- Research article
- Open Access
RNA expression of TLR10 in normal equine tissues
BMC Research Notesvolume 9, Article number: 353 (2016)
Toll like receptors are one of the major innate immune system pathogen recognition systems. There is little data on the expression of the TLR10 member of this family in the horse.
This paper describes the genetic structure of the Equine TLR10 gene and its RNA expression in a range of horse tissues. It describes the phylogenetic analysis of the Equine TLR1,6,10,2 annotations in the horse genome, firmly identifying them in their corresponding gene clades compared to other species and firmly placing the horse gene with other TLR10 genes from odd-toed ungulates. Additional 3’ transcript extensions to that annotated for TLR10 in the horse genome have been identified by analysis of RNAseq data. RNA expression of the equine TLR10 gene was highest in peripheral blood mononucleocytes and lymphoid tissue (lymph nodes and spleen), however some expression was detected in all tissues tested (jejunum, caudal mesenteric lymph nodes, bronchial lymph node, spleen, lung, colon, kidney and liver). Additional data on RNAseq expression of all equine TLR genes (1–4 and 6–10) demonstrate higher expression of TLR4 than other equine TLRs in all tissues.
The equine TLR10 gene displays significant homology to other mammalian TLR10 genes and could be reasonably assumed to have similar fuctions. Its RNA level expression is higher in resting state PBMCs in horses than in other tissues.
The toll-like receptors (TLRs) are a family of membrane receptors that recognise a wide range of pathogen associated molecular patterns (PAMPs) and are considered a crucial signaling component of the innate immune system. TLRs 1-13 have previously been identified in mammals . These genes have a distinctive structure consisting of an extracellular amino-terminal leucine-rich repeat (LRR) domain, responsible for ligand binding, a transmembrane domain, and an intracellular carboxyl terminal toll/IL (interleukin)-1 receptor domain (TIR) that is responsible for signal transduction. Most TLR genes have no introns within their TIR domains. The genetic structure of these genes usually consists of a large 5′ exon containing the TIR and or the LRR domains with or without smaller exons at the 3′ end of the gene, often containing non-coding regions .
Based on genetic sequence TLRs can be broadly divided into six subfamilies that have related PAMP recognition and signaling pathways (TLR1/2/6/10, 3, 4, 5, 7/8/9 and 11/12/13). TLRs 3 and 7/8/9 are located intracellularly and respond to bacterial and viral nucleic acids, inducing expression of type I interferons. TLR 1/2/6/10 and 4, 5 are expressed on the cell surface and sense cell wall and outer membrane components of bacterial, fungal and protozoal organisms activating a core signaling pathway including NFκB and other transcription factors leading to pro-inflammatory cytokine release .
In the horse, the sequences of TLR 1–4 and 6–9 have been described [4–6] with some studies describing expression levels of some classes of TLRs in individual tissues or disease states [4, 5, 7–12]. The presence of equine TLR5 is controversial. Its existence has been suggested by cytokine release in response to bacterial flagellin, the ligand for TLR5  and a recent report of a 454 bp fragment with high sequence similarity to the intracellular signaling domain of human TLR5 in an equine expressed sequence tag . However, no full length homologue has been identified in the published equine genome.
TLR10 is currently the only orphan receptor without a known ligand, or conclusive biological function. A pseudogene in rodents , and full length TLR10 genes have been identified in a range of mammals, including humans , sheep , cattle  and pigs . TLR10 is present as part of a 50 kb TLR6-TLR1-TLR10 gene cluster thought to have arisen by ancestral gene duplication events. These TLR1 subfamily proteins form heterodimers with TLR2 [3, 19] with varying ligand affinity.
