Tick-Pathogen Interactions and Vector Competence: Identification of Molecular Drivers for Tick-Borne Diseases
- 1SaBio. Instituto de Investigación en Recursos Cinegéticos CSIC-UCLM-JCCM, Ciudad Real, Spain
- 2Department of Veterinary Pathobiology, Center for Veterinary Health Sciences, Oklahoma State University, Stillwater, OK, USA
- 3Global Health and Tropical Medicine, Instituto de Higiene e Medicina Tropical, Universidade Nova de Lisboa, Lisboa, Portugal
- 4UMR BIPAR INRA-ANSES-ENVA, Maisons-Alfort, France
- 5Biology Centre, Czech Academy of Sciences, Institute of Parasitology, Ceske Budejovice, Czechia
- 6Faculty of Science, University of South Bohemia, České Budějovice, Czechia
- 7Facultad de Veterinaria, Universidad de Zaragoza, Zaragoza, Spain
- 8Animal and Plant Health Agency, Surrey, UK
- 9Faculty of Health and Medicine, University of Surrey, Guildford, UK
- 10Institute of Infection and Global Health, University of Liverpool, Liverpool, UK
- 11Institute for Parasitology and Tropical Veterinary Medicine, Freie Universität Berlin, Berlin, Germany
- 12Department of Microbiology, Medical School, Aristotle University of Thessaloniki, Thessaloniki, Greece
- 13National Center of Reference for Anaplasma, Babesia, Rickettsia and Theileria, Intituto Zooprofilattico Sperimentale della Sicilia, Sicily, Italy
Ticks and the pathogens they transmit constitute a growing burden for human and animal health worldwide. Vector competence is a component of vectorial capacity and depends on genetic determinants affecting the ability of a vector to transmit a pathogen. These determinants affect traits such as tick-host-pathogen and susceptibility to pathogen infection. Therefore, the elucidation of the mechanisms involved in tick-pathogen interactions that affect vector competence is essential for the identification of molecular drivers for tick-borne diseases. In this review, we provide a comprehensive overview of tick-pathogen molecular interactions for bacteria, viruses, and protozoa affecting human and animal health. Additionally, the impact of tick microbiome on these interactions was considered. Results show that different pathogens evolved similar strategies such as manipulation of the immune response to infect vectors and facilitate multiplication and transmission. Furthermore, some of these strategies may be used by pathogens to infect both tick and mammalian hosts. Identification of interactions that promote tick survival, spread, and pathogen transmission provides the opportunity to disrupt these interactions and lead to a reduction in tick burden and the prevalence of tick-borne diseases. Targeting some of the similar mechanisms used by the pathogens for infection and transmission by ticks may assist in development of preventative strategies against multiple tick-borne diseases.
Ectoparasites that derive nutrition through blood feeding (haematophagy) are efficient vectors of disease. Ticks are haematophagous ectoparasites of vertebrates. Approximately 10% of the 900 currently known tick species are of significant medical or veterinary importance. Besides causing direct damage associated with blood feeding and in some cases through the excretion of toxins within their saliva, the main relevance of ticks lies in the wide variety of pathogens they can transmit, including bacteria, viruses, protozoa, and helminths (Jongejan and Uilenberg, 2004). The continuous exploitation of environmental resources and the increase in human outdoor activities, which have allowed for the contact with tick vectors normally present in the field, has promoted the emergence and resurgence of tick-borne pathogens (Jongejan and Uilenberg, 2004).
As previously discussed (Beerntsen et al., 2000), the terms “vectorial capacity” and “vector competence” are often used to describe the ability of an arthropod to serve as a disease vector. However, while vectorial capacity is influenced by behavioral and environmental determinants affecting variables such as vector density, longevity, and competence, vector competence is a component of vectorial capacity that depends on genetic factors affecting the ability of a vector to transmit a pathogen (Beerntsen et al., 2000, Box 1). These genetic determinants affect traits such as tick host preferences, duration of tick attachment, tick-host-pathogen and microbiome-pathogen interactions, and susceptibility to pathogen infection (Ramamoorthi et al., 2005; Hajdušek et al., 2013; Narasimhan et al., 2014; Nuttall, 2014; Rynkiewicz et al., 2015; Vayssier-Taussat et al., 2015). Therefore, the elucidation of the mechanisms involved in tick-pathogen interactions that affect vector competence is essential for the identification of molecular drivers for tick-borne diseases, and exposes paradigms for controlling and preventing these diseases.
Box 1. Important determinants influencing the acquisition, maintenance and transmission of pathogens by ticks.
Although our understanding of tick-pathogen interactions is still limited, advances in this field are facilitated by the increasing number of available genomic resources, including metabolomics, transcriptomics, and proteomics datasets of various ticks and tick-borne pathogens (TBPs) (Nene et al., 2004; Ayllón et al., 2015a; Cramaro et al., 2015; Kotsyfakis et al., 2015; Villar et al., 2015a; Gulia-Nuss et al., 2016; de Castro et al., 2016), and the recently published genome from Ixodes scapularis, a vector of Borrelia burgdorferi and Anaplasma phagocytophilum in North America (Gulia-Nuss et al., 2016). Together with tools such as tick cell lines and the widespread adaptation of RNA interference (RNAi) to study tick gene function (Bell-Sakyi et al., 2007; de la Fuente et al., 2007), this has opened exciting possibilities to identify determinants affecting tick vector competence.
Most studies of tick-pathogen interactions focus on certain pathogens (e.g., de la Fuente et al., 2016) or on certain aspects of these interactions (e.g., Hajdušek et al., 2013). However, for a better understanding of tick-pathogen molecular interactions and their role in vector competence, a comprehensive analysis involving major pathogens is crucial. In this review, we provide an overview of tick-pathogen molecular interactions for TBPs that constitute a growing burden for human and animal health (Figure 1). Additionally, the impact of tick microbiome on these interactions was considered to further contribute to the identification of molecular drivers affecting vector competence and the development of novel control and prevention strategies for tick-borne diseases.
Figure 1. Model organisms: tick-borne pathogens that constitute a growing burden for human and animal health. The pathogens covered in this review include bacteria (A. phagocytophilum and B. burgdorferi), viruses (Crimean-Congo hemorrhagic fever virus, tick-borne encephalitis virus), and protozoa (Babesia spp.) transmitted by hard ticks (Ixodidae). The most prevalent diseases caused by these pathogens, main tick vectors, and disease distribution worldwide is shown in the figure.
In this review, we used different tick-borne microorganisms including bacteria (A. phagocytophilum and B. burgdorferi), viruses (Crimean-Congo hemorrhagic fever virus, tick-borne encephalitis virus, and louping ill virus), and protozoa (Babesia spp.) to illustrate their impact on vector competence, behavior and transmission (Figure 1).
Anaplasma phagocytophilum is an obligate intracellular rickettsial pathogen vectored primarily by Ixodes spp. and causes human granulocytic anaplasmosis (HGA), equine, and canine granulocytic anaplasmosis, and tick-borne fever (TBF) (de la Fuente et al., 2008). In the vertebrate host, A. phagocytophilum infects neutrophils where the pathogen multiplies within a parasitophorous vacuole or morula (Ayllón et al., 2015a; Severo et al., 2015). In the absence of transovarial passage, ticks must acquire infection in each generation during a bloodmeal. A. phagocytophilum initially infects tick midgut cells and then subsequently develops in the salivary glands for transmission to susceptible hosts during tick feeding. Bacteria from the B. burgdorferi sensu lato complex are transmitted by Ixodid ticks and cause various symptoms associated with Lyme disease (Radolf et al., 2012). B. burgdorferi s.l. are acquired by larvae or nymphs from an infected host as they are not transovarially transmitted (Rollend et al., 2013). In the tick, spirochetes colonize the midgut and then traverse into the hemocoel and migrate to salivary glands for transmission during tick feeding (Pal et al., 2004; Ramamoorthi et al., 2005; Zhang L. et al., 2011; Coumou et al., 2016).
Ticks transmit a range of viruses that are of significant public and veterinary health concern (Table 1). It is estimated that these viruses spend over 95% of their life cycle within the tick vector. Tick-borne encephalitis virus (TBEV) causes neurological disease in humans, whereas louping ill virus (LIV) causes neurological disease in sheep (Labuda and Nuttall, 2003). Ixodid ticks transmit these viruses to particular host species through a bite (Doherty and Reid, 1971; Mansfield et al., 2016). Crimean-Congo hemorrhagic fever virus (CCHFV) is transmitted to humans by the bite of infected ticks (Hyalomma spp. are the most competent vectors) or by direct contact with blood or tissues of viremic patients or animals, causing a disease characterized by fever, headache, myalgia, and hemorrhagic manifestations (Papa, 2010). If the appropriate receptors are present in the tick, following a blood meal TBEV and CCHFV enter vector host cells by endocytosis (Labuda and Nuttall, 2003; Simon et al., 2009; Garrison et al., 2013; Shtanko et al., 2014; Suda et al., 2016). These viruses replicate in the lining of the tick midgut where they disseminate to the hemolymph and subsequently infect different tissues reaching the highest titers in the salivary glands and reproductive organs to exit the cell via exocytosis (Dickson and Turell, 1992).
