Published in Volume
120, Issue 9
(September 1, 2010)J Clin Invest.
Copyright © 2010, American Society for Clinical Investigation
Anaplasma phagocytophilum induces Ixodes scapularis ticks to express an antifreeze glycoprotein gene that enhances their survival in the cold
1Section of Infectious Diseases, Department of Internal Medicine, Yale University School of Medicine, New Haven, Connecticut, USA.
2Howard Hughes Medical Institute, Chevy Chase, Maryland, USA.
3Department of Epidemiology and Public Health, Yale University School of Medicine, New Haven, Connecticut, USA.
4Department of Entomology, Connecticut Agricultural Experiment Station, New Haven, Connecticut, USA.
Address correspondence to: Erol Fikrig, Section of Infectious Diseases, Department of Internal Medicine, Yale University School of Medicine, Room 169, 300 Cedar Street, New Haven, Connecticut 06520-8022, USA. Phone: 203.785.4140; Fax: 203.785.3864; E-mail:
First published August 25, 2010
Received for publication March 3,
2010, and accepted in revised form June 16,
In the United States, Ixodes scapularis ticks overwinter in the Northeast and Upper Midwest and transmit the agent of human granulocytic anaplasmosis, Anaplasma phagocytophilum, among other pathogens. We now show that the presence of A. phagocytophilum in I. scapularis ticks increases their ability to survive in the cold. We identified an I. scapularis antifreeze glycoprotein, designated IAFGP, and demonstrated via RNAi knockdown studies the importance of IAFGP for the survival of I. scapularis ticks in a cold environment. Transfection studies also show that IAFGP increased the viability of yeast cells subjected to cold temperature. Remarkably, A. phagocytophilum induced the expression of iafgp, thereby increasing the cold tolerance and survival of I. scapularis. These data define a molecular basis for symbiosis between a human pathogenic bacterium and its arthropod vector and delineate what we believe to be a new pathway that may be targeted to alter the life cycle of this microbe and its invertebrate host.
Diverse arthropods have intimate relationships with microbes (1–5). Several examples include pheromonal symbiosis of desert locusts (6) and nutritional symbiosis of flower thrips (7) with environmentally acquired bacteria. Aphid-Buchnera and tsetse-Wigglesworthia obligate endosymbioses and Wolbachia-insect facultative endosymbioses are examples of arthropods having relationships with bacteria acquired by vertical transmission (8–10). Arthropods also transmit microbes to vertebrates, sometimes resulting in human illness (11), and little is known about whether these vectors can establish beneficial interactions with medically important pathogens.
The black-legged tick, Ixodes scapularis, can transmit several bacteria that cause disease in man, including Anaplasma phagocytophilum, the agent of human granulocytic anaplasmosis (12–16). I. scapularis are blood-sucking ectoparasites that ingest A. phagocytophilum while feeding on infected animals (16). Upon entering ticks, A. phagocytophilum establishes itself in the salivary glands of the ticks and is then transstadially maintained through different stages of the arthropod life cycle (17, 18). Persistence in the arthropod throughout the year is particularly important for a microbe, such as A. phagocytophilum, which cannot be transovarially transmitted from an infected adult female tick to its offspring (17, 18). I. scapularis larvae that feed in midsummer overwinter as nymphs, and nymphs that engorge in early summer overwinter as adults (18, 19). These ticks must survive multiple abiotic stress conditions, including freezing temperatures, desiccation, and ice encasement.
Arthropods have evolved physiological and behavioral strategies to withstand lower environmental temperatures that are collectively termed “freeze avoidance” or “freeze tolerance.” Each of these processes elicits different adaptive responses, and specific antifreeze proteins are involved (20–22). Antifreeze proteins are a diverse class of compounds that bind to ice crystals and restrict their growth (23–26). Antifreeze proteins require structural complementarity with ice to adsorb to its surface; however, the molecular mechanisms remain to be elucidated (27–30). Antifreeze proteins are classified into 2 main types, antifreeze proteins (AFPs) and antifreeze glycoproteins (AFGPs) (24, 29). AFPs and AFGPs are divided into 4 and 8 subtypes, respectively (24, 29, 30). A characteristic feature of AFGPs is the presence of repeating tripeptide units (alanine-alanine-threonine), in which the secondary hydroxyl group of the threonine residue is glycosylated with a disaccharide (30). Higher molecular mass glycoproteins of 20 to 33 kDa are referred to as AFGPs 1 to 4, and those less than 20 kDa are referred to as AFGPs 5 to 8 (24, 29, 30). AFGPs may also have the l-threonine residue substituted with l-arginine, and l-alanine residues substituted with l-proline (31, 32). Most experiments have focused on understanding the role of type 1 to 4 AFPs. A limited number of studies have been performed on AFGPs, due to their structural complexity and the difficulty in obtaining pure AFGP.
Since their identification in the body fluids of polar fishes (23, 33), AFPs have been found in more than 55 terrestrial arthropods, including insects, spiders, mites, and centipedes (20, 34–40). AFGPs in arthropods have not been reported. In the present study, we have identified an I. scapularis AFGP and determined whether I. scapularis has enhanced cold tolerance due to an association with A. phagocytophilum.
A. phagocytophilum–infected ticks survive better at cold temperatures. A. phagocytophilum survives the winter in tissues of I. scapularis. We therefore determined whether this bacterium influences the survival of ticks exposed to cold temperatures. Uninfected or A. phagocytophilum–infected ticks that were maintained at 23°C in laboratory were incubated at –20°C and analyzed for survival at various time points (Figure 1A). Survival curves showed the lethal time point50 (LT50) at –20°C for uninfected ticks to be approximately 25 minutes (Figure 1A). At the LT50, A. phagocytophilum–infected ticks were more cold tolerant (survival rate of 80%) than uninfected (survival rate of 40%) ticks (Figure 1A). None of the ticks, regardless of infection, survived when incubated for 45 minutes at –20°C (Figure 1A). We then performed 18 independent survival assays with multiple batches of ticks (10 ticks/group/experiment) at the LT50. We found increased survival rates for A. phagocytophilum–infected (73%, P < 0.001) ticks in comparison with uninfected (41%) controls (Figure 1B). After cold shock, ticks were monitored for their ability to move from a starting point after 10 minutes. The mobility (distance-traveled rate) of A. phagocytophilum–infected ticks after cold shock was higher (P < 0.0001) than controls, suggesting increased fitness of the A. phagocytophilum–infected ticks at cold temperatures (Figure 1C and Supplemental Figure 1; supplemental material available online with this article; doi:
A. phagocytophilum–infected nymphs survive better at cold temperatures.
(A) Survival of uninfected and A. phagocytophilum–infected (A. phag–infected) unfed nymphs at –20°C for 0, 10, 15, 20, 25, 30, 45, or 90 minutes. Data from 2 independent experiments with 10 ticks/group/time point/experiment are shown. The dashed box indicates the LT50 time point for ticks at –20°C. Mean ± SD error bars from 2 independent experiments are shown for comparison. (B) Survival of uninfected and A. phagocytophilum–infected unfed nymphs at the LT50 (–20°C, 25 minutes) from 18 independent experiments. Each circle represents 1 independent experiment (10 ticks/group/experiment). The difference in the survival between A. phagocytophilum–infected and uninfected nymphs is significant (P < 0.001). (C) Mobility (in cm) by uninfected or A. phagocytophilum–infected unfed nymphs after cold shock at LT50. Each circle represents 1 individual tick. Survival (D and F) and mobility (E and G) measurements of uninfected and A. phagocytophilum–infected unfed nymphs at LT50 in a sequential (D and E) and scrambled (F and G) cold tolerance assay. Each circle in D and F represents 1 independent experiment (10 ticks/group/experiment) and in E and G represents 1 individual tick. In all panels, white circles represent uninfected ticks and black circles represent A. phagocytophilum–infected ticks. For all panels, statistical significance was calculated using Mann-Whitney U nonparametric test. n = 70 (C); n = 60 (E); n = 30 (G) for both uninfected and A. phagocytophilum–infected ticks. Horizontal lines in B–G indicate the median of the readings from independent experiment/ticks.
