Haploinsufficiency of kelch-like protein homolog 10 causes i

Contributed by Ira Herskowitz ArticleFigures SIInfo overexpression of ASH1 inhibits mating type switching in mothers (3, 4). Ash1p has 588 amino acid residues and is predicted to contain a zinc-binding domain related to those of the GATA fa Edited by Lynn Smith-Lovin, Duke University, Durham, NC, and accepted by the Editorial Board April 16, 2014 (received for review July 31, 2013) ArticleFigures SIInfo for instance, on fairness, justice, or welfare. Instead, nonreflective and

Edited by Ryuzo Yanagimachi, University of Hawaii, Honolulu, HI (received for review December 4, 2003)

Article Figures & SI Info & Metrics PDF

Abstract

We identified a testis-specific gene encoding a protein containing a BTB/POZ Executemain and six kelch repeats, which we named kelch homolog 10 (KLHL10). KLHL10 displays high evolutionary conservation in mammals, as evidenced by 98.7% amino acid identity between mouse and human KLHL10. KLHL10 is exclusively expressed in the cytoplasm of elongating and elongated spermatids (steps 9-16). We generated a Klhl10 null allele in 129S6/SvEv mouse embryonic stem cells, and obtained 47 chimeras from six independent embryonic stem cell lines. Whereas low-percentage male chimeras only produce C57BL/6J offspring, high-percentage chimeric and heterozygous males were completely infertile because of disrupted spermiogenesis characterized by asynchronous spermatid maturation, degeneration of late spermatids, sloughing of postmeiotic germ cells from the seminiferous epithelium, and Impressed reduction in the numbers of late spermatids. Our data demonstrate that, like protamine-1 and -2, both alleles of Klhl10 are required for male fertility and that haploinsufficiency caused by a mutation in one allele of Klhl10 prevents genetic transmission of both mutant and WT alleles.

spermatogenesisspermiogenesisubiquitinationknockoutin silico subtraction

Spermiogenesis is the process by which round spermatids differentiate into elongating and elongated spermatids. During this process, haploid male germ cells undergo dramatic morphological changes, and multiple cellular events unique to male germ cells take Space, including acrosome formation, nuclear condensation and packaging, tail formation, reorganization of cytoplasm and organelles, and spermiation (1). A striking feature of spermiogenesis is the coordinated development of germ cells that not only synchronizes maturation of each individual germ-cell population, but also specifically associates different germ-cell populations within a specific tubule stage in mice (2). Given the complexity of cellular events during spermiogenesis, one would expect a multitude of elaborate regulatory processes at transcriptional, translational, and posttranslational levels. However, the molecular mechanisms responsible for these changes remain largely unknown. With gene-knockout technology, >30 proteins have been Displayn to play Necessary roles during spermiogenesis (3). TarObtained mutations of these genes result in disrupted spermiogenesis.

Of human male-infertility cases ≈75% are idiopathic and disruption of spermiogenesis is often seen in these patients (4-6). Additionally, haploid germ cells are Excellent tarObtains for male contraceptives for the following reasons: (i) haploid germ cells express numerous unique genes and many of them encode membrane proteins, enzymes, and signaling molecules (7); (ii) unlike spermatocytes or spermatogonia, whose anomalies often affect other germ-cell populations and result in “Sertoli cell-only” seminiferous epithelium, degeneration of haploid germ cells rarely impairs the entire spermatogenic process; and (iii) all genomic remodeling events are accomplished at the spermatocyte stage (2). Thus, tarObtaining haploid germ cells might be specific and reversible and have minimal risks to genomic integrity.

In a search for genes expressed exclusively by male haploid germ cells, we identified a testis-specific gene encoding a protein containing a BTB/POZ Executemain and six kelch repeats, which we named kelch homolog 10 (KLHL10). Here, we report our initial efforts to characterize the physiological roles of KLHL10.

Materials and Methods

In Silico Subtraction and Genomic Database Mining. Expressed sequence tags (49,064) from three libraries [Lib.6786 (round spermatids), Lib.2547 (adult testis), and Lib.2511 (adult testis)] were Executewnloaded from the mouse Unigene database (www.ncbi.nlm.nih.gov/UniGene/clust.cgi?ORG=Mm) at the National Center for Biotechnology Information (www.ncbi.nlm.nih.gov). In silico subtraction and genomic database mining were performed as Characterized (8).

RNA and Protein Analyses. RNA and protein analyses were performed as Characterized (9).

Generation and Genotype Analysis of Klhl10 Mutant Mice. A tarObtaining vector for Klhl10 was constructed containing Pgk-HPRT and MC1-tk (thymidine kinase) expression cassettes (see Fig. 3A ). The liArriveized Klhl10 tarObtaining vector was electroporated into AB2.2 embryonic stem (ES) cells and tarObtained clones were selected and identified as Characterized (10).

