1. Introduction
Coxiella burnetii is a Gram-negative, intracellular bacterium with a near worldwide distribution [
1,
2]. The zoonosis Q fever is caused by this bacterium, typically following inhalation of infectious particles generated by infected animals. Q fever encompasses a wide spectrum of clinical disease; however, the most common manifestation is a flulike illness known as acute Q fever [
3]. Due to the potentially debilitating nature of Q fever,
C. burnetii’s pronounced environmental stability, and aerosol infection potential, this pathogen is considered a biodefense threat and has been classified as a select agent by the U.S. Centers for Disease Control and Prevention (CDC)-Division of Select Agents and Toxins (DSAT) [
4].
C. burnetii Nine Mile II (NMII) Clone 4 (RSA439), is exempt from DSAT regulation and may be manipulated at BSL-2 conditions [
5]. This clonal strain expresses truncated lipopolysaccharide (LPS) due to a large chromosomal deletion and has been reported to exhibit avirulence in a guinea pig infection model [
6]. In contrast,
C. burnetii NMI is a virulent strain expressing full-length LPS and is commonly used as a positive control for virulence in animal studies. Beyond laboratory-generated strains such as NMII, clinically and environmentally derived
C. burnetii strains have been isolated from a wide array of organisms including cats, chiggers, cows, dogs, goats, humans, rodents, sheep, and ticks [
7,
8,
9]. These strains exhibit genetic and phenotypic diversity [
7,
10,
11] despite retaining full-length LPS and the type IVB secretion system (T4BSS), two core
C. burnetii virulence factors.
In 1959, the isolation of several novel “Dugway”
C. burnetii strains was reported [
12]. These strains were isolated from three rodent species (
Peromyscus maniculatus,
Dipodomys ordii, and
D. microps) from the Great Salt Lake Desert, Utah USA during a three-year collection period (1954–1957) [
12]. This marked the first report of
C. burnetii recovery from wild mammals. The unique biologic characteristics of the Dugway strains were reported soon after these strains were isolated. The authors encountered difficulty passaging yolk sac isolates in infected guinea pigs due to apparent avirulence, a hypothesis further bolstered by guinea pig infection studies [
13]. Additionally, hamsters appeared to be more susceptible to the Dugway strain infection and pathology than guinea pigs, also developing higher antibody titers following infection. These findings stood in contrast to results obtained for non-rodent derived isolates (e.g., dairy and clinical human isolates). Recent studies confirmed Dugway strain attenuation in guinea pig intraperitoneal [
11] and aerosol [
10] infection models. Genetic analysis of the Dugway 5J108-111 strain indicated that this strain has the largest genome with the fewest pseudogenes and insertion sequence elements compared to all other
C. burnetii strains [
14]. These data suggest that the Dugway strains supersede other isolates (e.g., NMI, K Q154, and G Q212) in terms of temporal lineage establishment. Dugway strains possess the unique QpDG plasmid [
15] and Dugway-specific plasmid-encoded effector proteins have been identified [
16]. It remains to be seen whether chromosomal and/or plasmid genomic sequences lie at the root of Dugway strains’ unique behavior. Further, phylogenetic analysis of various
C. burnetii strains based on
adaA gene variation suggested that Dugway strains may be the ancestor of all
C. burnetii strains [
17].
Likely related to host adaptation and tropism, these unique genetic and phenotypic features pose Dugway strains as valuable experimental tools and potential vaccine candidates. Avirulence and/or severe attenuation despite retention of primary virulence factors paired with Dugway strains’ unique genomic content all contribute to its intrigue and utility. Dugway strains possess desired qualities for whole-cell vaccines (WCV); however, protective efficacy has not yet been determined. Further, Q fever WCVs are known to cause potentially severe post-vaccination hypersensitivity responses in pre-immune individuals [
18], representing a major roadblock for widespread licensing of existing Q fever vaccines (e.g., Q-VAX
®). Although mechanisms of post-Q fever vaccination delayed-type hypersensitivity (DTH) are being uncovered using novel animal models [
19,
20], causative antigens have not yet been determined. Accordingly, despite Dugway strain uniqueness, the reactogenicity of Dugway-based WCVs has not been reported. Here, we sought to characterize Dugway-host interactions in vivo using guinea pig models of infection, vaccine challenge, and post-vaccination DTH. Further, these studies were designed to evaluate the feasibility of Dugway-based WCVs as an improved Q fever vaccine. Thus, we created a mutant Dugway ∆
dot/icm strain, lacking 23 or 26 genes within the
dot/icm apparatus encoding the TB4SS apparatus. This strategy has been used for
C. burnetii NMI and conferred attenuation, retained immunogenicity, and potentially reduced post-vaccination DTH magnitude [
21].
