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Experimental Diabetes Research
Volume 2009 (2009), Article ID 835650, 10 pages
http://dx.doi.org/10.1155/2009/835650
Research Article

Sequence Variation and Expression of the Gimap Gene Family in the BB Rat

1Diabetes and Endocrinology Research Center, University of Washington, 815 Mercer Street, Building A, S130, Seattle, WA 98109, USA
2Department of Biological and Chemical Sciences, Salish Kootenai College, 58138 Hwy 93, Pablo, P.O. Box 70, MT 59855, USA
3Department of Clinical Sciences, Clinical Research Center, Lund University, Entrance 72, Building 91:10, 20502 Malmö, Sweden
4Department of Medicine, University of Washington, 1959 N.E. Pacific Street, Seattle, P.O. Box 357710, WA 98195, USA
5Department of Comparative Medicine, University of Washington, 1959 N.E. Pacific Street, Seattle, P.O. Box 357190, WA 98195, USA
6Department of Internal Medicine, University of Iowa, 375 Newton Road, 3111B MERF, Iowa City, IA 52242, USA

Received 9 December 2008; Accepted 8 February 2009

Academic Editor: Anjan Kowluru

Copyright © 2009 Elizabeth A. Rutledge et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

Positional cloning of lymphopenia (lyp) in the BB rat revealed a frameshift mutation in Gimap5, a member of at least seven related GTPase Immune Associated Protein genes located on rat chromosome 4q24. Our aim was to clone and sequence the cDNA of the BB diabetes prone (DP) and diabetes resistant (DR) alleles of all seven Gimap genes in the congenic DR.lyp rat line with 2 Mb of BB DP DNA introgressed onto the DR genetic background. All (100%) rats are lymphopenic and develop type 1 diabetes (T1D) by 84 days of age while rats remain T1D and lyp resistant. Among the seven Gimap genes, the Gimap5 frameshift mutation, a mutant allele that produces no protein, had the greatest impact on lymphopenia in the rat. Gimap4 and Gimap1 each had one amino acid substitution of unlikely significance for lymphopenia. Quantitative RT-PCR analysis showed a reduction in expression of all seven Gimap genes in spleen and mesenteric lymph nodes when compared to . Only four; Gimap1, Gimap4, Gimap5, and Gimap9 were reduced in thymus. Our data substantiates the Gimap5 frameshift mutation as the primary defect with only limited contributions to lymphopenia from the remaining Gimap genes.

1. Introduction

Lymphopenia (lyp) is a prerequisite for spontaneous type 1 diabetes (T1D) in the BioBreeding (BB) diabetes prone (DP) rat [1]. Positional cloning of the lyp gene revealed a frame shift mutation in Gimap5 (previously known as Ian5 or Ian4L1). Gimap5 is a member of at least seven related GTPase Immune Associated Protein (Gimap) genes located within 150 Kilobases (Kb) on rat chromosome (RNO) 4 [2, 3]. rats, where 2 Mb of DP DNA was introgressed onto the BB diabetes resistant (DR) genetic background, are lymphopenic and 100% develop spontaneous T1D by 84 days of age [4].

The positional cloning and subsequent identification of the Gimap5 gene on RNO4 were in part established through generation of the DR.lyp congenic rat line along with recombination events following our method of marker assisted breeding of DP with F344 rats [2, 4, 5]. Analysis of the lyp phenotype in the F344 DNA recombinant rats helped us define the critical lyp interval as a region of approximately 33 Kb between D4Rhw6 (76.83 Mb) and IIsnp3 (77.16 Mb) containing Gimap1, Gimap5, and Gimap3 (formerly known as Ian2, Ian5, and Ian4, resp.) [2, 4]. Gimap5 was identified as the lyp gene in the BBDP rat through a frameshift mutation and premature truncation of the Gimap5 protein [2, 6] and can be rescued in a P1-derived artificial chromosome (PAC) transgenic rat [7]. However, potential contributions to lymphopenia and/or T1D from the other Gimap genes are still unknown. Similarly, how the mechanisms by which reduced Gimap5 transcript levels and the absence of the Gimap5 protein [2, 7, 8] contribute to lymphopenia and T1D are still being elucidated [913].

