Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Mice Lacking Hbp1 Function Are Viable and Fertile

  • Cassy M. Spiller ,

    Current address: School of Biomedical Sciences, The University of Queensland, Brisbane, Queensland, Australia

    Affiliation Institute for Molecular Bioscience, The University of Queensland, Brisbane, Queensland, Australia


  • Dagmar Wilhelm,

    Current address: Department of Anatomy & Neuroscience, The University of Melbourne, Melbourne, Victoria, Australia

    Affiliation Institute for Molecular Bioscience, The University of Queensland, Brisbane, Queensland, Australia

  • David A. Jans,

    Affiliation School of Biomedical Sciences, Monash University, Clayton, Victoria, Australia

  • Josephine Bowles,

    Affiliation School of Biomedical Sciences, The University of Queensland, Brisbane, Queensland, Australia

  • Peter Koopman

    Affiliation Institute for Molecular Bioscience, The University of Queensland, Brisbane, Queensland, Australia

Mice Lacking Hbp1 Function Are Viable and Fertile

  • Cassy M. Spiller, 
  • Dagmar Wilhelm, 
  • David A. Jans, 
  • Josephine Bowles, 
  • Peter Koopman


Fetal germ cell development is tightly regulated by the somatic cell environment, and is characterised by cell cycle states that differ between XY and XX gonads. In the testis, gonocytes enter G1/G0 arrest from 12.5 days post coitum (dpc) in mice and maintain cell cycle arrest until after birth. Failure to correctly maintain G1/G0 arrest can result in loss of germ cells or, conversely, germ cell tumours. High mobility group box containing transcription factor 1 (HBP1) is a transcription factor that was previously identified in fetal male germ cells at the time of embryonic cell cycle arrest. In somatic cells, HBP1 is classified as a tumour suppressor protein, known to regulate proliferation and senescence. We therefore investigated the possible role of HBP1 in the initiation and maintenance of fetal germ cell G1/G0 arrest using the mouse model. We identified two splice variants of Hbp1, both of which are expressed in XY and XX fetal gonads, but only one of which is localised to the nucleus in in vitro assays. To investigate Hbp1 loss of function, we used embryonic stem (ES) cells carrying a Genetrap mutation for Hbp1 to generate mice lacking Hbp1 function. We found that Hbp1-genetrap mouse mutant germ cells proliferated correctly throughout development, and adult males were viable and fertile. Multiple Hbp1-LacZ reporter mouse lines were generated, unexpectedly revealing Hbp1 embryonic expression in hair follicles, eye and limbs. Lastly, in a model of defective germ cell G1/G0 arrest, the Rb1-knockout model, we found no evidence for Hbp1 mis-regulation, suggesting that the reported RB1-HBP1 interaction is not critical in the germline, despite co-expression.


Germ cells are highly specialized cells that are uniquely capable of undergoing meiosis and represent our means to reproduce. During embryo development, two distinct cell cycle modes characterize the sex-specific pathways of germ cell differentiation. From 12.5 dpc in mice, germ cells enter G1/G0 arrest, signifying commitment to spermatogenesis [1], while entry into meiosis prophase I in the ovary signifies commitment to oogenesis [2]. The somatic cell environment of the gonads directs these two germ cell fates. Retinoic acid has been shown to modulate meiosis entry in the ovary, while being antagonistic to pro-spermatogonia development [35]. In the testis, very little is known regarding germ cell entry and maintenance of G1/G0 arrest. In humans, failure of this process to occur correctly has been linked to testicular germ cell tumours and their precursor, germ cell neoplasia in situ [6, 7]. This connection provides strong motivation for investigating cell cycle regulation in these specialised cells.

With no clear effector molecule or signalling pathway that seems likely to fulfil the role of inducing mitotic arrest in germ cells, investigations in many laboratories used microarray analysis and subtraction screens to identify genes expressed sex-specifically at the appropriate time. Using a subtraction screen, Smith and colleagues (2004) identified Hbp1, encoding the transcription factor high mobility group box containing transcription factor 1 (HBP1), as being expressed during the onset of mitotic arrest in mouse fetal testes [8]. From these data and what is currently known of HBP1 function in other systems, we hypothesised that HBP1 may be involved in the initiation or maintenance of mitotic arrest in fetal male germ cells.

HBP1 is a transcription factor that was first identified as an interacting factor of the cell cycle regulator retinoblastoma 1 (RB1) via a yeast two-hybrid screen [9]. HBP1 was subsequently shown to contain two RB1 interaction motifs, facilitating interaction with RB1 and related factor p130 [9, 10]. HBP1 shares DNA binding domain homology with members of the T cell-specific transcription factor lymphoid enhancer factor (TCF/LEF) [11] and the SRY-related HMG box (SOX) [12] families. The prominent feature of these families is their high mobility group (HMG) domain that sequence-specifically interacts exclusively with DNA [13]. Recent studies have identified a diverse range of gene targets for HBP1, including the MYC family (Myc and Mycn), cell cycle genes (cyclin D1), NADPH oxidase pathway (p46 phox), chromatin remodelling (histone H10) and myeloperoxidase (reviewed in [14]). Interestingly, in humans, MYC and deregulation of the germ cell mitosis-to-meiosis switch have been implicated in the genesis of germ cell neoplasia in situ [15, 16]. Via protein-protein interactions with cell cycle regulators (RB1, p130) and repression of specific gene targets, the role of HBP1 is to set up proliferation barriers and trigger differentiation in various cell contexts. Indeed, over-expression of HBP1 in vitro and in vivo results in cell cycle arrest even in the presence of optimal proliferation signals [10, 14, 17].

In this study we focused on Hbp1 expression and function in male fetal germ cells during the period of G1/G0 arrest (12.5 dpc—birth). We provide the first report of a splice variant of Hbp1 that is expressed in male and female gonads, and describe the phenotype of a novel Hbp1-knockout mutant mouse line. We also generated and analysed two Hbp1-LacZ reporter lines to uncover further unreported embryonic tissue expression, and investigated a role for Hbp1 in a model of defective germ cell G1/G0 arrest—the Rb1-knockout mouse.

Materials and Methods

Ethics statement

All mouse strains and experimental protocols were conducted in accordance with the Animal Ethics Committee of the University of Queensland (approval # IMB/131/09/ARC and SBMS/121/16/NHMRC/ARC/BREED).


