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The Ron/STK receptor tyrosine kinase is essential for peri-implantation development in the mouse
Rebecca S. Muraoka,1 William Y. Sun,2 Melissa C. Colbert,3 Susan E. Waltz,2 David P. Witte,4 Jay L. Degen,2 and Sandra J. Friezner Degen2
1Graduate Program in Developmental Biology, University of Cincinnati College of Medicine, Cincinnati, Ohio 45229-3039, USA2Division of Developmental Biology,3Division of Molecular Cardiovascular Biology, and4Division of Pathology, Children’s Hospital Research Foundation, Cincinnati, Ohio 45229-3039, USA
Address correspondence to: Sandra J.F. Degen, Division of Developmental Biology, Children’s Hospital Research Foundation, 3333 Burnet Avenue, Cincinnati, Ohio 45229-3039, USA. Phone: (513) 636-4816; Fax: (513) 636-4317; E-mail: [email protected]
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1Graduate Program in Developmental Biology, University of Cincinnati College of Medicine, Cincinnati, Ohio 45229-3039, USA2Division of Developmental Biology,3Division of Molecular Cardiovascular Biology, and4Division of Pathology, Children’s Hospital Research Foundation, Cincinnati, Ohio 45229-3039, USA
Address correspondence to: Sandra J.F. Degen, Division of Developmental Biology, Children’s Hospital Research Foundation, 3333 Burnet Avenue, Cincinnati, Ohio 45229-3039, USA. Phone: (513) 636-4816; Fax: (513) 636-4317; E-mail: [email protected]
Find articles by Sun, W. in: JCI | PubMed | Google Scholar
1Graduate Program in Developmental Biology, University of Cincinnati College of Medicine, Cincinnati, Ohio 45229-3039, USA2Division of Developmental Biology,3Division of Molecular Cardiovascular Biology, and4Division of Pathology, Children’s Hospital Research Foundation, Cincinnati, Ohio 45229-3039, USA
Address correspondence to: Sandra J.F. Degen, Division of Developmental Biology, Children’s Hospital Research Foundation, 3333 Burnet Avenue, Cincinnati, Ohio 45229-3039, USA. Phone: (513) 636-4816; Fax: (513) 636-4317; E-mail: [email protected]
Find articles by Colbert, M. in: JCI | PubMed | Google Scholar
1Graduate Program in Developmental Biology, University of Cincinnati College of Medicine, Cincinnati, Ohio 45229-3039, USA2Division of Developmental Biology,3Division of Molecular Cardiovascular Biology, and4Division of Pathology, Children’s Hospital Research Foundation, Cincinnati, Ohio 45229-3039, USA
Address correspondence to: Sandra J.F. Degen, Division of Developmental Biology, Children’s Hospital Research Foundation, 3333 Burnet Avenue, Cincinnati, Ohio 45229-3039, USA. Phone: (513) 636-4816; Fax: (513) 636-4317; E-mail: [email protected]
Find articles by Waltz, S. in: JCI | PubMed | Google Scholar
1Graduate Program in Developmental Biology, University of Cincinnati College of Medicine, Cincinnati, Ohio 45229-3039, USA2Division of Developmental Biology,3Division of Molecular Cardiovascular Biology, and4Division of Pathology, Children’s Hospital Research Foundation, Cincinnati, Ohio 45229-3039, USA
Address correspondence to: Sandra J.F. Degen, Division of Developmental Biology, Children’s Hospital Research Foundation, 3333 Burnet Avenue, Cincinnati, Ohio 45229-3039, USA. Phone: (513) 636-4816; Fax: (513) 636-4317; E-mail: [email protected]
Find articles by Witte, D. in: JCI | PubMed | Google Scholar
1Graduate Program in Developmental Biology, University of Cincinnati College of Medicine, Cincinnati, Ohio 45229-3039, USA2Division of Developmental Biology,3Division of Molecular Cardiovascular Biology, and4Division of Pathology, Children’s Hospital Research Foundation, Cincinnati, Ohio 45229-3039, USA
Address correspondence to: Sandra J.F. Degen, Division of Developmental Biology, Children’s Hospital Research Foundation, 3333 Burnet Avenue, Cincinnati, Ohio 45229-3039, USA. Phone: (513) 636-4816; Fax: (513) 636-4317; E-mail: [email protected]
Find articles by Degen, J. in: JCI | PubMed | Google Scholar
1Graduate Program in Developmental Biology, University of Cincinnati College of Medicine, Cincinnati, Ohio 45229-3039, USA2Division of Developmental Biology,3Division of Molecular Cardiovascular Biology, and4Division of Pathology, Children’s Hospital Research Foundation, Cincinnati, Ohio 45229-3039, USA
Address correspondence to: Sandra J.F. Degen, Division of Developmental Biology, Children’s Hospital Research Foundation, 3333 Burnet Avenue, Cincinnati, Ohio 45229-3039, USA. Phone: (513) 636-4816; Fax: (513) 636-4317; E-mail: [email protected]
Find articles by Degen, S. in: JCI | PubMed | Google Scholar
Published May 1, 1999 - More info
J Clin Invest. 1999;103(9):1277–1285. https://doi.org/10.1172/JCI6091.
