Centrins (Cetns) are highly conserved, widely expressed and multifunctional Ca2+-binding eukaryotic signature proteins best known for their roles in ciliogenesis and as critical components of the global genome nucleotide excision repair system. Two distinct Cetn subtypes, Cetn2-like and Cetn3-like, have been recognized and implicated in a range of cellular processes. In the course of morpholino-based loss of function studies in Xenopus laevis, we have identified a previously unreported Cetn2-specific function, namely in fibroblast growth factor (FGF) mediated signaling, specifically through the regulation of FGF and FGF receptor RNA levels. Cetn2 was found associated with the RNA polymerase II binding sites of the Cetn2-regulated FGF8 and FGFR1a genes, but not at the promoter of a gene (BMP4) whose expression was altered indirectly in Cent2 morphant embryos. These observations point to a previously unexpected role of Cetn2 in the regulation of gene expression and embryonic development.
Centrins (Cetn) are calmodulin-like eukaryotic signature proteins1. Cetn2-like and Cetn3-like subclasses of Cetns have been identified2,3. In the yeast Saccharomyces cerevisiae there is a single Cetn3-like Cetn gene, CDC31; its function is required for spindle pole body duplication4. The ciliated protozoa Tetrahymena thermophila contains (at least) four Cetn genes, three of which are expressed5.
Loss of either the Cetn2-like Cen1 or the Cetn3-like Cen2 genes produce non-redundant defects in basal body and cilia formation. While the Cetn2-like gene is essential for cell division, the Cetn3-like gene is not; cells null for the Cetn3-like Cen2 gene appear to divide normally but have aberrant basal body organization5,6,7.
The roles of Cetns in vertebrate cells appear to be more subtle and diverse. Mice have four distinct Cetn genes; Cetn2, Cetn3, and Cetn4 are typical intron containing genes, while Cetn1 lacks introns and is thought to have been generated by a retrotransposition event from Cetn28. Humans appear to lack a Cetn4-like gene9. Null mutations in mouse Cetn1 lead to infertility apparently due to defects in sperm development10 Zebrafish Cetn2 morphants11 and mice homozygous for a null mutation in Cetn212 have no reported cell division phenotypes but display ciliopathy-related phenotypes. Cetn3 and Cetn4 null phenotypes in the mouse have not, to our knowledge, been reported.
The removal of all three Cetn genes has been achieved in the chick hyper-recombinogenic DT40 cell line. Cetn2, Cetn3 and Cetn4 DT40 null cells display no apparent defects in centrosome formation or cell division but were hypersensitive to UV irradiation13. The radiation-sensitive phenotype observed in these cells was expected given the role of Cetn2 as an integral component of the nucleotide excision repair/xeroderma pigmentosum group C (XPC-RAD23-CETN2) complex14,15. Araki et al. reported that “almost 100% of CEN2 (sic) in the cell extract was co-precipitated with the anti-XPC antibody”14. While Cetns are certainly associated with centrosomes and basal bodies, the majority of cellular Cetn2 is apparently soluble and located throughout the cytoplasm and nucleus16. A number of other functions have been ascribed to Cetns, from the transport of heterotrimeric transducin G-proteins in retinal photoreceptor cells to interactions with heat shock proteins, the regulation of proteosome activity and the nuclear transport of RNAs and proteins3. It is clear that Cetn2 and Cetn3 have distinct functional roles in a number of systems.
Results and Discussion
The idiosyncratic aspects of X. laevis development can reveal gene functions hidden in other organisms17. We therefore set out to explore the roles of Cetns in early X. laevis development. Both X. laevis and X. tropicalis have multiple centrin genes, based on data accessed through Xenbase18. The gene/protein originally designated as Centrin (X. laevis: NCBI Reference Sequence: NP_001081398.1 and X. tropicalis: NP_001016387.1) or Centrin-1 (X. laevis: NCBI Reference Sequence: NP_001080127.1) display a Cetn2-like, rather than a Cetn1-like, genomic structure (see supplementary figure 1); we therefore refer to them as Cetn2 (see below). No Cetn1-like gene appears to be present in either X. laevis or X. tropicalis genomes. The Cetn3 and Cetn4 genes identified in X. laevis are similar in genomic structure to those found in mouse and human.