Animals were maintained in a recurrent photo cycle of 12h on-off in temperature controlled (22°C ± 2°C) rooms within the University of Queensland Biological Resource Centre. Mice received a diet of irradiated Meat Free Rat and Mouse Diet (Specialty Feeds, Glen Forrest, Australia) and fresh autoclaved water ad libitum. Mice were housed in filter-top static micro isolator cages with fine cord cob bedding and crinkle nest enrichment. Physical condition was monitored daily and provisions were in place to ensure any animals exhibiting adverse health received veterinary advice and/or immediate euthanasia to minimise pain and/or distress. Within the HGT colony, one mouse developed testicular teratoma and was euthanised by cervical dislocation immediately at external visualisation of the mass (detailed in Results). All other mice were euthanised by cervical dislocation at the experimental endpoint. Strains included: outbred CD1 mice and the We/We mutant strain on outbred Swiss background (Quackenbush strain) [18]. Rb1-/- mice were generated as previously described [19, 20] and maintained on a C57BL/6 background. Genotyping was performed as described previously [20].

Generation of the 2KbHbp1P_pHSP68_LacZ mouse lines

The 2 kb Hbp1 proximal promoter region was amplified from C57Bl/6 genomic DNA using the Expand High Fidelity PCR System (Roche, Indianapolis, USA) using primers Hbp1P2kb-F and Hbp1P2kb-R (S1 Table). The region included -2121 bp to +1 bp relative to the Hbp1 transcription start site and was cloned into a modified pBluescript vector containing LacZ driven by the minimal HSP68 promoter. Transgenic mouse lines were produced by standard methods [21]. Tail tip biopsies were genotyped for the presence of the β-galactosidase cassette using primers LacZ-F and LacZ-R (S1 Table). Positive Hbp1lacZ founders were then crossed to C57Bl/6 mice to generate lines, positive studs were identified and mated with C57Bl/6 wildtype females and embryos were collected for analysis.

Generation of Hbp1-genetrap mice

The Bay Genomics ES Cell Line RRF373 containing the β-geo splicetrap vector, pGT0Lxf [22] was obtained from the Mutant Mouse Regional Resource Centers (MMRRC, Davis, USA) ( The E14 mutant ES cell line (G418-resistant; 129P2/Ola) was used for blastocyst injection into C57Bl/6 blastocysts. Germline transmission was achieved by mating chimeric males to wild-type C57Bl/6 females, heterozygotes detectable by agouti coat colour. Intercrossing of the F1 heterozygotes generated 129P2/Ola/C57Bl/6 mixed background offspring and the line continued to be backcrossed to C57BL/6 over at least 7 subsequent generations.

Mice were genotyped by PCR from genomic DNA extracted by tail tip biopsy. Two separate PCR protocols were employed that allowed for detection of the β-geo cassette alone (primers LacZ-F and LacZ-R) in addition to a product spanning Hbp1 exon 5 and the β-geo cassette (primers Ex5_Geo-F and Ex5_Geo-R). Primers are listed in S1 Table.

Embryo collection and organ culture

Embryos were collected from timed matings, with noon of the day on which the mating plug was observed designated 0.5 dpc. Embryo sex was determined by gonadal morphology (the presence or absence of testis cords). Rb1-/- gonads were cultured as previously described [20, 23].

Cell lines

Human embryonic kidney (HEK293) cells [24] were cultured at 37°C, 5% CO2 in Dulbecco’s Modified Eagle Medium including 10% fetal calf serum. HEK293 cells were grown to 90% confluency on cover slips in 6-well plates, transfected with 4 μg of each Fl-Hbp1 or ΔHbp1 expression vector using Lipofectamine 2000 reagent (Invitrogen, Carlsbad, USA) as per manufacturers’ instructions. Cells were analysed after 24 h incubation at 37°C.

Whole mount in situ hybridisation

A 903 bp Fl-Hbp1 and a 573 bp ΔHbp1 3’UTR fragment were cloned from 12.5 dpc testis. Primers were Fl-Hbp1-F and Fl-Hbp1-R and ΔHbp1-F and ΔHbp1-R, listed in S1 Table. The amplified fragments were cloned into the pGEM-T-Easy vector (Promega, Madison, USA) and verified by sequencing. The sense and anti-sense probes were synthesised using T7 and SP6 RNA polymerases through in vitro transcription. Gonads/mesonephroi were dissected and fixed in 4% paraformaldehyde (PFA) in phosphate-buffered saline (PBS) for several hours at 4°C. Whole mount in situ hybridization (ISH) with digoxygenin (DIG) labelled RNA probes was carried out as described by [25]. The RNA probe was detected by incubation with BM Purple, AP Substrate (Roche, Indianapolis, USA).

Quantitative real time PCR and statistical analysis

Embryonic gonads (without mesonephros) were dissected in PBS and total RNA was immediately isolated using the Micro RNA kit (Qiagen, Hilden, Germany) as per manufacturers’ instructions including the optional DNaseI genomic DNA degradation step. cDNA was synthesised from 1 μg of RNA by reverse transcription (Superscript III, Invitrogen, Carlsbad, USA) using random primers (Promega, Madison, USA) according to manufacturers’ instructions. The ABIPrism-7000 Sequence Detector System was used to analyse relative cDNA levels. Primers are listed in S1 Table. All quantitative RT-PCR experiments were performed in triplicate and repeated on three separate biological samples. Results are represented as mean ±S.E.M of the experiments. Briefly, samples were analysed in 25 μl reactions containing 1 μl cDNA prepared as described above, SYBR Green PCR Master Mix (Applied Biosystems, Foster City, USA) and 3.75 μM each of forward and reverse primers. Cycling conditions began with an initial 10-min step at 95°C followed by 40 cycles of 95°C for 15 sec and 60°C for 1 min in a two-step thermal cycle. Dissociation curves were analysed for each primer set and cDNA samples were normalised against both 18S rRNA and Rps29 using the 2-ΔΔCT method. Statistical analysis was performed using Prism. Pairwise comparisons were analysed using two-tailed student t-tests.

HBP1-MYC constructs

Truncated Hbp1 cDNA constructs were amplified from 12.5 dpc testis cDNA using the Expand High Fidelity PCR System (Roche, Indianapolis, USA) with the common forward primer All-Hbp1-MYC-F containing a BamHI restriction site and individual reverse primers containing an XhoI restriction site, FlHbp1-MYC-R and ΔHbp1-MYC-R (S1 Table). These fragments were cloned into a modified pcDNA3.0 vector generating an N-terminal MYC-tagged protein and sequenced for verification.

Whole mount LacZ staining

Whole embryos and embryonic tissues were collected in ice-cold PBS and fixed for several hours in glutaraldehyde fixative (1% formaldehyde, 0.2, glutaraldehyde, 2 mM MgCl2, 5 mM EGTA and 0.02% NP-40 in PBS) at room temperature. Whole mount LacZ staining of these tissues was then performed as follows: Embryos were washed three times in PBS and stained for ß-galactosidase in 5mM K3Fe(CN)6, 5mM K4Fe(CN)6, 2mM MgCl2, 0.02% NaDeoxycholate, 0.02% NP-40 and 1mg/ml X-gal in phosphate buffered saline overnight at 37°C. After desired colour development was achieved, embryos were washed three times in PBS and post-fixed in 4% PFA in PBS for 30 min at 4°C.