© 1999 The American Society for Clinical Investigation
Received: December 17, 1998; Accepted: March 26, 1999
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Methods
Disruption of the mouse Ron gene. In construction of the targeting vector, exons 1–14 and part of exon 15 of the mouse Ron gene, isolated from a 129/Ola genomic library (15), were replaced by a 6.0-kb hypoxanthine phosphoribosyltransferase (HPRT) expression cassette, which also serves as a positive selection marker (Figure 1a). A 2.0-kb XbaI-BamHI fragment from the 5′ flanking sequence was used as the short arm of the targeting vector and was cloned into the XbaI and BamHI sites of a Bluescript plasmid (Stratagene, La Jolla, California, USA). A 3.1-kb SmaI fragment from the 3′ end of the mouse Ron gene, including part of exon 15 and exons 16–18, was used as the long arm of the targeting vector and was cloned into the SmaI site of the Bluescript plasmid containing the short arm. The HPRT expression cassette was cloned into the BamHI site of the Bluescript plasmid. A 2.0-kb cassette coding for the herpes simplex virus thymidine kinase gene (HSV-tk) was cloned into the HindIII and SalI sites of the Bluescript vector and used as a negative selection marker. The targeting vector was linearized with NotI prior to electroporation. The linearized targeting vector was introduced into mouse embryonic stem (ES) cells as previously described (24).
Figure 1Disruption of the mouse Ron gene in embryonic stem (ES) cells and mice. (a) Schematic representation and partial restriction map of the targeting vector (top) used to disrupt the endogenous mouse Ron gene (middle). The predicted organization of the targeted mouse Ron gene following homologous recombination is also shown (bottom). The targeting vector contains sequences homologous to the endogenous Ron gene (gray bars) flanking the HPRT expression cassette (white bar). The HSV-tk gene flanks the targeting vector at the 3′ end (dark gray bar). The exons of the endogenous Ron gene are numbered (1–19, black boxes). The primers used for PCR genotyping are indicated with arrows and are numbered 1–6. The probe used for Southern blot analysis is shown below the endogenous Ron gene. The BamHI fragments of genomic DNA that are complementary to the probe are indicated with the expected sizes (4.7 kb and 3.6 kb). B, BamHI. H, HindIII. S, SalI Sm, SmaI. X, XbaI. (b) Southern blot analysis of BamHI–digested DNA from selection-resistant ES cell clones. The wild-type allele (WT) is represented by a 4.7-kb fragment, while the targeted allele (Tg) is represented by a 3.6-kb fragment. ES9 was included as a wild-type control. (c) Southern blot analysis of BamHI–digested DNA from a single litter generated from a Ron+/– intercrossing. Offspring were genotyped at 7 days postnatal. Of the 12 littermates shown, 8 are Ron+/– (+/–) and 4 are Ron+/+ (+/+). (d) Genotype analysis by PCR of a single litter of E3.5 blastocysts generated from a Ron+/– intercrossing. The wild-type allele is represented by a 523-bp product generated from primers 1 and 2 (see a); the targeted allele is represented by a 274-bp product generated from primers 5 and 6.