Babesia spp. are tick-borne Apicomplexan protozoans which invade vertebrate host erythrocytes, where all hemoparasite phases occur (Yokoyama et al., 2006; Chauvin et al., 2009; Florin-Christensen and Schnittger, 2009). Babesia bovis and Babesia bigemina, transmitted mainly by Rhipicephalus microplus and Rhipicephalus annulatus, are considered the most important species for their great economic impact on the cattle industry. Humans are accidental hosts, but human babesiosis caused by Babesia microti is now considered an emerging zoonosis as cases are increasing yearly (Schnittger et al., 2012). Ticks become infected with Babesia parasites when ingesting blood cells containing piroplasms, which develop into male and female gametes in the tick midgut (Uilenberg, 2006). The zygotes then multiply and invade numerous tick organs including the ovaries, which results in transovarial passage for some species such as B. bovis and B. bigemina but not B. microti (Uilenberg, 2006). When ticks attach to a new host, the sporozoites mature and the parasites are transmitted with tick saliva and infect red blood cells (Uilenberg, 2006).
Biological Processes Involved in Tick-Pathogen Interactions
The objective of this paper is to review the information available on tick-pathogen molecular interactions and their role in vector competence. To address this objective, we discussed the main biological processes involved in tick-pathogen interactions. Additionally, the impact of tick microbiome on these interactions was considered. Although host-tick and host-pathogen molecular interactions also affect vector competence, this review focuses on tick-pathogen interactions for the identification of molecular drivers affecting vector competence that may result in the identification of tick-derived and pathogen-derived antigens for the development of novel control and prevention strategies for tick-borne diseases.
Role of Bacterial Proteins in Tick-Pathogen Interactions
Tick-pathogen protein-protein interactions play a crucial role during pathogen infection, persistence and transmission. The analysis of A. phagocytophilum proteins differentially represented during infection in ticks demonstrated that heat shock protein 70 (HSP70) and major surface protein 4 (MSP4) interact and bind to tick cells, thus playing a role in tick-pathogen interactions (Villar et al., 2015b). The type IV secretion system (T4SS) was proposed to be involved in the secretion of HSP70 and the MSP4 interaction with tick cells may induce the secretion of vesicles at the phagocytic cup to aid in adhesin secretion for rickettsial infection of tick cells (Villar et al., 2015b). Recent results have advanced our understanding of the molecular factors that are involved in the acquisition, persistence and transmission of B. burgdorferi in ticks (Rosa et al., 2005; Kung et al., 2013). An important protein involved in spirochete colonization of the tick midgut is the outer surface protein A (OspA), which binds to the tick receptor for OspA (TROSPA) (Pal et al., 2004). An I. scapularis dystroglycan like protein (ISDLP) as well as a tick receptor for the B. burgdorferi protein BBE31 (TRE31) help spirochetes traverse from the tick midgut into the hemocoel (Zhang L. et al., 2011; Coumou et al., 2016). B. burgdorferi outer surface protein C (OspC), produced when bacteria leave the tick midgut, binds to tick salivary protein 15 (Salp15) (Ramamoorthi et al., 2005), providing protection against mammalian antibody/complement-mediated immune response during bacterial transmission (Garg et al., 2006; Schuijt et al., 2011a). The TROSPA homolog in the B. bigemina vectors, R. microplus, and R. annulatus was proposed to be a putative receptor for Babesia ligands based on the decrease in infection after RNAi and vaccination experiments targeting this protein (Antunes et al., 2012; Merino et al., 2013). Flaviviruses and CCHFV enter vertebrate and vector host cells by attachment of viral envelope proteins to host receptors, which activates the actin-dependent clathrin-mediated endocytic pathway (Labuda and Nuttall, 2003; Simon et al., 2009; Garrison et al., 2013).
Intracellular bacteria induce cytoskeletal rearrangement to establish infection (Ireton, 2013). In I. scapularis, A. phagocytophilum remodels tick cytoskeleton by altering the ratio between monomeric globular G actin and filamentous F actin to facilitate infection through selective regulation of gene transcription in association with the RNA polymerase II and the TATA-binding protein (Sultana et al., 2010). In I. scapularis midgut cells, the up-regulation of Spectrin alpha chain or Alpha-fodrin in response to infection results in cytoskeleton remodeling that is used by A. phagocytophilum to facilitate infection (Ayllón et al., 2013, Figure 2A). Although not functionally characterized, a proteomics analysis in I. ricinus tick salivary glands showed the under-representation of cytoskeleton proteins in response to Borrelia infection, suggesting that some Borrelia strains promote a cytoskeleton rearrangement in ticks (Cotté et al., 2014, Figure 2B).
Figure 2. Tick-pathogen molecular interactions. (A) A. phagocytophilum (B) B. burgdorferi s.l., (C) TBEV, and (D) B. bovis/B. bigemina activate mechanisms (panel 1) and manipulate tick protective responses and other biological processes in order to facilitate infection (panel 2), while ticks respond to limit pathogen infection and preserve feeding fitness and vector competence for survival of both ticks and pathogens (panel 3). MG, midgut; HE, hemocyte; SG, salivary gland; MSPs, major surface proteins; HSPs, heat shock proteins; ER, endoplasmic reticulum.
Tick Cell Apoptosis
Apoptosis is an intrinsic immune defense mechanism in response to microbial infection that results in reduction of infected cells, but several pathogens have developed different strategies to inhibit cell apoptosis in order to enhance their infection, replication and survival (Ashida et al., 2011). Infection of tick salivary glands with A. phagocytophilum results in inhibition of the intrinsic apoptosis pathway through porin down-regulation, favoring bacterial infection (Ayllón et al., 2015a). Tick cells respond to infection via activation of the extrinsic apoptosis pathway, which limits A. phagocytophilum infection and promotes tick survival (Ayllón et al., 2015a). In tick midguts, A. phagocytophilum infection results in activation of the Janus kinase/signal transducers and activators of transcription (JAK/STAT) pathway, which inhibits apoptosis and promotes pathogen infection (Ayllón et al., 2015a). The ISE6 cultured cells, derived from embryonic I. scapularis, have provided a model for tick hemocyte responses to pathogen infection. In this cell line, A. phagocytophilum infection promotes protein misfolding in the endoplasmic reticulum (ER), counteracting the tick cell response to infection. However, tick cells respond by activating protein targeting and degradation, which reduces ER stress and apoptosis, thus favoring A. phagocytophilum infection (Villar et al., 2015a). Additionally, A. phagocytophilum may benefit from the tick cells ability to limit pathogen infection through phosphoenolpyruvate carboxykinase (PEPCK) inhibition that results in lower glucose metabolism and the reduction in the availability of essential metabolites for bacterial growth, which leads to the inhibition of cell apoptosis that increases infection in tick cells (Villar et al., 2015a). These results show that the inhibition of tick cell apoptosis is a physiologically relevant mechanism used by A. phagocytophilum to facilitate infection and multiplication in both tick and vertebrate host cells (de la Fuente et al., 2016, Figure 4). Infection of I. ricinus cells with flaviviruses leads to the differential expression of a large number of genes involved in a variety of cellular functions, including up-regulation of genes such as cytochrome c associated with cellular stress and apoptosis (Mansfield et al., 2017). However, the lack of detection of caspase genes, and the up-regulation of genes that inhibit apoptosis (including hsp70) suggest that flavivirus infection inhibits tick cell apoptosis in order to promote cell survival during infection as previously shown for A. phagocytophilum (Ayllón et al., 2015a; Alberdi et al., 2016).
Tick Innate Immune Response
Tick vector competence is influenced by the ability of transmitted pathogens to evade tick innate immune response (Hajdušek et al., 2013). Several humoral and cell-mediated immune response pathways are involved in tick innate immunity, and play a role in defense to Anaplasma, Borrelia, flavivirus, and Babesia infection or are manipulated by pathogens to facilitate infection (Turell, 2007; Hajdušek et al., 2013; Mansfield et al., 2017, Figure 2). With respect to the tick innate immune response, A. phagocytophilum subverts tick RNAi by mechanisms other than reduction of Tudor staphylococcal nuclease (Tudor-SN) levels to preserve a protein that is important for tick feeding (Ayllón et al., 2015b). In contrast, Subolesin (SUB), also involved in tick innate immune response for limiting pathogen infection (Naranjo et al., 2013; de la Fuente and Contreras, 2015), is not manipulated by A. phagocytophilum. SUB has been shown to be required for tick feeding and reproduction and for pathogen infection, and therefore the preservation of this protein is important for both tick and pathogen survival (de la Fuente and Contreras, 2015). In I. scapularis, the x-linked inhibitor of apoptosis protein (XIAP) interacts with the E2 conjugating enzyme Bendless affecting positive and negative regulators of the immune deficiency (IMD) pathway resulting in protection against infection by A. phagocytophilum (Severo et al., 2013).
After molting, tick nymphs attach and start feeding, displaying an altered midgut transcriptome when infected with B. burgdorferi (Rudenko et al., 2005). Some of the genes affected by infection include innate immune factors (defensin and thioredoxin peroxidase) that possibly limit tick Borrelia infection. Tick salivary protein 20 (Salp20) belongs to a protein family with complement-inhibitory activity that blocks the host alternative complement pathway and assists in Borrelia transmission (Hourcade et al., 2016). Tick salivary lectin pathway inhibitor (TSLPI) inhibits the human lectin complement pathway by interfering with the mannose binding lectin activity and enables transmission of Borrelia by protecting it from complement-mediated killing (Schuijt et al., 2011b; Wagemakers et al., 2016). Recently, Smith et al. (2016) showed that I. scapularis respond to interferon gamma acquired in the blood meal when parasitizing on B. burgdorferi-infected mice, leading to the up-regulation of the Rho-like GTPase and induction of antimicrobial peptides to inhibit pathogen infection.
