKI-1 [23]. Integrin-triggered p27KIP1 degradation has been observed in mammalian cells. For example, integrin crosstalk with receptor tyrosine kinase (RTK) induces the production of SCFSKP2 [54], a member of the SCF E3 ubiquitin ligase complex, which binds to the SKP1 [55], CUL1 [56] and FBX-1 [23] E3 ligase complex. This SCF complex targets CDK/cyclin inhibitors such as p27KIP1 and p21CIP1 [57].

We hypothesized that the SCF complex might play a similar role in the localization and level of CKI-1 in response to integrin signals. To test this hypothesis, we performed RNAi analysis of skpt-1/SKP2 [33], cul-1/CUL1 [58] and lin-23/F-Box [59] and monitored CKI-1 localization (Figure 5I, 5J, and 5K). We first examined skpt-1/SKP2 (RNAi) in the pat-3(+) background. CKI-1::GFP accumulation in the pat-3(+); skpt-1 (RNAi) nucleoplasm was almost identical to that seen in pat-3(sp) animals (Figure 5I). Similar results were obtained in cul-1 and lin-23 RNAi in the pat-3(+) strain (Figure 5J and 5K), suggesting ubiquitin-mediated protein degradation is responsible for the proper localization of CKI-1. RNAi of another E3 ligase complex gene, rbx-1/ROC1 [23], did not alter the localization pattern of CKI-1 (Table 1). Studies have also suggested that the DDB-1/CUL-4 associated factors (DCAF) complex is responsible for p27 degradation in mammals and Drosophila [60]. Our analysis of cul-4(RNAi) treated pat-3(+) animals suggests that this complex is unlikely to be involved in CKI-1 localization in C. elegans (Table 1). Taken together, our RNAi analyses suggested that the members of SCF complex play a role in the CKI-1 localization.

Immunoblot Analysis Demonstrates a Correlation between CKI-1 Overexpression and Mislocalization

We next investigated whether depletion of the focal adhesion and SCF complex genes would affect expression levels of CKI-1/p27KIP1 in addition to affecting nuclear localization patterns (Figures 5; Table 1). Immunoblot analyses of CKI-1::GFP were performed using protein extracts from RNAi-treated adult animals (Figure 5A and 5B). The amount of CKI-1::GFP generally increased in protein extracts of focal adhesion and SCF complex RNAi treated animals. Depletion of focal adhesion genes such as pat-3, ina-1, unc-97, unc-52, pat-6 and let-2 resulted in an up to 3-fold increase in CKI-1::GFP levels (Figure 3B, Table S1). RNAi of SCF E3 ligase genes such as skpt-1, lin-23, and cul-1 also produced significant increases in CKI-1::GFP levels. (Figure 3C, Table S1). Interestingly, even though nucleolar localization was not affected by pat-6 and let-2 RNAi, protein levels were significantly increased (Figure 3B). Our analysis suggested that disruption of integrin signaling or SCF–mediated protein degradation can result in the mislocalization as well as increased expression of CKI-1::GFP. However, the let-2 and pat-6 RNAi results suggest there may not be a direct relationship between protein levels and localization.

Discussion

In this study, integrin regulation of CKI-1 was assessed in vivo. Our analysis revealed that CKI-1/p27KIP1 had an abnormal localization pattern in the nucleoplasm of animals expressing a mutant integrin, pat-3(sp). In the mutant animals, CKI-1::GFP was overexpressed and clumped in the nucleoplasm, while in animals expressing wild type integrin, CKI-1::GFP was localized predominantly to the nucleolus (Figure 2). Further studies revealed that the amount of CKI-1::GFP protein was increased in the pat-3 mutant. To delineate the genetic pathway responsible for the upregulation of CKI-1/p27KIP1, we depleted focal adhesion and SCF E3 ubiquitin ligase genes in pat-3(+) animals and found that these genes are essential for the proper localization and expression of CKI-1::GFP. We conclude that the inhibition of integrin signaling and protein degradation significantly affects CKI-1 protein localization and expression level in vivo.

Previous studies have suggested a link between the mammalian integrin splice variant β1C and p27KIP1. For example, increased expression of β1C integrin elevated p27KIP1 in prostate cancer cell lines [13], [21], [61]. Our pat-3(sp) mutant splice form is an artificial variant [34], however, our study found that pat-3(sp) behaves similarly to the β1C variant of mammalian β1. pat-3(sp) increases CKI-1/p27KIP1 expression, possibly leading to a cell cycle arrest.

CKI-1 is Localized to the Nucleolus

Our observations of nuclear morphology and experiments using ncl-1 (RNAi) strongly suggest a nucleolar localization for CKI-1::GFP in pat-3(+). In contrast, CKI-1::GFP appeared clumped and was irregularly distributed in the nucleoplasm of pat-3(sp) animals, suggesting ectopic accumulation of CKI-1. This nucleolar to nuclear transition in CKI-1::GFP localization suggests a possible link between CKI-1 and nucleolar function.