To determine whether sequential cooling affected the survival of ticks, we incubated uninfected and A. phagocytophilum–infected ticks at different temperatures (23°C, 4°C, 0°C, –10°C, and –20°C) in a sequential manner for 1 hour at each respective temperature (see Methods). The increased survival and mobility of A. phagocytophilum–infected ticks in comparison with uninfected ticks that was seen upon rapid cold shock was also significant (P < 0.05) upon sequential cooling (Figure 1, D and E). To eliminate any bias in our studies, we performed a series of scrambled assays with a mixed population of A. phagocytophilum–infected and uninfected ticks at the LT50 (see Methods). Scrambled assays showed enhanced survival and mobility for A. phagocytophilum–infected (P < 0.05) ticks in comparison with the controls (Figure 1, F and G).
To determine whether the A. phagocytophilum burden was associated with increased arthropod cold tolerance, we performed studies with 25 uninfected and 25 A. phagocytophilum–infected ticks and quantified the A. phagocytophilum burden in each tick. After cold treatment, quantitative real-time PCR (QRT-PCR) was performed with p44 gene–specific primers to assess the A. phagocytophilum load. The results indicated a significant correlation between the A. phagocytophilum burden in each tick and its cold tolerance capacity (Figure 2). Collectively, the results from Figures 1 and 2 demonstrate a beneficial association between the presence of A. phagocytophilum within I. scapularis and the viability of ticks exposed to extreme cold temperatures.
Increased A. phagocytophilum burden correlates with increased cold tolerance of ticks.
A. phagocytophilum-burden in Live (L) or Dead (D) A. phagocytophilum–infected unfed ticks at LT50 (–20°C, 25 minutes) as determined by QRT-PCR. Uninfected ticks were used as controls. A. phagocytophilum burden was quantified with p44 gene–specific primers and normalized to tick beta-actin levels. Histograms represent the A. phagocytophilum burden in each individual tick (25 ticks/group/assay). Horizontal dotted line in the graph points to the threshold level of A. phagocytophilum burden required to increase cold tolerance in ticks. All of the dead A. phagocytophilum–infected ticks showed reduced bacterial loads that fell below the threshold level. 1 complete set of data from 3 independent experiments is shown.
Identification of an afgp gene in I. scapularis. Several insects and terrestrial arthropods have antifreeze proteins (20, 22, 35). We assessed whether I. scapularis has any antifreeze proteins and whether A. phagocytophilum influences the expression of these genes. An expressed sequence tag (EST) sequence that encodes a potential antifreeze protein (TC43064) was identified from the I. scapularis database. The sequence showed significant relatedness to a cod, Boreogadus saida, afgp gene rather than to insect afp genes. By RT-PCR, using primers designed from the 5′ and 3′ ends of the I. scapularis TC43064 sequence, an amplification product of approximately 900 bp was detected in cDNA generated from unfed I. scapularis ticks (Supplemental Figure 2). The PCR product was cloned into the pGEM-T Easy Vector and sequenced from both ends (Figure 3). The GC-rich TC43064 sequence contained a full-length open reading frame and coded predicted protein that, because of high similarity with B. saida AFGPs, was named I. scapularis AFGP (IAFGP; GenBank HM213906). Sequencing of additional cDNA clone obtained from different PCR primers (see Methods) yielded an additional 32 upstream nucleotides beyond the putative start codon of iafgp (Figure 3).
Nucleotide and predicted amino acid sequence of IAFGP. The nucleotide sequence of the iafgp gene was obtained by sequencing PCR product cloned in the pGEMT-Easy Vector. The deduced amino acid sequence is shown as a single letter below the nucleotide sequence. The in-frame putative IAFGP translational start and stop codons are indicated in bold. The amino acid sequence corresponding to N-terminal signal peptide is boxed (solid line). Ala-Ala-Thr repeats are underlined, and several O-glycosylation sites are indicated by asterisks. Upstream nucleotide sequence obtained from sequencing additional cDNA clone is shown in lower case. The Kozak sequence at 5′ end and polyadenylation signal at 3′ end are indicated in bold letters and enclosed in dashed boxes.
The iafgp sequence contained an open reading frame of 756 nucleotides with a 3′ untranslated region that included a polyadenylation signal sequence at position 146 from the stop codon (Figure 3). The full-length iafgp cDNA contained a KOZAK-compatible (41) ATG codon at the 5′ end, encoding a putative IAFGP protein with a predicted molecular mass of 23.2 kDa (Figure 3). Computer analysis (SignalP 3.0 Server; Technical University of Denmark) revealed a signal peptide cleavage site between amino acids 19 and 20 (Figure 3). The deduced IAFGP sequence showed approximately 70% identity with several other fish AFGPs (Supplemental Figure 3, A and B). Ala-Ala-Thr repeat sequences characteristic of fish AFGPs and posttranslational modification signals including O-glycosylation sites (determined at NetOGlyc 3.1 Server; Technical University of Denmark) were identified in IAFGP (Figure 3).
Expression of I. scapularis iafgp is developmentally regulated and induced at cold temperatures. We determined whether iafgp expression was regulated during tick development. The iafgp mRNA levels were assessed by QRT-PCR using β-actin as an internal control (Figure 4A). iafgp was expressed in larvae and nymphs and increased in adults (Figure 4A and Supplemental Figure 4). No difference in iafgp expression was seen between male and female adult ticks (Figure 4A and Supplemental Figure 4). To assess whether cold temperatures influenced iafgp mRNA levels, uninfected unfed ticks (20 ticks/temperature) were incubated at different temperatures (23°C, 10°C, 4°C, and 0°C). The expression levels of iafgp were increased (4-fold, P < 0.001) at lower (4°C and 0°C) temperatures in comparison with higher (23°C and 10°C) temperatures (Figure 4B).
Expression of iafgp is developmentally regulated and induced by cold and A. phagocytophilum.
(A) The expression of iafgp is developmentally regulated in I. scapularis ticks. Total RNA from unfed larvae (n = 10), unfed nymphs (n = 10), unfed adult males (n = 10 ticks), and unfed adult females (n = 10) was prepared in triplicate and the amount of iafgp transcripts was quantified by QRT-PCR and normalized to tick beta-actin. Error bars indicate + SD from the mean. (B) The expression of iafgp in nymphs is induced by cold temperatures. Total RNA from nymphs incubated at different temperatures (23°C, 10°C, 4°C, and 0°C) was prepared, and the iafgp transcript levels were quantified by QRT-PCR. Each circle represents 1 individual tick. The differences in iafgp levels at 4°C and 0°C in comparison with 23°C is significant (P < 0.05, Student’s t test). (C) Total RNA from uninfected nymphs (white circles) and A. phagocytophilum–infected nymphs (black circles) incubated at different temperatures (23°C, 10°C, 4°C, and 0°C) was prepared, and transcript levels of iafgp were quantified by QRT-PCR. Levels of iafgp were normalized to tick beta-actin. Each circle represents 1 individual tick. The elevated levels of iafgp transcripts in A. phagocytophilum–infected nymphs in comparison with the uninfected controls is significant at all tested temperatures (P < 0.05, Student’s t test). Horizontal lines in panels B and C indicate average of the readings from independent ticks.