Preliminary studies focusing on transcriptomic changes induced by TBEV infection of I. scapularis and I. ricinus cells have revealed the role of particular proteins within tick innate immune pathways that act to control infection (Weisheit et al., 2015). A similar approach has identified this response in tick cells infected with LIV and TBEV, with a range of transcripts being up and down-regulated (Weisheit et al., 2015; Mansfield et al., 2017). Flavivirus infection also induced transcripts associated with activation of innate immune pathways in tick cells, including JAK/STAT and Mitogen-activated protein kinase (MAPK) pathways (Mansfield et al., 2017), with additional up-regulation of genes with host resistance functions, including FK506 binding protein (FKBP) and the antiviral helicase Slh1 (Mansfield et al., 2017, Figure 2C). CCHFV is capable of evading the tick innate immune response. Following intracoelomic CCHFV inoculation, virus titers in male and female ticks are the same and infection rates and titers in salivary glands, ovaries, and testes increase upon blood feeding (Dickson and Turell, 1992). Therefore, viral replication in tissues associated with possible CCHFV transmission in infected ticks may be stimulated by attachment and feeding on susceptible hosts. This might reduce the stress induced by viral replication while ticks are waiting to find a vertebrate host, but increase the potential for viral transmission once the host is infested (Turell, 2007).
Using different methodologies, some molecules have been identified as being implicated in tick-Babesia interactions (Hajdušek et al., 2013). Genes involved in immunity, stress, and defense responses showed up-regulation in response to B. bovis infection (Heekin et al., 2012), while genes encoding for calreticulin, kunitz-type serine protease inhibitors and microplusin which exhibits antimicrobial activity, were differentially expressed in B. bovis/B. bigemina infected Rhipicephalus ticks (Rachinsky et al., 2007; Antunes et al., 2012; Heekin et al., 2013; Lu et al., 2016). Tick SUB (Almazán et al., 2005) was shown to be up-regulated in B. microti inoculated intrahemocoelically into Rhipicephalus haemaphysaloides (Lu et al., 2016) and B. bigemina-infected R. microplus (Merino et al., 2013) (Figure 2D). The putative role of SUB in B. bigemina infection in ticks was supported by showing a decrease in pathogen levels in ticks fed on cattle immunized with recombinant SUB (Merino et al., 2013).
Tick Cell Epigenetics
Intracellular pathogens manipulate the transcriptional programs of their host cells via epigenetic mechanisms, leading to stress, and inflammatory responses (Gómez-Díaz et al., 2012). Recently, A. phagocytophilum was shown to manipulate tick cell epigenetics to increase the levels of the histone modifying enzymes (HMEs), histone acetyltransferases (HATs; 300/CBP), and histone deacetylases (HDACs and Sirtuins) resulting in the inhibition of cell apoptosis to facilitate pathogen infection and multiplication (Cabezas-Cruz et al., 2016). The results of this study suggested that a compensatory mechanism might exist by which A. phagocytophilum differentially manipulates tick HMEs to regulate transcription and apoptosis in a tissue-specific manner to facilitate infection but preserving tick fitness to guarantee survival of both pathogens and ticks (Cabezas-Cruz et al., 2016). As previously discussed (Cabezas-Cruz et al., 2016), the mechanisms by which A. phagocytophilum affects tick cell epigenetics is unknown but effector proteins such as AnkA, secreted through T4SS or other secretion mechanisms probably control it (Garcia-Garcia et al., 2009a,b; Rennoll-Bankert et al., 2015). It has been previously demonstrated that A. phagocytophilum AnkA recruits host histone deacetylase 1 (HDAC1) and modifies neutrophils gene expression (Garcia-Garcia et al., 2009a,b; Rennoll-Bankert et al., 2015). Interestingly, the homolog of HDAC1 in I. scapularis was overrepresented upon A. phagocytophilum infection in tick salivary glands (Cabezas-Cruz et al., 2016). It remains to be tested whether A. phagocytophilum AnkA plays the same role in ticks as in vertebrate neutrophils.
Effect of Pathogen Infection on Tick Fitness
The characterization of I. scapularis-A. phagocytophilum molecular interactions revealed complex responses by both ticks and pathogens that were necessary for maintenance of tick health while ensuring robust vector capacity (Ayllón et al., 2015a; Villar et al., 2015a; Gulia-Nuss et al., 2016; de la Fuente et al., 2016). Several lines of evidence suggest that tick-pathogen associations evolved to form “intimate epigenetic relationships” that have the potential to increase tick fitness (Cabezas-Cruz et al., 2017). At the tick-pathogen interface, A. phagocytophilum induces an antifreeze glycoprotein (IAFGP) and heat shock proteins (HSPs) to increase tick survival and feeding fitness (Neelakanta et al., 2010; Busby et al., 2012). Neelakanta et al. (2010) demonstrated that I. scapularis ticks infected with A. phagocytophilum show enhanced fitness against freezing injury due to the induced expression of IAFGP. They further showed that improved survival of infected ticks correlated with higher bacterial infection, therefore providing a direct link between pathogen infection and tick fitness in unfavorable ecological conditions. The fact that Borrelia and TBEV-infected ticks choose a higher questing height suggests that these pathogens help ticks to survive under dry conditions. In agreement with this hypothesis, I. ricinus infected by B. burgdorferi move less toward a humid environment and their survival is higher in highly desiccating conditions (Hermann and Gern, 2010; Herrmann and Gern, 2012). The tick histamine release factor (tHRF), up-regulated in B. burgdorferi-infected I. scapularis during feeding, facilitates tick engorgement and B. burgdorferi infection by increasing the blood flow to the tick-bite site and modulating vascular permeability (Dai et al., 2010).
The recent development of high-throughput next generation sequencing technologies has highlighted the complexity of the tick microbiome that includes both pathogens and potential symbionts (Vayssier-Taussat et al., 2015). It is readily apparent that interactions frequently occur among tick microbial communities, as relationships between microorganisms existing in one environment can be competitive, exclusive, facilitating, or absent, with many potential implications for human and animal health that remain to be elucidated (Ahantarig et al., 2013; Vayssier-Taussat et al., 2015). Both positive and negative associations have been reported for pathogens (Mather et al., 1987; de la Fuente et al., 2003). However, the role of tick endosymbionts in pathogen transmission has only been studied in a few selected bacterial and tick species.
Symbionts may confer crucial and diverse benefits to their hosts, playing nutritional roles, or affecting fitness, development, reproduction, defense against environmental stress, and immunity (Ahantarig et al., 2013). Coxiella-like endosymbionts are believed to be the most common vertically transmitted agents in hard ticks (Bernasconi et al., 2002; Lee et al., 2004; Clay et al., 2008; Bonnet et al., 2013; Cooper et al., 2013). In Amblyomma americanum, the removal of Coxiella symbionts following antibiotic treatment reduced tick offspring production and increased time to oviposition (Zhong et al., 2007). In I. ricinus (Lo et al., 2006; Sassera et al., 2006; Montagna et al., 2013), Candidatus Midichloria mitochondrii is an intra-mitochondrial bacterium that has also been detected in other tick genera (Harrus et al., 2011; Williams-Newkirk et al., 2012). It has been ascribed a possible helper role in tick molting processes (Zchori-Fein and Bourtzis, 2011, Figure 3). Rickettsia-like symbionts have also been reported to infect hard ticks from several genera (Baldridge et al., 2004; Clay et al., 2008; Liu et al., 2013). One study reported that Rickettsia-infected Dermacentor variabilis have slightly greater motility than uninfected ticks, indirectly influencing disease risk (Kagemann and Clay, 2013). Francisella-like symbionts have been reported in several hard tick genera (Venzal et al., 2008; Ivanov et al., 2011; Michelet et al., 2013), but their effect on tick fitness and biology remains unknown. Being able to manipulate host reproduction and then to affect vector populations, Wolbachia spp. have also been identified in several hard tick genera (Engelstadter and Hurst, 2007; Andreotti et al., 2011; Reis et al., 2011; Zhang X. et al., 2011). Their role in pathogen transmission requires further attention, as reports suggest that this bacterium can protect some arthropods against microbial infections (Martinez et al., 2014). In I. ricinus, Wolbachia pipientis is known to be associated with the hymenoptera tick endoparasitoid Ixodiphagus hookeri (Plantard et al., 2012; Bohacsova et al., 2016), and Arsenophonus spp. symbionts (Dergousoff and Chilton, 2010). The latter, detected in several tick species (Clay et al., 2008; Dergousoff and Chilton, 2010; Reis et al., 2011), are responsible for sex-ratio distortion in arthropods, and some studies suggest that they can affect host-seeking success by decreasing tick motility in A. americanum and D. variabilis (Kagemann and Clay, 2013). Lastly, some Spiroplasma spp. detected in Ixodes spp. such as Spiroplasma ixodetis (Tully et al., 1995) may cause sex-ratio distortion in some insect species via male killing (Tabata et al., 2011).
Figure 3. Possible impact of tick microbiome on pathogen transmission. Tick microbiome may affect pathogen transmission either directly via nutrient competition or induced/reduced immunity, or indirectly by affecting tick populations (viability, reproduction) or fitness (affecting host-seeking success). MG, midgut; SG, salivary gland; OV, ovaries.