The latest version of the X. laevis genome (7.1 as searched through the Xenbase Blast function in March 2015) reveals two distinct Cetn2 (Cetn2a and Cetn2s) and Cetn3 (Cetn3l and Cetn3s) genes and apparently a single Cetn4 gene. Our studies focus on the Cetn2a, Cetn3l and Cetn4 genes. Cetn2a corresponds to the 172 amino acid polypeptide labeled cetn1 or centrin (see above); Cetn3l corresponds to the 167 amino acid polypeptide labeled Cetn3 (GenBank: AAI29791.1). We isolated full length cDNAs that correspond to Cetn2a, Cetn3l and Cetn4. An analysis of gene expression during early Xenopus embryogenesis by Yanai et al.19 (Fig. 1A) and our own RT-PCR data in X. laevis (Fig. 1B) indicate that Cetn2a, Cetn3l and Cetn4 RNAs are supplied maternally and are present at high levels throughout early development; we have not directly examined the expression levels of the Cetn2s or Cetn3s genes.
We used two different antibodies to localized Cetn proteins in X. laevis. The first is a rabbit antibody (anti-XlCetn)20 that recognizes Cetn2, Cetn3 and Cetn4 proteins based on its recognition of Cetn2a, Cetn3l and Cetn4 polypeptides expressed from injected RNAs (Fig. 1C and data not shown). The second antibody is a commercially available rabbit antibody (anti-HsCetn1) that reacts preferentially with X. laevis Cetn2a compared to Cetn3l (Fig. 1C). Because the anti-HsCetn1 antibody produced higher overall background labelling, we used the anti-XlCetn antibody for most staining studies. Both anti-Cetn antibodies stain the basal body region of epidermal ciliated cells (Fig. 1D–F). There is also discernible staining of the myotome; neuronal microtubules are not stained (Fig. 1G–J - anti-XlCetn staining shown). Basal body localization of all three Cetns was confirmed using C-terminally GFP tagged forms of Cetn2a, Cent3l and Cetn4 expressed from injected RNAs (see below).
To down-regulate the levels of specific Cetn proteins in embryos we commissioned Gene-Tools LLC to design anti-sense translation blocking modified DNA oligonucleotides (morpholinos or MOs) specific for Cetn2a, Cetn3L and Cetn4 RNAs (see supplemental figure. 2). The Cetn2s gene encodes a 201 amino acid long polypeptide that differs from Cetn2a primarily by the presence of a 29 amino acid insertion at its N-terminus. Similarly the Cetn3S gene encodes a 212 amino acid long polypeptide that differs from Cetn3l primarily by the presence of a 32 amino acid insertion at its N-terminus. Given the dramatic nature of the Cetn2 morphant phenotype (see below) we commissioned a second, completely non-overlapping anti-Cetn2 morpholino (Cetn2-MO2). The translation of the Cetn2s RNA is not expected to be altered by either of the Cetn2a morpholinos used in our studies; similarly expression of Cetn3s is not expected to be altered by the Cetn3l morpholino. Because of its dramatic nature, we concentrate the studies described here on the characterization of the Cetn2a morphant phenotype. Plasmids that encode versions of Cetn2a-GFP, Cetn3l-GFP and Cetn4-GFP that contain sequences that match the Cetn2a-MO1, Cetn3l-MO and Cetn4-MO morpholinos perfectly were created for specificity and rescue studies. The Cetn2-MO1 and Cetn2-MO2 morpholinos reduced the level of Cetn2 protein but not Cetn3 or Cetn4, while the Cetn3 and Cetn4 morpholinos specifically reduced the accumulation of their targets (Fig. 2).
In ectodermal explants, a single Cetn morpholino alone (10 ngs/embryo) did not dramatically or reproducibly disrupt the formation of cilia in multiciliated cells; cilia formation did appear to be disrupted when multiple Cetn morpholinos were used together (supplemental figure. 3 and data not shown). Cetn2 morphants exhibited embryonic phenotypes unlike those associated with a typical ciliopathy; they appeared similar to those associated with defects in FGF-mediated mesoderm formation21. This phenotype was distinct from that displayed by Cetn3 and Cetn4 morphants (supplemental figure. 3 and data not shown) as well as in Chibby (Cby) morphants (Cby is a basal body protein associated with the regulation of Wnt signaling)22.