The predicted structures of the Gimap proteins show common sequences and motifs, such as GTP-binding domains in the N-terminal half, but with differing C-terminal ends [2, 3]. Some C-terminal regions are consistent with transmembrane domains as in the case of Gimap1 and Gimap5, while others, as in Gimap9 and Gimap4, predict coiled coil domains [3, 14]. Both GIMAP4 and GIMAP7 from human Jurkat cells [3] localize to the endoplasmic reticulum and Golgi apparatus while mouse Gimap3 from murine IL-3-dependent 32D myeloid precursor cells was expressed at the outer mitochondrial membrane [15]. Conflicting reports show that GIMAP5, from human primary T cells [10] and from GIMAP5 transfected 293T cells [16], localizes to the centrosome, Golgi apparatus, or endoplasmic reticulum (ER), whereas Gimap5, cloned from Rat2 fibroblasts, localizes to a distinct subcellular fraction that is neither mitochondrial nor ER [11]. Gimap proteins may therefore have similar function, but different subcellular locations. At this time, there is a paucity of information as to the expression of the Gimap genes in specific cell types.

The fact that the Gimap genes are located together in a tight cluster on RNO4 (and in conserved synteny with many other species), combined with their sequence similarities, suggests the possibility that the proteins carry out similar function. While there is sufficient evidence to support the frameshift mutation in Gimap5 as the cause of lymphopenia, we could not exclude that either Gimap1 or Gimap3 play a role, as they are located within the lymphopenia critical interval between D4Rhw6 and IIsnp3 as well as within the PAC used in the transgenic rescue of lymphopenia [7]. In addition, it is possible that the remaining Gimap family members outside the lymphopenia critical interval play a role in T1D development. In order to substantiate the frameshift mutation in Gimap5 and the subsequent protein null allele as the cause of lymphopenia as well as explore a possible contribution by other Gimap family members, we sequenced and cDNA from rat thymus. In addition, we examined Gimap gene expression across multiple tissues and quantified mRNA expression of all annotated and putative Gimap genes in and rat thymus, spleen, and mesenteric lymph node (MLN).

2. Materials and Methods

2.1. Dr.lyp Congenic Rats

The DR.lyp (BBDR.BBDP-(D4Rhw17-SS99306861) (D4Rhw11-D4Rhw10)/Rhw) congenic rat line was derived from animals with two independent recombination events developed from our previously described introgression of the lymphopenia locus by cyclic cross-intercross breeding of BBDP with BBDR rats [17]. The first recombination event was flanked by simple sequence length polymorphism (SSLP) marker D4Rhw11 (76.81 Mb) and the second flanked by SSLP marker D4Rhw10 (77.81 Mb) [4]. Thus, the DP DNA in the DR.lyp rat line encompasses the lyp critical interval from D4Rhw6 (76.83 Mb) to IIsnp3 (77.16 Mb) [2]. In addition, the DR.lyp congenic rat line used in the present study also contains BBDP DNA at D4Rat102 (66.22 Mb) and D4Rat26 (69.18 Mb). The DR.lyp congenic rat line is kept in sister-brother breeding and produces Mendelian proportions of the (25%), (50%), and (25%) genotypes. are 100% lymphopenic and 100% diabetic.

2.2. Housing

Rats were housed in a specific pathogen—free facility at the University of Washington, Seattle, Washington, on a 12-hour light/dark cycle with 24-hour access to food (Harlan Teklad, Madison, Wis, USA) and water. All protocols were approved by the institutional animal use and care committee of the University of Washington, Seattle, Wash, USA. The University of Washington Rodent Health Monitoring Program was used to track infectious agents via a quarterly sentinel monitoring system. Excluded infectious agents are listed at http://depts.washington.edu/compmed/rodenthealth/index.html#excluded.

2.3. RNA Isolation

Thymus, spleen, and mesenteric lymph nodes were homogenized from 45–78-day-old DR.lyp rats (7 male, 8 female) immediately after dissection in RNA lysis solution (Stratagene, La Jolla, CA or Qiagen, Valencia, Calif, USA) either with a pestle (Kontes, Vineland, NJ, USA) and, if viscous, passed through a 20 gauge needle or a Kinematica Polytron PT 10/35 (Brinkmann, Westbury, NY, USA). Bone marrow was obtained by flushing the femora and tibia with Dulbecco’s modified medium (Life Technologies, Grand Island, NY, USA). Nucleated cells were separated with lympholyte-rat ( , Cedarlane Lab, Ontario, Canada) according to the manufacturer’s protocol. Total RNA was isolated using either RNeasy (Qiagen) or Absolutely RNA Miniprep Kit (Stratagene) followed by treatment with DNase. PolyA+ RNA was isolated with Oligotex Direct mRNA Midi/Maxi Kit, (Qiagen). Total RNA was quantitated with RiboGreen (Stratagene).