2. Materials and Methods
2.1. Coxiella burnetii Strains, Infection Stocks, and Whole-Cell Vaccines (WCV)
C. burnetii strains (NMI RSA 439, Dugway 7D 77-80, and Dugway Δ
dot/icm clone 7) were propagated in acidified citrate cysteine medium-2 or -D (ACCM-2 or ACCM-D) [
22] at 37 °C, 2.5% O
2, and 5% CO
2 and were stored at −80 °C in a cell-freezing medium (DMEM with 10% fetal bovine serum and 10% dimethyl sulfoxide) until use.
C. burnetii Dugway Δ
dot/icm was constructed as previously described for the NMI Δ
dot/icm strain [
21]. Whole-cell vaccine (WCV) stocks, used for vaccination and skin testing, were cultured as infection stocks and were fixed in 4% paraformaldehyde for at least 12 h, washed in sterile PBS, and ultimately resuspended in USP-grade saline prior to being stored at −80 °C.
C. burnetii infection stock concentrations were quantified using qPCR to enumerate genomic equivalents (GE) [
11] while WCV concentrations were determined via direct bacterial count, as previously described [
21,
23]. Lipopolysaccharide (LPS) from infection stocks was extracted via a modified hot phenol method and visualized by silver stain, as previously described [
24] (
Supplementary Figure S1). In accordance with standard operating procedures approved by the Rocky Mountain Laboratories Institutional Biosafety Committee, any manipulations of
C. burnetii stocks and infected animal tissue were performed in a BSL-3 laboratory.
2.2. Guinea Pigs
Four- to six-week-old Hartley guinea pigs were obtained from Charles River, Wilmington, MA, USA (strain code 051) and were acclimated for at least a week prior to experimental manipulation. Female guinea pigs were utilized in these studies to minimize potentially confounding sex-associated factors (e.g., behavior, body weight, hormonal effects) and are used in accordance with historical Q fever virulence studies [
10,
25]. Animals were housed in individually ventilated plastic cages (Allentown, Allentown, NJ, USA; two animals per cage) with hardwood Sani-chip bedding (PJ Murphy, Montville, NJ, USA). A high-fiber guinea pig diet (Teklad global high-fiber guinea pig diet; Envigo, Indianapolis, IN, USA, cat n. 2041) and chlorinated, reverse osmosis filtered tap water was administered ad libitum. A 12 h light–dark cycle was maintained in animal housing facilities which were kept at 68–72 °F and 40–60% relative humidity with a 50% set point. Six animals per group were utilized for the experiment evaluating virulence, while four animals per group were utilized in vaccine challenge and post-vaccination hypersensitivity experiments. Animals were housed in approved animal biosafety level 3 (ABSL-3) facilities and manipulated under ABSL-3 standard operating procedures approved by the Rocky Mountain Laboratories Institutional Biosafety Committee and an Institutional Animal Care and Use Committee-approved protocol. Animal experiments and procedures were performed in an Association for Assessment and Accreditation of Laboratory Animal Care-accredited NIH/NIAID animal facility.
2.3. Infection Model
On the day of infection, animals were placed under isoflurane-induced sedation using an anesthetic vaporizer with activated charcoal absorption filters (VetEquip Inc., cat. N. 901801 and 931401, Livermore, CA, USA) and subcutaneously implanted with an IPTT-300 transponder (BioMedic Data Systems, Seaford, DE, USA) above the shoulder using a large bore needle. Guinea pigs were then infected with 1 mL of 10
6–10
7 GE of
C. burnetii in USP-grade saline via intraperitoneal injection. Negative control animals were mock infected with USP-grade saline. Body weights, body temperatures, and any behavioral/clinical changes were recorded daily at a consistent time for 14 days following infection. Body temperatures were collected using a DAS-8007-P reader (BioMedic Data Systems) and a temperature of ≥39.5 °C was defined as fever [
10,
26,
27]. Fourteen days post-infection, animals were euthanized. Blood and spleens were collected at euthanasia and processed as previously described and bacterial outgrowth from spleen tissues was quantified by TaqMan qPCR (
groel gene) [
21].
2.4. WCV Challenge Model
On the day of vaccination, animals were sedated by isoflurane inhalation and implanted with IPTT-300 transponders as described above. Four guinea pigs per group were vaccinated subcutaneously in the upper back with 0.5 mL of USP-grade saline containing 25–2.5 μg of QVax
® or paraformaldehyde-fixed
C. burnetii. Negative control animals were mock vaccinated with USP-grade saline. Body weights, body temperatures, and behavioral/clinical changes were recorded daily following vaccination for a total duration of 28 days. At 28 days post-vaccination, animals were infected with 1 mL of 10
6 GE
C. burnetii (NMI) as described above. Upon euthanasia, blood, mesenteric lymph nodes, and spleens were collected and processed as previously described [
21].