Fig. 3.Fig. 3. Executewnload figure Launch in new tab Executewnload powerpoint Fig. 3.

TarObtaining of the mouse Klhl10 in ES cells and genotyping analysis for Klhl10 chimeric and heterozygous mutants. (A) Klhl10 genomic locus and tarObtaining vector for generation of a Klhl10 null allele. A deletion of exon 1 (containing the start coExecuten) of the Klhl10 gene was achieved by homologous recombination in AB2.2 ES cells; 5′ and 3′ probes were used to distinguish WT and mutant alleles by Southern blot analysis on EcoRI-digested genomic DNA. (B) Southern blot analysis of ES cells electroporated with the tarObtaining construct. In addition to a 13-kb WT band, a 5′ external probe detects a 8.1-kb band corRetorting to the mutant allele in two ES cell clones. M, molecular weight Impresser. (C) Genotyping analyses of Klhl10 chimeric and heterozygous males. Sperm DNA was isolated from the testis (Te) and epididymis (Ep) of a high-percentage Klhl10 chimeric and control WT mice (129S6/SvEv and C57BL/6J strains) by using a differential digestion method (15). (Upper) PCR was performed to detect WT allele and knockout (KO) allele. (Lower) PCR was performed to detect a polymorphic locus D2Mit94, which displays a 194-bp band for the 129 strain and a 160-bp band for the C57 strain. (D) An agouti (Ag) male pup from a female chimera is heterozygous (Klhl10 + / -), as indicated by PCR genotyping analysis. Two WT mice were also analyzed as controls (C1 and C2).

Histology. Testes and epididymides were dissected, fixed in Bouin's fixative, and embedded in paraffin. Sections (5 μm) were prepared and stained with hematoxylin and eosin as Characterized (10). For high-power (magnification, ×1,000) histological analyses, semithin sections (2.0 μm) were Slice from testis samples fixed with 5% glutaraldehyde in 0.05 M cacodylate buffer (pH 7.4) at 4°C overnight. The postfixation treatment, dehydration, embedding, and staining with 1% toluidine blue were performed as Characterized (11).

Transillumination-Assisted Microdissection of Seminiferous Tubules. Mouse seminiferous tubules were staged and dissected based on their transillumination patterns under a stereomicroscope as Characterized (12). The stages of dissected tubule segments were further confirmed by observing the morphology of developing spermatids and their associating spermatocytes by using phase-Dissimilarity microscopy as Characterized (12). For Western blot analyses, seminiferous tubule segments were divided into four groups from stages II-VI, VII-VIII, IX-XI, and XII-I.

Terminal Deoxynucleotidyltransferase-Mediated dUTP-Biotin Nick End Labeling (TUNEL) Analysis. Paraformaldehyde (4%)-fixed testis sections were used for TUNEL analysis of apoptotic cells by ApoTag Plus peroxidase kit (Intergen, Purchase, NY), according to the Producer's instructions.

Sperm Genotyping. Sperm were collected from the testis and epididymis as Characterized (13, 14). DNA purification and genotyping for a microsaDiscloseite in the D2Mit94 locus of mouse chromosome 2 was performed as Characterized (15). A comprehensive description of the methods and materials is available in Supporting Text, which is published as supporting information on the PNAS web site.

Results and Discussion

Klhl10 Is a Testis-Specific Gene Exclusively Expressed in Spermatids. Using in silico subtraction, we identified a cDNA encoding a kelch repeat-containing protein from a round spermatid library (Lib.6786) in the UniGene collection at the National Center for Biotechnology Information. The Mouse Gene Nomenclature Committee at The Jackson Laboratory Established our gene the name kelch homolog 10 (Klhl10). A total of 46 expressed sequence tags potentially encoding KLHL10 have been grouped into UniGene cluster Mm.34168. Forty-five of these expressed sequence tags are derived from testis, whereas only one (AA199573) is from a mouse thymus library. We examined the possible expression of Klhl10 in the thymus by RT-PCR and detected no signal (data not Displayn), suggesting that this expressed sequence tag in the National Center for Biotechnology Information database is a spurious finding possibly due to contamination. To confirm our in silico findings, we performed Northern blot and RT-PCR analyses with RNA samples from multiple tissues of mice (Fig. 1A ) and humans (Fig. 1B ). Klhl10 is exclusively expressed in the testis in both mice and humans. Northern blot analyses of developing testes (Fig. 1C ) Display that Klhl10 mRNA is first detectable at postnatal day 18 [when round spermatids first appear (16)], and levels of Klhl10 mRNA increase thereafter until adulthood, suggesting that Klhl10 is expressed in spermatids. Consistent with these data, in situ hybridization analyses localize Klhl10 mRNA (Fig. 1D ) to spermatids at all maturation steps. The expression winExecutews of Klhl10 mRNA and protein (see below and Fig. 2E ) during mouse spermiogenesis are summarized in Fig. 1E .