To test whether Cetn2 morpholinos disrupted FGF signaling, we used ectodermal and mesodermal explants, as described previously23. In culture, such explants normally elongate and form notochordal tissue within the mesodermal domain (Fig. 3A). When the mesodermal domain was taken from a Cetn2 morphant embryo, elongation was inhibited and notochordal tissue failed to form (Fig. 2B). When the ectodermal region was derived from a Cetn2 morphant, morphological extension was somewhat suppressed but notochordal tissue formed (Fig. 3C). Similar results were obtained using mesoderm only explants. Again, control explants displayed an extended morphology (Fig. 3D) and formed notochordal tissue (Fig. 3I). Cetn2 morphant explants failed to elongate (Fig. 3E) or form notochord (Fig. 3J). The morphological extension and notochord phenotypes displayed by Cetn2 morphant explants were rescued by Cetn2 (Fig. 3G,K) but not by Cetn3 (Fig. 3L) RNA injection. The Cetn2 morpholino elongation defect was similar to that seen in explants derived from embryos injected with RNA encoding a dominant negative form of FGF Receptor 1 (dnFGFR1)(Fig. 3F). That the Cetn2 morphant phenotype involves effects on FGF signaling was further suggested by the fact that the phenotype could be rescued by the injection of FGF8 RNA (Fig. 3M).
Together with retinoic acid, Wnt, FGF and BMP are three of the most prominent signaling pathways involved in early embryonic patterning, including mesoderm/notochord formation24. A preliminary RT-PCR analysis of the levels of Wnt8a, FGF8 and BMP4a RNAs in stage 11 control and Cetn2 morphant embryos revealed a dramatic decrease in FGF8 and an increase in BMP4a RNA levels, with no apparent change in Wnt8a RNA levels (Fig. 4A). This is a pattern of changing RNA levels quite distinct from that observed in ectodermal explants and whole embryos injected with morpholinos directed against either of two other cilia/basal body-associated proteins, Cby22 and EFHC1 (Zhao et al., in preparation). We confirmed this result using quantitative reverse transcription PCR (qPCR) of Cetn2 morphant embryos prepared by injecting either the MO1 or MO2 Cetn2 morpholinos. These morpholinos decreased the levels of FGF2, FGF4, FGF8, FGFR1a and FGFR1b RNAs but produced no significant change in FGFR2, FGFR3, or FGFR4a RNAs. The Cetn3 MO did not change the level of any FGF or FGFR RNA examined (Fig. 4B,C). In rescue studies, co-injection of Cetn2-GFP RNA could return the levels of FGF8 and FGFR1a to control levels, while Cetn3-GFP and Cetn4-GFP RNAs could not (Fig. 4D).
FGF and BMP have been found to regulate each other’s expression in the early embryo25. To determine whether the effects of Cetn2 morpholinos were direct or indirect, we injected RNA encoding the BMP antagonist Noggin26 into Cetn2 morphant embryos. Noggin RNA reduced the Cetn2 MO induced increase in the level of BMP4a RNA, but did not increase the level of FGF8 RNA (Fig. 4E). In contrast, the injection of FGF8 RNA reduced the Cetn2 MO induced increase in the level of BMP4a RNA, but failed to rescue the levels of FGFR1a RNA (Fig. 4F). This suggests that Cetn2 plays a direct role in the regulation of FGF8 and FGFR1a/b, while its effects on BMP4a RNA levels are indirect and the result of changes in FGF signaling.
Given Cetn2’s established presence in the nucleus (see above) and the effects of the Cetn2 morpholinos on FGF8 and FGFR1a RNA levels, it seemed plausible that Cetn2 might directly influence the expression of these genes through interactions with chromatin. We initially examined the FGF8 gene in X. tropicalis using anti-XlCetn, anti-HsCetn1 (which preferentially reacts with Cetn2 over Cetn3 - see above) and anti-RNA polymerase II antibodies. We found that Cetn co-localized with polymerase at these loci (Fig. 5A). Further experiments in X. laevis used RNAs encoding GFP-tagged forms of X. laevis Cetn2a, Cetn3l and Cetn4 (see Methods). In ectodermal explants derived from RNA injected fertilized eggs, myc-Cetn2-GFP (Fig. 5B,C) and Cetn4-GFP (SupFig. 4) polypeptides preferentially accumulated in ciliated cells and localized to the basal body region of cilia (Fig. 5D,E). myc-Cetn3-GFP was also found to accumulate preferentially in ciliated cells (Fig. 5F,G) and was localized to basal bodies (Fig. 5H,I), but its localization was not quite as cilia-specific as that observed for Cetn2. That said, in ectodermal explants expressing (from injected RNA) both a C-terminally RFP-tagged Cetn2 (Cetn2-RFP) and myc-Cetn3-GFP, we saw regions of high overlap, as well as regions of distinct Cetn2 and Cetn3 accumulation (Fig. 5J–M). In chromatin immunoprecipitation (ChIP) experiments, myc-Cetn2-GFP but not myc-Cetn3-GFP or GFP alone, co-localized with Pol II on the FGF8 and FGFR1a genes (Fig. 5N,O); neither Cetn localized with Pol II on the BMP4a gene (Fig. 5P), as expected for an indirect target of Cetn2-mediated regulation.