2.4. cDNA Cloning and Sequencing

cDNA synthesis was performed using SuperScript II Reverse Transcriptase (Invitrogen, Carlsbad, Calif, USA) according to the manufacturer’s recommendations. PCR products were amplified from thymus cDNA as follows: PCR products were generated by using either Herculase (Stratagene) or Roche Taq polymerase (Roche Diagnostics, Indianapolis, Ind, USA). Reactions with Herculase were 25  L, consisting of 100 ng cDNA, 0.5  L of Herculase polymerase, 2.5  L of the supplied buffer, 0.5  L of a mix of 10 mM each dNTP, and 2  L each 5  M primer. Amplification was carried out in a PTC-200 Peltier Thermal Cycler (Bio-Rad, Hercules, Calif, USA) with the following conditions: for 3 minutes, 35 cycles of for 30 seconds, for 30 seconds, for 6 minutes, and a final step of for 7 minutes. Reactions with Roche polymerase were 20  L, consisting of 100 ng cDNA, 0.1  L Roche Taq polymerase, 2.0  L of the supplied buffer, 0.5  L of a mix of 10 mM each dNTP, and 2  L each 5  M primer. Reactions were carried out with the following conditions: for 3 minutes, 35 cycles of for 45 seconds, for 45 seconds, for 2 minutes, and a final step of for 7 minutes. PCR products were cloned into pCRII with the TOPO-TA cloning kit (Invitrogen), sequenced using ABI BigDye v3.1 (Applied Biosystems, Foster City, Calif, USA), and analyzed on an ABI 3730XL sequencer (Applied Biosystems) at the University of Washington Biochemistry Sequencing Core in Seattle, WA. and RACE ( and , Rapid Amplification of cDNA Ends) was carried out with a Marathon cDNA Amplification kit (K1802-1, Clontech, Palo Alto, Calif, USA) using the protocol provided. Plasmids were transformed into XL1Blue (Stratagene) by electroporation of Top10 cells (Invitrogen) according to the protocol supplied with the cells. Plasmids were purified by using GenElute Plasmid Maxiprep Kit (Sigma, St. Louis, Mo, USA) or Plasmid Maxi Kit (Qiagen). GenBank accession numbers of the cloned genes and of RACE products are DQ125335–DQ125353.

2.5. Quantitative RT-PCR

RNA was collected from whole tissue, isolated using a Qiaqen RNeasy minikit (Valencia, Calif, USA), and aliquoted to minimize degradation from freezing/thawing. Quantitative real time polymerase chain reaction (qRT-PCR) was performed on anMx4000 Multiplex QPCR System (Stratagene) in duplex reactions with rat cyclophilin (NM_017101) as an internal control. Samples were run in triplicate using 100 ng of total RNA or 5 ng of polyA+ RNA. Twenty-five L reactions were run using a Brilliant Single-Step qRT-PCR Kit (2.5  L 10x core RT-PCR buffer, 5.5 mM , 300 nM each primer, 200 nM each probe, 0.3 mM dNTP, 75 nM passive reference dye, 1.6 units Stratascript RT, 2 units SureStart Taq DNA-polymerase). The PCR cycling conditions were as follows: for 30 minutes, for 10 minutes, and 40 cycles of for 30 seconds, for 1 minute. Probes were positioned in the regions of the transcripts where there is more variation between the different Gimap genes and subjected to BLAST alignment to ensure specificity. The primers and probes used for each gene are listed in Table 1. Primers were obtained from Integrated DNA Technologies (Coralville, Iowa, USA) or Qiagen Operon (Valencia, Calif, USA). Fluorescently labeled probes were obtained from Integrated DNA Technologies. Representative qRT-PCR products for each gene, from each tissue, were run on an agarose gel to check for primer pair binding specificity. Each assay was also optimized and validated with serial dilutions of RNA to produce a standard curve that was then translated into a reaction efficiency, or specificity, of each Gimap gene assay. Results from each assay were validated and normalized against cyclophilin. The standard curves, multiplexed with cyclophilin, showed the following reaction efficiencies: Gimap8: , Gimap7: , Gimap4: , Gimap6: , Gimap9: , Gimap1: , Gimap5: , Lr8: , and cyclophilin: .

tab1
Table 1: Probes and primers used in qRT-PCR.
2.6. Statistical Analysis

Three rats from different litters were used to determine the expression of Gimap genes in mesenteric lymph node, thymus, spleen, bone marrow, and kidney. To compare Gimap and Lr8 gene expression across multiple tissues, data was first normalized to cyclophilin then scaled and expressed as a percentage of Gimap5 mesenteric lymph node (MLN), the highest expressing gene overall. For analysis of Gimap expression in , , and rat thymus, spleen, and mesenteric lymph node, 15 rats (5 rats per genotype) were used from 5 litters consisting of 1 rat genotype from each litter. Mesenteric lymph node data for 1 litter was missing leaving 12 rats from 4 litters for analysis. Comparisons from bone marrow and kidney are not shown due to very low expression and high error in these tissues. Pairwise comparisons of the individual ratios were carried out using linear mixed effects models in S-PLUS (Insightful Corp., Seattle, Wash, USA) with a random intercept for each litter. A conditional -test was implemented to test the significance of terms in the fixed effects models. A two-tail test with a -value .05 was judged as significant.