Histological and immunofluorescence analysis

Embryos and gonads were dissected in ice-cold PBS and fixed in 4% PFA in PBS for several hours. Samples were then embedded in paraffin before sectioning at 7 μm on a microtome (Leica, Wetzlar, Germany). For morphological analysis sections were deparaffinised and stained with haematoxylin and eosin (H&E). Immunofluorescence with transfected cells [26] and on sections of mouse embryos [27] was performed as described previously.

Primary antibodies and dilutions used were: Anti-MYC (Cell Signalling Technology, Danvers, USA) 1:1000, anti-AMH (Santa Cruz Biotechnology, Dallas, USA) 1:200, anti-3βHSD (Prof J I Mason, The University of Edinburgh) 1:100, anti-MVH (AbCam, Cambridge, UK) 1:200, anti-E-cadherin (BD Bioscience, San Jose, USA) 1:200, anti-Ki67 (Clone TEC-3, DakoCyomation, Glostrup, Denmark) 1:50, DAPI (Sigma Aldrich, St Louis, USA) 1:2000. Secondary antibodies and dilutions were all from Molecular Probes (Eugene, USA) and used at 1:200: goat anti-rabbit Alexa Flour 488, donkey anti-rat Alexa Fluor 594, goat anti-mouse Alexa Fluor 594 and donkey anti-goat Alexa Fluor 488.

H&E section images were captured on an Olympus (Shinjuku, Japan) BX51 BF/DF microscope. Whole mount LacZ imaging was performed on an Olympus (Shinjuku, Japan) SZX-12 stereo dissecting microscope. Photographs were taken with an Olympus (Shinjuku, Japan) DP-70 camera using the default settings of the Olympus software DP Controller (version Immunofluorescence-labelled sections were imaged using Zeiss (Oberkochen, Germany) LSM-510 confocal microscope.

Western blotting

Standard Western blot analysis was performed with the following antibodies and dilutions: Anti-HBP1 (N-20, Santa Cruz Biotechnology, Dallas, USA) 1:200, anti-alpha-tubulin (Clone B-5-1-2, Sigma Aldrich, St Louis, USA) 1:500, donkey anti-goat conjugated to horse radish peroxidase (HRP) (Jackson Laboratories, Bar Harbor, USA) 1:2000, goat anti-mouse-HRP (Sigma Aldrich, St Louis, USA) 1:2000.


Hbp1 is expressed during mouse gonad development

Ensembl genome browser database analysis of the Hbp1 sequence revealed two putative Hbp1 splice variants. The shorter transcript (referred to as delta Hbp1; ΔHbp1) omits exons 10 and 11 of the full-length transcript (referred to as full length Hbp1; FL-Hbp1), resulting in and a truncated coding region and an alternative 3’ untranslated region (Fig 1A). The encoded proteins contain several conserved domains including RB binding, p38 docking and phosphorylation sites in addition to the HMG domain, which is truncated at amino acid (aa) 474 in the smaller protein (Fig 1B).

Fig 1. Alternative splicing of Hbp1 transcripts.

(A) Gene structure of the two Hbp1 splice variants. The full-length transcript comprises 11 exons and the truncated transcript is composed of the first 9 exons. Both transcripts contain identical 5’UTRs in addition to distinct 3’UTRs (open boxes), the specific riboprobes and real time PCR probes are depicted. (B) Location of HBP1 protein domains and nuclear localisation signals (NLS).

We investigated the expression of both transcripts in developing mouse gonads at 14.5 dpc using whole mount ISH. Using antisense riboprobes hybridizing to the unique 3’UTRs, we detected expression of FL-Hbp1 in the testis only, whereas ΔHbp1 was expressed in both XY and XX gonads (Fig 2A). Sense control riboprobes did not yield any staining (S1 Fig). To determine if the expression was present in germ and/or somatic cells, we analysed expression levels of both Hbp1 transcripts in the We/We mutant mouse model using quantitative real time RT-PCR (qRT-PCR). Mice homozygous for mutations in the W (dominant white spotting) locus (We/We) lack germ cells and die in utero at 14.5 dpc due to macrocytic anaemia [18]. Analysis of FL-Hbp1 and ΔHbp1 expression in 13.5 dpc We/We mutant gonads revealed that expression was significantly decreased in XY samples lacking germ cells indicating that it is largely restricted to, or dependent on, germ cells in XY gonads (Fig 2B). In XX gonads, expression was not significantly decreased, suggesting there may be a larger somatic component of FL-Hbp1 and ΔHbp1 expression in this organ (Fig 2B). Next, we used qRT-PCR to compare levels of Hbp1 expression in wild-type testes and ovaries over a wider time-course. In the XY gonad, the highest expression of FL-Hbp1 and ΔHbp1 was detected at 15.5 dpc and 14.5 dpc respectively. In the ovary, expression of FL-Hbp1 and ΔHbp1 appeared to generally decline over the timecourse, with lowest expression detected at 16.5 dpc (Fig 2C). Attempts to localise HBP1 protein expression by immunofluorescence using an antibody were unsuccessful, so we turned to in vitro experiments.

Fig 2. Detection of Fl-Hbp1 and ΔHbp1 transcripts in wildtype and We/We gonads.

(A) Detection of Fl-Hbp1 and ΔHbp1 in 14.5 dpc XX and XY gonads using whole mount in situ hybridisation (B) qRT-PCR analysis detected lower levels of Fl-Hbp1 and ΔHbp1 gene expression in 13.5 dpc XY and XX We/We mutant gonads which lack germ cells. Expression was normalised to 18S RNA (mean ± S.E.M of three independent experiments, each performed in triplicate) and wildtype controls set to 1. *P < 0.05; **P < 0.005. (C) qRT-PCR detected the Fl-Hbp1 and ΔHbp1 transcripts in gonad-only cDNA samples from 12.5–16.5 dpc in XX and XY gonads. Expression was normalised to 18S RNA (mean ± S.E.M of three independent experiments, each performed in triplicate).