Recently, Abraham et al. (2017) showed how A. phagocytophilum manipulates I. scapularis tick microbiota to promote infection. Firstly, they showed that IAFGP, apart from protecting ticks against cold injury (see above), has antimicrobial activity against biofilm-forming bacteria, particularly Staphylococcus aureus and Enterococcus faecalis. They further showed that by targeting biofilm-forming bacteria, A. phagocytophilum modifies the composition of gut microbiota and alters tick midguts permeability, which results in higher A. phagocytophilum infection in the vector (Abraham et al., 2017). Regarding the relationship between symbionts and pathogens, exclusion has been reported in Rickettsiales, which may be due to intra-family bacterial cross-immunity. Exclusion has been documented in Dermacentor ticks infected with Rickettsia peacockii or Rickettsia montana that limits Rickettsia rickettsii and Rickettsia rhipicephali distribution, respectively (Burgdorfer et al., 1981; Macaluso et al., 2002, Figure 3). It has also been reported that I. scapularis male ticks infected by a rickettsial endosymbiont had significantly lower rates of infection by B. burgdorferi than symbiont-free males, thus evidencing interactions among microbial species (Steiner et al., 2008). Further research showed that perturbation of the midgut microbiome in I. scapularis influences B. burgdorferi colonization of ticks through a transcriptional mechanism resulting in lower expression of peritrophin, which perturbs the integrity of the peritrophic matrix (Narasimhan et al., 2014). In A. americanum, the presence of Coxiella-related symbionts seems to influence Ehrlichia chaffeensis transmission (Klyachko et al., 2007), and infection with Arsenophonus appears to be negatively correlated with the frequency of Rickettsia sp. infection (Clay et al., 2008, Figure 3).
Conclusions and Future Directions for the Control of Tick-Borne Diseases
Over millions of years, arthropod vectors have co-evolved with a variety of microorganisms including bacteria, viruses, and protozoa to the point where they appear to co-exist with little impact on the vector (Beerntsen et al., 2000; Estrada-Peña et al., 2015; de la Fuente et al., 2015). These arthropods have become efficient vectors of pathogens to humans and other vertebrate hosts that are susceptible to infection and disease.
Present results show that different pathogens have developed similar strategies such as manipulation of the immune response to infect ticks and facilitate multiplication and transmission. Some of these strategies may be used by pathogens to infect both ticks and mammalian hosts (de la Fuente et al., 2016). Additionally, recent evidence demonstrates that the microbiome has an effect on tick fitness and pathogen infection and transmission, highlighting the importance of tick-microbiome interactions for vector competence. Overall, these results illustrate how pathogens activate mechanisms and manipulate tick protective responses and other biological processes in order to facilitate infection, while ticks respond to limit pathogen infection and preserve feeding fitness and vector competence for survival of both ticks and pathogens. However, how different molecular mechanisms make certain tick species suitable vectors for certain pathogens is still not fully characterized. The presence of tick receptors that are pathogen-specific affects vector competence for these pathogens, but other mechanisms are probably also involved in this process. Furthermore, the biological processes involved in tick-pathogen interactions are also affected in other arthropod vectors (Box 2).
Box 2. Are the biological processes involved in tick-pathogen interactions unique for ticks?
The answer to this question is that several of the processes involved in tick-pathogen interactions have also been identified in other vector-pathogen interactions (see for example, Beerntsen et al., 2000; Vlachou et al., 2005; Wang et al., 2010; Gómez-Díaz et al., 2012; Sabin et al., 2013; Ramphul et al., 2015; Eng et al., 2016; Shaw et al., 2017). For example, as described in ticks, receptor-ligand-like interactions mediate pathogen recognition and infection in mosquitoes (Beerntsen et al., 2000). Remodeling of the cytoskeleton seems to be a general mechanism for tick pathogen infection (Cotté et al., 2014; de la Fuente et al., 2016). Pathogens such as Dengue virus (DENV), West Nile virus (WNV), and Plasmodium parasites also affect mosquito cytoskeleton during infection (Vlachou et al., 2005; Wang et al., 2010). The finding that some pathogens manipulate tick immune response to facilitate infection has been also reported in mosquitoes infected with Plasmodium falciparum (Beerntsen et al., 2000). Similarly, the expression of immune response genes such as those involved in the JAK/STAT pathway may serve to limit bacterial and fungal proliferation in fruit fly and mosquitoes (Beerntsen et al., 2000). Apoptosis plays an important role in tick-pathogen interactions (de la Fuente et al., 2016). While inhibition of cell apoptosis by pathogens facilitates infection, host cell response may activate alternative apoptotic pathways to limit infection (de la Fuente et al., 2016). These findings have been also described in for example Aedes aegypti and Anopheles gambiae mosquitoes infected with DENV and P. falciparum, respectively (Ramphul et al., 2015; Eng et al., 2016). The control of tick cell epigenetics by A. phagocytophilum has been proposed as a mechanism used by the pathogen to facilitate infection and multiplication (Cabezas-Cruz et al., 2016). Similar mechanisms have been described to operate at the mosquito-Plasmodium interface (Gómez-Díaz et al., 2012).
However, the functional mechanisms by which these processes are affected at the vector-pathogen interface may vary between pathogen and vector species (Figure 4). The limited information available on the functional characterization of these processes in ticks and other arthropods limits the scope of the comparative analysis between different vectors. Nevertheless, recent results support that in some cases the protein function described in model insect species may be different in the evolutionarily distant ticks. Differences in vector competence may be genetically encoded by differences in the immune response pathways operating at each vector-pathogen interaction (Baxter et al., 2017). For example, Tudor-SN, a conserved component of the basic RNAi machinery with a variety of functions including immune response and gene regulation, is involved in defense against infection in Drosophila (Sabin et al., 2013) but not in ticks (Ayllón et al., 2015b). The IMD pathway is involved in protection against infection in arthropods, but recent results support the existence of two functionally distinct IMD circuits in insects and ticks (Shaw et al., 2017). Future comparative analyses between different vector species will provide additional information on the functional implication of the different biological processes in vector-pathogen interactions and vector competence (Gerold et al., 2017).
Figure 4. Pathogens inhibit vector cell apoptosis by different mechanisms. After infection of tick salivary glands, A. phagocytophilum inhibit apoptosis by decreasing the expression of the pro-apoptotic genes coding for proteins such as ASK1 and Porin. Porin down-regulation is associated with the inhibition of mitochondrial Cyt c release (Ayllón et al., 2015a). In contrast, A. phagocytophilum infection does not affect Bcl-2 levels, probably because this protein but not Porin is essential for tick feeding (Ayllón et al., 2015a). A. phagocytophilum also induces ER stress in tick cells which play a role in reducing the levels of MKK that inhibits apoptosis (Villar et al., 2015a). Another interesting mechanism of A. phagocytophilum to inhibit apoptosis is the manipulation of glucose metabolism by reducing the levels of PEPCK (Villar et al., 2015a). The capacity of A. phagocytophilum to downregulate gene expression in neutrophils was associated with HDAC1 recruitment to the promoters of target genes by the ankyrin repeat protein AnkA (Garcia-Garcia et al., 2009a,b; Rennoll-Bankert et al., 2015). Tick HDAC1 is overrepresented in A. phagocytophilum-infected salivary glands and chemical inhibition of this protein decreases A. phagocytophilum burden in tick cells (Cabezas-Cruz et al., 2016). Infection of tick cells with flaviviruses results in the up-regulation of genes such as hsp70 that inhibit apoptosis (Mansfield et al., 2017). N, Nucleus; M, Mitochondria; ER, Endoplasmic Reticulum; Cyt c, Cytochrome c; ASK1, Apoptosis signal-regulating kinase 1; MKK, Mitogen-activated Protein Kinase; HDAC1, Histone Deacetylase 1; AnkA, Ankyrin A; PEPCK, Phosphoenolpyruvate Carboxykinase; FOXO, Forkhead box O; Hid, Head involution defective; JNK, Jun amino-terminal kinases; Casp, caspases. The molecules and processes represented in green are up-regulated, while those represented in red are down-regulated in response to infection. The activity of the molecules represented in blue varies in response to infection.
The identification of the molecular drivers that promote tick survival, spread, and pathogen transmission provides the opportunity to disrupt these processes and lead to a reduction in tick burden and prevalence of tick-borne diseases. Targeting some of the similar mechanisms used by the pathogens for infection and transmission by ticks may be used to develop strategies against multiple tick-borne diseases. As shown for B. burgdorferi OspA (Gomes-Solecki, 2014), pathogen-derived proteins involved in interactions with tick cells and playing a role during infection provide targets for development of novel control strategies for pathogen infection and transmission. Similarly, tick-derived antigens such as SUB involved in different biological processes may be used to reduce vector infestations and pathogen infection in ticks feeding on immunized animals (de la Fuente and Contreras, 2015). One novel approach to control populations might be to target specific endosymbionts, which requires detailed knowledge of microbial communities and their impact on tick biology (Taylor et al., 2012). Finally, the surveillance of microbial populations in tick salivary glands may enable the early identification of pathogens likely to be transmitted to vertebrate host (Qiu et al., 2014). Overall, the combination of effective and early diagnostics along with tick vaccines and strategies such as harnessing genetics to improve livestock breeds, and the rational application of acaricides, antivirals and other therapeutic interventions will result in a more effective and environmentally friendly control of tick populations. In addition, transgenic or paratransgenic ticks and vertebrate host genetically modified to confer resistance to pathogen infection may be produced and combined with vaccine applications and other interventions (de la Fuente and Kocan, 2014).
JF, SA, SB, AD, AE, NJ, KM, AN, AP, NR, AF, ROMR conducted the literature research and wrote the paper. JF, AC, AP, SB, AN, NJ prepared the figures and tables. All authors provided critical review and revisions.
Part of the research included in this review was supported by the Ministerio de Economia y Competitividad (Spain) grant BFU2016-79892-P and the European Union (EU) Seventh Framework Programme (FP7) ANTIGONE project number 278976. SA and AD would like to acknowledge FCT for funds to GHTM - UID/Multi/04413/2013. MV was supported by the Research Plan of the University of Castilla-La Mancha (UCLM), Spain. The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
We thank members of our laboratories for fruitful discussions.