2.7. Bioinformatics

Predicted protein sequences were aligned using T-coffee (http://www.ch.embnet.org/software/TCoffee.html). Structure and topology of proteins were defined using HMMTOP (http://www.ensim.hu./hmmtop/index.html) or Protein Predict (http://cubic.bioc.columbia.edu/pp/). Subcellular locations were predicted using PSORT (http://psort.nibb.ac.jp/form2.html). The nomenclature used in this paper follows the official names determined by the rat nomenclature committee (Lois J. Maltais, Mouse Genome Database (MGD), Mouse Genome Informatics Web Site, The Jackson Laboratory, Bar Harbor, Maine, http://www.informatics.jax.org/) and is different from previous publications [2, 3, 18, 19].

3. Results

3.1. cDNA Cloning and Sequencing of Gimap8, Gimap9, Gimap4, Gimap6, and Gimap7 in and Rats

Gimap8, Gimap9, Gimap4, Gimap6, and Gimap7 (in the order as they appear on the chromosome) are located outside the lymphopenia critical interval (Figure 1). Sequence analysis of thymus cDNA encoding Gimap4 showed three single nucleotide polymorphisms (SNPs) at positions 216, 510, and 618, relative to the ATG start site, and two nucleotides deleted at position 922-923 in rats as compared to rats (Table 2). The first three base pair substitutions resulted in synonymous amino acid changes in the hypothetical protein sequence, while the deletion resulted in a frameshift mutation in the last three predicted amino acid residues and eliminated the normal stop codon at position 311. RACE from thymus cDNA showed that the reading frame continued for other 21 amino acids before generating a new stop codon (Table 2). This same frameshift mutation was also identified in F344/Rhw (nonlymphopenic) rats, which were used in the positional cloning of lymphopenia (Table 2). One nucleotide substitution was identified in Gimap7 at position 603, relative to the ATG start site, between and that resulted in a synonymous amino acid change in the hypothetical protein sequence (Table 2). No SNPs were found in the coding sequences of Gimap6, Gimap8, and Gimap9.

tab2
Table 2: Gimap family thymus cDNA sequencing in and rats.
835650.fig.001
Figure 1: Expanded map of Gimap interval in human, mouse, and rat.Gimap family orthology in human, mouse, and rat is shown along with an expanded map of the 2 Mb of DP DNA in the congenic DR.lyp rat line. The 33 Kb lymphopenia critical interval is indicated between the SSLP markers D4Rhw6 and IIsnp3. Ian aliases are in parentheses underneath the corresponding Gimap name.
3.2. cDNA Cloning and Sequencing of Gimap1 and Gimap3 in and Rats

Gimap1 and Gimap3 are located inside the lymphopenia critical interval (Figure 1). Sequence analysis of thymic cDNA showed a single SNP in the coding sequence of Gimap1 at nucleotide position 752, relative to the ATG start site, that produced an amino acid change in rats as compared to the (Table 2). The SNP produced a methionine (M) to threonine (T) substitution at amino acid 251, which is located near the C-terminus and is not in any of the predicted GTP binding domains. Sorting intolerant from tolerant (SIFT) analysis (http://blocks.fhcrc.org/sift/SIFT.html) predicted the T substitution to be tolerated at this position and did not predict to affect protein function.

Gimap3 is not annotated in the rat genome sequence. Genomic sequencing of the putative ortholog of mouse Gimap3 from base pair positions 76,846,091 to 76,852,162 on RNO 4 (the orthologous DNA interval to mouse Gimap3) in and rats revealed repetitive single or dinucleotide repeats throughout the region that likely resulted in early termination of the sequencing reactions. As such, no specific PCR products could be generated. Attempts were also made to amplify Gimap3 from and rat thymus cDNA; however, again, no specific PCR products were obtained. Comparative analysis of the Brown Norway (BN/Hsdmcwi) database sequence, available at the University of California Santa Cruz (UCSC; Nov. 2004 assembly), with the mouse Gimap3 database sequence (UCSC) failed to establish an open reading frame. The multiple repetitive elements added additional difficulty in locating potential exons or transcripts. No rat EST evidence could be found in the region orthologous to mouse Gimap3 and in human; GIMAP3 is annotated as a pseudogene. Lastly, no evidence of a Gimap3 transcript was found in northern blots of and or from qRT-PCR of rat thymus or spleen (data not shown). Therefore, Gimap3 is likely a pseudogene in rat.