TLR10 is known to be expressed in humans in a wide range of lymphoid tissues and cells, as well as in intestinal epithelial cells, dermal endothelial cells and placental trophoblasts [20–23]. TLR10 RNA expression has also been detected in pigs, cattle and sheep, primarily in lymphoid tissue such as peripheral blood leukocytes, lymph nodes and spleens, though trace levels of RNA have been detected in other tissues (Additional file 1: Table S1). Initial modeling studies have suggested that di and triacetylated lipopeptides may potentially interact with TLR10/1, TLR10/2 hetero-dimers and TLR10/10 homodimers . Co-immunoprecipitation experiments confirmed that, similar to TLR2/1, TLR2/10 complexes recruit the proximal adaptor MyD88 to the activated receptor complex. However, human TLR10, alone or in cooperation with TLR2, fails to activate typical TLR-induced signalling (such as NF-kB activation) downstream of the adapter molecules . The role of TLR10 in inflammation is controversial. TLR10 has been shown to mediate the inflammatory response in human intestinal epithelial cells and macrophages to intracellular Listeria monocytogenes infection in one study . While another study, using RNA silencing, blocking antibody and transfection suggests inhibitory properties leading to an anti-inflammatory effect .
There has been only one published report on TLR10 expression in the horse. This report used semi-quantitative PCR, based on predicted sequences, and suggested TLR10 expression in equine bronchial epithelium . To extend this understanding, this paper presents an initial description of the transcriptional profile of TLR10 in a variety of tissues in the horse, along with the previously described equine TLR genes.
Tissue samples for RNAseq: details of these samples, generation of RNAseq data and mapping to the horse genome have been published previously [27, 28]. Briefly, the samples consisted of five tissue samples (kidney, jejunum, liver, spleen and mesenteric lymph node) collected from an aged gelding, lymphocytes isolated by Ficoll Paque (GE healthcare) from a healthy 11 year old welsh mountain pony gelding and RNA from lymphocytes isolated from a healthy thoroughbred mare (the same horse whose DNA the horse genome is derived from) (Additional file 1: Table S2). The RNA samples were extracted, prepared and sequenced on a SOLiD 3 ABi sequencer to generate 50 bp reads. These reads were mapped to the equine reference genome EquCab2 and the transcriptome data was generated as in Moreton et al. . The data for the TLR genes was retrieved from the annotated transcriptome [data available at EBI sequence read archive (SRA) under the study accession number ERP001116 and at 10.7717/peerj.382/supp-6]. Relative expression is given as reads per kilobase per million reads (RPKM) .
Tissue samples for RT-qPCR based TLR10 expression analysis: Samples were collected post mortem from healthy animals euthanized for other reasons than this study. Approximately 5 mm3 tissue samples (kidney, spleen, liver, colon, lung, bronchial and mesenteric lymph nodes) were collected and stored in RNA later (Additional file 1: Table S2). Biopsies were homogenised using a 5 mm stainless steel ball-bearing in a Retsch® Bead Mill MM 301 at 30 shakes per second for 4 min (colon, lung, bronchial and mesenteric lymph nodes), 5 min (spleen) or 6 min (liver and kidney), RNA extraction was performed using the Nucleospin RNA II mini kit (Machery Nagel) according to manufacturer’s instructions. RNA was converted to cDNA using random hexamer primers (promega) and M-MLV reverse transcriptase (promega) as per manufacturer’s instructions. RNA quality was determined using RNA 6000 Nano Kit® Bioanalyser (Agilent technologies, Waldbronn, Germany), for RNA integrity numbers (RIN) see Additional file 1: Table S2. A cut off value of a RIN of 5 was set as the quality threshold for a sample to be included in the study as recommended for qPCR studies in Fleige and Pfaffl .
Tissues from all horses were considered to be in a “resting” state without obvious gross pathology.
For each predicted TLR like horse gene the longest open reading frame was translated and aligned with known TLR1,2,6 and 10 proteins from Swissprot. All known vertebrate TLR10 genes were identified and predicted protein sequences were identified. In each case, sequences were aligned using Muscle and a phylogenetic tree generated using PhyML under the LG model with 4 rate classes and NNI tree searching and 100 bootstrap replicates. The resulting trees were visualised using Figtree (http://tree.bio.ed.ac.uk/software/figtree/).
