- Research article
- Open Access
DNA vaccines encoding the envelope protein of West Nile virus lineages 1 or 2 administered intramuscularly, via electroporation and with recombinant virus protein induce partial protection in large falcons (Falco spp.)
Veterinary Research volume 46, Article number: 87 (2015)
As West Nile virus (WNV) can cause lethal diseases in raptors, a vaccination prophylaxis of free-living and captive populations is desirable. In the absence of vaccines approved for birds, equine vaccines have been used in falcons, but full protection against WNV infection was not achieved. Therefore, two DNA vaccines encoding the ectodomain of the envelope protein of WNV lineages 1 and 2, respectively, were evaluated in 28 large falcons. Four different vaccination protocols were used, including electroporation and booster-injections of recombinant WNV domain III protein, before challenge with the live WNV lineage 1 strain NY99. Drug safety, plasmid shedding and antibody production were monitored during the vaccination period. Serological, virological, histological, immunohistochemical and molecular biological investigations were performed during the challenge trials. Antibody response following vaccination was low overall and lasted for a maximum of three weeks. Plasmid shedding was not detected at any time. Viremia, mortality and levels, but not duration, of oral virus shedding were reduced in all of the groups during the challenge trial compared to the non-vaccinated control group. Likewise, clinical scoring, levels of cloacal virus shedding and viral load in organs were significantly reduced in three vaccination groups. Histopathological findings associated with WNV infections (meningo-encephalitis, myocarditis, and arteritis) were present in all groups, but immunohistochemical detection of the viral antigen was reduced. In conclusion, the vaccines can be used safely in falcons to reduce mortality and clinical signs and to lower the risk of virus transmission due to decreased levels of virus shedding and viremia, but full protection was not achieved in all groups.
West Nile virus (WNV) is a arthropod-borne Flavivirus belonging to the Flaviviridae family and the Japanese encephalitis serogroup complex . At least seven different lineages of WNV have been demonstrated by phylogenetic analysis [2,3], with lineages 1 and 2 being of high zoonotic importance . The virus is distributed worldwide, except for Antarctica [1,5] and epidemics in birds caused by linage 1 and 2 have been reported from different regions in Europe [6-8].
Following an enzootic life cycle, WNV is transmitted between arthropods, especially some mosquito species, and a wide range of vertebrates [9,10]. Birds are regarded as important virus reservoirs , whereas humans and mammals (especially horses) represent mainly dead-end hosts, potentially suffering from febrile disease, encephalitis, meningitis, poliomyelitis, and death [4,12,13]. In the latter, viremia may be low, but in reptilian and avian species, viral titers have been demonstrated to be high enough for re-infection of mosquitoes . Therefore, migratory birds play an important role in spreading WNV [15-17].
Besides asymptomatic courses, WNV infections may lead to severe morbidity and mortality in different avian species, especially in raptors, crows and domestic geese [18-27], which seemed to be particularly vulnerable to WNV. In raptors, natural WNV infections have been described in hawks [20,21,28-30], eagles [24-26,31-33], condors  and different falcon species, such as peregrine falcons (Falco peregrinus), gyrfalcons (F. rusticolus), prairie falcons (F. mexicanus), merlins (F. columbarius) and American kestrels (F. sparverius) [27,30]. Experimental WNV infection studies have been performed in single raptor species [27,35-37], demonstrating that falcons can act as amplifying hosts, developing viremia, virus shedding, and subclinical to fatal diseases.
Although WNV constitutes an obvious threat to free-ranging and captive birds of prey in public or private collections, zoos, falconries or commercial breeding centers, a vaccine destined for birds is not available. However, inactivated vaccines and subunit vaccines destined for horses, as well as experimental DNA vaccines, have been used in avian species and evaluated either by the development of neutralizing antibodies [34,38,39] or by experimental WNV challenge [40-51]. Inactivated WNV vaccines and recombinant canary pox vaccines showed limited efficacy in large falcons, especially if administered only twice before an experimental WNV lineage 1 challenge infection . Eventually, a triple application scheme of both vaccines (given at three-weekly-intervals) reduced the clinical signs sufficiently, decreased or even abolished WN-viral RNA shedding and prevented residual viral organ loads three weeks post-challenge. However, full protection against a clinical WNV infection was not always achieved.