Abraham, N. M., Liu, L., Jutras, B. L., Yadav, A. K., Narasimhan, S., Gopalakrishnan, V., et al. (2017). Pathogen-mediated manipulation of arthropod microbiota to promote infection. Proc. Natl. Acad. Sci. U.S.A. 114, E781–E790. doi: 10.1073/pnas.1613422114
Ahantarig, A., Trinachartvanit, W., Baimai, V., and Grubhoffer, L. (2013). Hard ticks and their bacterial endosymbionts (or would be pathogens). Folia. Microbiol. 58, 419–428. doi: 10.1007/s12223-013-0222-1
Alberdi, P., Mansfield, K. L., Manzano-Román, R., Cook, C., Ayllón, N., Villar, M., et al. (2016). Tissue-specific signatures in the transcriptional response to Anaplasma phagocytophilum infection of Ixodes scapularis and Ixodes ricinus tick cell lines. Front. Cell. Infect. Microbiol. 6:20. doi: 10.3389/fcimb.2016.00020
Almazán, C., Kocan, K. M., Blouin, E. F., and de la Fuente, J. (2005). Vaccination with recombinant tick antigens for the control of Ixodes scapularis adult infestations. Vaccine 23, 5294–5298. doi: 10.1016/j.vaccine.2005.08.004
Andreotti, R., Perez de Leon, A. A., Dowd, S. E., Guerrero, F. D., Bendele, K. G., and Scoles, G. A. (2011). Assessment of bacterial diversity in the cattle tick Rhipicephalus (Boophilus) microplus through tag-encoded pyrosequencing. BMC. Microbiol. 11:6. doi: 10.1186/1471-2180-11-6
Antunes, S., Galindo, R. C., Almazán, C., Rudenko, N., Golovchenko, M., Grubhoffer, L., et al. (2012). Functional genomics studies of Rhipicephalus (Boophilus) annulatus ticks in response to infection with the cattle protozoan parasite, Babesia bigemina. Int. J. Parasitol. 42, 187–195. doi: 10.1016/j.ijpara.2011.12.003
Ashida, H., Mimuro, H., Ogawa, M., Kobayashi, T., Sanada, T., Kim, M., et al. (2011). Host-pathogen interactions cell death and infection: a double-edged sword for host and pathogen survival. J. Cell. Biol. 195, 931–942. doi: 10.1083/jcb.201108081
Ayllón, N., Naranjo, V., Hajdušek, O., Villar, M., Galindo, R. C., Kocan, K. M., et al. (2015b). Nuclease Tudor-SN is involved in tick dsRNA-mediated RNA interference and feeding but not in defense against flaviviral or Anaplasma phagocytophilum rickettsial infection. PLoS ONE 10:e0133038. doi: 10.1371/journal.pone.0133038
Ayllón, N., Villar, M., Busby, A. T., Kocan, K. M., Blouin, E. Bonzón-Kulichenko, E. F., et al. (2013). Anaplasma phagocytophilum inhibits apoptosis and promotes cytoskeleton rearrangement for infection of tick cells. Infect. Immun. 81, 2415–2425. doi: 10.1128/IAI.00194-13
Ayllón, N., Villar, M., Galindo, R. C., Kocan, K. M., Šíma, R., López, J. A., et al. (2015a). Systems biology of tissue-specific response to Anaplasma phagocytophilum reveals differentiated apoptosis in the tick vector Ixodes scapularis. PLoS Genet. 11:e1005120. doi: 10.1371/journal.pgen.1005120
Baldridge, G. D., Burkhardt, N. Y., Simser, J. A., Kurtti, T. J., and Munderloh, U. G. (2004). Sequence and expression analysis of the ompA gene of Rickettsia peacockii, an endosymbiont of the Rocky Mountain wood tick, Dermacentor andersoni. Appl. Environ. Microbiol. 70, 6628–6636. doi: 10.1128/AEM.70.11.6628-6636.2004
Bell-Sakyi, L., Zweygarth, E., Blouin, E. F., Gould, E. A., and Jongejan, F. (2007). Tick cell lines: tools for tick and tick-borne disease research. Trends. Parasitol. 23, 450–457. doi: 10.1016/j.pt.2007.07.009
Bernasconi, M. V., Casati, S., Peter, O., and Piffaretti, J. C. (2002). Rhipicephalus ticks infected with Rickettsia and Coxiella in Southern Switzerland (Canton Ticino). Infect. Genet. Evol. 2, 111–120. doi: 10.1016/S1567-1348(02)00092-8
Bohacsova, M., Mediannikov, O., Kazimirova, M., Raoult, D., and Sekeyova, Z. (2016). Arsenophonus nasoniae and Rickettsiae infection of Ixodes ricinus due to parasitic wasp Ixodiphagus hookeri. PLoS ONE 11:e0149950. doi: 10.1371/journal.pone.0149950
Bonnet, S., de la Fuente, J., Nicollet, P., Liu, X., Madani, N., Blanchard, B., et al. (2013). Prevalence of tick-borne pathogens in adult Dermacentor spp. ticks from nine collection sites in France. Vector Borne Zoonotic Dis. 13, 226–236. doi: 10.1089/vbz.2011.0933
Burgdorfer, W., Hayes, S., and Mavros, A. (1981). “Non-pathogenic rickettsiae in Dermacentor andersoni: a limiting factor for the distribution of Rickettsia rickettsia,” in Rickettsia and Rickettsial Disease, ed W. Burgdorfer (New York, NY: Academic Press), 585–594.
Busby, A. T., Ayllón, N., Kocan, K. M., Blouin, E. F., de la Fuente, G., Galindo, R. C., et al. (2012). Expression of heat-shock proteins and subolesin affects stress responses, Anaplasma phagocytophilum infection and questing behavior in the tick, Ixodes scapularis. Med. Vet. Entomol. 26, 92–102. doi: 10.1111/j.1365-2915.2011.00973.x
Cabezas-Cruz, A., Alberdi, P., Ayllón, N., Valdés, J. J., Pierce, R., Villar, M., et al. (2016). Anaplasma phagocytophilum increases the levels of histone modifying enzymes to inhibit cell apoptosis and facilitate pathogen infection in the tick vector, Ixodes scapularis. Epigenetics 11, 303–319. doi: 10.1080/15592294.2016.1163460
Cabezas-Cruz, A., Estrada-Peña, A., Rego, R. O. M., and De la Fuente, J. (2017). Tick-pathogen ensembles: do molecular interactions lead ecological innovation? Front. Cell. Infect. Microbiol. 7:74. doi: 10.3389/fcimb.2017.00074
Chauvin, A., Moreau, E., Bonnet, S., Plantard, O., and Malandrin, L. (2009). Babesia and its hosts: adaptation to long-lasting interactions as a way to achieve efficient transmission. Vet. Res. 40, 37. doi: 10.1051/vetres/2009020
Clay, K., Klyachko, O., Grindle, N., Civitello, D., Oleske, D., and Fuqua, C. (2008). Microbial communities and interactions in the lone star tick, Amblyomma americanum. Mol. Ecol. 17, 4371–4381. doi: 10.1111/j.1365-294X.2008.03914.x
Cooper, A., Stephens, J., Ketheesan, N., and Govan, B. (2013). Detection of Coxiella burnetii DNA in wildlife and ticks in northern Queensland, Australia. Vector Borne Zoonotic Dis. 13, 12–16. doi: 10.1089/vbz.2011.0853
Cotté, V., Sabatier, L., Schnell, G., Carmi-Leroy, A., Rousselle, J. C., Arsène-Ploetze, F., et al. (2014). Differential expression of Ixodes ricinus salivary gland proteins in the presence of the Borrelia burgdorferi sensu lato complex. J. Proteomics. 96, 29–43. doi: 10.1016/j.jprot.2013.10.033
Coumou, J., Narasimhan, S., Trentelman, J. J., Wagemakers, A., Koetsveld, J., Ersoz, J. I., et al. (2016). Ixodes scapularis dystroglycan-like protein promotes Borrelia burgdorferi migration from the gut. J. Mol. Med. 94, 361–370. doi: 10.1007/s00109-015-1365-0
Cramaro, W. J., Revets, D., Hunewald, O. E., Sinner, R., Reye, A. L., and Muller, C. P. (2015). Integration of Ixodes ricinus genome sequencing with transcriptome and proteome annotation of the naive midgut. BMC Genomics 16:871. doi: 10.1186/s12864-015-1981-7
Dai, J., Narasimhan, S., Zhang, L., Liu, L., Wang, P., and Fikrig, E. (2010). Tick histamine release factor is critical for Ixodes scapularis engorgement and transmission of the Lyme disease agent. PLoS Pathog. 6:e1001205. doi: 10.1371/journal.ppat.1001205
de Castro, M. H., de Klerk, D., Pienaar, R., Latif, A. A., Rees, D. J., and Mans, B. J. (2016). De novo assembly and annotation of the salivary gland transcriptome of Rhipicephalus appendiculatus male and female ticks during blood feeding. Ticks Tick Borne Dis. 7, 536–548. doi: 10.1016/j.ttbdis.2016.01.014
de la Fuente, J., Blouin, E. F., and Kocan, K. M. (2003). Infection exclusion of the rickettsial pathogen Anaplasma marginale in the tick vector Dermacentor variabilis. Clin. Diagn. Lab. Immunol. 10, 182–184. doi: 10.1128/cdli.10.1.182-184.2003
de la Fuente, J., Estrada-Peña, A., Cabezas-Cruz, A., and Brey, R. (2015). Flying ticks: anciently evolved associations that constitute a risk of infectious disease spread. Parasit Vectors 8, 538. doi: 10.1186/s13071-015-1154-1
de la Fuente, J., Estrada-Peña, A., Cabezas-Cruz, A., and Kocan, K. M. (2016). Anaplasma phagocytophilum uses common strategies for infection of ticks and vertebrate hosts. Trends Microbiol. 24, 173–180. doi: 10.1186/s13071-015-1154-1
de la Fuente, J., Estrada-Peña, A., Venzal, J. M., Kocan, K. M., and Sonenshine, D. E. (2008). Overview: ticks as vectors of pathogens that cause disease in humans and animals. Front. Biosci. 13, 6938–6946. doi: 10.2741/3200
de la Fuente, J., Garcia-Garcia, J. C., Blouin, E. F., McEwen, B. R., Clawson, D., and Kocan, K. M. (2001). Major surface protein 1a effects tick infection and transmission of Anaplasma marginale. Int. J. Parasitol. 31, 1705–1714. doi: 10.1016/S0020-7519(01)00287-9
de la Fuente, J., and Kocan, K. M. (2014). “Development of vaccines for control of tick infestations and interruption of pathogen transmission,” in Biology of Ticks, 2nd Edn., ed D. Sonenshine and M Roe (New York, NY: Oxford University Press), 333–352.
