Generation and characterization of mice with a conditional null allele of the HtrA4 gene

Introduction

The mammalian high temperature requirement factor A4 (HtrA4) is one of four members of the HtrA family of serine proteases. First identified in bacteria as DegP (1), homologs of the HtrA family have been identified in vertebrates, invertebrates and humans (2). All HtrAs share one or multiple highly conserved C-terminal PDZ domains, which bind target proteins and regulate protein-protein interactions, whereas the N-terminus is variable and contains the signal and regulatory sequences (3). Members of the HtrA family are involved in a variety of human diseases (4,5). The most important previous study to date was a genome-wide association study, which identified a marked genetic linkage between specific overexpressed variants of the HtrA1 gene and the wet form of age-associated macular degeneration (6). HtrA1, 2 and 3 have also been implicated in osteoarthritis, cancer, Alzheimer's disease, Parkinson's disease and muscular dystrophy (7–14).

Among the HtrA family members, HtrA4 has rarely been investigated. The HtrA4 protein is predicted to be an oligomeric chaperone protease, which degrades misfolded secretory proteins (15). HtrA4 may exert its action by cleaving within the β-actin sequence to inhibit its ability to form insoluble fibers (16). The transcripts of HtrA4 were upregulated in the placenta of patients with severe pre-eclampsia (17). The role of HtrA4 remains to be fully elucidated in mice. Mouse HtrA4 is a protein of 483 amino acids, which shares 68.18% similarity in amino acid sequence with its human homolog. The mouse HtrA4 and HtrA1 proteins share a similar domain structure (4). The mouse HtrA4 gene is located on chromosome 8 (at 13.70 cM), and consists of nine exons. Exon 1 codes for the insulin-growth-factor-binding and Kazal protease inhibitor domains, exons 3–6 code for a trypsin-like catalytic domain, and exons 7–9 code for the PDZ domains.

The present study aimed to further characterize the cellular functions of HtrA4 in vivo, by generating an HtrA4 conditional allele in mice, which allows the inactivation of HtrA4 through Cre-mediated recombination in a cell-type-specific manner. In addition, the phenotype of the HtrA4 knockout mice was characterized.

Materials and methods

Animals

The mice with an HtrA4 floxed allele were generated by Ozgene (Bentley, Australia). Briefly, a flippase recognition target (FRT)-flanked phosphoglycerate kinase I (PGK)-neomycin cassette was inserted downstream of exon 5 of the HtrA4 gene. The loxP sites were inserted upstream of exon 4, downstream of exon 6, and in between exon 5 and the selection cassette. The construct was incorporated into the genomic DNA of embryonic stem (ES) cells from C57BL/6J mice by electroporation using GenePulser (Bio-rad Laboratories Inc., Hercules, CA, USA) at 230 V/500 µF and subsequent selection. The targeted ES cells were injected into C57BL/6J blastocysts, and the aggregates were transferred into the uterus of recipient mice to produce chimeric mice. The chimeric mice were crossed with C57BL/6J mice to generate HtrA4+/flox-neo mice, which were bred with Rosa26-FlpE mice (provided by Ozgene) to remove the FRT-flanked PGK-neo cassette. The HtrA4+/flox mice were subsequently crossed with Rosa26-Cre mice to create an HtrA4 null allele. All mice were maintained on a C57BL/6J background. The animals (equal male to female ratio) were housed in separate cages at 21±1°C with a 12 h light/dark cycle with access to water and standard rodent pellets, in a conventional, pathogen-free facility at Yale University School of Medicine (New Haven, CT, USA). The present study and all experiments were performed in accordance with the guidelines issued by the Institutional Animal Care and Use Committee at Yale University (New Haven, CT, USA). The genomic DNA was digested with ScaI restriction enzyme (New England Biolabs, Ipswich, MA, USA) and separated by electrophoresis in 0.8% agarose gel (Calbiochem, San Diego, CA, USA) for 12 h prior to Southern blot analyses. The following probes were used for Southern blot analysis of the ES cell clones and HtrA4 alleles in mice: The 3′ probe, a 537 bp polymerase chain reaction (PCR) product targeting the genome sequence beyond the 3′ end of the HtrA4 gene (primers: Forward, 5′-TGG TGT CAC TGG GTC TCC TTA AAGC-3′ and reverse, 5′-AGG GTT AGA TCG GGA TGT TTT AGGG-3′); the en probe, a 695 bp PCR product targeting genomic sequence on exon 8 (PCR primers: Forward, 5′-AAC CAG ATG GGG AAG AGA TAG GCTC-3′ and reverse, 5′-CAGATGCAGATGCAATACAAGCTGC-3′). Primers used for PCR genotyping of the HtrA4 alleles as follows: Primer a, 5′-GCT GGA GTT AGA GGT GGT TGT GGAC-3′ (forward); primer b, 5′-CAG GGA GAT GGT TTA GAA CAG TGG-3′ (reverse); and primer c, 5′-TGC CTG TAA ATG GAA AGC ATGA-3′ (reverse). All primers were obtained from Yale DNA Analysis facility, New Haven, CT, USA).