3.3. Predicted Protein Alignment

Alignment of the Gimap family predicted protein sequences in the rat (Figure 2) showed predicted GTP binding domains and conserved box characteristics for all of the Gimap proteins with the most divergent regions located near the C-terminal ends. Gimap1 and Gimap5 are predicted to contain transmembrane domains while Gimap4 and Gimap9 are predicted to contain coiled coil domains. Gimap8, Gimap7, and Gimap6 are predicted to have neither transmembrane nor coiled coil domains. Gimap8 was larger than the other Gimap proteins, containing 688 amino acids and three repeated GTP binding domains (Figure 2).

835650.fig.002
Figure 2: Alignment of predicted Gimap protein sequences in the rat. T-coffee predicted protein alignment from cloned cDNA is shown. Gimap8 is divided into three separate sequences (with the amino acid numbers indicated by each sequence). Shading indicates the GTP binding domain consensus regions (GTP) and the conserved domain (Conserved Box). The HMMTOP predicted transmembrane domain sequences for Gimap1 and Gimap5 and the coiled coil domains for Gimap4 and Gimap9 are underlined.
3.4. Gimap Expression Pattern across Multiple Tissues

The relative expression levels of the Gimap genes in mesenteric lymph node, thymus, spleen, bone marrow, and kidney were determined in the rat (Figure 3). All of the Gimap genes expressed more robustly in the mesenteric lymph nodes, thymus, and spleen as compared to bone marrow and kidney ( ). In the mesenteric lymph node, Gimap4, Gimap5, and Gimap8 were expressed significantly higher than Gimap9 ( ) while in kidney, Gimap4 and Gimap8 were expressed significantly higher than Gimap1 and Gimap9 ( ) (Figure 3). No significant expression differences were detected between any of the Gimap genes (Gimap8, 9, 4, 6, 7, 1, and 5) in thymus, spleen, and bone marrow. Overall, Lr8, a gene unassociated with the Gimap family but also within the 2 Mb of DP DNA in the congenic rat line, expressed predominantly in the spleen, an expression pattern unique relative to the Gimap family.

835650.fig.003
Figure 3: Tissue specific Gimap expression. The mean standard deviation is shown for ( ) Gimap gene expression. To compare Gimap gene expression across multiple tissues, data was first normalized to cyclophilin then scaled and expressed as a percentage of Gimap5 mesenteric lymph node (MLN), the highest expressing gene overall. Genes appear in the order at which they appear on rat chromosome 4. Tissues appear in the following order per gene: MLN (dots), thymus (white), spleen (hash marks), bone marrow (black), and kidney (stripes). Significance is represented as follows: is and is .
3.5. Gimap Expression in and Thymus, Spleen, and Mesenteric Lymph Node

In thymus, expression of Gimap4, Gimap9, Gimap1, and Gimap5 was significantly decreased in rats as compared to (Figure 4). In contrast, Gimap7 expression in thymus was higher in as compared to while Gimap8, Gimap6, and Lr8 showed no differential expression. Expression of all of the Gimap genes (8, 9, 4, 6, 7, 1, and 5) was reduced in rat spleen and mesenteric lymph node as compared to (Figure 4). We observed the same expression pattern whether the data were normalized to cyclophilin or to total RNA (data not shown). Data from bone marrow and kidney is not shown due to the very low expression in these tissues. The low expression observed in these tissues is not due to RNA degradation, but rather to the low mRNA levels relative to cyclophilin levels.

835650.fig.004
Figure 4: Gimap gene expression in the and rats. The mean standard deviation is shown for and rat Gimap gene expression in thymus ( ), spleen ( ) and mesenteric lymph node (MLN) ( ) after normalization to cyclophilin. Black columns represent and grey hatched columns represent . Data is expressed as a percentage of . Significant differences are follows; for , for , for . Genes appear in the order at which they appear on rat chromosome 4. The average Gimap expression in rat bone marrow and kidney s is shown in Figure 3.

4. Discussion

While the frameshift mutation in Gimap5 is likely necessary and sufficient for lymphopenia, the possibility remains that additional mutation(s) in the Gimap family may contribute to the development of lymphopenia, spontaneous T1D, or both in the rat. Aside from Gimap5, only Gimap1 and Gimap3 could potentially play a role in the development of lymphopenia, as they are the only remaining genes located within the 33 Mb interval critical for lymphopenia between D4Rhw6 and IIsnp3. The methionine to threonine base pair substitution at amino acid position 251 in Gimap1 is not located in any of the predicted GTP binding domains and SIFT analysis predicted that the mutation is not likely to alter normal Gimap1 protein function. Furthermore, the DR amino acid at position 251 is not conserved across species; human GIMAP1 has a valine at this same position [3]. Lastly, no Gimap3 transcript could be found and no open reading frame could be identified. We suspect that this region of the rat genome does not code for a protein, which is similar to the human GIMAP3 pseudogene [3] and unlike mouse Gimap3 [15]. Therefore, the sequence analysis of Gimap1 and Gimap3 supports the hypothesis that Gimap5 is the cause of lymphopenia in the rat. In addition, the sequence data from all of the remaining Gimap family members suggest that these genes are not likely to play a role in the onset of T1D diabetes. We cannot however exclude the possibility that there are mutations outside of the coding regions, such as in transcription factor binding sites or other regulatory sites, that play a role in the regulation of Gimap gene expression and/or the onset of T1D in the rat.