Expression of iafgp is influenced by A. phagocytophilum. As A. phagocytophilum influences the cold tolerance of ticks, we determined whether A. phagocytophilum also alters iafgp expression. A. phagocytophilum–infected ticks were incubated at different temperatures (23°C, 10°C, 4°C, and 0°C), and iafgp mRNA levels were compared with those of uninfected ticks (20 ticks/group/temperature). The expression of iafgp was elevated in A. phagocytophilum–infected ticks in comparison with the controls at all tested temperatures (Figure 4C; 3-fold, P < 0.05). These results show that iafgp expression is influenced by the presence of A. phagocytophilum within ticks.
iafgp-deficient ticks have reduced ability to survive at cold temperatures. To determine whether IAFGP directly plays a role in tick survival at cold temperatures, we generated iafgp-deficient uninfected ticks by RNA interference (RNAi). Mock and iafgp dsRNAs were synthesized in vitro. Mock dsRNA was prepared from empty L4440 vector that contained restriction enzyme site sequences (see Methods). Equal amounts (4.2 nanoliters) containing equal molecules of the respective dsRNAs were microinjected into the bodies of ticks, which were allowed to rest for 3 days at 23°C. At day 3, QRT-PCR showed a significant reduction of iafgp mRNA in iafgp-dsRNA–injected ticks compared with the mock-injected (7-fold, P < 0.01) controls (Figure 5A). The unchanged levels of tick beta-actin mRNA confirmed the specificity of RNAi. We then determined survival and mobility rates of mock- and iafgp-dsRNA–injected ticks at the LT50 (25 min, –20°C). We found a significant reduction in survival (P < 0.0001) and mobility (P < 0.0001) of iafgp-dsRNA–injected ticks in comparison with the mock-injected controls (Figure 5, B and C), demonstrating a direct role for IAFGP in tick cold tolerance. To further demonstrate that the reduced survival and mobility of ticks was due to specific silencing of iafgp, the survival and mobility assays were repeated by silencing another I. scapularis gene, trospA (Supplemental Figure 5). We found no significant differences in the survival and mobility of trospA-dsRNA–injected ticks in comparison with the mock-injected controls (Supplemental Figure 5).
Silencing of iafgp by RNAi reduces survival of ticks at cold temperatures.
(A) QRT-PCR showing reduced iafgp mRNA levels in iafgp-dsRNA–injected uninfected ticks compared with the mock-dsRNA control. (B) Survival of mock-dsRNA–injected and iafgp-dsRNA–injected ticks at the LT50 time point. (C) Mobility (in cm) by mock-dsRNA–injected and iafgp-dsRNA–injected ticks at LT50 time point (–20°C, 25 min). (A–C) White circles represent mock-dsRNA–injected ticks, and white triangles represent iafgp-dsRNA–injected ticks. QRT-PCR showing reduced iafgp mRNA levels (D) and A. phagocytophilum burden (E) in mock-injected (black circles) and iafgp-dsRNA–injected (black triangles) ticks partially fed (48 hours) on A. phagocytophilum–infected mice. (F) Survival percentage at –20°C, 50-minute time point of mock-dsRNA–injected (black circles) and iafgp-dsRNA–injected (black triangles) ticks partially fed (48 hours) on A. phagocytophilum–infected mice. Each circle in A, C, D, and E represents 1 individual tick, and each circle in B and F represents 1 independent experiment with 10 ticks/group/experiment. Statistics in A, D, and E were performed using 2-tailed Student’s t test and in B, C, and F using Mann-Whitney U test. n = 60 (C) for both mock and iafgp-dsRNA ticks. Horizontal lines in A, D, and E represent average and in B, C, and F represent median of the readings from independent experiments/ticks.
To understand whether increased cold tolerance in A. phagocytophilum–infected ticks is solely related to A. phagocytophilum–induced expression of iafgp, we generated iafgp-deficient ticks using RNAi. Mock- and iafgp-dsRNA–injected ticks were then allowed to feed on A. phagocytophilum–infected mice for 48 hours. Both groups of ticks were assessed for the A. phagocytophilum burden and cold tolerance (see Methods). The LT50 time point at –20°C for 48-hour–fed ticks was between 45 and 50 minutes. For our experiments, we considered incubation at –20°C, 50 minutes as cold treatment condition for fed ticks. QRT-PCR showed a reduction of iafgp mRNA levels in iafgp-dsRNA–injected ticks when compared with the mock-injected (3-fold, P < 0.05) ticks (Figure 5D). We found a reduction in the A. phagocytophilum burden (P < 0.05) and survival (P < 0.01) of iafgp-dsRNA–injected ticks in comparison with the controls (Figure 5, E and F). The survival rates of ticks were the same in the mock- and trospA-dsRNA–injected ticks (Supplemental Figure 5). These results show that the increased cold tolerance in A. phagocytophilum–infected ticks is directly related to the A. phagocytophilum–induced expression of iafgp.
A. phagocytophilum infection enhances the cold tolerance of tick cells. A. phagocytophilum can infect and persist in I. ricinus tick cell line (IRE/CTVM19) for an extended period of time. By RT-PCR, using primers designed from the 5′ and 3′ ends of iafgp gene followed by sequencing, we were able to identify I. ricinusiafgp gene from these cells (Supplemental Figure 6, A and B). We designated I. ricinusiafgp as iafgp-Iric (GenBank HM213905). The deduced amino acid sequence of IAFGP-IRIC showed 80% identity with IAFGP (Supplemental Figure 6C). Ala-Ala-Thr repeat sequences and O-glycosylation sites were also evident in IAFGP-IRIC (Supplemental Figure 6B). We then determined whether A. phagocytophilum also induces iafgp-Iric in vitro. These tick cells, when incubated at –5°C for 2 hours, demonstrated a significant induction of iafgp-Iric mRNA (3-fold, P < 0.01) in comparison with 28°C temperature (Figure 6A). A. phagocytophilum infection also induced iafgp-Iric expression in these cells (4-fold, P < 0.01; Figure 6B). To determine whether A. phagocytophilum infection increases cold tolerance in tick cells, we incubated the cells at –20°C for 10 minutes and stained with FM4-64 dye to analyze membrane integrity and internalization of the dye upon cold treatment (Figure 6C). We found less membrane disruption and internal membrane staining in A. phagocytophilum–infected cells (3-fold, P < 0.001) compared with controls (Figure 6, C and D). Uninfected and A. phagocytophilum–infected cells incubated at 28°C showed no phenotypic differences (Figure 6C). These results further show that A. phagocytophilum infection and an increase in iafgp-Iric expression are associated with the induction of cold tolerance in tick cells.