Gene expression analysis

The relevant tissues were collected from age and sex-matched mice of the wild-type and HtrA4−/− genotypes following intra-cardiac perfusion with cold phosphate-buffered saline (PBS). The tissues were snap frozen and homogenized in liquid nitrogen using a mortar and pestle. The homogenized tissues were incubated with TRIzol (Invitrogen; Thermo Fisher Scientific, Inc., Grand Island, NY, USA) for 30 min on ice, and total RNA was extracted using an RNeasy kit (Qiagen, Hilden, Germany) with optional DNase I treatment (Qiagen) according to the manufacturer's instructions. cDNA synthesis was conducted using the RevertAid First strand cDNA Synthesis kit (Thermo Fisher Scientific, Inc.) following the manufacturer's instruments. Reverse transcription-quantitative (RT-q)PCR was performed by the qPCR facility of Mt. Sinai School of Medicine (New York, NY, USA) with the following thermocycling conditions: 50°C for 2 min and 95°C for 2 min, followed by 40 cycles of 95°C for 15 s, and 60°C for 1 min. The RNA levels were normalized against the endogenous control, gene mouse β-actin. The primers used were: mHtrA4, 5′-CTT GGA TGG CGA CGT GAT TGGT-3′ and 5′-TCT GCA AAG GGG CCT TGC CTT-3′; β-actin, 5′-AGG TGA CAG CAT TGC TTC TG-3′ and 5′-GCT GCC TCA ACA CCT CAAC-3′. All reactions were performed in triplicate and a two-tailed t-test was used to determine statistical significance.

Immunohistochemistry

The mouse tissues were snap-frozen and embedded in optimal cutting temperature compound (Tissue-Tek; Miles, Inc., Elkhart, IN, USA), followed by serial sectioning at 6 µm. The tissue sections were cut at 6 µm using a Leica CM1850 cryostat (Leica Microsystems GmbH, Wetzlar, Germany) were air-dried and fixed in cold acetone for 2 min at room temperature. Following washing in PBS, the tissue sections were blocked for 15 min in 1% BSA in PBS. The slides were incubated with polyclonal goat anti-HtrA4 antibody (1:40; cat. no. sc-87773; Santa Cruz Biotechnology, Inc., Santa Cruz, CA, USA) overnight at 40°C. The tissue sections were washed three times and were incubated for 30 min with Texas Red conjugated rabbit anti-goat immunoglobulin (1:250; cat. no. TI-5000; Vector Laboratories, Burlingame, CA, USA). Following washing, the slides were mounted in VECTASHIELD® mounting medium, containing 4′,6-diamidino-2-phenylindole (Vector Laboratories) and were visualized under a Zeiss Axio Imager M1 fluorescence microscope (Zeiss, Jena, Germany). The tissue sections from HtrA4−/− mice were used as a negative control.