Our work reveals a new and unexpected role for Cetn2 as a transcriptional regulator of a subset of FGF and FGFR genes. The fact that Cetn2 was found to co-localize with Pol II at some, but not all genes suggests that its promoter association is dependent upon the presence of other proteins. In addition to its nuclear role as part of the XPC DNA repair complex, Cetn2 has been reported to be an integral component of the Trex2 complex, which appears to interact with both nuclear pores and RNA polymerase and has been implicated in the nuclear export of mRNAs27,28. This suggests that the Cetn2 morphant phenotype could, in part, involve changes in Trex2 function or other, as yet unidentified interactions. To resolve this issue, we are currently in the process of identifying Cetn2-associated proteins in Xenopus and other systems.
The role of Cetn2 as a regulator of mesodermal differentiation, as revealed by notochord formation, in Xenopus early embryonic development may seem at odds with the reported phenotypes of morpholino treated Zebrafish embryos and Cetn2 null mice. In the Zebrafish Danio rerio, depletion of Cetn2 led to a ciliopathy-related cyst formation phenotype11. A syndromic ciliopathy, including dysosmia and hydrocephalus was reported in Cetn2 null mice12. We anticipate that the phenotypic differences between these three vertebrates can be attributed to differences in developmental mechanisms and Cetn2-containing complexes, the patterns of centrin gene expression during embryonic development and perhaps some level of partial redundancy between the centrin genes, although neither Cetn3 or Cetn4 RNAs rescued the Cetn2 morphant gene expression phenotype. That said, a role of Cetn2 in the regulation of gene expression and its integral role in the functions of XPC, Trex2 and perhaps other complexes, indicates the need for more subtle analyzes of the physiological roles of Cetn2 in particular and Cetns as a class of proteins.
Materials and Methods
Embryos, their manipulation and analysis
X. laevis embryos were staged and explants were generated, following standard procedures29. Capped mRNAs were transcribed from linearized plasmid templates using mMessage mMachine kits (Ambion) following manufacturer’s instructions. At the two-cell stage embryo injections were directed equatorially. As an injection tracer, we routinely included RNAs (150 pgs/embryo) encoding either β-galactosidase, green fluorescent protein (GFP) or GFP-CAAX, which is membrane-associated. In the case of GFP/GFP-CAAX RNA injection, embryos were examined at stage 10-11 by fluorescent microscopy to confirm the accuracy of injection. RNA isolation, cDNA synthesis, RT-PCR and qPCR analyses were carried out as described previously22,23. Real-time (quantitative) PCR was carried out using a Mastercycler Epgradient Realplex device (Eppendorf). PCR reactions were set up using DyNAmo SYBR Green qPCR kits (Finnzymes). Each sample was normalized to the expression level of ornithine decarboxylase (ODC). The cycling conditions used were: 95°C for 5 minutes; then 40 cycles of 95°C for 15 seconds, 56°C for 15 seconds, 60°C for 30 seconds. The ΔΔCT method was used to calculate real-time PCR results. The primers used for RT-PCR analysis were Ornithine decarboxylase (ODC) [U 5′-CAG CTA GCT GTG GTG TGG-3′ D 5′-CAA CAT GGA AAC TCA CAC-3′]; Wnt8a [U 5′-TGA TGC CTT CAC TTC TGT GG-3′ D 5′-TCC TGC AGC TTC TTC TCT CC -3′]; BMP4 [U 5′-TGG TGG ATT AGT CTC GTG TCC -3′ D 5′-TCA ACC TCA GCA GCA TTC C -3′]; Noggin [U 5′-AGT TGC AGA TGT GGC TCT-3′ D 5′-AGT CCA AGA GTC TCA GCA -3′]; FGF8 [U 5′-TGG TGA CCG ACC AAC TAA GC D 5′-CGA TTA ACT TGG CGT GTG G ]; FGF2 [U 5′- AGA GGC TCT ACT GCA AGA ACG-3′ D 5′- TTC CTT CAT GGC AAG GTA GC-3′]; FGF4 [U 5′-GCA TGC CGT TCT CTT CTT CC -3′ D 5′-ACG TCG CAG TCT CTT GAT GC -3′]; FGFR1a [U 5′-GCG CAT TGG TGG ATA TAA GG -3′ D 5′- AGA CCG GCT TGT AGG ATT GG-3′]; FGFR1b [U 5′-GCG CAT TGG TGG ATA TAA GG -3′ D 5′-GAG ACC GGC TTG TAG GAT AGG -3′]; FGFR2 [U 5′- TCT GCA TGG TAG TGG TCT GC-3′ D 5′- CAG GAG TCG TGT TGT GAT CC-3′]; FGFR3 [U 5′- ACC AAG TGG TTC AAG GAT GG D 5′- TCG TCA TCC TCA TCA TCA CC]; FGFR4a [U 5′-ACA GTC AAG TTC CGC TGT CC -3′ D 5′-GCT GCC AAC TCT GTT CTC TAC C -3′]; and FGFR4b [U 5′-ACA CTG GAG CCT GGT AAT GG -3′ D 5′-GCT ACC TAC ACG TGC TGT GG -3′].