DNA WNV vaccines have been used with very promising results in crows [40,41], songbirds , and raptors [34,46]. In American robins (Turdus migratorius), American crows (Corvus brachyrhynchos) and fish crows (Corvus ossifragus), viremia levels were effectively reduced by the intramuscular administration of DNA vaccines. Additionally, in crows, higher survival rates in WNV challenge trials were achieved by vaccination compared to controls. California condors (Gymnogyps californianus) showed neutralizing antibody titers sixty days after vaccination, which have been considered as effective protection against naturally circulating WNV during the 2004 transmission season . In red-tailed hawks (Buteo jamaicensis), the stimulation of antibody development following twofold vaccination was very low (only 21.4% of the vaccinated birds had low titers), but a significant reduction in mean viremia levels was achieved after challenge . However, differences in seroconversion rate and virus shedding were not significant and the absence of morbidity and mortality in the control group during WNV challenge trial limits its validity for clinical protection.
In light of the observed drawbacks of other vaccination strategies in large falcons, we tested a DNA vaccine candidate in combination with different application schemes and confirmed its efficacy by live virus challenge. The vaccine encodes the envelope (E) protein of WNV, the major target for neutralizing antibodies . Our results indicate that protective immune responses are induced upon DNA vaccination. However, the level of protection is strongly dependent on the delivery system, with in-vivo electroporation (EP) being the most successful.
Materials and methods
Animals and viruses
In total, 28 captive-bred, mature (>6 month old) falcons (Falco rusticolus [n = 6]; F. cherrug [n = 1]; F. peregrinus [n = 3]; F. cherrug x F. rusticolus [n = 14]; F. peregrinus x F. rusticolus [n = 6]) originating from one collection were used for this study. All birds were healthy in clinical and endoscopic examination and were dewormed twice (3 week interval) prior to the trial (25 mg/kg fenbendazol orally, Panacur Suspension 2.5% ad us. vet., MSD Animal Health GmbH, Unterschleißheim, Germany and 25 mg/kg toltrazuril orally, Baycox 5% orale Suspension ad us. vet., Bayer Animal Health GmbH, Leverkusen, Germany). ELISA (ID Screen© WN competition ELISA, IDVet, Grabels, France) and the micro-virus neutralization test (VNT) confirmed the absence of pre-existing WNV specific antibodies. Additionally, the absence of Usutu virus specific antibodies was confirmed by VNT using the USUV strain Vienna_2001 (GenBank accession no. AY453411.1).
WNV lineage 1 NY99 (GenBank accession no. AF196835) was propagated and titrated on Vero E6 cells and used for virus challenge according to previous studies [37,51]. Virus identity was verified by sequencing the WNV E protein gene. Challenge virus doses contained 106 Tissue Culture Infection Dose 50 (TCID50) diluted in 1 mL minimal essential medium (MEM) and were injected subcutaneously in the inguinal region.
Construction of WNV DNA vaccine candidates
Two DNA vaccines containing a modified version of the pVax1 vector (Invitrogen, Karlsruhe, Germany) as the backbone were prepared according to Schneeweiss et al. .
The first vaccine (WNV-DNA-1) encoded the E protein ectodomain of WNV lineage 1 strains WNV 2000-crow3356 (GenBank accession no. AF404756.1), which is a close relative to the challenge WNV NY99 strain.
The second vaccine (WNV-DNA-2) encoded the E protein ectodomain of WNV lineage 2 with the sequence of the E protein of WNV strain goshawk Austria 361/10 (2009) (GenBank accession no. HM015884). DNA for intramuscular application was dissolved in 0.9% (w/v) sodium chloride.
All DNA‐preparations used for vaccination in this study were checked for their ability to express the E‐protein via transient transfection assays in cultured cells, as described in Schneeweiss et al.  before being injected into animals (data not shown).
Expression and purification of recombinant WNV proteins
The recombinant domain III of WNV 2000-crow3356 was generated as a fusion protein with the maltose binding protein (MBP), as described by Schneeweiss et al. . The MBP tag was enzymatically removed from domain III by factor X cleavage according to the manufacturers’ instructions (New England Biolabs, USA). Here, 250 μg of protein in 150 μL phosphate buffered saline (PBS) was mixed with 350 μL adjuvant Montanide ISA 70 VG (Seppic, France) (= 500 μL in total) and used for vaccination.