A. phagocytophilum infection and induction of iafgp expression enhances cold tolerance in tick cells.
(A) QRT-PCR showing the levels of iafgp transcripts in tick cells incubated at different temperatures (28°C, 4°C, 0°C, –5°C). (B) QRT-PCR showing the level of iafgp transcripts in uninfected (white bar) and A. phagocytophilum–infected (black bar) tick cells at 48 hours after infection. Results from 3 independent experiments are shown. Error bars indicate + SD from the mean. The level of iafgp transcripts was normalized to tick beta-actin. (C) Immunofluorescence images of tick cells stained with FM4-64 dye showing increased membrane disruption in uninfected cells in comparison with A. phagocytophilum–infected cells after cold shock at –20°C for 10 minutes. Uninfected and A. phagocytophilum–infected tick cells incubated at 28°C served as experimental controls. Representative images from 3 independent experiments are shown. Original magnification, ×65. Scale bar: 20 μM. (D) Quantitative assessment of the number of membrane-disrupted cells in uninfected (white circles) and A. phagocytophilum–infected (black circles) tick cells after cold shock at –20°C for 10 minutes is shown. Each circle represents 1 microscopic field. Statistics were performed using Student’s t test and the P values are shown. Horizontal lines in the graph indicate average of the readings from independent microscopic observations.
In vitro antifreeze activity of IAFGP mediates yeast survival at cold temperatures. To characterize the functional role of IAFGP, we developed a cold tolerance assay in yeast (see Methods). IAFGP was expressed in Saccharomyces cerevisiae EBY100 cells fused to the Aga2p mating agglutinin protein under the control of galactose-inducible promoter (Figure 7A). The expression of iafgp was induced by growing yeast transformants in SDGAA medium. 102 cells from an overnight culture were plated on SDGAA, and the number of viable cells before cold shock was determined by their colony-forming ability (Figure 7, B and C). From the same culture vial, cells were shifted to –20°C, and at 4 and 24 hours samples were thawed and 102 cells were plated on SDGAA plates to determine cell viability after cold shock. Yeast cells transformed with the empty plasmid pYD1 were used as experimental controls. Recovery of the plasmids (isolated from EBY100 transformants and transformed in E. coli) confirmed the presence of both iafgp and empty plasmids in respective yeast strains used in the cold-tolerance assay (Supplemental Figure 7). Cells containing empty vector showed a significant loss of viability after 24 hours incubation at –20°C in comparison with the cells expressing IAFGP (P < 0.01; Figure 7, B and C). These results demonstrate that expression of IAFGP increases cold tolerance in yeast.
IAFGP increases cold tolerance in yeast. (A) Schematic representation of the constructs used for testing IAFGP expression in yeast cells. Full-length iafgp (FL-iafgp) was cloned in frame with AGA2 in pYD1 vector and transformed into EBY100 yeast cells. (B) Representative images from 3 independent experiments of SDGAA plates containing pYD1/FL-iafgp and the pYD1 empty vector transformed yeast cells before and after 4 hours or 24 hours at –20°C. (C) Quantitative survival assessment of pYD1/FL-iafgp (black bars) and pYD1 empty vector (white bars) transformed yeast cells after 4 hours or 24 hours at –20°C. Data from 3 independent experiments with triplicate clones are shown. Error bars indicate + SD from the mean value. Statistics were performed using Student’s t test, and the P values are shown.
Arthropods and microbes have intimate interactions (4). Many microbes are parasitic or commensal, but some are advantageous to the host (1, 5, 9, 42–47). Studies have elucidated the role of microbial factors involved in beneficial relationships with arthropods (4, 42, 43); however, the host molecules that contribute to these beneficial relationships remain unknown. We have now identified an arthropod antifreeze glycoprotein, IAFGP, that is actively involved in a mutualistic interaction between A. phagocytophilum and I. scapularis, facilitating survival of both species at cold temperatures.
Several studies have examined the cold-hardiness of Ixodes ticks, but these studies have not assessed whether a microbe can influence its vector during cold exposure (48–50). As A. phagocytophilum overwinter in ticks (18), we determined whether this microbe altered I. scapularis gene expression and whether this was related to survival in the cold. We observed a significant increase in the expression of an antifreeze glycoprotein gene, iafgp, at cold temperatures when I. scapularis were infected with A. phagocytophilum compared with ticks that did not harbor this pathogen. We found no significant differences in iafgp expression between uninfected and Babesia microti–infected ticks, suggesting that iafgp expression is specifically influenced by the presence of A. phagocytophilum (Supplemental Figure 8). The increased survival, as determined by a series of rapid, sequential, and scrambled cold-tolerance assays, demonstrated enhanced cold tolerance of A. phagocytophilum–infected ticks. The mobility of ticks further confirmed increased fitness of A. phagocytophilum–infected ticks at cold temperatures. Finally, a higher A. phagocytophilum burden correlated with increased viability of ticks at cold temperatures. A direct correlation of AFGP concentration to antifreeze activity has been shown in other studies (24, 51, 30). Our data suggest that A. phagocytophilum induces the expression of iafgp, leading to elevated levels of IAFGP synthesis that enhance the cold tolerance of ticks — thereby facilitating survival of both I. scapularis and A. phagocytophilum at extreme temperatures.
The small genome size, low rate of horizontal gene transfer events, and absence of mobile genetic elements that are characteristic of many beneficial microbes (52) are also evident with A. phagocytophilum (53). Many arthropods contain specialized cells called bacteriocytes that are filled with “primary symbionts” that are mostly beneficial to the hosts (4, 43). The primary symbionts are vertically transmitted from parent to their offspring. Arthropods also harbor “secondary” symbionts that usually do not reside exclusively in these specialized organs and are found extracellularly or intracellularly in different tissues (4, 43). These symbionts are acquired by horizontal transmission such as direct intimate contact or indirect contamination via a vector or the environment. Unlike primary symbionts in which beneficial associations with the arthropod are maintained from generation to generation, secondary symbionts exhibit favorable associations with the host that are typically facultative (4). Our finding that, in the absence of vertical transmission, A. phagocytophilum that are acquired from mammals and maintained in ticks significantly contributed to the arthropod fitness during cold reflects a facultative beneficial relationship between this microbe and I. scapularis.
The frequency of A. phagocytophilum infection in I. scapularis varies among ticks in different parts of United States (12–15, 54). Factors that influence the efficient vector acquisition of the bacteria while feeding on vertebrates as well as the ecological and landscape changes, such as yearly temperature fluctuations, associated with tick activity, can potentially influence A. phagocytophilum infection rates (19, 55). If A. phagocytophilum–infected ticks persist better during winter, then illnesses that these ticks transmit may also increase with alterations in the climate. Our laboratory-based survival and mobility studies may provide insight in understanding the epidemiological distribution of A. phagocytophilum–infected ticks in the field.
The extended winter questing activity of Ixodes ticks has been systematically examined both in Europe and in the United States (56, 57). The fact that Ixodes ticks are active during the winter, when arthropods are usually quiescent, supports our data for a critical role of AFGPs during this season. Studies from Lee and Baust show that Ixodes uriae has the greatest overall range of thermal tolerance, from –30°C to +40°C, reported for any Antarctic terrestrial arthropod (48). The authors proposed that the regulation of the cold tolerance in I. uriae could be due to the presence of antifreeze proteins. Arthropods in nature seek refuge in areas (microenvironment) where they are protected from hard freezing. Chill injury is the most important condition they come across. In addition to the role as inhibitors of ice crystal growth, AFGPs protect membrane stability during low temperature stress and chill injury (58, 59). Hays et al. found that AFGPs prevent leakage from liposomes, suggesting that AFGPs interact with lipids to stabilize membranes at low temperature (60). Collectively, these studies suggest a role for AFGP during chill injury.