The nucleolus is the main site of ribosome biogenesis and ribosomal RNA (rRNA) synthesis [62]. The rRNAs are synthesized and assembled into a ribosomal complex in the nucleolus. In mammals, stressed ribosomal synthesis leads to cell cycle arrest via increased p27KIP1 levels [63]. In addition, mutations in the cytoplasmic tail of β4 integrin or p27 β4 binding protein (p27BBP/eIF6) result in an inability of β4 to localize to hemidesmosomes and a defect in assembly of the 80S ribosomal subunit, suggesting a connection between integrin signaling and ribosome biogenesis [64][66]. Although further studies are required, we speculate that the splice defective pat-3(sp) integrin may cause a decrease in ribosome biosynthesis.

Proper CKI-1 Localization is Linked to Integrin and Integrin-associated Molecules

Integrins are αβ heterodimers and both subunits are necessary for integrin function. Therefore, depletion of the α subunit would have the same effect as disruption of the β subunit, PAT-3. Indeed, CKI-1::GFP mislocalization and increased expression were observed when the α integrin gene ina-1 was depleted by RNAi, suggesting that CKI-1 upregulation is a result of disrupted integrin function and that integrin activity is normally required for proper CKI-1 localization and protein levels. In addition, RNAi analysis of the IPP complex showed that pat-4/ILK [46], [67], unc-97/PINCH [47] and pat-6/parvin [48] are also required for correct expression and/or localization of CKI-1. Some studies have suggested that these components act together and are degraded if pat-4/ILK or unc-97/PINCH is not present [68] but other studies, including ours, suggest these molecules may have independent roles [69], [70]. In addition, PINCH or parvin binding to ILK is mutually exclusive, suggesting that PINCH might provide a different mode of signaling than parvin [71], [72]. ILK has been shown to play an important role in cell proliferation in tissue culture [73] and PINCH is frequently upregulated in human cancers [74]. Disruption of ILK or PINCH inhibits cell proliferation and increases the expression level of p27KIP1 and pRb [75], suggesting that cells might generally respond to perturbed cell adhesion by inducing p27KIP1 expression and halting the cell cycle. In addition, our analysis links the ECM ligand, unc-52/perlecan, to CKI-1 localization, suggesting that perlecan-bound integrin might regulate CKI-1 by activating pat-4/ILK and unc-97/PINCH.

SCF E3 Ligase Complex is Required for the Proper Localization of CKI-1

This study revealed that ubiquitin-mediated protein degradation plays a crucial role in regulating CKI-1/p27KIP1. RNAi of SCF E3 ligase genes resulted in mislocalization of CKI-1::GFP. The E3 ligase includes a scaffold protein (CUL-1/CUL1) that assembles the ubiquitin ligation complex along with ubiquitin transferase (RBX-1/ROC1), an adaptor (SKPT-1/SKP2), and a substrate-binding protein (LIN-23/F-Box). The SKP2/Cullins/F-box (SCF) E3 ligase complex is involved in the degradation of cellular proteins such as cell cycle inhibitors, transcription factors and other signaling effectors [76]. It has been reported that phosphorylated p27KIP1 is degraded in an SCF-dependent manner and that the loss of SCF is associated with pathological conditions such as cancer [76][78]. Our RNAi analyses showed that SKPT-1/SKP2 [33], [55], LIN-23/F-Box [23], [59] and CUL-1/CUL1 [56], [58], [77] are required for the proper localization of CKI-1, while RBX-1/ROC1 showed no effect. This might indicate that SCF ligase forms a complex with a protein other than RBX-1 for the degradation of CKI-1.

Integrin Signaling May Influence the Cell Cycle by Regulating CKI-1 Level via SCF Ubiquitin Ligases

We propose a potential model for the role of integrin signaling in CKI-1 regulation. Our preferred model assumes the presence of functional integrin in the hypodermal cells. Integrin is activated by binding to ECM ligands and signaling is initiated and propagated by molecules such as pat-4/ILK and unc-97/PINCH to SCF ligase which degrades CKI-1 (Figure 6). pat-3(sp) may interfere with the formation of the SCF complex and the degradation of CKI-1 by inhibiting the function of wild-type PAT-3 integrins or by acting as a non-functional β subunit that significantly dilutes integrin signaling [8]. SAGE analysis indicates that pat-3 and ina-1 are expressed in hypodermal cells [79], [80] consistent with a previously identified role for ina-1/α integrin function in hypodermis [24]. Although we have identified a role for the SCF complex in CKI-1 degradation, our work does not specifically address whether SCF activation is directly linked to integrin signaling in a linear manner, as displayed in the model (Figure 6). Future genetic studies should determine the cell autonomy and epistatic relationships of the genes in the pathway from integrin to cell cycle control.

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Figure 6. Model for the integrin regulation of CKI-1.