Dergousoff, S. J., and Chilton, N. B. (2010). Detection of a new Arsenophonus-type bacterium in Canadian populations of the Rocky Mountain wood tick, Dermacentor andersoni. Exp. Appl. Acarol. 52, 85–91. doi: 10.1007/s10493-010-9340-5
Dickson, D. L., and Turell, M. J. (1992). Replication and tissue tropisms of Crimean-Congo hemorrhagic fever virus in experimentally infected adult Hyalomma truncatum (Acari: Ixodidae). J. Med. Entomol. 29, 767–773. doi: 10.1093/jmedent/29.5.767
Eng, M. W., van Zuylen, M. N., and Severson, D. W. (2016). Apoptosis-related genes control autophagy and influence DENV-2 infection in the mosquito vector, Aedes aegypti. Insect Biochem. Mol. Biol. 76, 70–83. doi: 10.1016/j.ibmb.2016.07.004
Estrada-Peña, A., de la Fuente, J., Ostfeld, R. S., and Cabezas-Cruz, A. (2015). Interactions between tick and transmitted pathogens evolved to minimise competition through nested and coherent networks. Sci. Rep. 5:10361. doi: 10.1038/srep10361
Estrada-Peña, A., Ortega, C., Sánchez, N., Desimone, L., Sudre, B., Suk, J. E., et al. (2011). Correlation of Borrelia burgdorferi sensu lato prevalence in questing Ixodes ricinus ticks with specific abiotic traits in the western Palearctic. Appl. Environ. Microbiol. 77, 3838–3845. doi: 10.1128/AEM.00067-11
Garcia-Garcia, J. C., Barat, N. C., Trembley, S. J., and Dumler, J. S. (2009a). Epigenetic silencing of host cell defense genes enhances intracellular survival of the rickettsial pathogen Anaplasma phagocytophilum. PLoS Pathog. 5:e1000488. doi: 10.1371/journal.ppat.1000488
Garcia-Garcia, J. C., Rennoll-Bankert, K. E., Pelly, S., Milstone, A. M., and Dumler, J. S. (2009b). Silencing of host cell CYBB gene expression by the nuclear effector AnkA of the intracellular pathogen Anaplasma phagocytophilum. Infect Immun. 77, 2385–2391. doi: 10.1128/IAI.00023-09
Garg, R., Juncadella, I. J., Ramamoorthi, N., Ananthanarayanan, S. K., Thomas, V., Rincón, M., et al. (2006). Cutting edge: CD4 is the receptor for the tick saliva immunosuppressor, Salp15. J. Immunol. 177, 6579–6583. doi: 10.4049/jimmunol.177.10.6579
Garrison, A. R., Radoshitzky, S. R., Kota, K. P., Pegoraro, G., Ruthel, G., et al. (2013). Crimean-Congo hemorrhagic fever virus utilizes a clathrin- and early endosome-dependent entry pathway. Virology 444, 45–54. doi: 10.1016/j.virol.2013.05.030
Gerold, G., Bruening, J., Weigel, B., and Pietschmann, T. (2017). Protein interactions during the flavivirus and hepacivirus life cycle. Mol. Cell. Proteomics 16(4 Suppl. 1), S75–S91. doi: 10.1074/mcp.r116.065649
Gomes-Solecki, M. (2014). Blocking pathogen transmission at the source: reservoir targeted OspA-based vaccines against Borrelia burgdorferi. Front. Cell Infect Microbiol. 4:136. doi: 10.3389/fcimb.2014.00136
Gómez-Díaz, E., Jordà, M., Peinado, M. A., and Rivero, A. (2012). Epigenetics of host-pathogen interactions: the road ahead and the road behind. PLoS Pathog. 8:e1003007. doi: 10.1371/journal.ppat.1003007
Gulia-Nuss, M., Nuss, A. B., Meyer, J. M., Sonenshine, D. E., Roe, R. M., Waterhouse, R. M., et al. (2016). Genomic insights into the Ixodes scapularis tick vector of Lyme disease. Nat. Commun. 7:10507. doi: 10.1038/ncomms10507
Hajdušek, O., Síma, R., Ayllón, N., Jalovecká, M., Perner, J., de la Fuente, J., et al. (2013). Interaction of the tick immune system with transmitted pathogens. Front. Cell Infect Microbiol. 3:26. doi: 10.3389/fcimb.2013.00026
Harrus, S., Perlman-Avrahami, A., Mumcuoglu, K. Y., Morick, D., Eyal, O., and Baneth, G. (2011). Molecular detection of Ehrlichia canis, Anaplasma bovis, Anaplasma platys, Candidatus Midichloria mitochondrii and Babesia canis vogeli in ticks from Israel. Clin. Microbiol. Infect 17, 459–463. doi: 10.1111/j.1469-0691.2010.03316.x
Heekin, A. M., Guerrero, F. D., Bendele, K. G., Saldivar, L., Scoles, G. A., Dowd, S. E., et al. (2013). The ovarian transcriptome of the cattle tick, Rhipicephalus (Boophilus) microplus, feeding upon a bovine host infected with Babesia bovis. Parasit. Vectors 6:276. doi: 10.1186/1756-3305-6-276
Heekin, A. M., Guerrero, F. D., Bendele, K. G., Saldivar, L., Scoles, G. A., Gondro, C., et al. (2012). Analysis of Babesia bovis infection-induced gene expression changes in larvae from the cattle tick, Rhipicephalus (Boophilus) microplus. Parasit. Vectors 5:162. doi: 10.1186/1756-3305-5-162
Hermann, C., and Gern, L. (2010). Survival of Ixodes ricinus (Acri: Ixodidae) under challenging conditions of temperature and humidity is influenced by Borrelia burgdorferi sensu laro infection. J. Med. Entomol. 47, 1196–1204. doi: 10.1603/ME10111
Herrmann, C., and Gern, L. (2012). Do the level of energy reserves, hydration status and Borrelia infection influence walking by Ixodes ricinus (Acari: Ixodidae) ticks? Parasitology 139, 330–337. doi: 10.1017/S0031182011002095
Hourcade, D. E., Akk, A. M., Mitchell, L. M., Zhou, H. F., Hauhart, R., et al. (2016). Anti-complement activity of the Ixodes scapularis salivary protein Salp20. Mol. Immunol. 69, 62–69. doi: 10.1016/j.molimm.2015.11.008
Ivanov, I. N., Mitkova, N., Reye, A. L., Hübschen, J. M., Vatcheva-Dobrevska, R. S., Dobreva, E. G., et al. (2011). Detection of new Francisella-like tick endosymbionts in Hyalomma spp. and Rhipicephalus spp. (Acari: Ixodidae) from Bulgaria. Appl. Environ. Microbiol. 77, 5562–5565. doi: 10.1128/AEM.02934-10
Johnson, N., Voller, K., Phipps, L. P., Mansfield, K. L., and Fooks, A. R. (2012). Rapid molecular detection methods for arboviruses of livestock of importance to Northern Europe. J. Biomed. Biotechnol. 2012:719402. doi: 10.1155/2012/719402
Kagemann, J., and Clay, K. (2013). Effects of infection by Arsenophonus and Rickettsia bacteria on the locomotive ability of the ticks Amblyomma americanum, Dermacentor variabilis, and Ixodes scapularis. J. Med. Entomol. 50, 155–162. doi: 10.1603/ME12086
Kleiboeker, S., Scoles, G. A., Burrage, T. G., and Sur, J. (1999). African swine fever virus replication in the midgut epithelium is required for infection of Ornithodoros ticks. J. Virol. 73, 8587–8598.