HBP1 variants display different cellular localization

As HBP1 is a transcription factor, it must gain access to the nucleus to perform its function. We therefore investigated the cellular localisation of both variants in cell culture. Bioinformatic analysis of the HBP1 amino acid sequence revealed the presence of two un-reported nuclear localisation signals (NLSs) flanking the HMG domain at positions aa 444–448 (NKCKR) and aa 514–518 (WKRKR) (Fig 1B). These putative NLSs are conserved within families of HMG-containing proteins including the SOX family of transcription factors [28]. As ΔHbp1 lacks the second NLS, we hypothesised that ΔHbp1 would not be efficiently localised to the nucleus. To investigate this, we generated both variants in-frame with a MYC tag and transfected them into HEK293 cells. Analysis by MYC immunofluorescence revealed mainly nuclear and some cytoplasmic localization of FL-HBP1 (containing both NLS sequences), but exclusively cytoplasmic localisation of ΔHBP1 (Fig 3). These data suggest that the C-terminal NLS is necessary for HBP1 nuclear localisation and importantly, has revealed a significant functional difference between FL-HBP1 and ΔHBP1.

Fig 3. Cellular localisation of Fl-HBP1 and ΔHBP1.

Myc-tagged HBP1 variants were transfected into HEK293 cells and immunostained for MYC expression. Cells were counterstained with DAPI to identify the nuclei and were visualised using confocal microscopy. FL-HBP1 was localised to the nucleus with some cytoplasmic staining also detected. ΔHBP1 remained in the cytoplasm. The control represents cells transfected without DNA. Scale Bar = 10μm.

The Hbp1 promoter is active in vivo

Next, we employed a transgenic approach using in vivo ß-galactosidase expression driven by the Hbp1 promoter for two reasons. First, this strategy allows identification of regulatory regions required for germ cell expression of Hbp1 in vivo, and secondly, the generation of a germ cell-LacZ expressing transgenic line that can be used in gonadal explant culture as an indication of G1/G0 arrested germ cells would provide an excellent tool for germ cell research. 2 kb of the Hbp1 proximal promoter was amplified and cloned into the pHSP68_LacZ expression vector [29]. Following pro-nuclear injection, two founding Hbp1Lacz lines were established and characterised by ß-galactosidase staining.

The first Hbp1lacZ founder line (Hbp1lacZ_1) displayed specific staining in several fetal somatic tissues including the brain, neural tube, eye, limb tips and hair follicles (Fig 4). Importantly, expression of LacZ driven by the 2 kb promoter region of Hbp1 was also detected in 14.5 dpc XY gonads but not in ovaries at this stage. The XY gonadal staining was not strong enough to identify individual LacZ-expressing cell types following sectioning (S2 Fig).

Fig 4. LacZ expression analysis of Hbp1lacZ_1.

LacZ expression, driven by the 2 kb Hbp1 proximal promoter, was assessed at embryonic stages 11.5 (A) and 14.5 dpc (B); wildtype (Wt); transgenic (Tg). Promoter activity was also detected in 14.5 dpc somatic tissues including the forebrain (C), hair follicles (D), eye (E), limb tips (F) and neural tube (G,H). Expression was also detected at 14.5 dpc in the XY (I), but not XX (J) gonad.

Analysis of the second Hbp1lacZ founder (Hbp1lacZ_2) revealed comparable LacZ expression to founder 1 in several fetal somatic tissues including the hair follicles and eye in addition to the forebrain (S3 Fig), suggesting that this might be a true reflection of the activity of this Hbp1 promoter region in vivo. Differences were seen in the cell types expressing LacZ within the neural tube, as Hbp1lacZ_2 stained within the dorsal root ganglia rather than the epithelia as seen for Hbp1lacZ_1. In addition to the tip of each expanding digit, expression was also detected in the limb proper, and there was an absence of LacZ expression in the hindbrain in Hbp1lacZ_2. Unlike Hbp1lacZ_1, there was no detectable LacZ expression within the fetal XY and XX gonads (S3 Fig).

Analysis of Hbp1-mutant mice

We next generated Hbp1 loss-of-function mice in order to investigate the effects on embryonic development. Hbp1 “gene-trap” mutant ES cells, containing a ß-galactosidase cassette insertion directly downstream of exon 5, were obtained from Bay Genomics (Fig 5A). The nature of the Hbp1 genetrap mutation potentially gives rise to a truncated protein containing the first 5 exons (218 aa). An expression construct of the Hbp1-mutant variant was cloned and expressed in HEK293 cells with a N-terminal MYC tag and revealed that the shortened protein is expressed exclusively within the cytoplasm (S4 Fig), suggesting that if this product is translated in vivo, it cannot have a nuclear function, including binding to DNA.

Fig 5. Morphological and protein expression analysis of Hbp1+/+ and Hbp1-/- mutant embryos.

(A) Gene structure of the two Hbp1 splice variants and the Hbp1 gene-trap variant which contains a ß-galactosidase cassette inserted directly downstream of exon 5. (B) Whole 14.5 dpc Hbp1+/+ and Hbp1-/- embryos were stained for LacZ expression. LacZ was detected in Hbp1-/- embryos in the eye, hair follicles, limbs, ears and mesonephros, but not testes at 14.5 or 16.5 dpc. (C) Western blot analysis was performed on whole 14.5 dpc Hbp1+/+, Hbp1+/- and Hbp1-/- embryo lysates. Anti-HBP1 detected reduced levels of HBP1 protein in the Hbp1+/- and Hbp1-/- samples compared to Hbp1+/+ control. TUBA1A was used as the loading control.

Following blastocyst injection of the Hbp1-mutant ES cells, breeding of chimeric male offspring resulted in germline transmission of the Hbp1-genetrapped allele. Heterozygotes for the mutation (Hbp1+/-) were viable and fertile and subsequent Hbp1+/- x Hbp1+/- matings yielded Hbp1-/- embryos for analysis. As with the adult heterozygous mutants, the homozygous embryos displayed normal gross morphology of all somatic tissues (Fig 5B). Both heterozygous and homozygous males were fertile fathering an average of 6.7 ±2.8 (n = 7) and 7.3 ±1.2 (n = 3) pups per litter respectively. Accordingly, adult testis gross morphology was comparable between wildtype controls and homozygous mutants with testis/body weight ratios of 0.24 ±0.03 and 0.28 ±0.01 respectively (n = 3). We observed one instance of testicular teratoma in a chimeric male founder (S5 Fig), but this phenomenon did not affect any of the Hbp1+/- males in the established colony (0/53 males).

We also stained Hbp1+/- embryos for LacZ expression taking advantage of the ß-galactosidase cassette insertion. Similarly to the Hbp1 promoter transgenic lines (Hbp1lacZ_1 and Hbp1lacZ-2), LacZ expression was detected in hair follicles, eye and limbs of embryos at 14.5 dpc. In contrast, no ß-galactosidase activity was detected in fetal gonads at 14.5 and 16.5 dpc, or in the neural tube or brain, unlike the promoter transgenic lines (Figs 5B and 4, S3 Fig). Although these analyses suggested that Hbp1 is endogenously expressed during the development of hair follicles, eye and limbs, adult Hbp1+/- (n = 67) and Hbp1-/- (n = 12) mice had no reported defects with hair growth, eyesight or limb morphology.