Genotype analysis. Southern blot analysis of BamHI–digested genomic DNA from selection-resistant ES cell clones or mouse tail biopsies was performed as described previously (24). The probe used for Southern blot analysis is derived from a region of the Ron gene that lies outside the proposed region of homologous recombination. Alternatively, genotype analysis on DNA from tail or ear biopsy was performed using a multiplex PCR reaction (24). The endogenous Ron allele was detected using primers 1 (5′-CCCTGCCGACTGCTGCCTAAGGACT-3′, exon 5) and 2 (5′-AGAGATGGCTTCCACTCGGAAGTGC-3′, exon 6), generating a 523-bp product (Figure 1a). The targeted Ron allele was detected by primers 3 (5′-CGTCAGGCCCGAGCCCGCCGGCCCGGGTCCC-3′, inside the HPRT expression cassette) and 4 (5′-CTGTACCTGCTCCGGAGGCACACTC-3′, exon 19, outside the region of homologous recombination), resulting in a 3.56-kb PCR product (Figure 1a). Once the targeted allele had been established in the F1 offspring by Southern blot analysis, primers 5 (5′-TATTACCAGTGAATGTTTGTCAGCAGTTCCC-3′, inside the HPRT expression cassette) and 6 (5′-TGTACCAGGGCACCGGAGAGACCGA-3′, Ron 5′ flanking sequences) were used, generating a 274-bp product (Figure 1a).
Generation of mouse colonies. Targeted ES cells were injected into C57Bl/6 blastocysts and transferred into pseudopregnant C57Bl/6 females to generate chimeric founders (performed by the ES Cell Gene Altered Mouse Service at the University of Cincinnati College of Medicine). Chimeric founders were crossed to NIH Black Swiss mice to generate F1 offspring. Hemizygous (Ron+/–) F1 males were crossed to NIH Black Swiss females to generate F2 offspring. Ron+/– F2 siblings were intercrossed to generate F3 offspring. All experiments described were performed in F3 offspring of the 129/Black Swiss mixed genetic background mice, except where indicated. For the 129/CD-1 mixed genetic background experiment, chimeric founders were crossed with CD-1 females to generate F1 offspring. CD-1/129 F1 offspring were intercrossed to produce the experimental F2 generation. The targeted Ron allele was also introduced into a C57Bl/6 background by crossing a chimeric founder with a C57Bl/6 mouse, followed by backcrossing to C57Bl/6 mice for 6 generations.
Developmental analysis. Offspring from timed matings between Ron+/– mice were isolated at specific developmental time points (Table 1). Prior to parturition, embryos were dissected cleanly away from potentially contaminating maternal tissue. Embryos isolated at E5.5 through E12.5 were genotyped by Southern blot analysis of whole-embryo DNA, or alternatively, genotyped by PCR analysis of yolk sac or whole-embryo DNA. For PCR analysis, the yolk sacs or embryos were digested in 10–100 μl of digestion buffer (500 mM KCl, 100 mM Tris-HCl [pH 8.3], 0.1 mg/mL gelatin, 0.45% Nonidet P-40, 0.45% Tween-20, and 0.1 mg/mL proteinase K) for 16 hours at 55°C, and the lysate was used for PCR analysis. Blastocysts isolated at E3.5 were flushed from uterine horns and individually cultured for 1 week in DMEM supplemented with 15% FBS and 4 mM L-glutamine.
Histologic analyses. Pregnant mice from timed matings between Ron+/– mice at E6.5 and E7.5 were sacrificed, and the entire gravid uterus was harvested, fixed in 10% buffered formalin, and cut into segments prior to embedding in paraffin. The entire embedded uterine segments were serially sectioned, mounted on slides, and stained with hematoxylin and eosin. All slides were examined microscopically.
In situ hybridization. Decidua containing the undisturbed mouse embryos were isolated at E7.5 and fixed in 4% paraformaldehyde in PBS (pH 7.4). Blastocysts were flushed from uterine horns, fixed directly into 4% paraformaldehyde, and centrifuged directly onto slides. A 35S-labeled, 1,100-nucleotide Ron antisense RNA probe from the 3′ end of mouse Ron cDNA and a 900-nucleotide Ron sense RNA control were synthesized and individually hybridized to cryosections of fixed tissue as described previously (15, 25).