When ECM ligand binds to integrin on the cell surface, the IPP complex delivers signals to the SCF E3 ligase complex resulting in sequestration of CKI-1/p27 to the nucleolus. In pat-3(sp), the mutant β integrin interferes with the function of wild-type pat-3(+). Consequently, integrin does not signal to the IPP complex. We suggest the reduced integrin signals may leave the SCF complex inactive. This allows an increase in the amount of CKI-1/p27 and alters the location of the protein in the nucleus.

https://doi.org/10.1371/journal.pone.0042425.g006

In addition to muscle and gonad morphogenesis, our work identifies another important function of integrin in C. elegans, the regulation of CKI-1/p27KIP1. This finding brings new insight onto cell cycle control. Integrins appear to regulate the level of p27KIP1 via signaling mediators such as pat-4/ILK and unc-97/PINCH and to maintain SCF ubiquitin ligase activity. Importantly, unc-52 RNAi produces a similar phenotype, suggesting that the cell-matrix interaction balances the amount of CKI-1 in the cell. This information will be useful in understanding the mechanism on how the cell-ECM interaction regulates cell cycle progression.

Materials and Methods

Animals and Culture

Caenorhabditis elegans were cultured on nematode growth medium (NGM) agar plates seeded with OP50 E. coli under standard conditions [81]. RW3600 qC1 dpy-19 (e1259) glp-1 (q339)/pat-3 (st564) III [38] were acquired from the Caenorhabditis Genetics Center (St. Paul, MN). The pat-3 transgenic rescued lines used in this study are listed in Table 2. All transgenic lines were cultured under standard conditions [81].

Mutant Pat-3 Constructs and Germline Tranformation

pPAT3 (+)-PB12K and mutant constructs for pPAT3-sp were created using overlap extension PCR and have been described previously [34]. Germline transformation was performed using the standard protocol for microinjections [82]. Briefly, pPAT3 constructs were mixed with cki-1::GFP [26] and rab-3::RFP or myo-3::RFP [83]. All rescued lines were made at a mixture of 5 µg/ml of pPAT3, 2 µg/ml of pVT352G (cki-1::GFP), and 100 µg/ml of pGH8 (rab-3::RFP) or 100 µg/ml of pCFJ104 (myo-3::RFP) in TE buffer (pH 7.5). This mixture was injected into a distal gonad of the RW3600 qC1 dpy-19(e1259) glp-1(q339)/pat-3(st564) III animal. F2 generation animals with 100% red progeny were isolated and more than 10 generations elapsed before the characterization of phenotypes and multiple lines were used for confirmation [84].

Phenotype Characterization and Nuclei Expression Pattern Identification

To characterize rescued lines, young adult worms were mounted in a drop of M9 buffer containing 1% NaN3 (Sigma Chemical Co., St. Louis, MO) or 0.5 mM levamisole on a 24×60 mm coverslip coated with 4% agarose and examined on a Nikon TE2000-U Diaphot epifluorescence microscope. Images were captured using a CoolSnap cf monochrome camera (Roper Scientific, Tucson, AZ) and analyzed with Metavue imaging software (version 7.5, Molecular Devices Co., Downingtown, PA). Typically, CKI-1::GFP became visible at the late L4 stage. In the wild-type rescue pat-3(+) animals, GFP was apparently nucleolar: a strong green spot on a larger green nucleus. To photograph the image, the camera was set at the exposure time of 2000 milliseconds. However, in pat-3(sp) animals, the CKI-1::GFP expression was much brighter than in the pat-3(+). For pat-3(sp), images were taken at the exposure time of 300 milliseconds. About 20 hypodermal nuclei in the midbody, an area including vulva at the ventral midline, of each animal was observed for nuclear morphology characterization. Displayed images are patterns seen most commonly under the described conditions.

To analyze the size of nucleoli, the area was measured using ImageJ software (version 1.33, National Institute of Health, Rockville, MD) [85]. To determine the nucleolar to nuclear ratio, the area value of nucleolus, a brighter spot on a nucleus, was divided by that of nucleus. Five measurements for each rescued line were averaged for comparison.

Reverse Transcription Polymerase Chain Reaction (RT-PCR)

To analyze cki-1, pat-3, and gpd-1/GAPDH mRNA levels, animals were partially synchronized by isolating embryos using 20% alkaline hypochlorite solution [86]. After 48 hours, forty L4 to young adult animals were picked into 10 µL of M9 buffer. RNA was extracted using 250 µL Tri-Reagent (Sigma-Aldrich, St. Louis, MO) and 50 µL chloroform (1/5 volume of Tri-Reagent) and RNA was precipitated from the extract with isopropanol. Approximately 1 µg of total RNA was used to synthesize cDNA with Transcriptor Reverse Transcription Kit (Roche, Carlsbad, CA) primed with random hexamers in a total 20 µL reaction volume. Total of 1 µL cDNA was used in PCR amplification with cki-1 primers, pat-3 primers, and with control gpd-1/GAPDH primers previously described [34]. Primer sequences listed below were used for amplification:

CKI1 Forward 2: 5′-GGAGTTCTACAGAACC-3′

CKI1 Reverse 2: 5′-CACCGGAGACAGCTTG-3′

PAT3PT Forward1: 5′-CTCAACGAAACTACACCCTGCC-3′

PAT3PT Reverse 1: 5′-TTAGTTGGCTTTTCCAGCGTATACTGG-3′.