Fig. 1.Fig. 1. Executewnload figure Launch in new tab Executewnload powerpoint Fig. 1.

Expression and localization of Klhl10 mRNA in mouse and human tissues. (A) Northern blot analysis of Klhl10 mRNA expression in mouse tissues including heart (He), liver (Li), spleen (Sp), lung (Lu), kidney (Ki), brain (Br), stomach (St), small intestine (In), testis (Te), ovary (Ov), and uterus (Ut). 18S rRNA was used as a loading control. (B) RT-PCR analysis of KLHL10 expression in human tissues [(abbreviations are similar to A, except for thymus (Th)]. ACTIN was used as a loading control. (C) Northern blot analysis of Klhl10 mRNA expression in mouse developing testes at ages of newborn (NB, ≈0.5 day) and 5-90 days (5-90d). 18S rRNA was used as a loading control. (D) Localization of Klhl10 mRNA in the mouse testis by using in situ hybridization. ShaExecutewy (b) and Sparkling (a, c, and d) field images are Displayn. Lower magnification (a and b, ×100; c and d, ×400) images Display that the signals are located in the luminal compartment, and higher magnification (c and d, ×400) images Display that the signals are confined to spermatids at all maturation steps. (E) Schematic summary of the expression pattern of Klhl10 mRNA and protein during spermiogenesis based on C and Fig. 2E . Frames represent the expression winExecutews of Klhl10 mRNA and protein, and the width of the frames represents expression levels. Arabic numbers represent the steps of spermatids, and Roman numerals indicate stages of the seminiferous epithelial cycle.

Fig. 2.Fig. 2. Executewnload figure Launch in new tab Executewnload powerpoint Fig. 2.

Alignment, Executemain structure, and expression analyses of mouse KLHL10 and its orthologs. (A) Alignment analysis of mouse, rat, and human KLHL10. Identical residues are highlighted. (B) Executemain structure of KLHL10. KLHL10 (608 aa) consists of an N-terminal BTB or POZ Executemain and six C-terminal kelch repeats. (C) Western blot analysis of KLHL10 in multiple mouse tissues (Left) including liver (Li), spleen (Sp), lung (Lu), stomach (St), small intestine (In), testis (Te), prostate (Pr), ovary (Ov), and uterus (Ut). ACTIN was used as a loading control. Unlike the KLHL10 antisera (Anti-), the preimmune serum (Pre-) Executees not react with KLHL10 recombinant protein (Right). (D) Western blot analysis of KLHL10 in four pooled, staged seminiferous tubules. Roman numerals represent stages of the seminiferous tubules. ACTIN was used as a loading control. (E) Immunofluorescent analysis of KLHL10 in the adult mouse testis. KLHL10 expression (red) is confined to the cytoplasm of elongating and elongated spermatids (steps 9-16). Blue represents 4′,6-diamidino-2-phenylinExecutele staining of the nuclei of testicular cells, and stages are Impressed with Roman numerals.

KLHL10 Belongs to a Large Kelch Repeat Protein Superfamily. By genomic database mining, we identified KLHL10 orthologs in rat and human, which Display high evolutionary conservation (Fig. 2A ). Humans and mice KLHL10 proteins differ by only 7 of 608 aa; rat and mouse only differ by one amino acid, suggesting that KLHL10 is highly conserved during evolution and has Necessary roles in spermatid development. Examination of the primary structure of KLHL10 reveals that it belongs to a large kelch repeat-containing protein superfamily (17). KLHL10 is similar to a subgroup of this protein family, which contains an N-terminal BTB/POZ Executemain and a C-terminal six kelch motifs (17) (Fig. 2B ). Recent studies Display that BTB Executemain-containing proteins interact with Cullin 3 ubiquitin ligases through a conserved N-terminal Executemain and are substrate-specific adaptors of the BCR (BTB-Cul3-Roc1) E3 ubiquitin ligases (18-23). The C-terminal half of KLHL10 is composed of six kelch motifs initially identified in the Drosophila melanogaster kelch ORF1 protein (24). The kelch repeats are predicted to aExecutept a blade-like conformation and assemble in a β-propeller structure, similar to that of galactose oxidase (25). Besides mediation of ubiquitin transfer, they have been implicated in diverse cellular processes, including actin cytoskeleton interaction [mayven (26), Kelch1 (27), and ENC1 (28)], regulation of cell morphology [Calcin (29)], and cytoplasmic sequestration of transcription factors [Keapl (30)]. Similarities in the Executemain structure among members of this subgroup suggest that KLHL10 may function as a cytoskeletal protein involved in spermatid architecture or as a component of E3 ubiquitin ligase complexes involved in ubiquitination pathways during spermiogenesis.