Northern and Western blot analysis. Freshly harvested mouse tissues were homogenized in 200 mM Tris-HCl (pH 8.0), 0.2% SDS, and 0.5% Triton X-100, and centrifuged at 15,000 rpm for 30 minutes at 4°C. Protein (20 μg) from the supernatant was analyzed for the presence of HGFL or Ron by Western blot analysis as described (26). HGFL was detected using a previously characterized rabbit polyclonal antibody against its single-chain form (10), and Ron was detected using a goat polyclonal antibody against the extracellular domain of mouse Ron (R&D Systems Inc., Minneapolis, Minnesota, USA). Specific antibody binding was visualized using a chemiluminescent system (ECL; Amersham Life Sciences Inc., Arlington Heights, Illinois, USA). For Northern blot analysis, total RNA was isolated from freshly harvested mouse liver, size fractionated, and transferred to a nylon membrane (GeneScreen Plus; Du Pont NEN Research Products, Boston, Massachusetts, USA). A full-length mouse HGFL cDNA (8) was labeled with [α-32P]dCTP and used as a probe, as described previously (24).
Production of HGFL. The production of recombinant HGFL was carried out by transfection of Chinese hamster ovary (CHO) cells with wild-type human HGFL cDNA cloned into pcDNA3, as described (26). This recombinant human HGFL has been previously shown to cause the activation of mouse peritoneal macrophages in a manner that is identical to the action of mouse HGFL (26).
Isolation, culture, activation, and measurement of NO of mouse peritoneal macrophages. Adult mouse peritoneal cavities were lavaged with 10 mL sterile, serum-free DMEM. Cells were centrifuged and plated in 35-mm wells with 106 cells per well. Peritoneal macrophages were treated with culture media from wild-type CHO cells or CHO cells expressing human HGFL. Cell morphology was observed at timed intervals thereafter using a phase-contrast microscope. Cells displaying a compact, spindle-shaped morphology with elongated cytoplasmic processes were considered activated. The percentage of activated macrophages per field was determined by blinded counting. The synthesis of NO by peritoneal macrophages was determined by measuring levels of nitrite, a stable by-product of NO, in the serum-free culture media of plated macrophages. The cells were treated with 1 μg/mL LPS from Escherichia coli (Sigma Chemical Co., St. Louis, Missouri, USA) and/or 100 U/mL recombinant mouse IFN-γ (Sigma Chemical Co.) in the presence or absence of 50–100 ng/mL human HGFL (see above). Culture media (100 μL) from the stimulated macrophages were added to 100 μl Greiss reagent (1% sulfanilamide and 0.1% naphthylethylene diaminehydrochloride in 2.5% H3PO4; Promega Corp., Madison, Wisconsin, USA). The absorbance of the resulting colorimetric reaction was measured at 540 nm. The nitrite levels in culture media were calculated by comparison with a standard curve. All samples were assayed in triplicate.
Challenge with LPS. Wild-type or Ron+/– mice were administered LPS (25 μg/g; Sigma Chemical Co.) in sterile PBS (1 mg/mL) by peritoneal injection (27). Mouse viability was determined at 24-hour intervals for 14 days following the administration of LPS.
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Results
Disruption of the mouse Ron gene in ES cells and mice. Disruption of the mouse Ron gene was performed in ES cells by homologous recombination (Figure 1a). Targeting resulted in the deletion of 300 bases upstream of exon 1 through the middle of exon 15, a region that encompasses the entire extracellular domain and transmembrane domain of the Ron gene product. Southern blot analysis identified 9 ES cell clones that contained the targeted Ron allele out of 114 selection-resistant clones screened (Figure 1b). Three independently derived ES clones were used to generate chimeric founders that were found to transmit the targeted Ron allele to their offspring.
Homozygous loss of Ron is embryonic lethal prior to E6.5. To examine the consequences of the targeted loss of both Ron alleles, hemizygous siblings (Ron+/–) were intercrossed and the genotypes of the progeny were determined by Southern blot analysis (Figure 1c). The transmission of the mutant Ron allele did not follow a Mendelian pattern of inheritance (Table 1). In total, 33.1% of the pups were wild-type (Ron+/+), while 66.9% of the pups were Ron+/–. No homozygous mutant (Ron–/–) mice were identified, indicating that the expected proportion of Ron–/– littermates dies at some point during embryonic development. This intrauterine death was observed for mice derived from all 3 ES cell lines used to generate gene-targeted mice.