All quantitative reverse transcriptase real time PCR (RT-qPCR) experiments were designed and performed to comply with the quality controls detailed in the MIQE guidelines . SYBR green RT-qPCR was performed on cDNA using primer sets for TLR10 and reference genes succinate dehydrogenase complex subunit A (SDHA) and Hypoxanthine phosphoribosyl transferase (HPRT) (Additional file 1: Table S3). Specificity of the PCR amplicons was confirmed by sequencing.
The Light Cycler 480 DNA SYBR green 1 master mix (Roche) in a 20 μl reaction volume was used according to manufacturer’s instructions. Cycling conditions consisted of 98 °C for 15 min then 45 cycles of 98 °C for 15 s, 58 °C for 30 s and 72 °C for 30 s. Reactions were performed on a Light Cycler 480 96 well plate real time PCR system (Roche). Serial dilutions of control cDNA were used to assess primer efficiency. Relative expression was calculated using the following formula : Corrected Ct value = Ct + (Nt – Ct′) * S/S′ where Ct = mean sample Ct, Nt = experimental reference gene mean, Ct′ = mean reference gene of sample, S = TLR slope, S′ = reference gene slope.
Transcripts with (RPKM > 0) were identified for TLR1-4 and TLR6-9 as well as TLR10, the latter has not been reported previously. The Ensembl Equus caballus database does not contain any annotations for TLR5. By comparison to known TLR1,6 and 10 protein sequences, two horse TLR1 transcripts were identified (ENSCAT00000002340 and rmCuff_TCONS_00039270) and single transcripts for TLR6 (ENSCAT00000001932) and TLR10 (ENSCAT00000022185).
Comparison of Equine transcripts to representative TLR1,2,6 and 10 genes shows the clear definition of ENSECAT00000002340 as equine TLR1, ENSECAT00000019013 as TLR2, ENSECAT00000001932 as TLR6 and ENSECAT00000022185 as TLR10 (Fig. 1). When TLR10 transcript ENSECAT00000022185 is aligned with representatives of vertebrate TLR10 sequences it is most closely related to the wild Przewalski horse (E. ferus przewalskii) and the southern white rhinoceros (Ceratotherium simum simum) and all odd-toes ungulates (Perissodactyla) (Fig. 2) as would be expected.
Sufficient read depth was available for transcript structure analysis for TLR10 (Fig. 3a). Gaps in the predicted transcripts compared with the ENSEMBL annotations over the 5′ exons are probably due to sub-optimal read coverage rather than real transcriptional variation. Additional 3′ transcript extensions are suggested by our transcript analysis when compared with the reference sequence annotations (Fig. 3a). The sequence covered by our predicted TLR10 transcript contains one large open reading frame with a short leader sequence. Basic structural domain analysis of this open reading frame using the SMART protein domain analysis suite demonstrated a typical mammalian TLR10 gene structure (Fig. 3b) consisting of a series of amino terminal LRR’s, a Leucine Rich Repeat C—terminal domain, a transmembrane domain and a carboxyl terminal TIR domain. Read depth was not consistently high enough for confident calling of SNPs on TLR10.
Each organ or cell type was found to have a distinct TLR expression profile (Additional file 2: Figure S1). Absolute TLR expression was highest in the lymphocyte samples (Additional file 2: Figure S1 A and B). Both lymphocyte samples had similar patterns of TLR expression with TLR4 expressed at the highest level (26 < RPKM < 70) followed by TLR2 and TLR1. TLR’s 6, 7, 8 and 10 were expressed at low levels (RPKM < 12) and TLR3 at trace levels (RPKM < 1). Apart from expression of TLR4 and 8 in the spleen, expression of any TLR in other tissues was at low or trace levels (RPKM < 5). Total number of reads and reads mapped per tissue were similar (Additional file 1: Table S2), indicating that the differences in RPKM reads for this class of gene is genuine and not due to differences in general read mapping density across tissues.
RNAseq data for TLR10 expression were very low in tissues other than PBMCs (Additional file 2: Figure S1). To confirm TLR10 mRNA expression from the RNAseq data, a range of tissues from further Thoroughbred Horses and Welsh Ponies were analyzed by RT-qPCR. TLR10 transcript was detected in all tissues tested: caudal mesenteric lymph nodes, bronchial lymph node, spleen, lung, colon, kidney and liver; with highest levels in the lymphoid tissues (lymph nodes and spleen) and lowest in liver (Fig. 4). Where samples for multiple horses were available for that tissue, TLR10 transcript levels were consistent within that tissue (Fig. 4a).