Falcon immunizations and WNV challenge studies
During the time of vaccination, falcons were housed in outdoor hexagonal aviaries with a ground area of 125 m2 and height of 6 m in a commercial breeding center. The area of the center was inspected and approved by the animal welfare (permission no.: 392016/2009) and species conservation authorities (permission no.: AZ 68.337-02/4.2) and approved as an area for genetic engineering (BS003115275-1 dt Az. 40611/5801/501) according to the German Genetic Engineering Act (Gentechnikgesetz, GenTG). Vaccination studies were approved (reference no. 7221.3-1.1.-056/10) on the basis of the EU council directive 86/609/EEC for the protection of animals used for experiments. Vaccines were administered under isoflurane inhalation anesthesia .
Each of the four vaccination groups (A-D) consisted of five randomly selected falcons plus two randomly selected, unvaccinated control falcons (which were merged into a control group E (n = 8) eventually).
Falcons in groups A and B were vaccinated by intramuscular injection (pectoral muscle) with a plasmid (700 μg per dose) encoding the E protein of the WNV lineage 1 (group A) or 2 (group B) and immune responses were boosted once after three weeks post-vaccination (wpv). Falcons in groups C and D received a plasmid (75 μg per dose) encoding WNV E protein lineage 1 by intramuscular injection into the lower leg muscles immediately followed by an in-vivo electroporation (EP) using the electric pulse generator Clinivet (IGEA, Modena, Italy) according to Schneeweiss et al. . For this purpose, feathers were plucked, exposing an area of 3 cm2 around the injection site, and the four-electrode array was placed on the skin to apply the electric pulses (Figure 1). While group C animals were boosted after three weeks in the same way, falcons of group D received two subcutaneous injections of recombinant WNV E protein domain III and ISA 70 adjuvant after two and four weeks. Depending on the assigned vaccination group, the control animals (group E) received injections of sodium chloride, EP and/or adjuvant, respectively, at the same time as the respective vaccinated birds. Each bird was kept under constant observation for 3 h after each treatment. During the seven weeks of the vaccination course, the health status of all falcons was assessed daily and a clinical examination was performed every seven days, including palpation of the vent, auscultation of the lungs and heart, and inspection of nares, pharynx, mucus membranes, feet, skin and muscles at the vaccination sites. Blood samples and swabs from the oropharynx and cloaca were taken weekly for WNV antibody determination by ELISA, VNT  and DNA plasmid detection by PCR, respectively.
After seven (groups A & B) or six weeks (groups C & D), respectively, falcons were transferred to an animal trial unit and challenged under biosafety level 3 conditions with WNV strain 1 NY99. Challenged falcons were examined daily for general condition, posture, plumage, behavior, excrements, neurological status, hydration status, respiration and food uptake . Measurements of body temperature, weight, condition score and hydration status were performed under isoflurane inhalation anesthesia, and samples were taken (blood, pharyngeal and cloacal swabs) on 0, 3, 6, 8, 10, 12, 14 and 19/20/21 days post-infection (dpi) . Clinical findings were documented using a clinical scoring system: a score of 0 referred to a healthy/inconspicuous status, 1 to a mildly affected status, score 2 to a moderately affected status and 3 to a severely affected status. Deceased animals were given a score of 4. Birds were euthanized on 19/20/21 dpi or earlier, when falcons showed seizures, torticollis, somnolence or apathy. Post-mortem examinations were performed on all dead birds, and included the sampling of organs (lung, heart, spleen, kidney, liver, and brain) and subsequent storage of samples in supplemented MEM at −70 °C and in formalin, as described earlier [37,51].
Sera were assayed by ID Screen© WN competition ELISA (IDVet) following the manufacturer’s instructions, with a 40% competition as a cut-off value. Additionally, VNT on Vero cells were conducted using two-fold dilutions (in MEM) and homologous challenge virus (100 TCID50) following the protocol by Seidowski et al. . Cytopathogenic effects were assessed after seven days using formalin-fixation and crystal violet staining, and neutralizing titers were calculated using the Behrens-Kaerber method, as previously described . Similarly, sera were checked for neutralizing antibodies against USUV using the strain Vienna_2001 (GenBank accession no. AY453411.1) for VNT.