Immunoblot Analysis

For quantitative analysis of CKI-1 protein levels in each strain, we first picked 30 young adults into 10 µL of M9 buffer and 10 µL of 2X Laemmli Sample Buffer (Bio-Rad Laboratories, Hercules, CA) premixed with 1∶1000 β-mercaptoethanol. Sample solutions were then boiled for 10 minutes at 100°C and electrophoresed through a 10% SDS-polyacrylamide gel at 180 V for 1 hour. Isolated proteins bands were electrotransferred onto a nitrocellulose membrane (Whatman Ltd., Dassel, Germany) using wet transfer at 100 V for 75 minutes in BSN transfer buffer with no methanol or SDS. This nitrocellulose membrane was then blocked for 1 hour in 5% milk solution at room temperature. Rabbit polyclonal IgG anti-GFP antibody (ab290, Abcam Inc., Cambridge, MA) at 1∶2000 was applied overnight at 4°C as primary antibody and goat anti-rabbit IgG HRP conjugated (ab6721, Abcam Inc., Cambridge, MA) at 1∶5000 was applied for 1 hour at RT. For control blots, LS25, a monoclonal antibody against UNC-54, or MH33, a monoclonal antibody against a gut specific intermediate filament protein, were diluted at 1∶1000 and 1∶2000. The primary antibody solutions were applied and detected by the goat anti-mouse IgG HRP conjugated (Sigma Chemical, Mo) secondary antibody. ECL chemiluminescence reagents (Thermo Fisher Scientific, Rockford, IL) were added to the membrane for 1 minute before exposure to the ULTRA-LUM gel imager (Ultra-Lum Inc., Claremont, CA) and analyzed with UltraQuant software (Ultra-Lum Inc., Claremont, CA). Individual band intensity was quantified using ImageJ software (version 1.66, National Institute of Health, Rockville, MD) that measured the integrated density of each band to analyze the intensity of bands.

RNA-mediated Interference of Gene Expression (RNAi) Analysis

C. elegans RNA interference analysis was performed using the bacterial feeding method [87], [88]. In addition to the standard RNAi protocol, we synchronized the stage of animals; embryos were collected using the standard 20% alkaline hypochlorite solution method [86]. After washes, collected embryos were placed onto RNAi plates, which were incubated in 20°C for 3 to 4 days until young adulthood before characterization. About 20 hypodermal nuclei in the midbody of transgenic worms were observed for the characterization of nuclear morphology using Metavue software. To verify the efficiency, all RNAi animals were examined for behavioral phenotypes linked to the RNAi gene. For example, focal adhesion gene RNAi was subjected to thrashing assays [89] because uncoordinated (Unc) phenotypes were previously reported for RNAi of these genes (Figure S2). Each RNAi-inducing plasmid (Geneservice, Hinxton, UK) used in this study was isolated and sequenced in order to verify the gene targeted by the construct.

Supporting Information

Figure S1.

ncl-1(RNAi) increases the size of the nucleolus in CKI-1::GFP in pat-3 transgenic animals. Panel A: ncl-1(RNAi); pat-3(+). The area of CKI-1::GFP is 2.4 times (P<.001) the size of the area seen in the no RNAi control in panel B: CKI-1::GFP in pat-3(+) background.

https://doi.org/10.1371/journal.pone.0042425.s001

(TIF)

Figure S2.

Locomotion defects of RNAi animal. Panel A: Number of body bends in 30 seconds was measured in pat-3(+) animals treated with RNAi of pat-3, ina-1, unc-97, unc-52, pat-6, let-2, and unc-112 genes. The number of body bends was compared to that of L4440, the negative control RNAi. Black bars indicate the average number of body bends for each RNAi tested. Horizontal bars indicate the standard error of each test. N = 10. *indicates P<.0001 (compared to L4440). Panel B: Number of body bends in 30 seconds was measured in pat-3(+) animals treated with RNAi of rbx-1, cul-4, skpt-1, lin-23, and cul-1 genes. The number of body bends was compared to that of L4440, the negative control RNAi. Bars indicate the average number of body bends for each RNAi tested. Horizontal bars indicate the standard error of each test. N = 10. *indicates P<.0001 (compared to L4440).

https://doi.org/10.1371/journal.pone.0042425.s002

(TIF)

Acknowledgments

The authors thank Dr. Victor Ambros for the VT352G cki-1::GFP DNA construct and appreciate the many people who read and offered comments on the manuscript.

Author Contributions

Conceived and designed the experiments: ML. Performed the experiments: SK EJY JC EC. Analyzed the data: SK EJY EC ML. Contributed reagents/materials/analysis tools: EC ML. Wrote the paper: SK EJY EC ML.