To precisely identify the time frame in which Ron–/– embryos undergo developmental failure, litters from Ron+/– intercrosses were dissected cleanly from the uterus, microscopically examined, and genotyped at specific time points during gestation (Table 1). As early as E7.5, the ratio of Ron+/+ to Ron+/– embryos was approximately 1:2 (Table 1), but Ron–/– embryos were not identified at this or later time points, suggesting that Ron–/– embryos die prior to E7.5. The Ron+/– embryos were phenotypically indistinguishable from their wild-type littermates upon gross morphologic examination.
To determine if Ron–/– embryos develop to at least the blastocyst stage, at E3.5 blastocysts were flushed from the uterine horns of Ron+/– females bred to Ron+/– males, and individually cultured. The cultured blastocysts were monitored daily over a period of 7 days and then genotyped by PCR analysis (Figure 1d). At this stage of development, all 3 possible genotypes were observed, and the expected Mendelian ratio of inheritance was recovered (Table 1). Ron–/– embryos were not morphologically distinguishable from their Ron+/+ or Ron+/– counterparts. Ron–/– blastocysts were able to hatch from the zona pellucida in culture, and the trophoblast outgrowths were able to attach to the tissue culture plate. The inner cell masses of Ron–/– blastocysts appeared normal and proliferated at approximately the same rate as the inner cell masses derived from Ron+/+ blastocysts, as determined by daily visual observation of blastocyst growth.
Analysis of embryos collected from Ron+/– breeding pairs later in gestation indicated that Ron–/– embryos continued to develop at least until E5.5. The frequency of Ron–/– embryos at E5.5 was found to be 20%, close to what is expected based on a normal Mendelian transmission pattern. In contrast, at E6.5 only 4.0% of the embryos analyzed were found to be Ron–/– (Table 1). This frequency falls below the expected Mendelian ratio of inheritance for the mutant Ron allele (P < 0.003 in χ2 analysis). The observation that the ratio of Ron+/– to Ron+/+ is approximately 2:1 suggests that there is little or no loss of Ron+/– embryos at this developmental stage. This was further determined by detailed histologic analyses of the uterine contents of pregnant mice from hemizygous matings. At E6.5, 88 implantation sites were analyzed by complete serial section analysis of the harvested uterine specimens. These analyses showed that despite the evidence of decidualization, only 82 sites were found to contain embryos. The other sites showed no residual evidence of any embryonic structures, suggesting that despite induction of the decidual reaction in the uterine mucosa, the embryos failed to successfully implant. Of the identified embryos, none showed any degenerative changes or histologic abnormalities. The presence of Ron–/– embryos at E5.5 and E6.5 demonstrates that Ron–/– embryos are able to implant and initiate decidualization of the uterus, but loss of the null embryos appears to start to occur shortly after the initiation of implantation.
Prenatal death is observed in various genetic backgrounds. To explore the potential influence of genetic background on the Ron–/– phenotype, chimeric founders were crossed with CD-1 females, generating Ron+/– offspring with a mixed genetic background of CD-1/129. When these heterozygous siblings were mated, it was again found that Ron+/+ and Ron+/– offspring were present at a ratio of approximately 1:2, but no term Ron–/– mice were present (Table 1). This intrauterine death was also observed in mice with a highly enriched C57/Bl6 background (6 generations of backcrossing). Therefore, the intrauterine death of Ron–/– embryos is consistently observed across various genetic backgrounds.
Ron is expressed at the blastocyst stage. The fact that Ron–/– embryos fail around E6.5 would imply that Ron is both present and of biologic importance prior to this point in development. To determine if Ron is expressed prior to this developmental roadblock, Ron expression was examined by in situ hybridization. At E3.5, blastocysts are composed of 2 distinct cell types: the cells of the trophectoderm and those of the inner cell mass. Ron expression was observed in the trophectodermal cells, a cell population that represents the earliest extraembryonic structure (Figure 2, a and b). The inner cell mass, which contributes to the embryo proper, was completely devoid of Ron expression. This exclusively extraembryonic trend of Ron expression continued at least through E7.5 of peri-implantation development (Figure 2). Therefore, Ron expression commences as early as E3.5, which precedes the developmental failure of Ron–/– embryos.