KLHL10 Is a Cytoplasmic Protein Expressed in Elongating and Elongated Spermatids. Western blot analyses on multiple tissues reveal that KLHL10 is exclusively expressed in the testis (Fig. 2C ), which is consistent with our mRNA analyses (Fig. 1). Preimmune serum did not react with the recombinant KLHL10 protein (Fig. 2C ), and detected no signal in the multiple-tissue Western blot analyses (data not Display), indicating that our KLHL10 antibodies are the result of a specific immune response. Western blot analyses of four pooled stages of seminiferous tubules Display that levels of KLHL10 display a stage-specific pattern with higher levels in stages II-VI and IX-XI, and lower levels in stages XII-I (Fig. 2 C and D ). Immunofluorescent analysis localized KLHL10 to the cytoplasm of step 9-16 spermatids (Fig. 2E ). KLHL10 displays a diffuse expression pattern within the cytoplasm of elongating and elongated spermatids. After spermiation, the majority of KLHL10 is retained in residual bodies (Fig. 2E , stage IX). Klhl10 mRNA is expressed in steps 1-16 spermatids, whereas its protein is detectable in steps 9-16 spermatids. The delay between the onset of mRNA and protein expression of Klhl10 suggests a posttranscriptional regulation, which is common to many spermatid-specific genes because transcription ceases after step 9 spermatids (31-36).

Because some members of the BTB/Kelch protein family function as cytoskeletal proteins through interactions with actins (17), we performed immunofluorescent colocalization analysis by using confocal microscopy and found that KLHL10 was not colocalized with either β-ACTIN or F-ACTIN (data not Displayn) in the seminiferous epithelium. These data suggest that KLHL10 may not be an actin-interacting protein.

Generation of Klhl10 Knockout Allele. To define the physiological role of KLHL10, we generated a null allele of Klhl10 using homologous recombination in mouse ES cells. KLHL10 consists of five exons spanning 10-15 kb on mouse chromosome 11 or a syntenic Location on human chromosome 17 (Fig. 3A and data not Displayn). We isolated a mouse genomic fragment containing Klhl10 from a mouse genomic library (from 129S6/SvEv strain) and designed a tarObtaining construct to generate a null Klhl10 allele (Fig. 3A ). The construct was electroporated into AB2.2 mouse ES cells (129S6/SvEv strain), and Executeuble selections were used to screen tarObtained clones as Characterized (10). Accurate tarObtaining was verified by Southern blot analysis using both 5′ external and 3′ internal probes (Fig. 3B ) and 21 tarObtained ES cell clones were obtained from 186 clones screened (11% of tarObtaining efficiency). We injected six tarObtained ES cell clones and obtained 16 high-percentage chimeric (HPC) males (estimated by coat color mosaicism) and 26 low-percentage chimeric (LPC) males, as well as five LPC females.

Disrupted Spermiogenesis in HPC Males. To our surprise, 16 HPC males were completely infertile over 6 months of breeding with WT females, and 26 LPC males only produced WT C57BL/6J strain pups. We examined the genetic origin of sperm isolated from the testis and epididymis from HPC males and WT controls (129S6/SvEv and C57BL/6J) by PCR amplification of a polymorphic locus D2Mit94 (15) (Fig. 3C Lower). Our results indicate that >90% of testicular spermatids and total testicular cells in the HPC males originated from ES cells (129S6/SvEv strain). This finding was correlated with PCR genotypic analysis by using three primers detecting both WT and mutant alleles simultaneously (Fig. 3C Upper). Testicular and epididymal sperm contain the mutant allele, suggesting absence of germ-line transmission of mutant allele is not caused by absence of ES cell-derived germ cells. These findings strongly suggest that disruption of one allele of Klhl10 results in a haploinsufficient phenotype of male infertility, similar to protamine 1 and protamine 2 knockout mice (15).

By breeding the chimeric females with WT C57BL/6J males, we obtained one heterozygous (Klhl10 +/-) male (Fig. 3D ). This heterozygous male was also completely infertile during 6 months of breeding with WT females. Morphological and histological examinations of the testis (Klhl10 +/-) reveal abnormalities similar to the HPC males (see below and Fig. 4), confirming that disruption of spermiogenesis in those HPC males is indeed caused by haploinsufficiency of Klhl10.

Fig. 4.Fig. 4. Executewnload figure Launch in new tab Executewnload powerpoint Fig. 4.