While we can exclude the involvement of the members of the Gimap family proximal to D4Rhw6 (Gimap8, Gimap9, Gimap4, Gimap6, and Gimap7) in the development of lymphopenia, we cannot exclude that they may play a role in the development of T1D. Coding sequence analysis of these family members revealed that only Gimap4 had genetic differences, specifically a two-base pair deletion, that would result in a nonsynonymous amino acid change between the nondiabetic and the diabetes susceptible (Table 2). Although the effect of this variation is unknown, we did discover this same deletion in the nonlymphopenic, diabetes resistant F344 rat. F344 DNA introgressed through this interval on the background protects from onset of T1D [4] suggesting that the deletion mutation in Gimap4 is not deleterious. In addition, the predicted protein sequences of both human (AK001972) and mouse (NP_778155.2) Gimap4 show that the 23 C-terminal amino acids are similar to those of (data not shown). It is therefore unlikely that the Gimap4 two-base pair deletion mutation in the rat is functionally relevant to development of T1D or lymphopenia, rather it is likely an additional natural isoform [20].

All of the Gimap genes were predominantly expressed in organs of the immune system: mesenteric lymph node, thymus, and spleen, consistent with previous findings of a role of the Gimap gene family in lymphocyte development [21]. Interestingly, there was an overall reduction in expression of all seven Gimap genes in rat spleen and mesenteric lymph node and four (Gimap4, Gimap9, Gimap1, and Gimap5) of the seven genes in rat thymus. In contrast, Lr8, a gene unrelated to the Gimap family located 69 Kb downstream of Gimap5, (Figure 1) [22, 23] showed no differential expression between and . It is not clear why Gimap5 transcript levels are reduced as the single cytosine residue deletion results in a frameshift mutation and a premature truncation in the protein. One hypothesis is that during protein synthesis, the incomplete (truncated) protein may destabilize the RNA/protein complexes and cause mRNA degradation [24, 25]. Another hypothesis for reduction in rat Gimap gene transcripts is a difference in organ composition from those of rats. Reduced T cells numbers in rats could lead to a difference in cellular composition and may explain the lower observed expression of all of the Gimap genes. As the function of Gimap proteins remains rather poorly defined, it would be a useful addendum if in vitro knockdown experiments were designed to test the functional changes that might derive from reduced expression of Gimap5. These types of experiments could determine if the mutation is significant in functional terms or if the altered expression is the most critical feature.

The Gimap gene family is conserved throughout evolution from plants to humans [3]. Members of the Gimap gene family are implicated in a variety of basic cellular processes. These include protection against plant pathogens [26] and okadaic acid and gamma radiation [16]. Gimap family members have also been found to be important for T cell development [27], B cell activation [28], B cell malignancy [29], and apoptosis [8, 30]. In addition, Gimap5 deficient mice have been shown to have impaired maturation and survival of CD4 and CD8 positive T cells [13].

In conclusion, positional cloning of the lymphopenia gene in the spontaneously T1D prone BB DP rat revealed a frameshift mutation in the GTPase Immune Associated Protein Gimap5 [2, 6]. Our coding sequence analysis of the remaining members of the Gimap family revealed that Gimap4 and Gimap1 each had coding variation between and . However, the amino acid differences do not appear to have functional effects substantiating the Gimap5 frameshift mutation as the cause of lymphopenia. Quantitative real time PCR analysis showed a reduction in expression of all seven Gimap genes in spleen and mesenteric lymph nodes when compared to while only four, Gimap1, Gimap4, Gimap5, and Gimap9, were reduced in thymus. Further understanding of the nature of the Gimap family will aid in our goal of characterizing the pathways involved in the development of lymphopenia and T1D.

Acknowledgments

This work was supported by the National Institutes of Health (AI42380) and the Molecular and Genetics Core (E. A. R., B. V., J. L. H., and M. R. P.) of the University of Washington Diabetes and Endocrinology Research Center (DK17047), a Junior Faculty Award (D. H. M), and a Mentor Based Postdoctoral Fellowship Award (Å. L.) from the American Diabetes Association.