The RNAi studies, in which the selective knockdown of iafgp directly interferes with the survival and mobility of I. scapularis ticks, confirms the role of IAFGP in tick fitness at extreme cold temperatures. We noted no changes in survival or mobility with iafgp-dsRNA–treated ticks at warmer (28°C) temperatures (data not shown), suggesting that the effects of the dsRNA on tick survival after cold shock were not due to indirect effects on any aspect of tick biology. Three scenarios may be envisioned that may elucidate the involvement of IAFGP in cold tolerance. First, IAFGP may inhibit ice crystal growth inside ticks, thereby protecting them from lethal stress and damage caused by freezing. Second, IAFGP may prevent (a) denaturation of macromolecules, (b) rupture of cell membrane by blocking ion fluxes across membranes or by inhibiting the leakage of liposomes, and (c) osmotic shrinkage with water loss in cells during freezing. Third, IAFGP may work in concert with other cold tolerance strategies of arthropods such as accumulation of polyhydroxyl alcohols and glycerol to increase the overall cold-tolerance capacity. With any of these models, our finding that iafgp-deficient ticks were reduced in their ability to survive after cold shock suggests a critical role for IAFGP in I. scapularis during the winter.
The mechanism by which IAFGP binds ice water molecules during freezing in ticks is currently not understood. We hypothesize that IAFGP may either directly bind to the ice by hydrogen bonding or by the entropic and enthalpic interactions from hydrophobic residues. The demonstration of reduced membrane disruption of A. phagocytophilum–infected tick cells that express more iafgp and increased cold tolerance upon direct expression of IAFGP in yeast supports this role. These data also suggest a mechanism of IAFGP function at the ice water molecule interface and corroborate the observations seen with other antifreeze proteins (61, 62).
In summary, these data show how an arthropod and a microbe interact to adapt to cold temperature. This beneficial interaction may enhance the long-term coexistence and fitness of both species. This study is not only important in developing an understanding of the molecular basis of mutualism between bacteria and arthropods but also may potentially form the basis for future strategies to interfere with the life cycle of vector-borne human diseases.
Bacterial isolates and ticks. A. phagocytophilum isolate NCH-1 (63) was used throughout this study and will be referred to herein as the A. phagocytophilum. This isolate infects humans and persists in ticks during its different developmental stages. E. coli strain DH5α (Invitrogen) was used as a cloning host for generating different plasmids. Where necessary, the antibiotic ampicillin was used at a final concentration of 50 μg/ml. I. scapularis ticks comprising uninfected, A. phagocytophilum–infected nymphs, uninfected larvae, and uninfected male and female adults and Babesia–infected ticks were obtained from a continuously maintained tick colony at the Department of Epidemiology and Public Health, Yale University. Larvae were fed on either uninfected or A. phagocytophilum–infected mice and allowed to molt to generate uninfected or A. phagocytophilum–infected unfed nymphs. To generate 48-hour–fed A. phagocytophilum–infected nymphs, mock and iafgp-dsRNA–injected ticks were allowed to feed on A. phagocytophilum–infected mice and collected at 48 hours after engorgement. Mice were obtained from Jackson Laboratories and housed at Yale Animal Resources Center. We used female C3H/HeJ mice (Jackson laboratories), 4 to 6 weeks of age, for all our experiments. All tick-feeding experimental protocols followed Yale University institutional guidelines for care and use of laboratory animals and were approved by the Institutional Animal Care and Use Committee (IACUC) at Yale University. Tick rearing was conducted in an incubator at 23°C with 85% relative humidity and a 14-hour light/10-hour dark photoperiod regiment.
Infection rate assessment in ticks. Genomic DNA from A. phagocytophilum–infected unfed nymphs was extracted using DNeasy kit (QIAGEN) and processed for PCR with primers specific for the A. phagocytophilump44 gene (64). 10% of the unfed nymphs from each infection group were individually tested by PCR to confirm A. phagocytophilum infection. A. phagocytophilum infection rates ranged from 80% to 95% from each group. PCR reactions were performed with Taq DNA polymerase (Roche) with conditions as follows: 94°C for 3 minutes initial denaturation followed by 94°C for 1 minute, 54°C for 1 minute, and 72°C for 1 minute for 28 cycles. PCR products were analyzed on 1.5% agarose gels.
Identification of antifreeze glycoprotein gene in I. scapularis. The iafgp (TC43064) full-length nucleotide sequence was identified with BLAST search performed at the Gene Index Project (
http://compbio.dfci.harvard.edu/tgi/) in the I. scapularis EST database using B. saida (NCBI DQ427107) nucleotide sequence as query. EST sequences were further analyzed using DNASTAR software. Total RNA from unfed, uninfected I. scapularis ticks was isolated using QIAGEN RNeasy Kit (QIAGEN), processed for cDNA synthesis using iScript cDNA synthesis (Bio-Rad), and used as a template for RT-PCR. RT-PCR was performed using Master Amp PCR Optimization Kit (Epicentre Technologies). The iafgp gene fragment was amplified using oligonucleotides 5′-ATGACGACTCTGCTTCGTCTGACTATCCT-3′ and 5′-CGTTATTTATTCCCRCGTTTTCAT-3′. The generated PCR products were cloned into pGEM-T easy vector (Promega) and sequenced using primers 5′-CGCCAGGGTTTTCCCAGTCACGAC-3′, 5′-TAATACGACTCACTATA-3′, and 5′-CACACAGGAAACAGCTATGAC-3′ from both ends at KECK DNA Sequencing Facility, Yale University. To obtain additional 32-bp upstream nucleotide sequence (KOZAK sequence) beyond the putative start codon of iafgp gene, PCR was performed using 5′-GAGACTCCAAAGGGACCAACCTA-3′ and 5′-CGTTATTTATTCCCRCGTTTTCAT-3′ and sequenced from the 5′ end with the pGEMT sequencing primer (mentioned above). Figure 3 in the text shows sequence of both 32 bp upstream sequence and iafgp coding sequence. Amino acid sequence similarity and identity of IAFGP were determined by aligning deduced IAFGP amino acid sequences with fish AFGPs from B. saida, Chaenodraco wilsoni, Pogonophryne scotti, Dissostichus mawsoni, Chaenocephalus aceratus, Trematomus hansoni, Notothenia neglecta, Notothenia microlepidota, Harpagifer antarcticus, and Eleginus gracilis using DNASTAR software. Accession numbers for these protein sequences are shown in the legend of Supplemental Figure 3.
Cold treatment for ticks to quantify iafgp mRNA levels. A. phagocytophilum–infected and uninfected control unfed nymphs that were maintained at 23°C in an incubator were split into 4 groups with 20 ticks/group in individual 0.5-ml tubes. These tubes were incubated at 23°C for 2 hours and immediately shifted to different temperatures (10°C, 4°C, and 0°C). One group of ticks was continued with incubation at 23°C as controls. 100 μl of RLT buffer (QIAGEN RNeasy kit) was calibrated in 20 individual tubes/temperature. Ticks and buffer solution were incubated for 4 hours at respective temperatures. After cold treatment, ticks were immediately processed for homogenization in individual tubes with RLT buffer incubated at respective temperatures. For 4°C and 0°C incubations, homogenization was performed in 4°C cold room. All ticks were immediately processed for RNA extraction followed by cDNA synthesis. The mRNA level of iafgp was measured by QRT-PCR.