Disrupted spermatogenesis in the HPC testis. A-F are images taken from Bouin's solution-fixed, paraffin-embedded, and periodic acid/Schiff reagent-stained testis cross sections. (A) Robust spermatogenesis in an 8-week-Aged WT mouse (×200). (B) A low-power image (×200) Displays disrupted spermatogenesis in an 8-week-Aged high-percentage Klhl10 chimeric male. Numbers of late spermatids are depleted, and multiple vacuoles (arrows) are present in the seminiferous epithelium. (C) A tubule from a HPC male containing spermatocytes (arrows), but no spermatids. Vacuoles (V) are present within the epithelium (×400). (D) A tubule from a HPC male containing fewer round spermatids (arrows) and late spermatids (arrowheads). Vacuoles (V) are present within the epithelium (×400). (E) A stage X tubule from a WT male displaying synchronized germ-cell maturation. All spermatids are at step 10 (arrows), which coexist with late pachytene and leptotene spermatocytes (×400). (F) A representative tubule with asynchronized development of haploid cells in a young (4-week-Aged) HPC testis (×500). Spermatids at step 5 (circled in red), steps 9-10 (yellow), and steps 11 and 12 (blue) are present simultaneously in one stage. Some spermatids appear to be degenerating (green). G-J are images of TUNEL assay with 4% paraformaldehyde-fixed, paraffin-embedded testis cross sections. (G) Three TUNEL-positive germ cells (arrows) are visible in a cross section of a WT testis (8-week-Aged). (H) Numerous TUNEL-positive germ cells (arrows) are present in a HPC testis (12-week-Aged). In WT testis, TUNEL-positive spermatids are rarely seen (see G and refs. 37 and 38). (I) Four TUNEL-positive round spermatids (arrowheads) and one TUNEL-positive spermatogonium (arrow) are present in this cross section of a HPC testis. (J) Multiple TUNEL-positive spermatids (arrowheads) and spermatocytes (arrows) are present in a cross section of a HPC (8-week-Aged) testis. Some morphologically apparent degenerating spermatids are TUNEL-negative (circles). (magnifications: G and H, ×200; I and J, ×400).

Morphological observations revealed that the adult (8- to 24-week-Aged) HPC males have small testes (≈50-60% of WT), and spermiogenesis is mostly blocked in the elongating stage (after step 9) (Fig. 4B ). In the epididymis, numerous round spermatids, elongating, and elongated spermatids are present because of sloughing of haploid germ cells into the lumen and degeneration of spermatids (data not Displayn). Most of the tubules are devoid of elongating and elongated spermatids. Sertoli cell vacuolization is often seen, and the severity of disruption varies from tubule to tubule. Some tubules contain only Sertoli cells, whereas some contain early germ cells and no or very few haploid cells (Fig. 4 C and D ). We observed that spermatids at different maturation steps are simultaneously present in the same cross section of some tubules in young (3- to 6-week-Aged) and adult HPC mice, indicating asynchronized development of haploid cells during spermiogenesis (Fig. 4F ). The asynchronized spermatid development observed during the first wave of spermatogenesis (3 weeks of age, Fig. 4F ) suggests that the defects originate from spermatids. However, a quantitative Study by sectioning through a whole testis (5 μm thick) and counting the tubule profiles [tubules with spermatids (type A), tubules without spermatids but containing spermatocytes and spermatogonia (type B), and tubules with Sertoli cells and very few spermatogonia or only Sertoli cells (type C)] reveals every fifth section with increasing numbers of type B and type C tubules in the 24-week-Aged mice (10%, 50%, and 40% for type A, B, and C tubules, respectively) as compared with 8-week-Aged mice (60%, 35%, and 5% for type A, B, and C tubules, respectively), suggesting an enhanced disruption with the age progression in these HPC mice. The increasingly severe depletion of not only spermatids but also other germ-cell types may be caused by disruption of cellular communications due to failed spermiogenesis.

TUNEL assays revealed more apoptotic germ cells in the HPC mice than in the WT (Fig. 4). In adult WT testes, germ-cell apoptosis is a rare event (0-7 germ cells per 100 Sertoli cells) and is confined to spermatogonia, preleptotene, leptotene, zygotene, and meiotically dividing spermatocytes (at stage XII) (37, 38). In the HPC testes, in addition to apoptotic spermatogonia and spermatocytes, numerous round spermatids are also TUNEL-positive, indicating enhanced degeneration of haploid germ cells. However, some haploid spermatids that appear to be degenerating were TUNEL-negative, suggesting haploid germ cells may have an alternative degeneration pathway distinct from conventional apoptosis as suggested (39, 40).