References

  1. 1. Arnaout MA, Mahalingam B, Xiong JP (2005) Integrin structure, allostery, and bidirectional signaling. Annu Rev Cell Dev Biol 21: 381–410.
  2. 2. Hynes RO (2002) Integrins: bidirectional, allosteric signaling machines. Cell 110: 673–687.
  3. 3. Fornaro M, Languino LR (1997) Alternatively spliced variants: a new view of the integrin cytoplasmic domain. Matrix Biol 16: 185–193.
  4. 4. Belkin AM, Retta SF, Pletjushkina OY, Balzac F, Silengo L, et al. (1997) Muscle β1D integrin reinforces the cytoskeleton-matrix link: Modulation of integrin adhesive function by alternative splicing. J Cell Biology 139: 1583–1595.
  5. 5. Baudoin C, Van der Flier A, Borradori L, Sonnenberg A (1996) Genomic organization of the mouse β1 gene: conservation of the β1D but not of the β1B and β1C integrin splice variants. Cell Adhes Commun 4: 1–11.
  6. 6. Armulik A (2002) Splice variants of human β1 integrins: origin, biosynthesis and functions. Front Biosci 7: d219–227.
  7. 7. Balzac F, Retta SF, Albini A, Melchiorri A, Koteliansky VE, et al. (1994) Expression of β1B integrin isoform in CHO cells results in a dominant negative effect on cell adhesion and motility. J Cell Biol 127: 557–565.
  8. 8. Balzac F, Belkin AM, Koteliansky VE, Balabanov YV, Altruda F, et al. (1993) Expression and functional analysis of a cytoplasmic domain variant of the β1 integrin subunit. J Cell Biol 121: 171–178.
  9. 9. Altruda F, Cervella P, Tarone G, Botta C, Balzac F, et al. (1990) A human integrin β1 subunit with a unique cytoplasmic domain generated by alternative mRNA processing. Gene 95: 261–266.
  10. 10. Languino LR, Ruoslahti E (1992) An alternative form of the integrin β1 subunit with a variant cytoplasmic domain. J Biol Chem 267: 7116–7120.
  11. 11. Meredith J Jr, Takada Y, Fornaro M, Languino LR, Schwartz MA (1995) Inhibition of cell cycle progression by the alternatively spliced integrin β1C. Science 269: 1570–1572.
  12. 12. Fornaro M, Tallini G, Bofetiado CJ, Bosari S, Languino LR (1996) Down-regulation of β1C integrin, an inhibitor of cell proliferation, in prostate carcinoma. Am J Pathol 149: 765–773.
  13. 13. Fornaro M, Manzotti M, Tallini G, Slear AE, Bosari S, et al. (1998) β1C integrin in epithelial cells correlates with a nonproliferative phenotype: forced expression of β1C inhibits prostate epithelial cell proliferation. Am J Pathol 153: 1079–1087.
  14. 14. Wozniak MA, Desai R, Solski PA, Der CJ, Keely PJ (2003) ROCK-generated contractility regulates breast epithelial cell differentiation in response to the physical properties of a three-dimensional collagen matrix. J Cell Biol 163: 583–595.
  15. 15. Paszek MJ, Zahir N, Johnson KR, Lakins JN, Rozenberg GI, et al. (2005) Tensional homeostasis and the malignant phenotype. Cancer Cell 8: 241–254.
  16. 16. Mettouchi A, Klein S, Guo W, Lopez-Lago M, Lemichez E, et al. (2001) Integrin-specific activation of Rac controls progression through the G(1) phase of the cell cycle. Mol Cell 8: 115–127.
  17. 17. Walker JL, Assoian RK (2005) Integrin-dependent signal transduction regulating cyclin D1 expression and G1 phase cell cycle progression. Cancer Metastasis Rev 24: 383–393.
  18. 18. Fornaro M, Tallini G, Zheng DQ, Flanagan WM, Manzotti M, et al. (1999) p27(kip1) acts as a downstream effector of and is coexpressed with the β1C integrin in prostatic adenocarcinoma. J Clin Invest 103: 321–329.
  19. 19. Guo Y, Sklar GN, Borkowski A, Kyprianou N (1997) Loss of the cyclin-dependent kinase inhibitor p27(Kip1) protein in human prostate cancer correlates with tumor grade. Clin Cancer Res 3: 2269–2274.
  20. 20. Del Pizzo JJ, Borkowski A, Jacobs SC, Kyprianou N (1999) Loss of cell cycle regulators p27(Kip1) and cyclin E in transitional cell carcinoma of the bladder correlates with tumor grade and patient survival. Am J Pathol 155: 1129–1136.
  21. 21. Fornaro M, Manes T, Languino LR (2001) Integrins and prostate cancer metastases. Cancer Metastasis Rev 20: 321–331.