Figure 2In situ hybridization of wild-type embryos at E3.5 and E7.5. The embryos were stained with hematoxylin and eosin and hybridized with a probe complementary to the 3′ end of the mouse Ron transcript. Two distinct orientations of the blastocysts are shown: (a) orientation highlighting the trophectoderm of the blastocysts, and (b) orientation highlighting the inner cell mass. The light-field exposure is shown in the left panels, and the dark-field exposure is shown in the right panels. The bottom panel shows the dark-field exposure of a wild-type embryo isolated with the intact decidua at E7.5. TPHD, trophectoderm. ICM, inner cell mass. EE, extraembryonic tissue. E, embryonic tissue.
HGFL is present in the uterus at E4.5–E6.5. Based on the fact that Ron–/– embryos fail prior to E6.5, it was of interest to determine if the ligand for Ron, HGFL, is present in uterine tissue at this stage. Expression of HGFL was measured by Western blot analysis of uterine tissue from pregnant wild-type females at 4.5 and 6.5 days postcoitus, and from virgin females (Figure 3a). HGFL is present in mouse uterine tissue at both days 4.5 and 6.5 of pregnancy. The nongravid uterine tissue was devoid of detectable HGFL. Although these results do not establish that HGFL is synthesized within uterine tissue, it is clear that HGFL is present in the uterine environment at a time when Ron is expressed within the embryonic trophectoderm and when development is terminated in Ron–/– embryos. Therefore, a critical developmental signaling system may link maternal HGFL and embryonic Ron.
Figure 3Expression of HGFL in the liver and maternal uterus. (a) Expression of HGFL in the pregnant uterus. Uterine tissue was dissected from pregnant wild-type females at 4.5 and 6.5 days postcoitus, or from virgin (0) females. Liver was dissected from virgin females as a positive control for HGFL expression. Proteins were electrophoresed and Western blot analysis was performed. The expected size of HGFL (80 kDa) is indicated, as are the sizes of the molecular weight markers. The identity of the higher-molecular-weight band is unknown, but this band does not correspond to the size expected for HGFL. (b) Expression of Ron in the liver of Ron+/+ and Ron+/– mice. Western blot analysis was performed on protein isolated from the livers of wild-type and Ron+/– mice. The expected size of Ron (∼170 kDa) is indicated, as are the sizes of the molecular weight markers. (c) Expression of HGFL RNA in the livers of Ron+/+ and Ron+/– mice. Total RNA was isolated from the livers of Ron+/+ and Ron+/– mice and analyzed for expression of HGFL mRNA by Northern blot analysis. The position of the mouse HGFL mRNA is indicated, as are the positions of the 18S and 28S ribosomal RNAs. The ethidium bromide–stained agarose gel is shown (at right) to indicate the equivalent loading of samples.
Defects in morphologic changes in macrophages in Ron+/–mice. Ron+/– mice displayed no obvious abnormalities, as determined by gross morphology, weight gain, survival, and fertility (data not shown). Ron was expressed at approximately 75% of wild-type levels in Ron+/– mouse liver (Figure 3b). Similar levels were seen in colon and lung tissue from Ron+/– mice (data not shown). Therefore, it appears that a reduction in Ron gene dosage does not present a significant liability to the overall health of unchallenged mice. To explore the possibility of a gene dosage effect on specific cellular functions, macrophage activation was compared in Ron+/+ and Ron+/– mice. The total number of resident peritoneal macrophages derived from Ron+/– mice did not differ from the number derived from Ron+/+ mice (data not shown). However, macrophages derived from Ron+/+ and Ron+/– mice differed dramatically in regard to HGFL-produced macrophage activation, as judged by morphologic changes during activation from cells with large, round nuclei to spindle-shaped cells with condensed, dark nuclei (Figure 4a). Without stimulation by HGFL, the background level of macrophage activation was similar in macrophages derived from Ron+/+ and Ron+/– mice (Figure 4, a and b). The presence of HGFL stimulated an increase in the number of activated macrophages in both Ron+/+ and Ron+/– cultures. However, the level of HGFL-induced macrophage activation was dependent on the dosage of the Ron gene, with considerably fewer Ron+/– macrophages becoming activated in response to HGFL. The differential in the number of activated macrophages was maintained through a 24-hour period, suggesting that the difference in levels of activation was not due to a delay in the response of Ron+/– macrophages to HGFL. In addition, HGFL-activated Ron+/– macrophages are morphologically distinct from their wild-type counterparts in that they do not condense or form spindles to the same degree as the wild-type macrophages; however, they still extend long cytoplasmic processes similar to those of the wild-type macrophages (Figure 4a).