Morpholinos and plasmids
Cetn coding sequences were isolated from maternal RNA by RT-PCR and subcloned into pCS2 plasmids, following protocols used previously to isolate Cby coding sequences22; where indicated such constructs had N-terminal myc and C-terminal GFP sequences30. We also generated plasmids that encode Cetn-GFP chimeras that either perfectly matched or were maximally mismatched to their respective morpholinos. Plasmids encoding either N- or C-terminally tagged Cetn2-RFP were obtained from Sergie Sokol (Mount Sinai School of Medicine) and John Wallingford (U. Texas, Austin). Plasmids encoding FGF8 and a dominant-negative form of FGFR1 were supplied by Enrique Amaya (U. Manchester). Morpholinos against X. laevis centrins were designed and synthesized by Gene Tools. These included two non-overlapping morpholinos against Cetn-2a [MO1 5′CTTGTAGTTAGAAGCCATATCACAC 3′ and MO2 5′TGCACACACCAACCTTCGACCTCGC 3′], a Cetn-3l morpholino [5′CATCAGTCCTCACAGCCAGGCTCAT 3′] and a Cetn-4 morpholino [5′CTGGTTTACGCAGAACAGAGGCCAT 3′](supplemental figure. 2). In each case, a NIH-Blast search of the morpholino sequence revealed only a single hit in X. laevis, namely the targeted Cetn RNA. A plasmid encoding membrane-bound GFP, GFP-CAAX, was supplied by Kristen Kwan (U. Utah). Statistical analyses were based on values expressed as mean ± standard deviation and analyzed using the unpaired student’s t-test. p < 0.05 was considered as significant in all analyses.
Immunocytochemistry and imaging
Embryos were fixed and stained as described by Dent et al.31. The mouse monoclonal anti-acetylated α-tubulin antibody was used to visualized ciliated cells32. The rabbit anti-Xenopus Cetn antibody (anti-XlCetn) was supplied by Sergie Sokol20. The rabbit anti-human Cetn1 antibody (anti-HsCetn1) was purchased from Sigma. The anti-HsCetn1 antibody is directed against the C-terminal 15 amino acids of Cetn1; a similar sequence exists at the C-termini of X. laevis Cetn2 (13/15 identical) and Cetn4 proteins (12/15 identical), but is absent from the Cetn3 (5/15 identical)(data not shown). Notochord was visualized using the mouse monoclonal anti-keratin sulfate antibody MZ15 obtained from the Developmental Studies Hybridoma Bank33. Immunoperoxidase-stained explants were bleached before staining while immunofluorescently-labeled embryos were not. Fluorescent images were collected using a Zeiss 510 Confocal Laser Scanning Microscope.