Klyachko, O., Stein, B. D., Grindle, N., Clay, K., and Fuqua, C. (2007). Localization and visualization of a coxiella-type symbiont within the lone star tick, Amblyomma americanum. Appl. Environ. Microbiol. 73, 6584–6594. doi: 10.1128/AEM.00537-07
Kotsyfakis, M., Schwarz, A., Erhart, J., and Ribeiro, J. M. (2015). Tissue-and time-dependent transcription in Ixodes ricinus salivary glands and midguts when blood feeding on the vertebrate host. Sci. Rep. 5:9103. doi: 10.1038/srep09103
Lee, J. H., Park, H. S., Jang, W. J., Koh, S. E., Park, T. K., Kang, S. S., et al. (2004). Identification of the Coxiella sp. detected from Haemaphysalis longicornis ticks in Korea. Microbiol. Immunol. 48, 125–130. doi: 10.1111/j.1348-0421.2004.tb03498.x
Liu, L. M., Liu, J. N., Liu, Z., Yu, Z. J., Xu, S. Q., Yang, X. H., et al. (2013). Microbial communities and symbionts in the hard tick Haemaphysalis longicornis (Acari: Ixodidae) from north China. Parasit. Vectors 6:310. doi: 10.1186/1756-3305-6-310
Lo, N., Beninati, T., Sassera, D., Bouman, E. A., Santagati, S., Gern, L., et al. (2006). Widespread distribution and high prevalence of an alpha-proteobacterial symbiont in the tick Ixodes ricinus. Environ. Microbiol. 8, 1280–1287. doi: 10.1111/j.1462-2920.2006.01024.x
Lu, P., Zhou, Y., Yu, Y., Cao, J., Zhang, H., Gong, H., et al. (2016). RNA interference and the vaccine effect of a subolesin homolog from the tick Rhipicephalus haemaphysaloides. Exp. Appl. Acarol. 68, 113–126. doi: 10.1007/s10493-015-9987-z
Macaluso, K. R., Sonenshine, D. E., Ceraul, S. M., and Azad, A. F. (2002). Rickettsial infection in Dermacentor variabilis (Acari: Ixodidae) inhibits transovarial transmission of a second Rickettsia. J. Med. Entomol. 39, 809–813. doi: 10.1603/0022-2585-39.6.809
Mansfield, K. L., Cook, C., Ellis, R., Bell-Sakyi, L., Johnson, N., Alberdi, P., et al. (2017). Tick-borne pathogens induce differential expression of genes promoting cell survival and host resistence in Ixodes ricinus cells. Parasit. Vectors 10:81. doi: 10.1186/s13071-017-2011-1
Mansfield, K. L., Johnson, N., Banyard, A. C., Núñez, A., Baylis, M., Solomon, T., et al. (2016). Innate and adaptive immune responses to tick-borne flavivirus infection in sheep. Vet. Microbiol. 185, 20–28. doi: 10.1016/j.vetmic.2016.01.015
Martinez, J., Longdon, B., Bauer, S., Chan, Y. S., Miller, W. J., Bourtzis, K., et al. (2014). Symbionts commonly provide broad spectrum resistance to viruses in insects: a comparative analysis of Wolbachia strains. PLoS Pathog. 10:e1004369. doi: 10.1371/journal.ppat.1004369
Merino, O., Antunes, S., Mosqueda, J., Moreno-Cid, J. A., Pérez de la Lastra, J. M., et al. (2013). Vaccination with proteins involved in tick-pathogen interactions reduces vector infestations and pathogen infection. Vaccine 31, 5889–5896. doi: 10.1016/j.vaccine.2013.09.037
Michelet, L., Bonnet, S., Madani, N., and Moutailler, S. (2013). Discriminating Francisella tularensis and Francisella-like endosymbionts in Dermacentor reticulatus ticks: evaluation of current molecular techniques. Vet. Microbiol. 163, 399–403. doi: 10.1016/j.vetmic.2013.01.014
Montagna, M., Sassera, D., Epis, S., Bazzocchi, C., Vannini, C., Lo, N., et al. (2013). “Candidatus Midichloriaceae” fam. nov. (Rickettsiales), an ecologically widespread clade of intracellular alphaproteobacteria. Appl. Environ. Microbiol. 79, 3241–3248. doi: 10.1128/AEM.03971-12
Naranjo, V., Ayllón, N., Pérez de la Lastra, J. M., Galindo, R. C., Kocan, K. M., Blouin, E. F., et al. (2013). Reciprocal regulation of NF-kB (Relish) and Subolesin in the tick vector, Ixodes scapularis. PLoS ONE 8:e65915. doi: 10.1371/journal.pone.0065915
Narasimhan, S., Rajeevan, N., Liu, L., Zhao, Y. O., Heisig, J., Pan, J., et al. (2014). Gut microbiota of the tick vector Ixodes scapularis modulate colonization of the Lyme disease spirochete. Cell. Host. Microbe. 15, 58–71. doi: 10.1016/j.chom.2013.12.001
Neelakanta, G., Sultana, H., Fish, D., Anderson, J. F., and Fikrig, E. (2010). Anaplasma phagocytophilum induces Ixodes scapularis ticks to express an antifreeze glycoprotein gene that enhances their survival in the cold. J. Clin. Invest. 120, 3179–3190. doi: 10.1172/JCI42868
Nene, V., Lee, D., Kang'a, S., Skilton, R., Shah, T., and de Villiers, E., et al. (2004). Genes transcribed in the salivary glands of female Rhipicephalus appendiculatus ticks infected with Theileria parva. Insect. Biochem. Mol. Biol. 34, 1117–1128. doi: 10.1016/j.ibmb.2004.07.002
Pal, U., Li, X., Wang, T., Montgomery, R. R., Ramamoorthi, N., Desilva, A. M., et al. (2004). TROSPA, an Ixodes scapularis receptor for Borrelia burgdorferi. Cell 119, 457–468. doi: 10.1016/j.cell.2004.10.027
Plantard, O., Bouju-Albert, A., Malard, M. A., Hermouet, A., Capron, G., and Verheyden, H. (2012). Detection of Wolbachia in the tick Ixodes ricinus is due to the presence of the hymenoptera endoparasitoid Ixodiphagus hookeri. PLoS ONE 7:e30692. doi: 10.1371/journal.pone.0030692
Qiu, Y., Nakao, R., Ohnuma, A., Kawamori, F., and Sugimoto, C. (2014). Microbial population analysis of the salivary glands of ticks; a possible strategy for the surveillance of bacterial pathogens. PLoS ONE 9:e103961. doi: 10.1371/journal.pone.0103961
Rachinsky, A., Guerrero, F. D., and Scoles, G. A. (2007). Differential protein expression in ovaries of uninfected and Babesia-infected southern cattle ticks Rhipicephalus (Boophilus) microplus. Insect Biochem. Mol. Biol. 37, 1291–1308. doi: 10.1016/j.ibmb.2007.08.001
Radolf, J. D., Caimano, M. J., Stevenson, B., and Hu, L. T. (2012). Of ticks, mice and men: understanding the dual-host lifestyle of Lyme disease spirochaetes. Nat. Rev. Microbiol. 10, 87–99. doi: 10.1038/nrmicro2714
Ramamoorthi, N., Narasimhan, S., Pal, U., Bao, F., Yang, X. F., Fish, D., et al. (2005). The Lyme disease agent exploits a tick protein to infect the mammalian host. Nature 436, 573–577. doi: 10.1038/nature03812
Ramphul, U. N., Garver, L. S., Molina-Cruz, A., Canepa, G. E., and Barillas-Mury, C. (2015). Plasmodium falciparum evades mosquito immunity by disrupting JNK-mediated apoptosis of invaded midgut cells. Proc. Natl. Acad. Sci. U.S.A. 112, 1273–1280. doi: 10.1073/pnas.1423586112
Reis, C., Cote, M., Paul, R. E., and Bonnet, S. (2011). Questing ticks in suburban forest are infected by at least six tick-borne pathogens. Vector Borne Zoonotic Dis. 11, 907–916. doi: 10.1089/vbz.2010.0103
Rennoll-Bankert, K. E., Garcia-Garcia, J. C., Sinclair, S. H., and Dumler, J. S. (2015). Chromatin-bound bacterial effector ankyrin A recruits histone deacetylase 1 and modifies host gene expression. Cell Microbiol. 17, 1640–1652. doi: 10.1111/cmi.12461
Rollend, L., Fish, D., and Childs, J. E. (2013). Transovarial transmission of Borrelia spirochetes by Ixodes scapularis: a summary of the literature and recent observations. Ticks Tick Borne Dis. 4, 46–51. doi: 10.1016/j.ttbdis.2012.06.008
Rudenko, N., Golovchenko, M., Edwards, M. J., and Grubhoffer, L. (2005). Differential expression of Ixodes ricinus tick genes induced by blood feeding or Borrelia burgdorferi infection. J. Med. Entomol. 42, 36–41. doi: 10.1093/jmedent/42.1.36
Rynkiewicz, E. C., Hemmerich, C., Rusch, D. B., Fuqua, C., and Clay, K. (2015). Concordance of bacterial communities of two tick species and blood of their shared rodent host. Mol. Ecol. 24, 2566–2579. doi: 10.1111/mec.13187
Sassera, D., Beninati, T., Bandi, C., Bouman, E. A., Sacchi, L., Fabbi, M., et al. (2006). “Candidatus Midichloria mitochondrii,” an endosymbiont of the tick Ixodes ricinus with a unique intramitochondrial lifestyle. Int. J. Syst. Evol. Microbiol. 56, 2535–2540. doi: 10.1099/ijs.0.64386-0
Schuijt, T. J., Coumou, J., Narasimhan, S., Dai, J., Deponte, K., Wouters, D., et al. (2011b). A tick mannose-binding lectin inhibitor interferes with the vertebrate complement cascade to enhance transmission of the Lyme disease agent. Cell Host Microbe. 10, 136–146. doi: 10.1016/j.chom.2011.06.010
Schuijt, T. J., Narasimhan, S., Daffre, S., DePonte, K., Hovius, J. W., Van't Veer, C., et al. (2011a). Identification and characterization of Ixodes scapularis antigens that elicit tick immunity using yeast surface display. PLoS ONE 6:e15926. doi: 10.1371/journal.pone.0015926
Severo, M. S., Choy, A., Stephens, K. D., Sakhon, O. S., Chen, G., Chung, D. W., et al. (2013). The E3 ubiquitin ligase XIAP restricts Anaplasma phagocytophilum colonization of Ixodes scapularis ticks. J. Infect Dis. 208, 1830–1840. doi: 10.1093/infdis/jit380
Severo, M. S., Pedra, J. H. F., Ayllón, N., Kocan, K. M., and de la Fuente, J. (2015). “Anaplasma,” in Molecular Medical Microbiology, 2nd Edn., ed Y. W. Tang, M. Sussman, D. Liu, I. Poxton, and J. Schwartzman (New York, NY: Academic Press; Elsevier), 2033–2042.