References

  1. H. Markholst, S. Eastman, D. Wilson, B. E. Andreasen, and Å. Lernmark, “Diabetes segregates as a single locus in crosses between inbred BB rats prone or resistant to diabetes,” The Journal of Experimental Medicine, vol. 174, no. 1, pp. 297–300, 1991. View at Publisher · View at Google Scholar
  2. A. J. MacMurray, D. H. Moralejo, A. E. Kwitek, et al., “Lymphopenia in the BB rat model of type 1 diabetes is due to a mutation in a novel immune-associated nucleotide (Ian)-related gene,” Genome Research, vol. 12, no. 7, pp. 1029–1039, 2002. View at Publisher · View at Google Scholar
  3. J. Krücken, R. M. U. Schroetel, I. U. Müller, et al., “Comparative analysis of the human gimap gene cluster encoding a novel GTPase family,” Gene, vol. 341, no. 1-2, pp. 291–304, 2004. View at Publisher · View at Google Scholar
  4. J. M. Fuller, A. E. Kwitek, T. J. Hawkins, et al., “Introgression of F344 rat genomic DNA on BB rat chromosome 4 generates diabetes-resistant lymphopenic BB rats,” Diabetes, vol. 55, no. 12, pp. 3351–3357, 2006. View at Publisher · View at Google Scholar
  5. D. H. Moralejo, H. A. Park, S. J. Speros, et al., “Genetic dissection of lymphopenia from autoimmunity by introgression of mutated Ian5 gene onto the F344 rat,” Journal of Autoimmunity, vol. 21, no. 4, pp. 315–324, 2003. View at Publisher · View at Google Scholar
  6. L. Hornum, J. Rmer, and H. Markholst, “The diabetes-prone BB rat carries a frameshift mutation in Ian4, a positional candidate of Iddm1,” Diabetes, vol. 51, no. 6, pp. 1972–1979, 2002. View at Publisher · View at Google Scholar
  7. M. Michalkiewicz, T. Michalkiewicz, R. A. Ettinger, et al., “Transgenic rescue demonstrates involvement of the Ian5 gene in T cell development in the rat,” Physiological Genomics, vol. 19, no. 2, pp. 228–232, 2004. View at Publisher · View at Google Scholar
  8. M. Pandarpurkar, L. Wilson-Fritch, S. Corvera, et al., “Ian4 is required for mitochondrial integrity and T cell survival,” Proceedings of the National Academy of Sciences of the United States of America, vol. 100, no. 18, pp. 10382–10387, 2003. View at Publisher · View at Google Scholar
  9. S. Ilangumaran, M. Forand-Boulerice, S. M. Bousquet, et al., “Loss of GIMAP5 (GTPase of immunity-associated nucleotide binding protein 5) impairs calcium signaling in rat T lymphocytes,” Molecular Immunology, vol. 46, no. 6, pp. 1256–1259, 2009. View at Publisher · View at Google Scholar
  10. U. Dalberg, H. Markholst, and L. Hornum, “Both Gimap5 and the diabetogenic BBDP allele of Gimap5 induce apoptosis in T cells,” International Immunology, vol. 19, no. 4, pp. 447–453, 2007. View at Publisher · View at Google Scholar
  11. M. Keita, C. Leblanc, D. Andrews, and S. Ramanathan, “GIMAP5 regulates mitochondrial integrity from a distinct subcellular compartment,” Biochemical and Biophysical Research Communications, vol. 361, no. 2, pp. 481–486, 2007. View at Publisher · View at Google Scholar
  12. R. Kupfer, J. Lang, C. Williams-Skipp, M. Nelson, D. Bellgrau, and R. I. Scheinman, “Loss of a gimap/ian gene leads to activation of NF-κB through a MAPK-dependent pathway,” Molecular Immunology, vol. 44, no. 4, pp. 479–487, 2007. View at Publisher · View at Google Scholar
  13. R. D. Schulteis, H. Chu, X. Dai, et al., “Impaired survival of peripheral T cells, disrupted NK/NKT cell development, and liver failure in mice lacking Gimap5,” Blood, vol. 112, no. 13, pp. 4905–4914, 2008. View at Publisher · View at Google Scholar
  14. O. Stamm, J. Krücken, H.-P. Schmitt-Wrede, W. P. M. Benten, and F. Wunderlich, “Human ortholog to mouse gene imap38 encoding an ER-localizable G-protein belongs to a gene family clustered on chromosome 7q32-36,” Gene, vol. 282, no. 1-2, pp. 159–167, 2002. View at Publisher · View at Google Scholar