Chromatin immunoprecipitation (ChIP) was performed following the protocol described in Blythe et al.34. Briefly, at stage 11 uninjected embryos, or embryos injected with GFP, CETN2-GFP, or CETN3-GFP RNAs were cross-linked with 1% formaldehyde for 30 minutes; cross-linking was stopped with a 10 min wash in 0.125M Glycine/PBS, followed by three washes in PBS. Samples were resuspended in RIPA buffer (50 mM Tris-HCl, pH 7.4, 1% NP-40 (Sigma I3021), 0.25% Na-Deoxycholate,150 mM NaCl, 1 mM EDTA, 0.1% SDS, 0.5 mM DTT, 5mM Na-Butyrate, Protease Inhibitor Cocktail (Sigma P8340), Phosphatase Inhibitor Cocktail I (SigmaP2850), Phosphatase Inhibitor Cocktail II (Sigma P5726). Chromatin was sonicated on ice to an average size of 200-500 base pairs using a Bioruptor (Diagenode) . Immunoprecipitation was performed using Dynabeads Protein G (Life Technologies) coupled to 2 μg GFP antibody (ICL, Inc) or Pol II antibody (Diagenode) at 4°C overnight. The bound chromatin was eluted and cross-links were reversed at 65°C overnight. ChIP DNA was extracted with phenol-chloroform and qPCR was performed. Below is a list of the primers used in ChIP studies. X. tropicalis CHIP primers: Fgf8 [primer 1 U 5′- TGA CTT TGC GCT CTG ACT TT-3′ D 5′- AAA AGA AAC AGC CGA GAT GC-3′]; [primer 2 U 5′- GCA TCT CGG CTG TTT CTT TT -3′ D 5′- GAT AGT GAT GGG GAG AGC CT -3′]; [primer 3 U 5′- CAGGCTCTCCCCATCACTAT -3′ D 5′- GAG TAG AAA CAC GCT GCA CT-3′]; [primer 4 U 5′- CCT CTC TTC CAG ACT CGG CT -3′ D 5′- GGA GTC GGA TTG CAG TGG AG-3′]; [primer 5 U 5′-TGA GCT ACA TCA CCT CCA TC-3′ D 5′-GAA GAG AAG GTC CAG TTA GCA -3′]. X. laevis CHIP primers: FGFR1a [primer 1 U 5′-ACA GAG TGG CAA TTA TAC AGA GG -3′ D 5′-CAC CTC ACA GCC ACA ATA CC -3′]; [primer 2 U 5′-GAG AGG CTG TGA GCA TAA TGG-3′ D 5′-TGC TAC TAT AGG CAC CAT CAC C-3′]; [primer 3 U 5′-GGA GAG AGA TGG TGC CTA TGG -3′ D 5′-TCT TCC TAC TAC ACT TGC TGT CC-3′]; [primer 4 U 5′-TGG TGC CTA TAG TAG CAG TGG -3′ D 5′-CTC CAG AGC ACA AGC ATG G-3′]; FGF8 [primer 1 U 5′-CAC TCA CAC TGT GTC TCT CAG G -3′ D 5′-CCG GCC AAT AAC ACT AGA AGC-3′]; [primer 2 U 5′-TCA GCT CAG ACA CAC CAA GC -3′ D 5′-TTC TCT CTC TCT CTC GCT TCC -3′]; [primer 3 U 5′- TCA GCT CAG ACA CAC CAA GC -3′ D 5′- CAA GGA GGC GAG TTA CTT CC -3′]; [primer 4 U 5′- AGT AAC TCG CCT CCT TGT CG -3′ D 5′- GCC TCT CAA GAG CAA GAT GC -3′]; [primer 5 U 5′- GAC AGT AGC GCA ACA CTC G -3′ D 5′- GCC TCT CAA GAG CAA GAT GC -3′]; BMP4a [primer 1 U 5′- TTG GCT GTC AAG AAT CAT GG -3′ D 5′- CAG CAG GAA GTA GCC AGA GC -3′]; [primer 2 U 5′- ACA CGG CTC TGG CTA CTT CC -3′ D 5′- AGC CTG GCC AAT GAA TGC -3′]; [primer 3 U 5′- GGA CAT ATC GCA GGC TAT CG -3′ D 5′- TCA GAT AGT CAC CGC CAT CC -3′]; [primer 4 U 5′- GAG ACG CTC TCA GTC AGA TTA GC -3′ D 5′- CAA GGA CAG TTC CAC AGA GG -3′].
Note added in proof
Recently, human centrin 2 has been shown to regulate primary cilia formation through controlling CP11035.
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We thank Nick Galati with help with confocal imaging, Sergei Sokol for anti-centrin antibody; plasmids were obtained from Sergie Sokol, John Wallingford, Kris Kwon, Enrique Amaya and Richard Harland. The work was supported by NIH grant GM74746 (and supplement) to MW and in part through GM84133 to MWK.
The authors declare no competing financial interests.
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Shi, J., Zhao, Y., Vonderfecht, T. et al. Centrin-2 (Cetn2) mediated regulation of FGF/FGFR gene expression in Xenopus. Sci Rep 5, 10283 (2015). https://doi.org/10.1038/srep10283
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