For mLN and splenic flow cytometric analysis, single-cell suspensions were aliquoted into 96-well U-bottom plates at a density of 1 × 106 cells per well. Cells were washed in a staining buffer (PBS + 1% bovine serum albumin) and stained using a cocktail of antibodies specific for guinea pig cell surface antigens, including B Cells (clone: MsGp10, fluorophore: S/N unconjugated, BioRad, Hercules, CA, USA, cat. N. MCA567) with secondary antibody (anti-mouse IgG1, clone: RMG1-1, fluorophore: AF700, BioLegend, San Diego, CA, USA, cat. N. 406632), CD4 (clone: CT7, fluorophore: RPE, BioRad, cat. n. MCA749PE), and CD8 (clone: CT6, fluorophore: FITC, BioRad, cat. n. MCA752F). Following surface staining, cells were washed in staining buffer and fixed overnight at 4 °C using Cytofix (BD, San Jose, CA, USA, cat. n. 554655). Following fixation, cells were washed in staining buffer and analyzed on a BD FACSymphony flow cytometer using FacsDiva software (BD Biosciences). Data analysis was performed with FlowJo 10.0 software (TreeStar Inc., Ashland, OR, USA). A minimum of 20,000 events were captured for each sample. Single-stained compensation controls and fluorescence minus one staining controls were included to help set gating boundaries.
2.5. Post-Vaccination Hypersensitivity Modeling
The guinea pig post-vaccination hypersensitivity model was performed as previously described [
21]. Briefly, four guinea pigs per group were infected with 10
6 GE of NMI or mock infected with saline and monitored for 42 days. Next, animals were sedated by isoflurane inhalation and skin tested with 0.1 mL of 25, 2.5, and 0.25 μg of
C. burnetii WCV in USP-grade saline via intradermal injection at three separate sites on the shaved back. Negative control animals were mock skin tested with USP-grade saline. Body weights, body temperatures, behavioral/clinical changes, and skin metrics were recorded daily for 21 days post-skin tests. Skin-testing sites were shaved one day prior to intradermal inoculation (“skin testing”) and one day prior to subsequent skin metric measurement. Erythema diameter and induration severity were measured as previously described [
21]. Animals were euthanized 21 days following skin testing. Blood, mesenteric lymph nodes, spleens, and skin biopsies were collected for subsequent analysis, as previously described [
21].
2.6. Histology
Histology was performed as previously described [
20]. Briefly, skin biopsies were fixed in 10% Neutral Buffered Formalin for 48 h, placed in tissue cassettes, and processed with a Sakura VIP-6 Tissue Tek (Torrance, CA, USA) on a 12 h automated schedule using a graded series of ethanol, xylene, and PureAffin. Embedded tissues were sectioned at 5 μm, mounted and dried overnight at 42 °C prior to staining with hematoxylin and eosin using established methods. Biopsy specimens were evaluated using an Olympus BX53 microscope (Tokyo, Japan).
2.7. Statistical Analysis
Statistical analyses were conducted using GraphPad Prism version 7.0 (GraphPad Software, La Jolla, CA, USA). Statistical evidence for differences in group means was assessed using two-sample Welch t tests, allowing for unequal variances between groups. For each comparison, we computed Wald-type 95% confidence intervals and describe statistical significance with two-sided p-values. We represent p-values in equal to or below 0.05 with a single asterisk (*), p-values equal to or below 0.01 with a double asterisk (**), and p-values equal to or below 0.001 with a triple asterisk (***) unless otherwise indicated. Error bars represent the standard deviation of a group mean.
4. Discussion
Initial reports regarding Dugway strain characteristics included attenuation or avirulence in a guinea pig model of infection [
12] and high infectivity and antibody responsiveness in a hamster model of infection [
13]. Compared to high antibody titers induced by virulent strains in hamsters, guinea pigs, and mice, Dugway isolates only induced comparable titers in hamsters. More recently, Dugway strain avirulence in guinea pig infection models has been replicated [
10,
11]. Building on these studies, we address the potential of Dugway strain virulence, heterologous WCV protective capacity, and post-vaccination reactogenicity. Our guinea pig infection study data indicate that Dugway isolate 7D 77-80 displays similar virulence potential to the exempted NMII strain (RSA 439, clone 4), widely considered to be avirulent or severely attenuated [
6,
25]. This assessment is based on the effect of infection on body temperature, weight, and changes to the size and histological composition of the spleen. Animals inoculated with Dugway Δ
dot/icm yielded a similar clinical profile compared to the saline mock-infected control group, apart from slight splenomegaly in animals inoculated with 10
7 GE. This data complements former reports of Dugway strain attenuation in the guinea pig model [
10,
11,
13] and avirulence in Δ
dot/icm strains [
21]. Considering the physiologic relevance of the guinea pig model with humans in the context of Q fever [
28,
29] and the lack of any reported human infections involving Dugway strains, they are likely to exhibit attenuation in humans. Other phase I
C. burnetii isolates exhibit attenuation in guinea pig infection models, including G Q212, Priscilla/MSU Goat Q177, and P Q238 [
10,
11]. These isolates are derived from human heart valve samples (G Q212 and P Q238) and a goat cotyledon following abortion (Priscilla/MSU goat Q177). Together, this information indicates factors beyond plasmid type and LPS influence