Survival rate measurement by rapid cold shock. Survival rate of ticks was determined with modifications from Vandyk et al. (65). For generating I. scapularis survival curve, unfed A. phagocytophilum–infected or uninfected nymphs that were maintained at 23°C in an incubator were split into 8 groups with 10 ticks/group in individual glass tubes with ventilated covers that allow aeration. Tubes containing ticks were incubated at 23°C for an additional 2 hours and directly shifted to –20°C on a flat metal surface of the freezer (Hotpoint). A range of time in minutes was chosen at –20°C to determine LT50, at which point 50% tick mortality was observed. After cold treatment at –20°C for 0, 10, 15, 20, 25, 30, 45, and 90 minutes, glass vials containing ticks were immediately shifted to 4°C for 1 hour and room temperature for 1 hour to reacclimatize ticks. After reacclimatization at room temperature, a breath test was performed by blowing air into the glass tubes and immediately ticks were placed side-by-side (1 cm apart) in a line on Whatman filter paper. Any tick moving out of the line within 10 minutes was considered to have survived the cold temperature. Percentage of tick survival at –20°C was determined for each time point, and survival curve was generated from 2 independent experiments with 10 ticks/group/time point using Microsoft Excel. Eighteen independent experiments (10 ticks/group/experiment) with different batches of A. phagocytophilum–infected or uninfected unfed nymphs were then performed to determine whether the presence of A. phagocytophilum influences tick survival at the LT50 time point (25 minutes, –20°C). Rapid cold treatment for mock and iafgp-dsRNA–injected A. phagocytophilum–infected nymphs (48-hour fed ticks) was performed for 50 minutes at –20°C followed by incubation at 4°C for 1 hour and room temperature for 1 hour to reacclimatize ticks. After reacclimatization ticks were analyzed for survival as described before.
Survival rate measurement by sequential cold shock. To determine the survival rate of ticks after sequential cooling, A. phagocytophilum–infected or uninfected unfed nymphs (10 ticks/group/experiment) that were maintained at 23°C were sequentially incubated at 4°C for 1 hour, 0°C for 1 hour, and –10°C for 1 hour and assayed for survival rate at LT50. Further details are provided in Supplemental Methods.
Survival rate measurement by scrambled assay. To eliminate any bias in the measurement of survival rate of A. phagocytophilum–infected unfed nymphs in comparison with the unfed uninfected controls, scrambled assays were performed. A. phagocytophilum–infected and uninfected unfed nymphs (10 ticks/group/experiment) were mixed in equal numbers. Glass tubes containing mixed groups of ticks were treated the same way as in rapid cold shock experiments. After cold treatment at LT50 (–20°C, 25 minutes), ticks were placed in a line and then numbered from 1 to 20. Survival was determined and documented for each numbered tick. After survival assay, all ticks were processed for DNA extraction (QIAGEN) and PCR to classify them as uninfected (no PCR product with p44 gene primers) or A. phagocytophilum–infected ticks (PCR positive with p44 gene primers). Six independent experiments were performed, and statistical significance (P < 0.05) was calculated using Mann-Whitney U test.
Tick mobility measurements. Along with the survival assays (rapid cold shock experiments, sequential cold shock experiments, and scrambled assays), unfed nymphs were also monitored for mobility on Whatman filter paper. After cold shock and further processing as mentioned in rapid cold shock experiments, ticks were immediately placed in a line 1 centimeter apart and monitored for movement from starting point (point where ticks were placed at the start of the assay) to the end point (point where ticks have moved after 10 minutes of observation). Distance from the start point and end point was measured in centimeters for each individual tick. Ticks that did not move after 10 minutes were scored as zero. Mobility (distance traveled) measurement for both categories of ticks (uninfected and A. phagocytophilum–infected unfed nymphs) from 5 independent experiments was then analyzed using GraphPad Prism software, and statistical significance (P < 0.05) was calculated using the Mann-Whitney U test.
QRT-PCR analysis. Total RNA from unfed nymphs, unfed larvae, unfed adult male and female ticks, or tick cell line was converted to cDNA. The generated cDNA was used as a template for the amplification of iafgp mRNA. QRT-PCR was performed using iQ-SYBR Green Supermix (Bio-Rad). The levels of iafgp were quantified using oligonucleotides 5′-ATGAAGACTCTGCTTCCTCTGACTATCCT-3′ and 5′-GGTGTAGCCGCCCTTTTGG-3′. Standard curve was prepared using 10-fold serial dilutions of known quantities of iafgp gene cloned in pGEMT-Easy Vector. As an internal control and to normalize the amount of template, tick β-actin amplicons were quantified with published primers (66). Standard curve for tick actin was prepared using 10-fold serial dilutions of known quantities from 0.5 ng to 0.000005 ng.
dsRNA synthesis and tick microinjections. The pGEMT-iafgp plasmid was used as a template to amplify DNA encoding a fragment of iafgp. The iafgp gene-specific primers containing BglII (5′-GAAGATCTGTTGCCGGCGTGCTCG-3′) and KpnI (5′-GGGGTACCCTTCCGTATCCGAGCCCGTA-3′) restriction enzyme sites were used in the PCR. The fragment containing iafgp sequence was purified and cloned into BglII-KpnI sites of the L4440 double T7 Script II vector (67). dsRNA complementary to iafgp sequence was synthesized using the MEGAscript RNAi Kit (Ambion Inc.) following manufacturer’s instructions. Mock dsRNA was prepared from empty L4440 vector that contained restriction enzyme site sequences. Microinjections of mock and iafgp dsRNAs were performed as described (67). Briefly, 1 μg of L4440 empty vector or iafgp-containing vector was used as a template to prepare dsRNA. The prepared dsRNA was eluted in 50 μl of injection buffer (Ambion Inc.). Microinjections were made (4.2 nl/tick, 1 × 1012 molecules/μl) into the bodies of unfed nymphs as mentioned previously (67). Microinjected ticks were incubated either at room temperature for 3 days in a desiccator or fed on A. phagocytophilum–infected mice for 48 hours and analyzed for iafgp silencing by QRT-PCR. Silencing was confirmed using primers that were used for QRT-PCR and with 5′-CGGCTACGGGCTCGGA-3′ and 5′-GTTATTTATTCCCACGTTTTCATTTG-3′. Silencing of trospA gene was performed as described (68).
Tick cell line experiments. Ixodes ricinus tick cell line (IRE/CTVM19, maintained at 28°C without CO2) was used throughout our experiments (69). A. phagocytophilum infection was maintained in human promyelocytic cell line (HL-60; ATCC) maintained at 37°C, 5% CO2 in IMDM (Gibco; Invitrogen) with 20% FCS. For infecting tick cell line with A. phagocytophilum, bacteria were collected from A. phagocytophilum–infected HL-60 cells by centrifugation for 10 minutes at 3889 g. Cell pellets were resuspended in IMDM, lysed by 6 passages through a 25-gauge needle followed by 6 more passages through a 27-gauge needle, and the lysates were centrifuged at 350 g for 3 minutes to obtain cell-free bacteria in the supernatants that were used to infect the tick cell line. To quantify iafgp expression in tick cells, uninfected or A. phagocytophilum–infected tick cells were incubated at 28°C, 4°C, 0°C, and –5°C for 2 hours and immediately processed for RNA extraction, cDNA synthesis, and QRT-PCR. Cold shock experiments are described in the Supplemental Methods.