Detection of plasmid shedding
During the vaccination period, pharyngeal and cloacal swabs were examined for the presence of WNV plasmid DNA originating from WNV-DNA-1 and WNV-DNA-2. For this purpose, swabs were incubated in PBS and DNAs were extracted using E.Z.N.A Plasmid Mini Kit I (Omega bio-tek, Norcross, GA, USA). Afterwards, 10 μL eluate was examined by PCR using Taq polymerase (NEB, Ipswich, MA, USA) in a Biometra Thermocycler and four different primers (WPN-L1-fwd: 5′-CCTCCCTTGGAGCAGTGCTGGA-3′; WPN-L1-rev: 5′-CCTCCCTTGGAGCAGTGCTGGA-3′; WPN-L2-fwd 5′-TTGTGCATGGCCCGACGACT-3′; WPN-L2-rev: 5′-CCGGCCAGAGCTTGGTGCAAT-3′) with 394 and 379 base pairs, respectively. A detection level of 0.5 pg plasmid was determined per PCR.
Virus isolation and viral genome detection
Virus isolation was performed according to Angenvoort et al.  using serial dilutions of organ homogenate supernatants and bovine serum albumin-1 (BA-1) dilutions for the inoculation of Vero cells. After seven days, cells were formalin-fixed and stained with crystal violet; virus titers were calculated using the Spearman and Kaerber method, as described recently . Viral RNAs were isolated from oral and cloacal swabs, from organ homogenate supernatants using the QIAamp® Viral RNA Kit (Qiagen) and from blood in BA-1 using the RNeasy® Mini Kit (Qiagen) according to the manufacturer’s instructions . In parallel with these samples, an internal control RNA (IC RNA) containing 2 × 105 copies/μL was extracted. Viral RNA and IC RNA were stored at −70 °C for further analysis. Two qRT-PCRs, amplifying the 5′NTR-region or the NS2A-region, respectively, were used for WNV virus detection and quantification as described before . Cycle threshold (Ct) values below 35 were regarded as positive, from 35 to 40 as suspicious and above 40 as negative.
Histological and immunohistochemical examinations
Formalin-fixed tissue samples were embedded in paraffin, cut into 3 μm sections, rehydrated and stained with hematoxylin/eosin (H&E) or by using monoclonal antibodies (mabs) to WNV in immunohistochemistry (IHC). Mab 15R4 (kindly provided by P. Emmerich, Bernhard Nocht Institut, Hamburg, Germany) and mab 3B2 (kindly provided by Davide Lelli, Istituto Zooprofilattico Sperimentale della Lombardia e dell’Emilia Romagna, Brescia, Italy), were diluted in goat serum (1:20 and 1:80, respectively) and the slides were immunostained as described before . Briefly, endogenous peroxidase was blocked using H2O2/methanol for 30 min. As a pretreatment, a Proteinase K digestion for 15 min at 37 °C using a concentration of 4 μg/mL (mab 15R4) and heating with citrate buffer (pH 6.0) for 10 min (mab 3B2) were applied, respectively. The slides were finally developed using Mouse Envision HRP (Dako Diagnostics, Dako Deutschland GmbH, Hamburg, Germany) and diaminobenzidine. Hearts, spleens, brains and the virus injection sites were evaluated and scored for their percentage of positive tissues/cells according to previous studies . Thereby, an organ score of 0 was negative (= no cells affected), 1 was mildly affected (<1% positive cells), 2 was moderately affected (≥1% and <5% positive cells) and 3 was severely affected (≥5% positive cells).
WNV antibodies were compared within and between birds from vaccination and control groups using Fisher’s exact test. The mean duration of illness and clinical scores of all days for each falcon were compared using one-sided Wilcoxon rank sum test with continuity correction. All time points were calculated separately, except 19, 20 and 21 dpi, which were averaged to one terminal time point. For testing the duration of illness, a clinical score of 4 was excluded from the analysis. Each group was compared to the control group separately, whereby p-values below α-levels of 0.05 were classified as significant.
Levels of oral and cloacal virus shedding and of viremia were analyzed using ANOVA including all sampling days. The duration of virus shedding and viremia were evaluated using one-sided Wilcoxon rank sum test with continuity correction and a cut-off Ct value of 35.0. Likewise, this test was used for the analysis of viral organ loads (in heart, spleen, kidney, brain). All statistical tests were performed using R software .
The efficacy of two different WNV DNA vaccines in falcons was determined by a) assessing their tolerance, safety and potency to elicit specific antibody responses and b) by challenging the vaccinated and control birds with a semi-lethal WNV NY99 dose.