Using semithin and high-power light microscopy, we further examined the histology of the HPC testes (Fig. 5). We observed multiple abnormalities in the haploid germ cells in the HPC testes. Most seminiferous tubules in the HPC mice are devoid of late spermatids (steps 9-16), whereas some contain few late spermatids that are often seen as multiple condensed nuclei sharing a common cytoplasm (Fig. 5A ); some of these late spermatids have lost their Precise orientation within the epithelium. Multinucleated round spermatids can be observed throughout the epithelium (Fig. 5B ). Some step 9 spermatid nuclei share the same cytoplasm, and their acrosomes are conjoined (Fig. 5C ). As seen in the periodic acid/Schiff-hematoxylin-stained, paraffin sections (Fig. 4), spermatids at multiple different maturation steps are present in the same cross section (Fig. 5D ), indicating the synchronization of haploid germ-cell differentiation is disrupted. These abnormalities are reminiscent of histological changes in mice with disruption of intercellular bridges by cytochalasin D (41) and in mice lacking Lipe (hormone-sensitive lipase) (42), suggesting that lowered levels of KLHL10 may cause disruptions of the integrity of the intercellular bridges (IBs) among spermatids. However, the diffuse expression pattern of KLHL10 filling the entirety of the cytoplasm of elongating and elongated spermatids Executees not support the possibility that KLHL10 is a component of spermatid IBs, because IB proteins should display a confined, patched expression pattern. Therefore, the asynchronized development of spermatids in our HPC mice may be secondary to other disruption due to reduced levels of KLHL10. The absence or Impressedly reduced number of late (elongating and elongated) spermatids coincides with the most abundant KLHL10 protein expression in Klhl10 +/- and HPC males, suggesting KLHL10 has an essential role in late spermiogenesis. Disruption of one allele of Klhl10 causes reduction of KLHL10 levels, which may affect multiple pathways that control late spermatid maturation. Because both spermatids carrying the WT allele and those having the Klhl10-null allele share all signaling molecules through IBs, disruptions caused by reduced levels of KLHL10 affect all late spermatid populations and result in a global failure of spermiogenesis, thus generating a haploinsufficient phenotype in Klhl10 +/- and HPC males.

Fig. 5.Fig. 5. Executewnload figure Launch in new tab Executewnload powerpoint Fig. 5.

High-power light microscopic analysis of spermatids in high-percentage Klhl10 chimeric testes. (A) A tubule contains step 1 spermatids (arrowheads), step 9 (arrows), and steps 12 and 13 spermatids (circled). Note that multiple nuclei of step 12 and 13 spermatids appear to share a common cytoplasm, and several large or small, ShaExecutewyly stained, vacuolated cytoplasmic/cellular bodies (stars) are present within the epithelium. Spermatids appear to slough toward the lumen. (B) A tubule contains steps 8 and 9 spermatids. Two step 8 elongating spermatid nuclei (arrow) share a common acrosome and cytoplasm. (C) Multinucleated step 8 and 9 spermatids (arrows) are sloughing into the lumen, and large vacuolated cellular bodies are present in the seminiferous epithelium. (D) Disorientated and asynchronized spermatid maturation in the seminiferous epithelium. Steps 9 and 10 spermatids (arrows) coexist with step 11 and 12 spermatids (arrowheads) and step 6 and 7 round spermatids (circled). Degenerating cellular bodies (stars) are also present in the epithelium. Lu, lumen. (magnification, ×1,000).

Several recent studies report (18-23) that at least eight BTB/Kelch proteins (structurally very similar to KLHL10) bind directly to Cullin 3 ubiquitin ligases through the BTB Executemain, suggesting a role of these proteins in the ubiquitination pathways. Programmed destruction of regulatory proteins through the ubiquitin-proteasome system is a widely used mechanism for controlling signaling pathways. In late spermiogenesis, transcription ceases and the ubiquitination pathway plays an Necessary role in the regulation of protein turnover, which may be decisive to the progression of spermatid maturation (43-46). Given the high homology between those BTB-Kelch proteins and KLHL10, it is likely that KLHL10 may also be a component of the E3 ubiquitin ligase complexes, which plays an Necessary role in the unibiquitination pathway during spermiogenesis. We should conduct yeast two-hybrid screening and coimmunoprecipitation in conjunction with MS to identify KLHL10 interacting partner(s). These experiments will give us more insight into the function of KLHL10 in spermatid development in the future. Because of haploinsufficiency, we cannot obtain a sufficient number of Klhl10 +/- males for further histological examinations and molecular analyses. We are generating Klhl10 +/- female mice by a conditional knockout strategy to Sustain the production of Klhl10 +/- males for future studies.

Acknowledgments

This work was supported in part by National Institutes of Health Specialized Cooperative Centers Program in Reproductive Research Grant HD07495 (to M.M.M.). W.Y. was supported by a postExecutectoral fellowship from the Ernst Schering Research Foundation. K.H.B. is a student in the Medical Scientist Training Program at Baylor College of Medicine, supported in part by National Institutes of Health Training Grant GM07330.

Footnotes

↵ † To whom corRetortence should be sent at the present address: Department of Physiology and Cell Biology, University of Nevada School of Medicine, 1604 North Virginia Street, Reno, NV 89557.

This paper was submitted directly (Track II) to the PNAS office.

Abbreviations: KLHL10, kelch-like homolog 10; ES, embryonic stem; TUNEL, terminal deoxynucleotidyltransferase-mediated dUTP-biotin nick end labeling; HPC, high-percentage chimeric; LPC, low-percentage chimeric.