  15. L. Dahéron, T. Zenz, L. D. Siracusa, C. Brenner, and B. Calabretta, “Molecular cloning of Ian4: a BCR/ABL-induced gene that encodes an outer membrane mitochondrial protein with GTP-binding activity,” Nucleic Acids Research, vol. 29, no. 6, pp. 1308–1316, 2001. View at Publisher · View at Google Scholar
  16. T. Sandal, L. Aumo, L. Hedin, B. T. Gjertsen, and S. O. Døskeland, “Irod/Ian5: an inhibitor of γ-radiation- and okadaic acid-induced apoptosis,” Molecular Biology of the Cell, vol. 14, no. 8, pp. 3292–3304, 2003. View at Publisher · View at Google Scholar
  17. S. Bieg, G. Koike, J. Jiang, et al., “Genetic isolation of iddm 1 on chromosome 4 in the biobreeding (BB) rat,” Mammalian Genome, vol. 9, no. 4, pp. 324–326, 1998. View at Publisher · View at Google Scholar
  18. J. Krücken, M. Epe, W. P. M. Benten, N. Falkenroth, and F. Wunderlich, “Malaria-suppressible expression of the anti-apoptotic triple GTPase mGIMAP8,” Journal of Cellular Biochemistry, vol. 96, no. 2, pp. 339–348, 2005. View at Publisher · View at Google Scholar
  19. T. Nitta, M. Nasreen, T. Seike, et al., “IAN family critically regulates survival and development of T lymphocytes,” PLoS Biology, vol. 4, no. 4, article e103, pp. 1–13, 2006. View at Publisher · View at Google Scholar
  20. C. Carter, C. Dion, S. Schnell, et al., “A natural hypomorphic variant of the apoptosis regulator Gimap4/IAN1,” The Journal of Immunology, vol. 179, no. 3, pp. 1784–1795, 2007.
  21. J.-J. Filén, S. FiLén, R. Moulder, et al., “Quantitative proteomics reveals GIMAP family proteins 1 and 4 to be differentially regulated during human T helper cell differentiation,” Molecular & Cellular Proteomics, vol. 8, no. 1, pp. 32–44, 2009. View at Publisher · View at Google Scholar
  22. J. Lurton, T. M. Rose, G. Raghu, and A. S. Narayanan, “Isolation of a gene product expressed by a subpopulation of human lung fibroblasts by differential display,” American Journal of Respiratory Cell and Molecular Biology, vol. 20, no. 2, pp. 327–331, 1999.
  23. H. Nakajima, M. Takenaka, J.-Y. Kaimori, et al., “Gene expression profile of renal proximal tubules regulated by proteinuria,” Kidney International, vol. 61, no. 5, pp. 1577–1587, 2002. View at Publisher · View at Google Scholar
  24. P. A. Frischmeyer and H. C. Dietz, “Nonsense-mediated mRNA decay in health and disease,” Human Molecular Genetics, vol. 8, no. 10, pp. 1893–1900, 1999. View at Publisher · View at Google Scholar
  25. J. T. Mendell, N. A. Sharifi, J. L. Meyers, F. Martinez-Murillo, and H. C. Dietz, “Nonsense surveillance regulates expression of diverse classes of mammalian transcripts and mutes genomic noise,” Nature Genetics, vol. 36, no. 10, pp. 1073–1078, 2004. View at Publisher · View at Google Scholar
  26. T. L. Reuber and F. M. Ausubel, “Isolation of arabidopsis genes that differentiate between resistance responses mediated by the RPS2 and RPM1 disease resistance genes,” The Plant Cell, vol. 8, no. 2, pp. 241–249, 1996. View at Publisher · View at Google Scholar
  27. G. M. C. Poirier, G. Anderson, A. Huvar, et al., “Immune-associated nucleotide-1 (IAN-1) is a thymic selection marker and defines a novel gene family conserved in plants,” The Journal of Immunology, vol. 163, no. 9, pp. 4960–4969, 1999.
  28. M. Cambot, S. Aresta, B. Kahn-Perlès, J. de Gunzburg, and P.-H. Roméo, “Human immune associated nucleotide 1: a member of a new guanosine triphosphatase family expressed in resting T and B cells,” Blood, vol. 99, no. 9, pp. 3293–3301, 2002. View at Publisher · View at Google Scholar
  29. T. Zenz, A. Roessner, A. Thomas, et al., “hlan5: the human ortholog to the rat lan4/lddm1/lyp is a new member of the Ian family that is overexpressed in B-cell lymphoid malignancies,” Genes & Immunity, vol. 5, no. 2, pp. 109–116, 2004. View at Publisher · View at Google Scholar
  30. J. A. Lang, D. Kominski, D. Bellgrau, and R. I. Scheinman, “Partial activation precedes apoptotic death in T cells harboring an IAN gene mutation,” European Journal of Immunology, vol. 34, no. 9, pp. 2396–2406, 2004. View at Publisher · View at Google Scholar