Echocardiography

Echocardiograms were obtained for lightly anesthetized mice (1% isofluorane inhalation) using a Micro-Ultrasounds instrument (Vevo 770 Imaging system; Visual Sonics, Inc., Toronto, ON, Canada). Enlarged two-dimensional views were used to determine a short-axis plane at the level of the papillary muscles and the M-mode was obtained at this level. Measurements were obtained using the Vevo 770 analysis software.

Western blotting

Mouse tissues were harvested from 5-month-old HtrA4−/− mice and their control littermates following intra-cardiac perfusion with cold PBS. The tissues were lysed in radioimmunoprecipitation assay buffer (EMD Millipore, Billerica, MA, USA), supplemented with protease inhibitor cocktails (Roche Diagnostics, Mannheim, Germany), and the protein concentrations were measured by Bradford assay (Bio-Rad Laboratories, Inc.) using a Bio-Rad 415 Visible Spectrophotometer (Bio-Rad Laboratories, Inc.). The lysates were separated using a 12% Mini-protean TGX gel (Bio-Rad Laboratories, Inc.) and electroblotted onto polyvinylidene fluoride membranes (EMD Millipore). The membranes were blocked with 5% non-fat milk and were incubated overnight at 4°C with goat anti-HtrA4 antibody (1:500; Santa Cruz Biotechnology, Inc.). Following washing, the membranes were probed with horseradish peroxidase-conjugated rabbit anti-goat secondary antibody (1:2,500; cat. no. sc-2768; Santa Cruz Biotechnology, Inc.). Western blotting signals were detected by enhanced chemiluminescence (Thermo Fisher Scientific) and exposed on X-ray films. The membranes were stripped using Mild Antibody Stripping Solution (EMD Millipore) and reblotted with mouse anti-β-actin antibody (1:10,000; Sigma-Aldrich, St. Louis, MO, USA) as a loading control.

Statistical analysis

The data are expressed as the mean ± standard error of the mean. The statistical difference between two groups was evaluated using a two-tailed Student's t-test. All statistical analyses were performed using SPSS 17.0 (SPSS Inc., Chicago, IL, USA). P<0.05 was considered to indicate a statistically significant result.

Results

Generation of a conditional null allele of the HtrA4 gene in mice

The targeting construct was generated by flanking exons 4, 5 and 6 with loxP sites (Fig. 1A). Upon Cre excision, these three exons were removed and translation was terminated. A PGK-neo selection cassette, flanked by FRT sites, was inserted between exons 5 and 6. Exons 1–3 were preserved, as their transcripts were overlapping with a non-coding mRNA transcript of the Plekha2 gene. The targeting construct was linearized with AclI and introduced into the Bruce4 ES cell line by electroporation. Following neomycin selection and Southern blot analysis, two ES cell clones with the correct integration were identified. These ES cell clones were injected into blastocysts in order to develop chimeras, and each cell exhibited a successful germline transmission of the HtrA4 conditional allele, which is termed HtrA4flox-neo. To produce the HtrA4flox allele, HtrA4flox−neo/+ mice were bred with Flp deleter transgenic mice to remove the FRT-flanked PGK-neo cassette. The presence of all alleles was confirmed by Southern blotting (data not shown).