Yeast survival assays. S. cerevisiae strain EBY100 (Invitrogen) was used in all our analyses. The full-length iafgp gene was PCR amplified with oligonucleotides 5′-CGGAATTCATGACGACTCTGCTTCGTCTGACT-3′ and 5′-CCGCTCGAGCGCAGCCGCCGTAGCT-3′ containing EcoRI and XhoI sites, respectively, from pGEMT-iafgp plasmid DNA as a template. The obtained PCR product was digested with EcoRI-XhoI and cloned into pYD1 vector (Invitrogen) digested with EcoRI-XhoI generating pYD1/FL-iafgp. The plasmids pYD1/FL-iafgp or pYD1 (without insert) were transformed into EBY100 competent cells, and cold tolerance assays were performed as mentioned in the Supplemental Methods.
GenBank accession numbers. The GenBank accession numbers for I. scapularisafgp (iafgp) and I. ricinusafgp (iafgp-Iric) are HM213906 and HM213905, respectively.
Statistics. The statistical significance of differences observed in data sets was analyzed using Microsoft Excel and GraphPad Prism Software. For data with small variations and normal distribution, such as levels of iafgp expression in ticks or p44 levels in A. phagocytophilum–infected nymphs, a 2-tailed Student’s t test was performed to compare 2 means. For data with large variations and/or a nonparametric distribution, such as survival and mobility measurements, a 2-tailed Mann-Whitney U test was performed to compare 2 medians. Supplemental Table 1 shows sum of ranks in all experimental samples compared using Mann-Whitney U test. P < 0.05 was considered significant in all statistical analyses.
View Supplemental data
We thank A. Shaw for helpful discussions and D. Beck, K. DePonte, and L. Rollend for technical assistance. This work was supported by USDA grant 58-0790-6-139 and NIH grants 41440 and 32947. G. Neelakanta is a recipient of a postdoctoral fellowship from the Arthritis Foundation. E. Fikrig is an investigator of the Howard Hughes Medical Institute.
Conflict of interest: The authors have declared that no conflict of interest exists.
Citation for this article:J Clin Invest. 2010;120(9):3179–3190. doi:10.1172/JCI42868.
See the related Commentary beginning on page 3087.
Braendle C, Miura T, Bickel R, Shingleton AW, Kambhampati S, Stern DL. Developmental origin and evolution of bacteriocytes in the aphid-Buchnera symbiosis.
PLoS Biol. 2003;1(1):E21.
Bandi C, Dunn AM, Hurst GD, Rigaud T. Inherited microorganisms, sex-specific virulence and reproductive parasitism. Trends Parasitol. 2001;17(2):88–94.
Herbert EE, Goodrich-Blair H. Friend and foe: the two faces of Xenorhabdusnematophila.
Nat Rev Microbiol. 2007;5(8):634–646.
Dale C, Moran NA. Molecular interactions between bacterial symbionts and their hosts. Cell. 2006;126(3):453–465.
Kikuchi Y, Hosokawa T, Fukatsu T. Insect-microbe mutualism without vertical transmission: a stinkbug acquires a beneficial gut symbiont from the environment every generation. Appl Environ Microbiol. 2007;73(13):4308–4316.
Dillon R, Charnley K. Mutualism between the desert locust Schistocercagregaria and its gut microbiota.
Res Microbiol. 2002;153(8):503–509.
de Vries EJ, Jacobs G, Breeuwer JA. Growth and transmission of gut bacteria in the Western flower thrips, Frankliniellaoccidentalis.
J Invertebr Pathol. 2001;77(2):129–137.
Douglas AE. Nutritional interactions in insect-microbial symbioses: aphids and their symbiotic bacteria Buchnera. Annu Rev Entomol. 1998;43:17–37.
Pais R, Lohs C, Wu Y, Wang J, Aksoy S. The obligate mutualist Wigglesworthiaglossinidia influences reproduction, digestion, and immunity processes of its host, the tsetse fly.
Appl Environ Microbiol. 2008;74(19):5965–5974.
Werren JH, Baldo L, Clark ME. Wolbachia: master manipulators of invertebrate biology.
Nat Rev Microbiol. 2008;6(10):741–751.
Waterfield NR, Wren BW, Ffrench-Constant RH. Invertebrates as a source of emerging human pathogens. Nat Rev Microbiol. 2004;2(10):833–841.
Belongia EA. Epidemiology and impact of coinfections acquired from Ixodes ticks.
Vector Borne Zoonotic Dis. 2002;2(4):265–273.
Steiner FE, et al. Infection and co-infection rates of Anaplasmaphagocytophilum variants, Babesia spp., Borrelia burgdorferi, and the rickettsial endosymbiont in Ixodesscapularis (Acari: Ixodidae) from sites in Indiana, Maine, Pennsylvania, and Wisconsin.
J Med Entomol. 2008;45(2):289–297.
Holman MS, et al. Anaplasma phagocytophilum, Babesia microti, and Borrelia burgdorferi in Ixodes scapularis, southern coastal Maine.
Emerg Infect Dis. 2004;10(4):744–746.
Adelson ME, et al. Prevalence of Borrelia burgdorferi, Bartonella spp., Babesia microti, and Anaplasma phagocytophila in Ixodes scapularis ticks collected in Northern New Jersey.
J Clin Microbiol. 2004;42(6):2799–2801.
Anderson JF, Magnarelli LA. Biology of ticks. Infect Dis Clin North Am. 2008;22(2):195–215.
Noda H, Munderloh UG, Kurtti TJ. Endosymbionts of ticks and their relationship to Wolbachia spp. and tick-borne pathogens of humans and animals.
Appl Environ Microbiol. 1997;63(10):3926–3932.
Yuval B, Spielman A. Duration and regulation of the developmental cycle of Ixodesdammini (Acari: Ixodidae).
J Med Entomol. 1990;27(2):196–201.
Brownstein JS, Holford TR, Fish D. A climate-based model predicts the spatial distribution of the Lyme disease vector Ixodes scapularis in the United States.
Environ Health Perspect. 2003;111(9):1152–1157.
Duman JG. Antifreeze and ice nucleator proteins in terrestrial arthropods. Annu Rev Physiol. 2001;63:327–357.
Bale JS. Insects and low temperatures: from molecular biology to distributions and abundance. Philos Trans R Soc Lond B Biol Sci. 2002;357(1423):849–862.
Doucet D, Walker VK, Qin W. The bugs that came in from the cold: molecular adaptations to low temperatures in insects. Cell Mol Life Sci. 2009;66(8):1404–1418.
DeVries AL. Glycoproteins as biological antifreeze agents in antarctic fishes. Science. 1971;172(988):1152–1155.
Harding MM, Anderberg PI, Haymet AD. ‘Antifreeze’ glycoproteins from polar fish. Eur J Biochem. 2003;270(7):1381–1392.
Jia Z, Davies PL. Antifreeze proteins: an unusual receptor-ligand interaction. Trends Biochem Sci. 2002;27(2):101–106.
Feeney RE, Burcham TS, Yeh Y. Antifreeze glycoproteins from polar fish blood. Annu Rev Biophys Biophys Chem. 1986;15:59–78.
DeVries AL. Antifreeze glycopeptides and peptides: interactions with ice and water. Methods Enzymol. 1986;127:293–303.
Ben RN. Antifreeze glycoproteins--preventing the growth of ice. Chembiochem. 2001;2(3):161–166.
Davies PL, Sykes BD. Antifreeze proteins. Curr Opin Struct Biol. 1997;7(6):828–834.
Davies PL, Baardsnes J, Kuiper MJ, Walker VK. Structure and function of antifreeze proteins. Philos Trans R Soc Lond B Biol Sci. 2002;357(1423):927–935.