In summary, equine TLR10 shows conserved domain architecture and high sequence similarity to its mammalian counterparts. Equine TLR10 mRNA is expressed in a wide range of tissues with highest levels in lymphoid tissues.
The similarity of the predicted Equine TLR10 protein with the other described mammalian TLR10’s ) implies functional conservation between the equine and other TLR10’s. Our transcriptome assembly and annotation would suggest additional 3′ exons to the reference genome annotation for equine TLR10. These extensions may be tissue specific and remain to be confirmed with Sanger sequencing of mRNA.
The transcription profile for the complete TLR repertoire in the normal horse tissues examined here would also additionally suggest that TLR4 is an important sentinel signaling molecule in horse lymphoid tissue (spleen and PBMCs). This would correlate with the known susceptibility of horses to bacterial LPS (the ligand for TLR4) .
The results presented here demonstrate transcription of TLR10 in the horse in a wide range of tissues with expression location and levels similar to that in other mammalian species (Additional file 1: Table S1). This paper provides a starting point for further studies of activities of this gene in the horse. Presumably given it’s homology with TLR10 in other species it is likely to form heterodimers with TLR2, however confirmation of the function of TLR10 in any mammalian species will require further work.
toll like receptor
peripheral blood mononucleocyte cells
reverse transcriptase quantitative polymerase chain reaction
succinate dehydrogenase complex subunit A
hypoxanthine phosphoribosyl transferase
Roach JC, Glusman G, Rowen L, Kaur A, Purcell MK, Smith KD, Hood LE, Aderem A. The evolution of vertebrate Toll-like receptors. Proc Natl Acad Sci USA. 2005;102(27):9577–82.
Kanzok SM, Hoa NT, Bonizzoni M, Luna C, Huang Y, Malacrida AR, Zheng L. Origin of Toll-like receptor-mediated innate immunity. J Mol Evol. 2004;58(4):442–8.
Guan Y, Ranoa DR, Jiang S, Mutha SK, Li X, Baudry J, Tapping RI. Human TLRs 10 and 1 share common mechanisms of innate immune sensing but not signaling. J Immunol. 2010;184(9):5094–103.
Zhang YW, Davis EG, Blecha F, Wilkerson MJ. Molecular cloning and characterization of equine Toll-like receptor 9. Vet Immunol Immunopathol. 2008;124(3–4):209–19.
Astakhova NM, Perelygin AA, Zharkikh AA, Lear TL, Coleman SJ, MacLeod JN, Brinton MA. Characterization of equine and other vertebrate TLR3, TLR7, and TLR8 genes. Immunogenetics. 2009;61(7):529–39.
Wade CM, Giulotto E, Sigurdsson S, Zoli M, Gnerre S, Imsland F, Lear TL, Adelson DL, Bailey E, Bellone RR, et al. Genome sequence, comparative analysis, and population genetics of the domestic horse. Science. 2009;326(5954):865–7.
Werners AH, Bull S, Vendrig JC, Smyth T, Bosch RR, Fink-Gremmels J, Bryant CE. Genotyping of Toll-like receptor 4, myeloid differentiation factor 2 and CD-14 in the horse: an investigation into the influence of genetic polymorphisms on the LPS induced TNF-alpha response in equine whole blood. Vet Immunol Immunopathol. 2006;111(3–4):165–73.
Figueiredo MD, Vandenplas ML, Hurley DJ, Moore JN. Differential induction of MyD88- and TRIF-dependent pathways in equine monocytes by Toll-like receptor agonists. Vet Immunol Immunopathol. 2009;127(1–2):125–34.
Schneberger D, Caldwell S, Suri SS, Singh B. Expression of toll-like receptor 9 in horse lungs. Anat Rec. 2009;292(7):1068–77.