Figure 4Analysis of macrophage activation, NO synthesis, and septic shock. (a) Resident peritoneal macrophages isolated from Ron+/+ or Ron+/– mice (–HGFL) were treated with 100 ng/mL recombinant human HGFL (+HGFL) and analyzed for morphologic changes, including nuclear condensation, spindle formation, and cytoplasmic elongations. (b) Resident peritoneal macrophages were stimulated with media containing 100 ng/mL recombinant human HGFL (gray bars), or with control media (black bars). Macrophage activation was determined by blinded counting at 1–3 hours following HGFL treatment. Results are presented as the number of activated macrophages per total number of macrophages. Error bars represent the SD (P < 0.009, calculated using the Mann-Whitney test; n = 12 for each genotype; each experiment was repeated 3 times). (c) Resident peritoneal macrophages were stimulated with 1 μg/mL LPS and 100 U/mL IFN-γ in the absence (hatched bars) or presence (gray bars) of 100 ng/mL recombinant human HGFL, or left untreated (black bars). All NO values were calculated in reference to the amount of NO in untreated wild-type macrophages, which was set at a value of 1. The levels of NO in untreated macrophages from Ron+/+ and Ron+/– mice did not differ significantly. All values represent the average values obtained from 3 sets of mice (n = 12 for each genotype). Each experiment was assayed in triplicate. Error bars represent the SD (P < 0.03, calculated using the Mann-Whitney test). (d) Increased susceptibility of Ron+/– mice to LPS-induced septic shock. Ron+/+ or Ron+/– mice were administered 25 μg/g LPS by peritoneal injection and then monitored daily for mortality over a 14-day period. Results are presented as “cumulative survival,” which is the number of surviving mice per total number of mice treated with LPS (n = 8 for each genotype). The 2 groups of mice were compared by Kaplan-Meier survival analysis and were found to be statistically different, with a P value of 0.0011 by the Mantel-Cox test.
Defective NO regulation and increased susceptibility to septic shock in Ron+/– mice. To determine whether Ron gene dosage altered HGFL-induced NO synthesis, the levels of nitrite (a stable by-product of NO) released into the media were compared in cultures of peritoneal macrophages derived from Ron+/+ or Ron+/– mice. LPS in the presence of INF-γ increased the levels of NO released by macrophages almost 40-fold, regardless of whether the cells were derived from Ron+/+ or Ron+/– mice (Figure 4c). The presence of HGFL reduced NO release markedly. However, the HGFL-mediated suppression of NO release was distinctly dependent on gene dosage, with Ron+/+ macrophages releasing far less NO than Ron+/– macrophages in the presence of HGFL.
NO plays a critical role in the inflammatory response, and elevated NO levels have been implicated in tissue damage and endotoxic shock in mice. Therefore, Ron+/– mice were tested for their susceptibility to LPS-induced death. Treatment with LPS was not lethal to the majority of Ron+/+ mice, with 87.5% of Ron+/+ mice surviving beyond 14 days (Figure 4d). In striking contrast, this same dose of LPS was lethal to the majority of Ron+/– mice, with only 12.5% of Ron+/– mice surviving.
HGFL expression is unaltered in Ron+/– mice. To determine if the there is any compensatory upregulation of HGFL expression in Ron+/– mice, hepatic expression of HGFL was examined in both Ron+/+ and Ron+/– mice. Northern blot analysis of hepatic RNA demonstrated that expression of HGFL is essentially identical in Ron+/+ and Ron+/– mice (Figure 3c). Therefore, differences observed in macrophage function are not related to altered levels of HGFL in Ron+/– mice.
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