Geoghegan KF, Osuga DT, Ahmed AI, Yeh Y, Feeney RE. Antifreeze glycoproteins from Polar fish. Structural requirements for function of glycopeptide 8. J Biol Chem. 1980;255(2):663–667.
Burcham TS, Osuga DT, Rao BN, Bush CA, Feeney RE. Purification and primary sequences of the major arginine-containing antifreeze glycopeptides from the fish Eleginusgracilis.
J Biol Chem. 1986;261(14):6384–6389.
DeVries AL, Wohlschlag DE. Freezing resistance in some Antarctic fishes. Science. 1969;163(871):1073–1075.
Graham LA, Liou YC, Walker VK, Davies PL. Hyperactive antifreeze protein from beetles. Nature. 1997;388(6644):727–728.
Duman JG, Bennett V, Sformo T, Hochstrasser R, Barnes BM. Antifreeze proteins in Alaskan insects and spiders. J Insect Physiol. 2004;50(4):259–266.
Sjursen H, Somme L. Seasonal changes in tolerance to cold and desiccation in Phauloppia sp. (Acari, Oribatida) from Finse, Norway.
J Insect Physiol. 2000;46(10):1387–1396.
Tursman D, Duman JG, Knight CA. Freeze tolerance adaptations in the centipede, Lithobius forficatus. J Exp Zool. 1994;268(5):347–353.
Sinclair BJ, Chown SL. Haemolymph osmolality and thermal hysteresis activity in 17 species of arthropods from sub-Antarctic Marion Island. Polar Biol. 2002;25(12):928–933.
Patterson JL, Kelly TJ, Duman JG. Purification and com-position of a thermal hysteresis producing protein from the milkweed bug Oncopeltus fasciatus.
J Comp Physiol. 1981;142(4):539–542.
Duman JG. Environmental effects on antifreeze levels in larvae of the darkling beetle, Meracantha contracta.
J Exp Zool. 1977;201(2):333–337.
Kozak M. An analysis of 5′-noncoding sequences from 699 vertebrate messenger RNAs. Nucleic Acids Res. 1987;15(20):8125–8148.
Koropatnick TA, et al. Microbial factor-mediated development in a host-bacterial mutualism. Science. 2004;306(5699):1186–1188.
Baumann P. Biology of bacteriocyte-associated endosymbionts of plant sap-sucking insects. Annu Rev Microbiol. 2005;59:155–189.
Hurst GD, Werren JH. The role of selfish genetic elements in eukaryotic evolution. Nat Rev Genet. 2001;2(8):597–606.
Scarborough CL, Ferrari J, Godfray HC. Aphid protected from pathogen by endosymbiont. Science. 2005;310(5755):1781.
Hance T, Bolvin G. Effect of parasitism by Anaphessp. (Hymenoptera: Mymaridae) on the cold hardiness of Listronotus oregonensis (Coleoptera: Curculionidae) eggs.
Can J Zool. 1993;71:759–764.
Block W, Turnock WJ, Jones TH. Cold resistance and overwintering survival of the cabbage root fly, Delia radicum (Anthoomyiidae) and its parasitoid, Trybliographa rapae (Cynipidae), in England.
Lee RE, Baust JG. Cold-hardiness in the Antarctic tick, Ixodes uriae.
Physiol Zoology. 1987;60(4):499–506.
Dautel H, Knulle W. The supercooling ability of ticks (Acari, Ixodoidea). J Comp Physiol B. 1996;166(8):517–524.
Burks CS, Stewart RJ, Needham GR, Lee RE. The role of direct chilling injury and inoculative freezing in cold tolerance of Amblyomma americanum, Dermacentor variabilis and Ixodes scapularis.
Physiol Entomol. 1996;21:44–50.
Wen D, Laursen RA. Structure-function relationships in an antifreeze polypeptide. The role of charged amino acids. J Biol Chem. 1993;268(22):16396–16400.
Feldhaar H, Gross R. Insects as hosts for mutualistic bacteria. Int J Med Microbiol. 2009;299(1):1–8.
Hotopp JC, et al. Comparative genomics of emerging human ehrlichiosis agents. PLoS Genet. 2006;2(2):e21.
Courtney JW, Dryden RL, Wyleto P, Schneider BS, Massung RF. Characterization of Anaplasma phagocytophila and Borrelia burgdorferi genotypes in Ixodes scapularis ticks from Pennsylvania.
Ann N Y Acad Sci. 2003;990:131–133.
Kurtenbach K, Hanincova K, Tsao JI, Margos G, Fish D, Ogden NH. Fundamental processes in the evolutionary ecology of Lyme borreliosis. Nat Rev Microbiol. 2006;4(9):660–669.
Carroll JF, Kramer M. Winter activity of Ixodes scapularis (Acari: Ixodidae) and the operation of deer-targeted tick control devices in Maryland.
J Med Entomol. 2003;40(2):238–244.
Dautel H, Dippel C, Kammer D, erkhausen A, Kahl O. Winter activity of Ixodes ricinus in a Berlin forest.
Int J Med Microbiol. 2008;298(suppl 1):50–54.
Tablin F, et al. Membrane reorganization during chilling: implications for long-term stabilization of platelets. Cryobiology. 2001;43(2):114–123.
Rubinsky B, Arav A, Fletcher GL. Hypothermic protection--a fundamental property of “antifreeze” proteins. Biochem Biophys Res Commun. 1991;180(2):566–571.
Hays LM, Feeney RE, Crowe LM, Crowe JH, Oliver AE. Antifreeze glycoproteins inhibit leakage from liposomes during thermotropic phase transitions. Proc Natl Acad Sci U S A. 1996;93(13):6835–6840.
Chao H, et al. A diminished role for hydrogen bonds in antifreeze protein binding to ice. Biochemistry. 1997;36(48):14652–14660.
Wierzbicki A, Taylor MS, Knight CA, Madura JD, Harrington JP, Sikes CS. Analysis of shorthorn sculpin antifreeze protein stereospecific binding to (2-10) faces of ice. Biophys J. 1996;71(1):8–18.
Magnarelli LA, Ijdo JW, Stafford KC 3rd, Fikrig E. Infections of granulocytic ehrlichiae and Borrelia burgdorferi in white-tailed deer in Connecticut. J Wildl Dis. 1999;35(2):266–274.
IJdo JW, Wu C, Telford SR 3rd, Fikrig E. Differential expression of the p44 gene family in the agent of human granulocytic ehrlichiosis. Infect Immun. 2002;70(9):5295–5298.
Vandyk JK, Bartholomew DM, Rowley WA, Platt KB. Survival of Ixodes scapularis (Acari: Ixodidae) exposed to cold.
J Med Entomol. 1996;33(1):6–10.
Neelakanta G, et al. Outer surface protein B is critical for Borrelia burgdorferi adherence and survival within Ixodes ticks.
PLoS Pathog. 2007;3(3):e33.
Narasimhan S, et al. Disruption of Ixodes scapularis anticoagulation by using RNA interference.
Proc Natl Acad Sci U S A. 2004;101(5):1141–1146.
Pal U, et al. TROSPA, an Ixodes scapularis receptor for Borrelia burgdorferi.
Pedra JH, et al. Fucosylation enhances colonization of ticks by Anaplasmaphagocytophilum. [published online ahead of print March 19, 2010].Cell Microbiol.doi:10.1111/j.1462-5822.2010.01464.