Leise BS, Yin C, Pettigrew A, Belknap JK. Proinflammatory cytokine responses of cultured equine keratinocytes to bacterial pathogen-associated molecular pattern motifs. Equine Vet J. 2010;42(4):294–303.
de Laat MA, Clement CK, McGowan CM, Sillence MN, Pollitt CC, Lacombe VA. Toll-like receptor and pro-inflammatory cytokine expression during prolonged hyperinsulinaemia in horses: implications for laminitis. Vet Immunol Immunopathol. 2014;157(1–2):78–86.
Frellstedt L, Waldschmidt I, Gosset P, Desmet C, Pirottin D, Bureau F, Farnir F, Franck T, Dupuis-Tricaud MC, Lekeux P, et al. Training modifies innate immune responses in blood monocytes and in pulmonary alveolar macrophages. Am J Respir Cell Mol Biol. 2014;51(1):135–42.
Kwon S, Gewirtz AT, Hurley DJ, Robertson TP, Moore JN, Vandenplas ML. Disparities in TLR5 expression and responsiveness to flagellin in equine neutrophils and mononuclear phagocytes. J Immunol. 2011;186(11):6263–70.
Hasan U, Chaffois C, Gaillard C, Saulnier V, Merck E, Tancredi S, Guiet C, Briere F, Vlach J, Lebecque S, et al. Human TLR10 is a functional receptor, expressed by B cells and plasmacytoid dendritic cells, which activates gene transcription through MyD88. J Immunol. 2005;174(5):2942–50.
Chuang T, Ulevitch RJ. Identification of hTLR10: a novel human Toll-like receptor preferentially expressed in immune cells. Biochim Biophys Acta. 2001;1518(1–2):157–61.
Chang JS, Russell GC, Jann O, Glass EJ, Werling D, Haig DM. Molecular cloning and characterization of Toll-like receptors 1-10 in sheep. Vet Immunol Immunopathol. 2009;127(1–2):94–105.
Opsal MA, Vage DI, Hayes B, Berget I, Lien S. Genomic organization and transcript profiling of the bovine toll-like receptor gene cluster TLR6-TLR1-TLR10. Gene. 2006;384:45–50.
Shinkai H, Muneta Y, Suzuki K, Eguchi-Ogawa T, Awata T, Uenishi H. Porcine Toll-like receptor 1, 6, and 10 genes: complete sequencing of genomic region and expression analysis. Mol Immunol. 2006;43(9):1474–80.
Govindaraj RG, Manavalan B, Lee G, Choi S. Molecular modeling-based evaluation of hTLR10 and identification of potential ligands in Toll-like receptor signaling. PLoS One. 2010;5(9):e12713.
Hornung V, Rothenfusser S, Britsch S, Krug A, Jahrsdorfer B, Giese T, Endres S, Hartmann G. Quantitative expression of toll-like receptor 1-10 mRNA in cellular subsets of human peripheral blood mononuclear cells and sensitivity to CpG oligodeoxynucleotides. J Immunol. 2002;168(9):4531–7.
Fitzner N, Clauberg S, Essmann F, Liebmann J, Kolb-Bachofen V. Human skin endothelial cells can express all 10 TLR genes and respond to respective ligands. Clin Vaccine Immunol: CVI. 2008;15(1):138–46.
Requena T, Gazquez I, Moreno A, Batuecas A, Aran I, Soto-Varela A, Santos-Perez S, Perez N, Perez-Garrigues H, Lopez-Nevot A, et al. Allelic variants in TLR10 gene may influence bilateral affectation and clinical course of Meniere’s disease. Immunogenetics. 2013;65(5):345–55.
Mulla MJ, Myrtolli K, Tadesse S, Stanwood NL, Gariepy A, Guller S, Norwitz ER, Abrahams VM. Cutting-edge report: TLR10 plays a role in mediating bacterial peptidoglycan-induced trophoblast apoptosis. Am J Reprod Immunol. 2013;69(5):449–53.