Figure 1 Validation of mice harboring the HtrA4 conditional null allele. (A) Schematic representation of the floxed and deleted alleles of HtrA4 conditional null mice. The exons are presented as rectangles. A total of three loxP sites (white triangles) were inserted between exons 3/4, 5/6 and 6/7. The floxed sequences were deleted following Cre excision. The horizontal arrows refer to the primers used for genotyping. (B) Polymerase chain reaction genotyping of HtrA4 conditional null mice was performed. Primers a, b and c were used together for genotyping the tissue samples from the mice. HtrA4+/− mice were obtained by crossing HtrA4+/flox with Rosa26-Cre mice, and HtrA4−/− mice were obtained by intercrossing the HtrA4+/− mice. Primers a and b produced a 311 bp band for the wild-type allele, and a 354 bp band for the HtrA4 floxed allele. Primers a and c produced a 534 bp band for a complete HtrA4 knockout allele. (C) Reverse transcription-quantitative polymerase chain reaction of the gene expression of HtrA4 in organs from wild-type and HtrA4−/− mice. The data are presented as the mean ± standard error of the mean of three individual mice of the identical genotype (*P<0.05 and **P<0.01, compared with the wild-type. HtrA4, high temperature requirement factor A4.

Confirmation of Cre-mediated excision of the HtrA4 gene in mice

To assess the in vivo excision of the HtrA4flox allele, the HtrA4flox/+ mice were bred with Rosa26-Cre transgenic mice to delete the floxed region (18), generating the HtrA4 deletion mutants (Fig. 1A). The complete deletion of exons 4–6 was demonstrated by RT-qPCR, thereby confirming the effectiveness of the Cre excision (Fig. 1B). The HtrA4flox/+;Rosa26-Cre mice were crossed with C57/B6 mice to obtain HtrA4+/− mice lacking the Rosa26-Cre transgene. HtrA4+/− mice were intercrossed to obtain mice homozygotes of HtrA4 deletion (HtrA4−/−; Fig. 1B). The HtrA4−/− mice exhibited normal growth, without any obvious phenotypic differences. Among the surviving pups of the interbreeding of HtrA4+/− mice, the ratio of the identified HtrA4−/− genotype was no less than the expected Mendelian ratio, suggesting a lack of HtrA4 deletion-associated embryonic or neonatal lethality. To examine the expression pattern of HtrA4 and to confirm the loss of transcription of the HtrA4 gene in the HtrA4−/− mice, the total mRNA was extracted from 11 organs (brain, heart, lung, kidney, spleen, bladder, eye, testis, stomach, intestine and skeletal muscle) from the mice and the level of transcription of the HtrA4 gene was determined by RT-qPCR using primers, which were targeted to the floxed region. In wild-type mice, HtrA4 was expressed at a low level in the majority of organs, with the exception of the heart (Fig. 1C). HtrA4 transcription was absent in tissues from the HtrA4−/− mice (Fig. 1C).

Morphology and function of the HtrA4−/− mouse heart

The proteins from mouse tissues were extracted for western blot analysis. Among the 11 organs examined, the HtrA4 protein was only detected in the heart, which is consistent with the results from the mRNA analysis (Fig. 2A). The HtrA4 protein expression pattern was further assessed by immunofluorescence using an antibody targeting the C-terminus of the HtrA protein, together with an antibody against α-smooth muscle actin, the marker for vascular smooth muscle cells. Consistent with the Western blotting results, only the heart revealed a detectable level of protein expression in the coronary vessels, which was absent in the hearts of the HtrA4−/− mice (Fig. 2B). The expression of HtrA4 was restricted in the endothelial cells lining the inside layers of the smooth muscle cells (Fig. 2B). Therefore, the Cre-excised allele represented a null allele of HtrA4. Upon the loss of HtrA4, the size, weight and tissue morphology of the heart, and the heart rate (in beats/min) were demonstrated to be unaffected (Fig. 2C–F). Subsequently, the pumping action of the mouse heart was examined by echocardiography. The diameters of the left ventricle were measured at the papillary muscle level (Fig. 3A). The left ventricular end diastolic and end systolic diameters were similar in the wild-type and HtrA4−/− mice (Fig. 3B). As shown in Fig. 3C, the fractional shortening and ejection fraction, which are major indicators for heart function, were not affected in the heart of the HtrA4−/− mice. In addition, the mass of the left ventricles and cardiac output of the HtrA4−/− mice were also similar to the wild-type mice (Fig. 3D and E). Therefore, the loss of HtrA4 failed to affect the morphology or function of the heart.