Shaw, D. K., Wang, X., Brown, L. J., Oliva, C. A. S., Reif, K. E., Smith, A. A., et al. (2017). Infection-derived lipids elicit an immune deficiency circuit in arthropods. Nat. Commun. 8:14401. doi: 10.1038/ncomms14401
Shtanko, O., Nikitina, R. A., Altuntas, C. Z., Chepurnov, A. A., and Davey, R. A. (2014). Crimean-Congo hemorrhagic fever virus entry into host cells occurs through the multivesicular body and requires ESCRT regulators. PLoS Pathog. 10:e1004390. doi: 10.1371/journal.ppat.1004390
Simon, M., Johansson, C., and Mirazimi, A. (2009). Crimean-Congo hemorrhagic fever virus entry and replication is clathrin-, pH- and cholesterol-dependent. J. Gen. Virol. 90(Pt 1), 210–215. doi: 10.1099/vir.0.006387-0
Smith, A. A., Navasa, N., Yang, X., Wilder, C. N., Buyuktanir, O., Marques, A., et al. (2016). Cross-Species Interferon signaling boosts microbicidal activity within the tick vector. Cell Host Microbe 20, 91–98. doi: 10.1016/j.chom.2016.06.001
Steiner, F. E., Pinger, R. R., Vann, C. N., Grindle, N., Civitello, D., Clay, K., et al. (2008). Infection and co-infection rates of Anaplasma phagocytophilum variants, Babesia spp., Borrelia burgdorferi, and the rickettsial endosymbiont in Ixodes scapularis (Acari: Ixodidae) from sites in Indiana, Maine, Pennsylvania, and Wisconsin. J. Med. Entomol. 45, 289–297. doi: 10.1093/jmedent/45.2.289
Suda, Y., Fukushi, S., Tani, H., Murakami, S., Saijo, M., Horimoto, T., et al. (2016). Analysis of the entry mechanism of Crimean-Congo hemorrhagic fever virus, using a vesicular stomatitis virus pseudotyping system. Arch. Virol. 161, 1447–1454. doi: 10.1007/s00705-016-2803-1
Sultana, H., Neelakanta, G., Kantor, F. S., Malawista, S. E., Fish, D., Montgomery, R. R., et al. (2010). Anaplasma phagocytophilum induces actin phosphorylation to selectively regulate gene transcription in Ixodes scapularis ticks. J. Exp. Med. 207, 1727–1743. doi: 10.1084/jem.20100276
Tabata, J., Hattori, Y., Sakamoto, H., Yukuhiro, F., Fujii, T., Kugimiya, S., et al. (2011). Male killing and incomplete inheritance of a novel spiroplasma in the moth Ostrinia zaguliaevi. Microb. Ecol. 61, 254–263. doi: 10.1007/s00248-010-9799-y
Taylor, M., Mediannikov, O., Raoult, D., and Greub, G. (2012). Endosymbiotic bacteria associated with nematodes, ticks and amoebae. FEMS Immunol. Med. Microbiol. 64, 21–31. doi: 10.1111/j.1574-695X.2011.00916.x
Tully, J. G., Rose, D. L., Yunker, C. E., Carle, P., Bové, J. M., Williamson, D. L., et al. (1995). Spiroplasma ixodetis sp. nov., a new species from Ixodes pacificus ticks collected in Oregon. Int. J. Syst. Bacteriol. 45, 23–28. doi: 10.1099/00207713-45-1-23
Turell, M. J. (2007). “Role of ticks in the transmission of Crimean-Congo hemorrhagic fever virus,” in Crimean-Congo Hemorrhagic Fever: A Global Perspective, ed O. Ergonul and C. A. Whitehouse (Dordrecht: Springer Press), 143–154.
Vayssier-Taussat, M., Kazimirova, M., Hubalek, Z., Hornok, S., Farkas, R., Cosson, J. F., et al. (2015). Emerging horizons for tick-borne pathogens: from the “one pathogen-one disease” vision to the pathobiome paradigm. Future Microbiol. 10, 2033–2043. doi: 10.2217/fmb.15.114
Venzal, J. M., Estrada-Peña, A., Castro, O., de Souza, C. G., Félix, M. L., Nava, S., et al. (2008). Amblyomma triste Koch, 1844 (Acari: Ixodidae): hosts and seasonality of the vector of Rickettsia parkeri in Uruguay. Vet. Parasitol. 155, 104–109. doi: 10.1016/j.vetpar.2008.04.017
Villar, M., Ayllón, N., Alberdi, P., Moreno, A., Moreno, M., Tobes, R., et al. (2015a). Integrated metabolomics, transcriptomics and proteomics identifies metabolic pathways affected by Anaplasma phagocytophilum infection in tick cells. Mol. Cell Proteomics. 14, 3154–3172. doi: 10.1074/mcp.M115.051938
Villar, M., Ayllón, N., Kocan, K. M., Bonzón-Kulichenko, E., Alberdi, P., et al. (2015b). Identification and characterization of Anaplasma phagocytophilum proteins involved in infection of the tick vector, Ixodes scapularis. PLoS ONE 10:e0137237. doi: 10.1371/journal.pone.0137237
Vlachou, D., Schlegelmilch, T., Christophides, G. K., and Kafatos, F. C. (2005). Functional genomic analysis of midgut epithelial responses in Anopheles during Plasmodium invasion. Curr. Biol. 15, 1185–1195. doi: 10.1016/j.cub.2005.06.044
Wagemakers, A., Coumou, J., Schuijt, T. J., Oei, A., Nijhof, A. M., van 't Veer, C., et al. (2016). An Ixodes ricinus tick salivary lectin pathway inhibitor protects Borrelia burgdorferi sensu lato from human complement. Vector Borne Zoonotic Dis. 16, 223–228. doi: 10.1089/vbz.2015.1901
Wang, J. L., Zhang, J. L., Chen, W., Xu, X. F., Gao, N., Fan, D. Y., et al. (2010). Roles of small GTPase Rac1 in the regulation of actin cytoskeleton during dengue virus infection. PLoS Negl. Trop. Dis. 4:e809. doi: 10.1371/journal.pntd.0000809
Weisheit, S., Villar, M., Tykalová, H., Popara, M., Loecherbach, J., Watson, M., et al. (2015). Ixodes scapularis and Ixodes ricinus tick cell lines respond to infection with tick-borne encephalitis virus: transcriptomic and proteomic analysis. Parasit. Vectors 8, 599. doi: 10.1186/s13071-015-1210-x
Williams-Newkirk, A. J., Rowe, L. A., Mixson-Hayden, T. R., and Dasch, G. A. (2012). Presence, genetic variability, and potential significance of “Candidatus Midichloria mitochondrii” in the lone star tick Amblyomma americanum. Exp. Appl. Acarol. 58, 291–300. doi: 10.1007/s10493-012-9582-5
Yokoyama, N., Okamura, M., and Igarashi, I. (2006). Erythrocyte invasion by Babesia parasites: current advances in the elucidation of the molecular interactions between the protozoan ligands and host receptors in the invasion stage. Vet. Parasitol. 138, 22–32. doi: 10.1016/j.vetpar.2006.01.037
Zhang, L., Zhang, Y., Adusumilli, S., Liu, L., Narasimhan, S., Dai, J., et al. (2011). Molecular interactions that enable movement of the Lyme disease agent from the tick gut into the hemolymph. PLoS Pathog. 7:e1002079. doi: 10.1371/journal.ppat.1002079
Zhang, X., Norris, D. E., and Rasgon, J. L. (2011). Distribution and molecular characterization of Wolbachia endosymbionts and filarial nematodes in Maryland populations of the lone star tick (Amblyomma americanum). FEMS Microbiol. Ecol. 77, 50–56. doi: 10.1111/j.1574-6941.2011.01089.x
Keywords: tick, Anaplasma, flavivirus, Babesia, Borrelia, microbiome, immunology, vaccine
Citation: de la Fuente J, Antunes S, Bonnet S, Cabezas-Cruz A, Domingos AG, Estrada-Peña A, Johnson N, Kocan KM, Mansfield KL, Nijhof AM, Papa A, Rudenko N, Villar M, Alberdi P, Torina A, Ayllón N, Vancova M, Golovchenko M, Grubhoffer L, Caracappa S, Fooks AR, Gortazar C and Rego ROM (2017) Tick-Pathogen Interactions and Vector Competence: Identification of Molecular Drivers for Tick-Borne Diseases. Front. Cell. Infect. Microbiol. 7:114. doi: 10.3389/fcimb.2017.00114
Received: 06 February 2017; Accepted: 22 March 2017;
Published: 07 April 2017.
Edited by:Joao Santana Silva, University of São Paulo, Brazil
Reviewed by:Peter Kraiczy, Goethe University Frankfurt, Germany
X Frank Yang, Indiana University School of Medicine, USA
Copyright © 2017 de la Fuente, Antunes, Bonnet, Cabezas-Cruz, Domingos, Estrada-Peña, Johnson, Kocan, Mansfield, Nijhof, Papa, Rudenko, Villar, Alberdi, Torina, Ayllón, Vancova, Golovchenko, Grubhoffer, Caracappa, Fooks, Gortazar and Rego. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) or licensor are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Ryan O. M. Rego, firstname.lastname@example.org