  22. 22. Kamai T, Takagi K, Asami H, Ito Y, Oshima H, et al. (2001) Decreasing of p27(Kip1)and cyclin E protein levels is associated with progression from superficial into invasive bladder cancer. Br J Cancer 84: 1242–1251.
  23. 23. Carrano AC, Pagano M (2001) Role of the F-box protein Skp2 in adhesion-dependent cell cycle progression. J Cell Biol 153: 1381–1390.
  24. 24. Baum PD, Garriga G (1997) Neuronal migrations and axon fasciculation are disrupted in ina-1 integrin mutants. Neuron 19: 51–62.
  25. 25. Gettner SN, Kenyon C, Reichardt LF (1995) Characterization of βpat-3 heterodimers, a family of essential integrin receptors in C. elegans. J Cell Biol 129: 1127–1141.
  26. 26. Hong Y, Roy R, Ambros V (1998) Developmental regulation of a cyclin-dependent kinase inhibitor controls postembryonic cell cycle progression in Caenorhabditis elegans. Development 125: 3585–3597.
  27. 27. Ambros V (1999) Cell cycle-dependent sequencing of cell fate decisions in Caenorhabditis elegans vulva precursor cells. Development 126: 1947–1956.
  28. 28. Feng H, Zhong W, Punkosdy G, Gu S, Zhou L, et al. (1999) CUL-2 is required for the G1-to-S-phase transition and mitotic chromosome condensation in Caenorhabditis elegans. Nat Cell Biol 1: 486–492.
  29. 29. Kostic I, Roy R (2002) Organ-specific cell division abnormalities caused by mutation in a general cell cycle regulator in C. elegans. Development 129: 2155–2165.
  30. 30. Kostic I, Li S, Roy R (2003) cki-1 links cell division and cell fate acquisition in the C. elegans somatic gonad. Dev Biol 263: 242–252.
  31. 31. Buck SH, Chiu D, Saito RM (2009) The cyclin-dependent kinase inhibitors, cki-1 and cki-2, act in overlapping but distinct pathways to control cell cycle quiescence during C. elegans development. Cell Cycle 8: 2613–2620.
  32. 32. Boxem M, van den Heuvel S (2001) lin-35 Rb and cki-1 Cip/Kip cooperate in developmental regulation of G1 progression in C. elegans. Development 128: 4349–4359.
  33. 33. Kim Y, Kipreos ET (2007) The Caenorhabditis elegans replication licensing factor CDT-1 is targeted for degradation by the CUL-4/DDB-1 complex. Mol Cell Biol 27: 1394–1406.
  34. 34. Xu X, Ahn JH, Tam P, Yu EJ, Batra S, et al. (2010) Analysis of conserved residues in the βpat-3 cytoplasmic tail reveals important functions of integrin in multiple tissues. Dev Dyn 239: 763–772.
  35. 35. Deshaies RJ, Joazeiro CA (2009) RING domain E3 ubiquitin ligases. Annu Rev Biochem 78: 399–434.
  36. 36. Fire A, Xu SQ, Montgomery MK, Kostas SA, Driver SE, et al. (1998) Potent and specific genetic interference by double-stranded RNA in Caenorhabditis elegans. Nature 391: 806–811.
  37. 37. Chen N, Harris TW, Antoshechkin I, Bastiani C, Bieri T, et al. (2005) WormBase: a comprehensive data resource for Caenorhabditis biology and genomics. Nucleic Acids Res 33 Database Issue. D383–389.
  38. 38. Williams BD, Waterston RH (1994) Genes critical for muscle development and function in Caenorhabditis elegans identified through lethal mutations. J Cell Biol 124: 475–490.
  39. 39. Giancotti FG, Ruoslahti E (1999) Integrin signaling. Science 285: 1028–1032.
  40. 40. Philipp-Staheli J, Payne SR, Kemp CJ (2001) p27(Kip1): regulation and function of a haploinsufficient tumor suppressor and its misregulation in cancer. Exp Cell Res 264: 148–168.
  41. 41. Hedgecock EM, White JG (1985) Polyploid tissues in the nematode Caenorhabditis elegans. Dev Biol 107: 128–133.
  42. 42. Hedgecock EM, Herman RK (1995) The ncl-1 gene and genetic mosaics of Caenorhabditis elegans. Genetics 141: 989–1006.
  43. 43. Frank DJ, Roth MB (1998) ncl-1 is required for the regulation of cell size and ribosomal RNA synthesis in Caenorhabditis elegans. J Cell Biol 140: 1321–1329.
  44. 44. Moerman DG, Williams BD (2006) Sarcomere assembly in C. elegans muscle. WormBook. 1–16.
  45. 45. Qadota H, Benian GM (2010) Molecular structure of sarcomere-to-membrane attachment at M-Lines in C. elegans muscle. J Biomed Biotechnol 2010: 864749.
  46. 46. Mackinnon AC, Qadota H, Norman KR, Moerman DG, Williams BD (2002) C. elegans PAT-4/ILK functions as an adaptor protein within integrin adhesion complexes. Curr Biol 12: 787–797.