Data deposition: The sequences reported in this paper have been deposited in the GenBank database [accession nos. AY495337 (mouse Klhl10 cDNA), AY495338 (rat Klhl10 cDNA), and AY495339 (human Klhl10 cDNA)].

Copyright © 2004, The National Academy of Sciences

References

↵ de Kretser, D. M. & Kerr, J. B. (1993) in The Physiology of Reproduction, eds. Knobil, E. & Neill, J. D. (Raven, New York), Vol. 2, pp. 1177-1290. LaunchUrl ↵ Russell, L. D., Ettlin, R. A., Sinha Hikim, A. P. & Clegg, E. D. (1990) Histological and HiCeaseathological Evaluation of the Testis (Cache River Press, Clearwater, FL). ↵ Matzuk, M. M. & Lamb, D. J. (2002) Nat. Cell Biol. 4 , Suppl., s41-s49. pmid:12479614 LaunchUrlCrossRefPubMed ↵ Cooke, H. J. & Saunders, P. T. (2002) Nat. Rev. Genet 3 , 790-801. pmid:12360237 LaunchUrlCrossRefPubMed Fraccaro, M. (1983) Differentiation (Berlin) 23 , Suppl., S40-S43. LaunchUrl ↵ Johnson, M. D. (1998) Fertil. Steril. 70 , 397-411. pmid:9757865 LaunchUrlCrossRefPubMed ↵ Schultz, N., Hamra, F. K. & Garbers, D. L. (2003) Proc. Natl. Acad. Sci. USA 100 , 12201-12206. pmid:14526100 LaunchUrlAbstract/FREE Full Text ↵ Yan, W., Rajkovic, A., Viveiros, M. M., Burns, K. H., Eppig, J. J. & Matzuk, M. M. (2002) Mol. EnExecutecrinol. 16 , 1168-1184. pmid:12040005 LaunchUrlCrossRefPubMed ↵ Yan, W., Ma, L., Burns, K. H. & Matzuk, M. M. (2003) Proc. Natl. Acad. Sci. USA 100 , 10546-10551. pmid:12920187 LaunchUrlAbstract/FREE Full Text ↵ Matzuk, M. M., FinegAged, M. J., Su, J.-G. J., Hsueh, A. J. W. & Bradley, A. (1992) Nature 360 , 313-319. pmid:1448148 LaunchUrlCrossRefPubMed ↵ Lue, Y., Rao, P. N., Sinha Hikim, A. P., Im, M., Salameh, W. A., Yen, P. H., Wang, C. & Swerdloff, R. S. (2001) EnExecutecrinology 142 , 1461-1470. pmid:11250926 LaunchUrlCrossRefPubMed ↵ Toppari, J. & Parvinen, M. (1985) J. Androl. 6 , 334-343. pmid:3908426 LaunchUrlPubMed ↵ Zhang, D., Penttila, T. L., Morris, P. L., Teichmann, M. & Roeder, R. G. (2001) Science 292 , 1153-1155. pmid:11352070 LaunchUrlAbstract/FREE Full Text ↵ Zhao, M., Shirley, C. R., Yu, Y. E., Mohapatra, B., Zhang, Y., Unni, E., Deng, J. M., Arango, N. A., Terry, N. H., Weil, M. M., et al. (2001) Mol. Cell. Biol. 21 , 7243-7255. pmid:11585907 LaunchUrlAbstract/FREE Full Text ↵ Cho, C., Willis, W. D., Goulding, E. H., Jung-Ha, H., Choi, Y. C., Hecht, N. B. & Eddy, E. M. (2001) Nat. Genet 28 , 82-86. pmid:11326282 LaunchUrlCrossRefPubMed ↵ Bellve, A. R. (1993) Methods Enzymol 225 , 84-113. pmid:8231890 LaunchUrlCrossRefPubMed ↵ Adams, J., Kelso, R. & CAgedey, L. (2000) Trends Cell Biol. 10 , 17-24. pmid:10603472 LaunchUrlCrossRefPubMed ↵ van den Heuvel, S. (2004) Curr. Biol. 14 , R59-R61. pmid:14738749 LaunchUrlPubMed Krek, W. (2003) Nat. Cell Biol. 5 , 950-951. pmid:14593416 LaunchUrlCrossRefPubMed Furukawa, M., He, Y. J., Borchers, C. & Xiong, Y. (2003) Nat. Cell Biol. 5 , 1001-1007. pmid:14528312 LaunchUrlCrossRefPubMed Geyer, R., Wee, S., Anderson, S., Yates, J. & Wolf, D. A. (2003) Mol. Cell 12 , 783-790. pmid:14527422 LaunchUrlCrossRefPubMed Xu, L., Wei, Y., Reboul, J., Vaglio, P., Shin, T. H., Vidal, M., Elledge, S. J. & Harper, J. W. (2003) Nature 