In order to determine if HBP1 protein was translated in the heterozygous and homozygous mutants, whole 14.5 dpc embryo lysates were investigated by Western blot analysis using an HBP1 polyclonal antibody that recognises an epitope near the N-terminus of the protein. This analysis revealed greatly reduced levels of expression in both the Hbp1+/- and Hbp1-/- embryos compared to wildtype Hbp1+/+ control (Fig 5C). No lower molecular weight protein was apparent in the Hbp1+/- and Hbp1-/- embryos, suggesting that the truncated 218aa protein (detectable with the polyclonal antibody used; predicted molecular weight of 53 kDa) is either not translated, or is readily degraded.

We next made a thorough assessment of testis development in Hbp1-/- mutant embryos. Because the Hbp1 gene-trap mutation was ubiquitous in these embryos, somatic cells were also assessed for any phenotype that may arise due to the ablation of HBP1. Using H&E staining we found normal testis morphology at 12.5, 14.5 and 16.5 dpc (S6 Fig). Using immunofluorescence, we further found that expression of somatic cell markers AMH (Sertoli cells) and 3ßHSD (Leydig cells) were similar between genotypes at 14.5 dpc (S7 Fig).

To investigate the hypothesis that HBP1 controls G1/G0 arrest in fetal XY germ cells, proliferation marker Ki67 was assessed in the germ cell population, marked by expression of MVH. Here we found that germ cells were proliferating (Ki67-positive) equally at 12.5 dpc in both Hbp1+/+ and Hbp1-/- samples, but were not proliferating (Ki67-negative) at 14.5 and 16.5 dpc in either mutants or wild type controls (Fig 6A). Lastly, we assessed pluripotency marker OCT3/4 in the germ cell population. We detected OCT3/4 expression in germ cells of both genotypes at 14.5 dpc, but not at 16.5 dpc (Fig 6A). Although Hbp1-/- XY gonads appeared to have a normal morphology and profile of marker protein expression as detected by immunofluorescence, we next investigated gene expression in these samples, in an effort to identify a subtler phenotype in the absence of Hbp1. We performed qRT-PCR for a variety of germ cell and cell cycle markers in 16.5 dpc gonad samples from which mesonephroi had been removed (Fig 6B). Consistent with the immunofluorescence data, there were no significant changes to the germ cell markers Mvh or Oct3/4, and p63, a marker of G1/G0 arrest, was also unchanged. Additionally, somatic markers Fgf9 and Sox9, retinoblastoma family members Rb1, p130 and p107 and cell cycle regulators p21, p27 and p57 were comparable between controls and Hbp1-/- samples. Therefore, having determined that the Hbp1-mutant embryos showed normal morphology, fertility and viability, we conclude that HBP1 is dispensable for correct embryo development and subsequent adult survival.

Fig 6. Immunohistochemical and gene expression analysis of Hbp1+/+ and Hbp1-/- embryonic gonads.

(A) Proliferation marker Ki67 in germ cells (MVH-positive cells) was detected in both Hbp1+/+ and Hbp1-/- gonads at 12.5 dpc, but was absent in germ cells of 14.5 and 16.5 dpc gonads of both genotypes. Pluripotency marker OCT3/4 was expressed similarly in germ cells (MVH-positive cells) in Hbp1+/+ and Hbp1-/- gonads at 14.5 dpc and was undetectable at 16.5 dpc. Scale bar = 50μm. (B) qRT-PCR analysis of Hbp1+/+ and Hbp1-/- 16.5 dpc gonad samples revealed comparable expression between of various germ cell and somatic cell markers. Germ cell markers: Mvh, Oct3/4and G1/G0 arrest indicator p63, somatic cell markers Fgf9 and Sox9, Retinoblastoma family members Rb1, p130 and p107, and cell cycle regulators p21, Ccnd1-3 and p53 displayed no significant difference between Hbp1+/- and Hbp1-/- samples. Samples normalised to 18S RNA (mean ± S.E.M of three independent experiments, each performed in triplicate). *P < 0.05; **P < 0.005; ns = not significant.

It remained possible that Hbp1 might play a role in ameliorating the phenotypes of other experimentally-produced mouse mutants showing defective germ cell cycle control. In Rb1 loss-of-function (Rb1-/-) mutant mice, some XY germ cells fail to enter G1/G0 arrest at 14.5 dpc unlike the wildtype control [20]. Despite this aberration, arrest is achieved in the total germ cell population by 16.5 dpc, likely due to compensation by CDK inhibitors Cdkn1b and Cdkn2b which are upregulated in mutant germ cells [20]. We investigated whether Hbp1 might similarly be upregulated in the absence of Rb1 in order to achieve eventual G1/G0 arrest in these cells. Using qRT-PCR, we found a small but significant increase in levels of both FL-Hbp1 and ΔHbp1 in Rb1-/- gonads at 14.5 dpc (Fig 7A and 7B). However, because germ cell number is increased in Rb1-/- mutants due to their cell cycle defect (measured by Mvh expression; Fig 7C), we also normalized FL-Hbp1 and ΔHbp1 expression to Mvh to account for this germ cell number increase. We found that FL-Hbp1 and ΔHbp1 expression was unchanged at 14.5 dpc but significantly decreased at 16.5 dpc in germ cells of Rb1-/- mutant gonads (Fig 7D and 7E). These data suggest that in XY germ cells Hbp1, at least at the RNA level, is unlikely to contribute to the back-up mechanism performed by other CDK inhibitors to compensate for Rb1 failure to achieve G1/G0 arrest by 16.5 dpc.

Fig 7. Hbp1 expression in Rb+/+ and Rb-/- mutant XY gonads.

Using qRT-PCR analysis, normalizing gene expression to 18SRNA, both Fl-Hbp1 (A) and ΔHbp1 (B) gene expression was significantly increased in Rb-/- mutant XY gonads at 14.5 dpc. In 16.5 dpc Rb-/- cultured XY gonads, there was no significant difference in either Fl-Hbp1 or ΔHbp1 gene expression, although germ cell marker Mvh was significantly increased at this timepoint (C). When gene expression was normalized to germ cell marker Mvh, both Fl-Hbp1 (D) and ΔHbp1 (E) gene expression was significantly decreased in 16.5 dpc Rb-/- cultured XY gonads. (mean ± S.E.M of three independent experiments, each performed in triplicate; wildtype controls (Rb+/+) set to 1). *P < 0.05; **P < 0.005.