  47. 47. Hobert O, Moerman DG, Clark KA, Beckerle MC, Ruvkun G (1999) A conserved LIM protein that affects muscular adherens junction integrity and mechanosensory function in Caenorhabditis elegans. J Cell Biol 144: 45–57.
  48. 48. Lin X, Qadota H, Moerman DG, Williams BD (2003) C. elegans PAT-6/Actopaxin plays a critical role in the assembly of integrin adhesion complexes in vivo. Curr Biol 13: 922–932.
  49. 49. Wickstrom SA, Lange A, Montanez E, Fassler R (2010) The ILK/PINCH/parvin complex: the kinase is dead, long live the pseudokinase! EMBO J. 29: 281–291.
  50. 50. Rogalski TM, Williams BD, Mullen GP, Moerman DG (1993) Products of the unc-52 gene in Caenorhabditis elegans are homologous to the core protein of the mammalian basement membrane heparan sulfate proteoglycan. Genes Dev 7: 1471–1484.
  51. 51. Rogalski TM, Gilchrist EJ, Mullen GP, Moerman DG (1995) Mutations in the unc-52 gene responsible for body wall muscle defects in adult Caenorhabditis elegans are located in alternatively spliced exons. Genetics 139: 159–169.
  52. 52. Merz DC, Alves G, Kawano T, Zheng H, Culotti JG (2003) UNC-52/perlecan affects gonadal leader cell migrations in C. elegans hermaphrodites through alterations in growth factor signaling. Dev Biol 256: 173–186.
  53. 53. Sibley MH, Graham PL, von Mende N, Kramer JM (1994) Mutations in the α2(IV) basement membrane collagen gene of Caenorhabditis elegans produce phenotypes of differing severities. Embo J 13: 3278–3285.
  54. 54. Jonason JH, Gavrilova N, Wu M, Zhang H, Sun H (2007) Regulation of SCF(SKP2) ubiquitin E3 ligase assembly and p27(KIP1) proteolysis by the PTEN pathway and cyclin D1. Cell Cycle 6: 951–961.
  55. 55. Bai C, Sen P, Hofmann K, Ma L, Goebl M, et al. (1996) SKP1 connects cell cycle regulators to the ubiquitin proteolysis machinery through a novel motif, the F-box. Cell 86: 263–274.
  56. 56. Lyapina SA, Correll CC, Kipreos ET, Deshaies RJ (1998) Human CUL1 forms an evolutionarily conserved ubiquitin ligase complex (SCF) with SKP1 and an F-box protein. Proc Natl Acad Sci U S A 95: 7451–7456.
  57. 57. Carrano AC, Eytan E, Hershko A, Pagano M (1999) SKP2 is required for ubiquitin-mediated degradation of the CDK inhibitor p27. Nat Cell Biol 1: 193–199.
  58. 58. Kipreos ET, Lander LE, Wing JP, He WW, Hedgecock EM (1996) cul-1 is required for cell cycle exit in C. elegans and identifies a novel gene family. Cell 85: 829–839.
  59. 59. Hebeisen M, Roy R (2008) CDC-25.1 stability is regulated by distinct domains to restrict cell division during embryogenesis in C. elegans. Development 135: 1259–1269.
  60. 60. Higa LA, Yang X, Zheng J, Banks D, Wu M, et al. (2006) Involvement of CUL4 ubiquitin E3 ligases in regulating CDK inhibitors Dacapo/p27Kip1 and cyclin E degradation. Cell Cycle 5: 71–77.
  61. 61. Moro L, Perlino E, Marra E, Languino LR, Greco M (2004) Regulation of β1C and β1A integrin expression in prostate carcinoma cells. J Biol Chem 279: 1692–1702.
  62. 62. Lo SJ, Lee CC, Lai HJ (2006) The nucleolus: reviewing oldies to have new understandings. Cell Res 16: 530–538.
  63. 63. Donati G, Montanaro L, Derenzini M (2012) Ribosome biogenesis and control of cell proliferation: p53 is not alone. Cancer Res 72: 1602–1607.
  64. 64. Gandin V, Miluzio A, Barbieri AM, Beugnet A, Kiyokawa H, et al. (2008) Eukaryotic initiation factor 6 is rate-limiting in translation, growth and transformation. Nature 455: 684–688.
  65. 65. Chendrimada TP, Finn KJ, Ji X, Baillat D, Gregory RI, et al. (2007) MicroRNA silencing through RISC recruitment of eIF6. Nature 447: 823–828.
  66. 66. Sanvito F, Piatti S, Villa A, Bossi M, Lucchini G, et al. (1999) The β4 integrin interactor p27(BBP/eIF6) is an essential nuclear matrix protein involved in 60S ribosomal subunit assembly. J Cell Biol 144: 823–837.
  67. 67. Xu X, Rongali SC, Miles JP, Lee KD, Lee M (2006) pat-4/ILK and unc-112/Mig-2 are required for gonad function in Caenorhabditis elegans. Exp Cell Res 312: 1475–1483.