Regan T, Nally K, Carmody R, Houston A, Shanahan F, Macsharry J, Brint E. Identification of TLR10 as a key mediator of the inflammatory response to Listeria monocytogenes in intestinal epithelial cells and macrophages. J Immunol. 2013;191(12):6084–92.
Oosting M, Cheng SC, Bolscher JM, Vestering-Stenger R, Plantinga TS, Verschueren IC, Arts P, Garritsen A, van Eenennaam H, Sturm P, et al. Human TLR10 is an anti-inflammatory pattern-recognition receptor. Proc Natl Acad Sci USA. 2014;111(42):E4478–84.
Quintana AM, Landolt GA, Annis KM, Hussey GS. Immunological characterization of the equine airway epithelium and of a primary equine airway epithelial cell culture model. Vet Immunol Immunopathol. 2011;140(3–4):226–36.
Moreton J, Malla S, Aboobaker AA, Tarlinton RE, Emes RD. Characterisation of the horse transcriptome from immunologically active tissues. PeerJ. 2014;2:e382.
Brown K, Moreton J, Malla S, Aboobaker AA, Emes RD, Tarlinton RE. Characterisation of retroviruses in the horse genome and their transcriptional activity via transcriptome sequencing. Virology. 2012;433(1):55–63.
Mortazavi A, Williams BA, McCue K, Schaeffer L, Wold B. Mapping and quantifying mammalian transcriptomes by RNA-Seq. Nat Methods. 2008;5(7):621–8.
Fleige S, Pfaffl MW. RNA integrity and the effect on the real-time qRT-PCR performance. Mol Aspects Med. 2006;27(2–3):126–39.
Bustin SA, Benes V, Garson JA, Hellemans J, Huggett J, Kubista M, Mueller R, Nolan T, Pfaffl MW, Shipley GL, et al. The MIQE guidelines: minimum information for publication of quantitative real-time PCR experiments. Clin Chem. 2009;55(4):611–22.
Kogut MH, Genovese KJ, He H, Kaiser P. Flagellin and lipopolysaccharide up-regulation of IL-6 and CXCLi2 gene expression in chicken heterophils is mediated by ERK1/2-dependent activation of AP-1 and NF-kappaB signaling pathways. Innate immunity. 2008;14(4):213–22.
Seabury CM, Cargill, EJ, Womack JE. Sequence variability and protein domain architectures for bovine Toll-like receptors 1, 5, and 10. Genomics. 2007;90(4):502–15.
Senior JM, Proudman CJ, Leuwer M, Carter SD. Plasma endotoxin in horses presented to an equine referral hospital: correlation to selected clinical parameters and outcomes. Equine Vet J. 2011;43(5):585–9.
RT, LA and GM performed laboratory work, JM and RE performed bio-informatic and phylogenetic analysis, RT and ST designed the study, performed the qPCR data analysis and wrote the manuscript. ST directly supervised LA and GM and assisted with LA’s funding award. RT was primary grant holder for the funding that produced the manuscript. All authors read and approved the final manuscript.
The experimental work in this study was supported by a University of Nottingham New Researchers Grant awarded to R Tarlinton and an MSD Animal Health Connect Bursary awarded to L Alder. The funding bodies did not play a role in the experimental work, manuscript preparation or submission.
The authors declare that they have no competing interests.
Availability of data and materials
Data from the sequencing portion of this study are available at EBI Sequence Read Archive (SRA) under the study accession number ERP001116 and at 10.7717/peerj.382/supp-6.
Statement of ethics and consent to participate
The samples used in this study were primarily sourced from post-mortem material (abattoir or research institute donated animals). Consent was given by the donor of the animal for the use of its tissues in research. Ethical approval was obtained from the University of Nottingham, school of Veterinary Medicine and Science Clinical Ethical Review panel. Data from another study (Moreton et al. , Characterisation of the horse transcriptome from immunologically active tissues)  has been re-analysed in this study. Permission to reuse this data was obtained from these authors. That study included a small number of blood samples from horses that were bled under a home office project licence (number PPL 40/3354) and under a North American Institutional Animal Care and Use Committee (Cornell University, protocol # 1986–0216) protocol. These details are in the original publication.