The embryonic differentiation of XX and XY germ cells diverges at 12.5 dpc with XX germ cell entry into the first phase of meiosis and XY germ cell entry into G1/G0 arrest [1]. XY germ cells are particularly fascinating as they maintain a prolonged period of G1/G0 arrest throughout development and postnatal life, prior to entering mitosis and meiosis after puberty [30]. Aberrations in the entry or maintenance of G1/G0 arrest have led to instances of both germ cell loss and conversely, proliferation and therefore cancer, such as observed in Pten-/- [31], Dazl-/- [32] and Ter mutations [33]. It is also believed that loss of correct germ cell-cell cycle control and differentiation is responsible for germ cell neoplasia in situ (previously known as carcinoma in situ [34]), the precursor cell to human testicular germ cell tumours, for which there is no suitable mouse model. Comparison of germ cell and somatic cell tumours has revealed both common and unique gene and protein expression patterns, including for cell cycle regulators such as RB1 [6, 7]. It is possible that germ cells are subject to a different type of cell cycle regulation, which would not be surprising considering their unique ability to undergo meiosis.

Although we do not know what factor(s) may be responsible for initiating this cell cycle state, several cell cycle factors have been identified as being up-regulated or activated during fetal germ cell G1/G0 arrest. Particularly, activation of p27(KIP1), p15(INK4b) and p16(INK4a) and RB1 occurs at this time, in addition to upregulation of p21(Cdkn1a) [20, 35]. While these kinases and phospho-proteins comprise the machinery used to achieve and maintain G1/G0 arrest, the regulation of these factors within germ cells remains unclear. The transcription factor HBP1, identified by our group in a subtraction screen [8], is an interesting candidate for germ cell-specific regulation of this event due to its established role in cell cycle arrest and wide range of interacting factors. The work described here characterised the expression and functional role of Hbp1 in the initiation and maintenance of XY germ cell mitotic arrest.

Using several techniques, Hbp1 expression was enriched within the XY gonad during G1/G0 arrest as reported previously [8]. Further to the analysis presented by Smith and colleagues (2004), qRT-PCR analysis revealed maximal expression of FL-Hbp1 at 14.5–15.5 dpc in the XY gonads. As germ cells are reported to begin entry into G1/G0 arrest as early as 12.5 dpc [35, 36] it seems more likely that the role of HBP1 in these cells is related to the maintenance/reinforcement of this arrest rather than its initiation.

Expression of a second Hbp1 splice variant was also detected in germ cells at this stage and we considered that it might reflect a novel mechanism of Hbp1 regulation and function. Subcellular visualization in vitro revealed that only FL-HBP1 is translocated into the nucleus, likely requiring both NLSs within the HMG domain. The SOX family member SRY utilises two similar NLS sequences flanking its HMG domain which associate with importin beta for nuclear localisation and RanGTP for disassociation [28]; we predict a similar mechanism may be used by HBP1, however this is yet to be confirmed. In contrast to FL-HBP1, ΔHBP1, which lacks this C-terminal NLS, remained within the cytoplasm. This suggests that FL-HBP1 can function as a transcription factor in XY germ cells, while ΔHBP1 presumably has an alternate role, independent of DNA binding. Within the cytoplasm ΔHBP1 could potentially regulate levels of HBP1 binding partners such as RB1 and p130, or perform a dominant-negative function by preventing FL-HBP1 nuclear import, although no evidence for HBP1 dimerization has emerged to date. Identification of ΔHBP1 binding partner(s) may be informative in identifying a role for this factor.

Using transgenic reporter lines we investigated activity of the endogenous 2kb Hbp1 proximal promoter. Because of potential integration effects from the reporter transgenic lines, we compared LacZ expression between these and with the genetrap Hbp1 knockout line to uncover likely sites of endogenous Hbp1 reporter activity during embryonic development. Comparison of all lines suggests potential action of HBP1 within the eye, hair follicles and limbs, which have not been reported to date. Several other tissues such as the forebrain and neural tube displayed reporter line-specific LacZ expression suggesting that the transgene was vulnerable to integration effects and/or that the entire Hbp1 promoter contains repressive elements for these tissues outside of the 2kb promoter investigated.

Given the role of HBP1 in cell cycle arrest (reviewed in [12]), its XY germ cell expression, and in vivo transcriptional regulation determined using the LacZ reporter and genetrap lines; we predicted that Hbp1 loss-of-function would display a fetal germ cell proliferation defect and possible aberrations in hair follicle, eye and limb development. The Hbp1-mutant mouse line we generated successfully ablated HBP1 protein and transcript levels, yet showed normal gross embryonic development and fetal germ cell G1/G0 arrest and differentiation. Specifically, germ cell identity, cell number and cell cycle state assessed by both mRNA and protein expression was comparable between mutants and controls. Adult Hbp1+/+ and Hbp1-/- mutants were viable and fertile (at least until 6 months of age), with no gross defects in any tissue or organ observed, despite reports of Hbp1 functioning in an array of adult tissues including muscle, adipocyte, erythroid and liver (reviewed in [12]).

Recently, Dong and colleagues (2016) reported a conditional Hbp1 loss-of-function model. Following ubiquitous deletion using the Ella-Cre recombinase [37], they observed defects in the oocyte reserve in adult females [35]. This phenotype was attributed to altered mitochondrial function in granulosa cells, and confirmed by using conditional deletion in the granulosa cells and germ cells separately [38]. In the absence of Hbp1, for unknown reasons and despite a general increase in ovarian reserve due to decreased apoptosis, mutant females were infertile by 7 months. We might expect the same phenotype in the Hbp1 genetrap-derived mutant mice analysed here, but although we routinely mated heterozygous and homozygous genetrapped Hbp1 females at ages younger than 7 months, we did not analyse any mice beyond that age.

An in vitro interaction between HBP1 and RB1 has been reported multiple times in the literature. In muscle cells the specific ratio of RB1/HBP1 has been shown to affect the regulation of the MyoD family and differentiation in C2C12 cells [10, 12]. We previously reported the function of RB1 in affecting correct timing of G1/G0 arrest in XY fetal germ cells, as in its absence germ cells exhibit a delay in G1/G0 entry and subsequent increase in total numbers [20]. In this study we investigated a role for HBP1 in the Rb1-/- model but found no evidence that transcriptional upregulation of Hbp1 compensates for Rb1 loss in the germ cells. Because Hbp1-/- germ cells affect correct G1/G0 arrest, it seems that, in vivo, the germline does not utilize an RB1-HBP1 interaction, or it has little biological significance, despite co-expression of both factors. Further analysis of HBP1 and RB1 protein level as well as binding partners in these mutants is required to confirm this conclusion.