Figure 2 Expression of HtrA4 in the mouse heart. (A) Immunoblots were performed to determine the protein expression levels of HtrA4 and β-actin in heart extracts from WT and HtrA4−/− mice. (B) Immunofluorescence staining of HtrA4 and α-smooth muscle actin on cardiac tissue sections from WT and HtrA4−/− mice was performed. Arrows indicate endothelial cells (magnification, ×60). (C) Images of the heart from a 3-month-old HtrA4−/− mouse and its WT littermate were captured. (D) Hematoxylin and eosin staining of a cardiac tissue section from WT and HtrA4−/− mice (magnification, ×10) was performed. (E) The weight of the hearts from 3-month-old WT and HtrA4−/− mice were plotted in a histogram (n=6; P=0.40). (F) The heart rates in beats/min of the 3-month-old WT and HtrA4−/− mice were compared (n=15; P=0.17). n.s., non-significant; WT, wild-type; HtrA4, high temperature requirement factor A4.

Figure 3 Echocardiographic analysis of the cardiac function of HtrA4−/− mice. (A) Short-axis echocardiography demonstrated that the diameters of the left ventricles of the WT and HtrA4−/− mice were similar. The arrows show the size of the intraventricular diameters during diastole. (B) The LVEDD and LVESD of the left ventricles of the WT and HtrA4−/− mice were measured (n=6; P=0.73 and P=0.55, for LVEDD and LVESD, respectively). (C) The EF and FS of the left ventricles of WT and HtrA4−/− mice were determined (n=6; P=0.39 and P=0.34, for %EF and %FS, respectively). (D) The masses of the left ventricle from the WT and HtrA4−/− mice were measured and corrected by echocardiography (n=10; P=0.33). (E) The cardiac output of the WT and HtrA4−/− mice was determined (n=9; P=0.61). The results of these experiments were n.s. comparing WT with HtrA4−/− mice. EF, ejection fraction; FS, fractional shortening; LVEDD, left ventricular end diastolic diameter; LVESD, left ventricular end systolic diameter; HtrA4, high temperature requirement factor A4; n.s., non-significant; WT, wild-type.

Morphology and function of the HtrA4−/− mouse placenta

The embryonic development of the HtrA4−/− mice was analyzed. At embryonic day 13.5, the HtrA4−/− embryos, including the yolk sacs, exhibited a similar developmental pattern compared with their wild-type littermates (Fig. 4A). No HtrA4 expression was detectable by immunofluorescence at this stage of embryonic development, including in the embryonic heart. The HtrA4 transcript has been detected in human placenta (GenBank accession no. BC057765), therefore, the placenta of wild-type females with wild-type embryos and HtrA4−/− females with HtrA4−/− embryos were examined. The macroscopic morphology of the wild-type and HtrA4−/− placentas was similar (Fig. 4B). A positive staining of HtrA4 was observed only on the decidual layer of the placenta of wild-type mice, and not on the HtrA4−/− placenta (Fig. 4C). Concerning the sections with hematoxylin and eosin staining, HtrA4−/− placentas demonstrated normal tissue structure and cell morphology (Fig. 4D). In addition, intercrossing of the HtrA4−/− mice produced a similar number of offsprings from each litter as the intercrossing of wild-type mice (Fig. 4E), indicating a normal placental function.