C. burnetii virulence potential.
Despite an incomplete understanding of protective antigens involved in WCV immunity, the role of full-length LPS/
O-antigen has been well-established [
25]. Given the presence of full-length LPS in Dugway strains, heterologous protection displayed by Dugway WCV was expected. In a direct comparison to QVax
®, Dugway WCV demonstrated similar efficacy with neither breakthrough fever nor splenomegaly as evidenced at the lowest dose of QVax
®. Despite clear protective efficacy after challenge infection, demonstrated by a lack of fever, body weight change, and splenomegaly,
C. burnetii was detectable via qPCR in spleens of all vaccinated animals. Notably, at 14 days post-infection,
C. burnetii splenic burden appears to be low and difficult to detect, likely due to host clearance. Regardless, sterilizing immunity was not achieved for QVax
® or Dugway WCV, although the absence of clinical disease is notable. Further, a significant increase in mLN CD8
+ T cell frequency in the Saline:NMI group following infection was not reflected in vaccinated, challenged animals. This observation recalls data reported in earlier studies [
21] and may indicate a role for cytotoxic CD8
+ T cells in primary immunity. Here, we present a comprehensive assessment of fever in the guinea pig model in response to QVax
® dose escalation in the intraperitoneal guinea pig infection model. This data will likely prove useful for future comparative vaccine studies, as QVax
® is considered the gold standard for protection against Q fever.
In a guinea pig PVH model, the Dugway strain appeared to be as reactive as NMI and QVax
®. Further, regardless of sensitization strain (Dugway or NMI), Dugway skin-tested animals appeared to experience reactogencitiy comparable to NMI skin-tested animals. Histological characterization of skin-testing sites also appeared comparable between strains. This indicates common PVH antigens shared among Dugway and Nine Mile strains. As previously reported [
21], Δ
dot/icm strains appeared to be less reactive based on several experimental endpoints, including erythema and induration. Indeed, Dugway Δ
dot/icm demonstrated the most promising reduction in reactogenicity. Beyond the potential contribution of the T4BSS, additional antigens remain to be identified. Newly developed murine PVH models may provide utility in further studies [
19,
20].
The host species from which Dugway strains were isolated from may contribute to their unique characteristics in guinea pig models. Dugway strains were isolated from deer mice (
Peromyscus maniculatus) and kangaroo rats (
Dipodomys ordii and
D. microps). Despite the recent identification of
C. burnetii DNA in deer mice (Canada) and wild rodents (Spain), further strain characterization was not performed [
30,
31]. In laboratory settings, deer mice, kangaroo rats, and other wild rodent species were shown to be susceptible to intraperitoneal
C. burnetii infection, albeit to a lesser degree than guinea pigs [
32,
33]. Due to the environmental range of
C. burnetii, a hypothesis exists that describes wild rodents as disease reservoirs with the potential involvement of ticks in the natural lifecycle of the bacterium separate from or associated with the genesis of the livestock lifecycle of infection [
9,
32,
33]. It is tempting to suggest that wild rodent host adaptation may influence
C. burnetii characteristics such as virulence and behavior in a distinct host, such as a guinea pig or human. Further study is needed to address this hypothesis and the Dugway strain group will likely prove a valuable resource in this effort.
The presented data build upon historic findings relating to unique C. burnetii Dugway strains. Our characterization of Dugway host-pathogen interactions in vivo reveals an attenuated strain with vaccine potential. Specifically, the Dugway Δdot/icm strain appears to be a viable WCV candidate, exhibiting significantly reduced reactogenicity. The unique behavior of Dugway isolates paired with the large amount of unique genomic material contained in these isolates raises many important questions. For example, why are Dugway strains attenuated, what do novel genomic regions encode and are they functionally relevant, and does host adaptation play a role in Dugway strain behavior? This manuscript highlights Dugway strain behavior in vivo and provides a framework for future studies to address these inquiries. Indeed, the unique background and phenotype of the Dugway strain group provide a valuable experimental platform for the study C. burnetii pathogenesis and mechanisms of virulence.