  68. 68. Fukuda T, Chen K, Shi X, Wu C (2003) PINCH-1 is an obligate partner of integrin-linked kinase (ILK) functioning in cell shape modulation, motility, and survival. J Biol Chem 278: 51324–51333.
  69. 69. Clark KA, McGrail M, Beckerle MC (2003) Analysis of PINCH function in Drosophila demonstrates its requirement in integrin-dependent cellular processes. Development 130: 2611–2621.
  70. 70. Zhang Y, Chen K, Tu Y, Velyvis A, Yang Y, et al. (2002) Assembly of the PINCH-ILK-CH-ILKBP complex precedes and is essential for localization of each component to cell-matrix adhesion sites. J Cell Sci 115: 4777–4786.
  71. 71. Wang X, Fukuda K, Byeon IJ, Velyvis A, Wu C, et al. (2008) The structure of α-parvin CH2-paxillin LD1 complex reveals a novel modular recognition for focal adhesion assembly. J Biol Chem 283: 21113–21119.
  72. 72. Montanez E, Wickstrom SA, Altstatter J, Chu H, Fassler R (2009) α-parvin controls vascular mural cell recruitment to vessel wall by regulating RhoA/ROCK signalling. EMBO J 28: 3132–3144.
  73. 73. Grashoff C, Aszodi A, Sakai T, Hunziker EB, Fassler R (2003) Integrin-linked kinase regulates chondrocyte shape and proliferation. EMBO Rep 4: 432–438.
  74. 74. Wang-Rodriguez J, Dreilinger AD, Alsharabi GM, Rearden A (2002) The signaling adapter protein PINCH is up-regulated in the stroma of common cancers, notably at invasive edges. Cancer 95: 1387–1395.
  75. 75. Cruet-Hennequart S, Maubant S, Luis J, Gauduchon P, Staedel C, et al. (2003) α(v) integrins regulate cell proliferation through integrin-linked kinase (ILK) in ovarian cancer cells. Oncogene 22: 1688–1702.
  76. 76. Skaar JR, Pagano M (2009) Control of cell growth by the SCF and APC/C ubiquitin ligases. Curr Opin Cell Biol 21: 816–824.
  77. 77. Tsvetkov LM, Yeh KH, Lee SJ, Sun H, Zhang H (1999) p27(Kip1) ubiquitination and degradation is regulated by the SCF(Skp2) complex through phosphorylated Thr187 in p27. Curr Biol 9: 661–664.
  78. 78. Chu I, Sun J, Arnaout A, Kahn H, Hanna W, et al. (2007) p27 phosphorylation by Src regulates inhibition of cyclin E-Cdk2. Cell 128: 281–294.
  79. 79. Griffith OL, Pleasance ED, Fulton DL, Oveisi M, Ester M, et al. (2005) Assessment and integration of publicly available SAGE, cDNA microarray, and oligonucleotide microarray expression data for global coexpression analyses. Genomics 86: 476–488.
  80. 80. Pleasance ED, Marra MA, Jones SJ (2003) Assessment of SAGE in transcript identification. Genome Res 13: 1203–1215.
  81. 81. Brenner S (1974) The genetics of Caenorhabditis elegans. Genetics 77: 71–94.
  82. 82. Mello CC, Kramer JM, Stinchcomb D, Ambros V (1991) Efficient gene transfer in C.elegans: extrachromosomal maintenance and integration of transforming sequences. EMBO J 10: 3959–3970.
  83. 83. Frokjaer-Jensen C, Davis MW, Hopkins CE, Newman BJ, Thummel JM, et al. (2008) Single-copy insertion of transgenes in Caenorhabditis elegans. Nat Genet 40: 1375–1383.
  84. 84. Lee M, Cram EJ, Shen B, Schwarzbauer JE (2001) Roles for βpat-3 integrins in development and function of Caenorhabditis elegans muscles and gonads. J Biol Chem 276: 36404–36410.
  85. 85. Dello SA, van Dam RM, Slangen JJ, van de Poll MC, Bemelmans MH, et al. (2007) Liver volumetry plug and play: do it yourself with ImageJ. World J Surg 31: 2215–2221.
  86. 86. Wood WB (1988) The Nematode. Caenorhabditis elegans. Cold Spring Harbor Laboratory Press.
  87. 87. Timmons L, Tabara H, Mello CC, Fire AZ (2003) Inducible systemic RNA silencing in Caenorhabditis elegans. Mol Biol Cell 14: 2972–2983.
  88. 88. Fire A, Xu S-Q, Montgomery MK, Kostas SA, Driver SE, et al. (1998) Potent and specific genetic interference by double-stranded RNA in Caenorhabditis elegans. Nature 319: 806–811.
  89. 89. Lee M, Shen B, Schwarzbauer JE, Ahn J, Kwon J (2005) Connections between integrins and Rac GTPase pathways control gonad formation and function in C. elegans. Biochim Biophys Acta 1723: 248–255.
  90. 90. Francis R, Waterston RH (1991) Muscle cell attachment in Caenorhabditis elegans. Journal of Cell Biology 114: 465–479.