Figure 4 Expression of HtrA4 in the mouse placenta. (A) E13.5 WT and HtrA4−/− embryos and yolk sacs. (B) The placenta of E13.5 WT embryo/WT mother and HtrA4−/− embryo/HtrA4−/− mother are illustrated. (C) Immunofluorescence staining of HtrA4 in the mouse placenta of E13.5 WT embryo/WT mother and the HtrA4−/− embryo/HtrA4−/− mother are shown (magnification, ×20) The red coloration represents the staining taken up by HtrA4. (D) Hematoxylin and eosin staining of of the mouse placenta of E13.5 WT embryo/WT mother and HtrA4−/− embryo/HtrA4−/− mother (magnification, ×10) was performed. (E) The fertility of the WT/WT and HtrA4−/−/HtrA4−/−-crossed mice was examined. Each bar represents the mean ± standard error of the number of pups per litter from intercrossing of wild-type and HtrA−/− mice (n=15, P=0.72). n.s., non-significant;. WT, wild-type; HtrA4, high temperature requirement factor A4.

Discussion

The HtrA family of proteins perform vital roles in physiological processes, including apoptosis and cell signaling (15,19). Previously, HtrA proteins 1, 2 and 3 were identified as potential drug targets for the treatment of cancer and neurodegenerative disorders (4,5,19). Although the protein structure of HtrA4 is similar to the other three family members, HtrA4 has received little attention. In the present study, a conditional null HtrA4 allele in mice was successfully generated, and the phenotype of the HtrA4-deficient mice was characterized.

Although the gene inactivation of HtrA4−/− was successfully achieved, no obvious differences in the phenotype between HtrA4−/− adult mice and embryos was identified in the present study. The function of HtrA4 under normal conditions may be redundant, however, it is possible that HtrA4 may be activated in a pathological situation. Similar to human HtrA4, mouse HtrA4 was also expressed in the placenta. In the placenta of patients with pre-eclampsia, the protein expression of HtrA4 was increased (17). In addition, HtrA4 is a target gene of the placental transcription factor, glial cells missing 1 (20). HtrA4 represses the fusogenic activity of syncytin-1 and promotes trophoblast invasion (20). It is possible that HtrA4 works in association with the other HtrA family members. HtrA1 was upregulated in the mouse model of arthritis, and contributed to cartilage degradation (8). Another member of the HtrA family, HtrA2, was increased in the rat testis in response to experimental cryptorchidism (21). The mouse model described in the present study may be useful in studying the roles of HtrA4 in pathogenesis (17,19,20).

In the present study, it was observed that the mouse HtrA4 protein is specifically expressed in the endothelial cells of coronary vessels. However, a loss of HtrA4 failed to induce abnormalities in the morphology and function of the heart. The protein structure of HtrA4 is very similar to that of HtrA1, which is highly expressed in endothelial cells, smooth muscle cells and perivascular fibroblasts (22). In the vascular system, HtrA1 regulates transforming growth factor-β (TGF-β) signaling, and is involved in the pathogenesis of cerebral autosomal recessive arteriopathy with subcortical infarcts and leukoencephalopathy (23). The N-termini of the HtrA1 and HtrA4 proteins contain predicted cleavable signal peptides and a fragment of insulin growth factor-binding protein (IGFBP)7 (15). IGFBP and kinase interaction domains in HtrA1 and HtrA4 revealed a similarity to follistatin, which is a potent antagonist of TGF-β signaling (24–26). In addition, HtrA1 inhibited TGF-β signaling under a variety of cellular conditions (27). Therefore, HtrA4 may also interact with the TGF-β family of proteins, although its function may be compensated by HtrA1.

Taken together, the conditional null HtrA4 allele in mice was generated and validated by effective Cre excision, which led to the loss of transcription and protein expression levels of HtrA4. This novel mouse line provides opportunities to address the tissue and cell type-specific roles of HtrA4 under different physiological and pathological conditions.

Acknowledgments

The present study was funded by the Rosebay Medical Foundation and Yale Medical School Dean's Research Fund, the National Natural Science Foundation of China (grant no. 81370269), and the Shandong Taishan Scholarship. The authors would like to thank Professor Frank Giordano, Dr Yan Huang and Mr. Steve Viviano of Yale University for their scientific input and technical assistance.

References