In summary, we have profiled expression of Hbp1 within the XY germ cell population at a time appropriate to the maintenance of their G1/G0 arrest. We have shown that FL-HBP1 can be translocated to the nucleus to presumably function as a transcription factor. In vivo expression of Hbp1 was detected in the gonad as well as various other somatic tissues, suggesting that HBP1 may play a wider role in somatic tissue development/specification also. Genetic deletion of Hbp1 revealed normal fetal germ cell cycle control, suggesting that its role, if any, in the germline is not fundamental.

Supporting Information

S1 Fig. Sense controls of Fl-Hbp1 and ΔHbp1 in-situ hybridisation probes.

No signal was detected for either Fl-Hbp1 or ΔHbp1 sense control probes in 14.5 dpc gonads using whole mount in situ hybridisation.


S2 Fig. LacZ expression section analysis of Hbp1lacZ_1.

LacZ expression was detected in sections of 14.5 dpc Hbp1lacZ_1 testes, although resolution of cell type was not possible. Scale bar = 50μm; Meso = mesonephros.


S3 Fig. LacZ expression analysis of Hbp1lacZ_2.

LacZ expression, driven by the 2 kb Hbp1 proximal promoter, was detected at embryonic stages 12.5 (A) and 14.5 dpc in wildtype (Wt) and transgenic (Tg) embryos (B). Promoter activity was also detected in 14.5 dpc somatic tissues including the forebrain (C), hair follicles and eye (D), limb (E) and neural tube (F). Expression was not detected in either testes or ovaries at 14.5 dpc (G,H).


S4 Fig. Cellular localisation of HBP-genetrap variant.

Myc-tagged HBP1-genetrap variant was transfected into HEK293 cells and immunostained for MYC expression which revealed cytoplasmic localisation of the tagged protein. Cells were counterstained with DAPI to identify the nuclei and were visualised using confocal microscopy. Scale Bar = 10μm.


S5 Fig. Histological analysis of teratoma harvested from an HBP1-genetrap chimera at 6 months.

Externally an enlarged growth was evident (A, arrow). Internally, the growth was highly vascularised and had grown into the wall of the abdomen (B, arrow). H&E staining of sections revealed a teratoma with no normal spermatogenic tubules present (C) but multiple differentiated somatic cell types (D,E). Sale bar = 200μm.


S6 Fig. Immunohistochemical analysis of Hbp1+/+ and Hbp1-/- embryonic gonads.

H&E staining of XY Hbp1++- and Hbp1-/- gonads revealed comparable morphology of somatic and germ cells at timepoints 12.5, 14.5 and 16.5 dpc. Scale bar = 50μm.


S7 Fig. Immunohistochemical analysis of somatic markers in Hbp1+/+ and Hbp1-/- embryonic gonads.

Investigation of Sertoli cell marker AMH and Leydig marker 3ßHSD revealed visually similar fluorescence intensity and localisation in Hbp1+/+ and Hbp1-/- 14.5 dpc gonads. E-CAD (E-cadherin) marks germ cells. Apparent differences in total cord number between genotypes are due to the artefact of section position and gonad orientation. Scale bar = 50μm.


S1 Table. Primer names, sequences and product sizes (bp).



We thank Drs Graham Kay and Ian Tonks for kindly providing us with the RbF2/F2 mouse line. We also thank Tara Davidson, Desmond Tutt and Danielle Little for transgenic mouse production and animal husbandry. Confocal imaging was performed at the Australian Cancer Research Foundation’s (ACRF) Cancer Biology Imaging Facility, QLD, Australia. DAJ and PK are Senior Principal Research Fellows of the National Health and Medical Research Council of Australia.

Author Contributions

  1. Conceptualization: CS DW DAJ PK.
  2. Data curation: CS.
  3. Formal analysis: CS DW PK.
  4. Funding acquisition: DAJ JB PK.
  5. Investigation: CS DW.
  6. Methodology: CS DW DAJ PK.
  7. Project administration: CS DW PK.
  8. Supervision: DW DAJ JB PK.
  9. Writing – original draft: CS.
  10. Writing – review & editing: DW JB PK.