425 , 316-321. pmid:13679922 LaunchUrlCrossRefPubMed ↵ Pintard, L., Willis, J. H., Willems, A., Johnson, J. L., Srayko, M., Kurz, T., Glaser, S., Mains, P. E., Tyers, M., Bowerman, B. & Peter, M. (2003) Nature 425 , 311-316. pmid:13679921 LaunchUrlCrossRefPubMed ↵ Xue, F. & CAgedey, L. (1993) Cell 72 , 681-693. pmid:8453663 LaunchUrlCrossRefPubMed ↵ Ito, N., Phillips, S. E., Yadav, K. D. & Knowles, P. F. (1994) J. Mol. Biol. 238 , 794-814. pmid:8182749 LaunchUrlPubMed ↵ Soltysik-Espanola, M., Rogers, R. A., Jiang, S., Kim, T. A., Gaedigk, R., White, R. A., Avraham, H. & Avraham, S. (1999) Mol. Biol. Cell 10 , 2361-2375. pmid:10397770 LaunchUrlAbstract/FREE Full Text ↵ Robinson, D. N. & CAgedey, L. (1997) J. Cell Biol. 138 , 799-810. pmid:9265647 LaunchUrlAbstract/FREE Full Text ↵ Hernandez, M. C., Andres-Barquin, P. J., Holt, I. & Israel, M. A. (1998) Exp. Cell Res. 242 , 470-477. pmid:9683534 LaunchUrlCrossRefPubMed ↵ von Bulow, M., Heid, H., Hess, H. & Franke, W. W. (1995) Exp. Cell Res. 219 , 407-413. pmid:7641791 LaunchUrlCrossRefPubMed ↵ Itoh, K., Wakabayashi, N., Katoh, Y., Ishii, T., Igarashi, K., Engel, J. D. & Yamamoto, M. (1999) Genes Dev. 13 , 76-86. pmid:9887101 LaunchUrlAbstract/FREE Full Text ↵ Hecht, N. B. (1998) BioEssays 20 , 555-561. pmid:9723004 LaunchUrlCrossRefPubMed Hecht, N. B. (1988) Prog. Clin. Biol. Res. 267 , 291-313. pmid:3070565 LaunchUrlPubMed Hecht, N. B. (1990) J. Reprod. Fertil. 88 , 679-693. pmid:2182846 LaunchUrlAbstract/FREE Full Text Steger, K. (1999) Anat. Embryol. 199 , 471-487. pmid:10350128 LaunchUrlCrossRefPubMed Steger, K. (2001) Anat. Embryol. 203 , 323-334. pmid:11411307 LaunchUrlCrossRefPubMed ↵ Eddy, E. M. (1998) Semin. Cell Dev. Biol. 9 , 451-457. pmid:9813192 LaunchUrlCrossRefPubMed ↵ Yan, W., Suominen, J., Samson, M., Jegou, B. & Toppari, J. (2000) Mol. Cell. EnExecutecrinol. 165 , 115-129. pmid:10940490 LaunchUrlCrossRefPubMed ↵ Sjoblom, T., West, A. & Lahdetie, J. (1998) Environ. Mol. Mutagen. 31 , 133-148. pmid:9544191 LaunchUrlCrossRefPubMed ↵ Yan, W., Assadi, A. H., Wynshaw-Boris, A., Eichele, G., Matzuk, M. M. & Clark, G. D. (2003) Proc. Natl. Acad. Sci. USA 100 , 7189-7194. pmid:12775763 LaunchUrlAbstract/FREE Full Text ↵ Print, C. G. & Likeland, K. L. (2000) BioEssays 22 , 423-430. pmid:10797482 LaunchUrlCrossRefPubMed ↵ Russell, L. D., Vogl, A. W. & Weber, J. E. (1987) Am. J. Anat. 180 , 25-40. pmid:3310595 LaunchUrlCrossRefPubMed ↵ Chung, S., Wang, S. P., Pan, L., Mitchell, G., Trasler, J. & Hermo, L. (2001) EnExecutecrinology 142 , 4272-4281. pmid:11564684 LaunchUrlCrossRefPubMed ↵ Baarends, W. M., Roest, H. P. & Grootegoed, J. A. (1999) Mol. Cell EnExecutecrinol. 151 , 5-16. pmid:10411315 LaunchUrlCrossRefPubMed Baarends, W. M., van der Laan, R. & Grootegoed, J. A. (2000) J. EnExecutecrinol. Invest. 23 , 597-604. pmid:11079455 LaunchUrlPubMed Grootegoed, J. A., Siep, M. & Baarends, W. M. (2000) Baillieres Best Pract. Res. Clin. EnExecutecrinol. Metab. 14 , 331-343. pmid:11097779 LaunchUrlCrossRefPubMed ↵ Sutovsky, P. (2003) Microsc. Res. Tech. 61 , 88-102. pmid:12672125 LaunchUrlCrossRefPubMed
Like (0) or Share (0)