  1. 1. Hilscher W. [Kinetics of prespermatogenesis and spermatogenesis]. Verh Anat Ges. 1974;68:39–62. Epub 1974/01/01. pmid:4478730
  2. 2. McLaren A. Meiosis and differentiation of mouse germ cells. Symp Soc Exp Biol. 1984;38:7–23. Epub 1984/01/01. pmid:6400220
  3. 3. Bowles J, Knight D, Smith C, Wilhelm D, Richman J, Mamiya S, et al. Retinoid signaling determines germ cell fate in mice. Science. 2006;312(5773):596–600. Epub 2006/04/01. pmid:16574820
  4. 4. Bowles J, Feng CW, Spiller C, Davidson TL, Jackson A, Koopman P. FGF9 suppresses meiosis and promotes male germ cell fate in mice. Dev Cell. 2010;19(3):440–9. Epub 2010/09/14. pmid:20833365
  5. 5. Koubova J, Menke DB, Zhou Q, Capel B, Griswold MD, Page DC. Retinoic acid regulates sex-specific timing of meiotic initiation in mice. Proc Natl Acad Sci U S A. 2006;103(8):2474–9. pmid:16461896
  6. 6. Bartkova J, Rajpert-De Meyts E, Skakkebaek NE, Lukas J, Bartek J. Deregulation of the G1/S-phase control in human testicular germ cell tumours. APMIS. 2003;111(1):252–65; discussion 65–6. Epub 2003/05/23. pmid:12760379
  7. 7. Bartkova J, Lukas C, Sorensen CS, Meyts ER, Skakkebaek NE, Lukas J, et al. Deregulation of the RB pathway in human testicular germ cell tumours. J Pathol. 2003;200(2):149–56. Epub 2003/05/20. pmid:12754735
  8. 8. Smith JM, Bowles J, Wilson M, Koopman P. HMG box transcription factor gene Hbp1 is expressed in germ cells of the developing mouse testis. Dev Dyn. 2004;230(2):366–70. pmid:15162515
  9. 9. Lavender P, Vandel L, Bannister AJ, Kouzarides T. The HMG-box transcription factor HBP1 is targeted by the pocket proteins and E1A. Oncogene. 1997;14(22):2721–8. pmid:9178770
  10. 10. Tevosian SG, Shih HH, Mendelson KG, Sheppard KA, Paulson KE, Yee AS. HBP1: a HMG box transcriptional repressor that is targeted by the retinoblastoma family. Genes Dev. 1997;11(3):383–96. pmid:9030690
  11. 11. Schilham MW, Wilson A, Moerer P, Benaissa-Trouw BJ, Cumano A, Clevers HC. Critical involvement of Tcf-1 in expansion of thymocytes. J Immunol. 1998;161(8):3984–91. pmid:9780167
  12. 12. Shih HH, Tevosian SG, Yee AS. Regulation of differentiation by HBP1, a target of the retinoblastoma protein. Mol Cell Biol. 1998;18(8):4732–43. pmid:9671483
  13. 13. Bewley CA, Gronenborn AM, Clore GM. Minor groove-binding architectural proteins: structure, function, and DNA recognition. Annu Rev Biophys Biomol Struct. 1998;27:105–31. pmid:9646864
  14. 14. Yee AS, Paulson EK, McDevitt MA, Rieger-Christ K, Summerhayes I, Berasi SP, et al. The HBP1 transcriptional repressor and the p38 MAP kinase: unlikely partners in G1 regulation and tumor suppression. Gene. 2004;336(1):1–13. pmid:15225871
  15. 15. Jorgensen A, Nielsen JE, Almstrup K, Toft BG, Petersen BL, Rajpert-De Meyts E. Dysregulation of the mitosis-meiosis switch in testicular carcinoma in situ. J Pathol. 2013;229(4):588–98. pmid:23303528
  16. 16. Almstrup K, Leffers H, Lothe RA, Skakkebek NE, Sonne SB, Nielsen JE, et al. Improved gene expression signature of testicular carcinoma in situ. Int J Androl. 2007;30(4):292–302. pmid:17488342
  17. 17. Shih HH, Xiu M, Berasi SP, Sampson EM, Leiter A, Paulson KE, et al. HMG box transcriptional repressor HBP1 maintains a proliferation barrier in differentiated liver tissue. Mol Cell Biol. 2001;21(17):5723–32. pmid:11486012
  18. 18. Buehr M, McLaren A, Bartley A, Darling S. Proliferation and migration of primordial germ cells in We/We mouse embryos. Dev Dyn. 1993;198(3):182–9. pmid:8136523
  19. 19. Tonks ID, Hacker E, Irwin N, Muller HK, Keith P, Mould A, et al. Melanocytes in conditional Rb-/- mice are normal in vivo but exhibit proliferation and pigmentation defects in vitro. Pigment Cell Res. 2005;18(4):252–64. pmid:16029419
  20. 20. Spiller CM, Wilhelm D, Koopman P. Retinoblastoma 1 protein modulates XY germ cell entry into G1/G0 arrest during fetal development in mice. Biol Reprod. 2010;82(2):433–43. pmid:19864318
  21. 21. Hogan B. Manipulating the mouse embryo: a laboratory manual. 2nd ed. Plainview, N.Y.: Cold Spring Harbor Laboratory Press; 1994. xvii, 497 p. p.
  22. 22. Brennan J, Skarnes WC. Gene trapping in mouse embryonic stem cells. Methods Mol Biol. 2008;461:133–48. pmid:19030794
  23. 23. Martineau J, Nordqvist K, Tilmann C, Lovell-Badge R, Capel B. Male-specific cell migration into the developing gonad. Curr Biol. 1997;7(12):958–68. pmid:9382843
  24. 24. Graham FL, Smiley J, Russell WC, Nairn R. Characteristics of a human cell line transformed by DNA from human adenovirus type 5. J Gen Virol. 1977;36(1):59–74. pmid:886304
  25. 25. Hargrave M, Bowles J, Koopman P. In situ hybridization of whole-mount embryos. Methods Mol Biol. 2006;326:103–13. pmid:16780196
  26. 26. Beverdam A, Wilhelm D, Koopman P. Molecular characterization of three gonad cell lines. Cytogenet Genome Res. 2003;101(3–4):242–9. pmid:14684990
  27. 27. Wilhelm D, Martinson F, Bradford S, Wilson MJ, Combes AN, Beverdam A, et al. Sertoli cell differentiation is induced both cell-autonomously and through prostaglandin signaling during mammalian sex determination. Dev Biol. 2005;287(1):111–24. pmid:16185683
  28. 28. Forwood JK, Harley V, Jans DA. The C-terminal nuclear localization signal of the sex-determining region Y (SRY) high mobility group domain mediates nuclear import through importin beta 1. J Biol Chem. 2001;276(49):46575–82 pmid:11535586
  29. 29. Kothary R, Clapoff S, Darling S, Perry MD, Moran LA, Rossant J. Inducible expression of an hsp68-lacZ hybrid gene in transgenic mice. Development. 1989;105(4):707–14. pmid:2557196
  30. 30. Pedersen T, Peters H. Proposal for a classification of oocytes and follicles in the mouse ovary. J Reprod Fertil. 1968;17(3):555–7. pmid:5715685
  31. 31. Kimura T, Suzuki A, Fujita Y, Yomogida K, Lomeli H, Asada N, et al. Conditional loss of PTEN leads to testicular teratoma and enhances embryonic germ cell production. Development. 2003;130(8):1691–700. Epub 2003/03/07. pmid:12620992
  32. 32. Lin Y, Page DC. Dazl deficiency leads to embryonic arrest of germ cell development in XY C57BL/6 mice. Dev Biol. 2005;288(2):309–16. pmid:16310179
  33. 33. Noguchi T, Noguchi M. A recessive mutation (ter) causing germ cell deficiency and a high incidence of congenital testicular teratomas in 129/Sv-ter mice. J Natl Cancer Inst. 1985;75(2):385–92. pmid:3860691
  34. 34. Hoei-Hansen CE, Almstrup K, Nielsen JE, Brask Sonne S, Graem N, Skakkebaek NE, et al. Stem cell pluripotency factor NANOG is expressed in human fetal gonocytes, testicular carcinoma in situ and germ cell tumours. Histopathology. 2005;47(1):48–56. pmid:15982323
  35. 35. Western PS, Miles DC, van den Bergen JA, Burton M, Sinclair AH. Dynamic regulation of mitotic arrest in fetal male germ cells. Stem Cells. 2008;26(2):339–47. pmid:18024419
  36. 36. Tam PP, Snow MH. Proliferation and migration of primordial germ cells during compensatory growth in mouse embryos. J Embryol Exp Morphol. 1981;64:133–47. pmid:7310300
  37. 37. Lakso M, Pichel JG, Gorman JR, Sauer B, Okamoto Y, Lee E, et al. Efficient in vivo manipulation of mouse genomic sequences at the zygote stage. Proc Natl Acad Sci U S A. 1996;93(12):5860–5. pmid:8650183
  38. 38. Dong Z, Huang M, Liu Z, Xie P, Dong Y, Wu X, et al. Focused screening of mitochondrial metabolism reveals a crucial role for a tumor suppressor Hbp1 in ovarian reserve. Cell Death Differ. 2016.