Vaccine tolerance and safety
Following vaccination and sampling, behavior, food uptake, movement or general health of the falcons were not affected at any time. The body weight of the vaccinated and control animals varied only slightly between +3.5% and −6.6%. In group B, two birds (F32, F33) developed an edematous/gelatinous texture of pectoral muscle 1 wpv. One falcon in group D demonstrated 0.4 cm × 0.5 cm sized, yellowish, dense skin texture at the vaccination site 1 and 2 weeks after boost vaccination (F56, 5-6 wpv) with recombinant WNV protein. The vaccination sites of all other birds were macroscopically unsuspicious. In none of the oral and fecal swabs from the falcons was WNV plasmid DNA detected at any time.
Vaccination induced antibody responses
Antibody responses are shown in Figures 2 and 3. All control birds (group E) remained negative by ELISA and VNT. In group A, one bird (F25) was ELISA-positive from 5 wpv onwards. At the same time, two other falcons (F29, F30) had low antibody titers of 1:10 by VNT, which lasted for 3 weeks in one bird. All other individuals of this group remained negative in both tests throughout the complete trial.
In group B, one falcon (F31) was ELISA-positive 4 wpv and another falcon (F33) had a low antibody titer of 1:20 5 wpv by VNT. Both individuals were negative at all other time points examined and all of the other birds of this group remained negative throughout the entire vaccination period.
Three falcons in group C (F49, F52, F53) were positive by ELISA from 4 wpv onwards. One of these (F52) and one other falcon (F50) had antibody titers of 1:15 and 1:10 by VNT, respectively, lasting for 1-2 weeks.
None of the birds in group D were positive by ELISA and only two birds (F57, F58) had an antibody titer of 1:15 by VNT 6 wpv.
In groups A and C, but not in groups B and D, Fisher’s exact test demonstrated a significantly increased presence of WNV antibodies compared to group E.
Clinical signs following WNV NY99 challenge
Details on the clinical scores and development of body weights are provided in Figure 4. In the control group E, two of the eight control birds (F55, F27) had to be euthanized 3 dpi and 14 dpi, respectively, due to severe central nervous signs (clinical score 3) such as seizures, torticollis, ataxia and an inability to stand. Two other birds (F42, F51) were found dead on 5 dpi and 8 dpi, respectively, after showing greenish discoloration of urates, enophthalmos, inappetence and ruffled feathers on the previous day. Similar symptoms (clinical scores 2-3) were observed in the four other control birds between 3 dpi and 11 dpi temporarily, but clinical signs ceased afterwards. All control birds dropped their weight from 1.56% to 27.01% (median: 5.75%).
Four falcons of group A had clinical scores equal to or above 2 and two falcons (F26, F29) died on 4 dpi and 8 dpi, respectively. Body weight dropped slightly in the three survivor birds (0.7-7.1%) and decreased rapidly and severely in the two deceased falcons (21.9% and 10.5%, respectively). Median weight loss of all birds in group A was 6.8%.
In group B, two falcons (F31, F33) had clinical scores of 2 on one day and one falcon (F35) had clinical scores of 2 and 3 over several days. No bird died and weight losses ranged from 0.76% to 10.9% (median: 9.6%).
One falcon (F50) of group C had a clinical score of 2 on one day (7 dpi) and another bird (F54) had this score after ten days. However, clinical score in the latter increased to 3 for one day. No falcon died and the weight loss in four birds ranged from 9.1% to 16% (median: 11.6%), whereas in one bird (F54), it was up to 27.1%.
In group D, one falcon (F60) had a clinical score of 2 and one falcon (F59) had a clinical score of 3. The latter animal was euthanized on 18 dpi because of ataxia, hypermetria and weight loss of 30.9%. The other birds in this group dropped weight from 1.5% to 12% (median: 8.7%).
In groups B, C and D, but not in group A, significantly reduced clinical scores were demonstrated by Wilcoxon rank sum test compared to the control group E (p-values 0.01154, 0.02391, 0.04592; for group A 0.1703).
Virus shedding, viremia and antibody response after challenge infection
Oral and cloacal virus shedding data are shown in Figures 5 and 6, virus genome detection in the blood in Figure 7 and virus re-isolation data from blood in Figure 8. Serology results are depicted in Figures 9 and 10.
All birds of the challenge control group (group E) shed WNV orally and in their feces from 3 dpi onwards, with Ct values varying from 17.48 to 34.75. However, in the four surviving control birds (F13, F24, F36, F43), viral genomes were sometimes not detected (F36 at 20 dpi and F13, F24, F43 after 8-14 dpi). Viral genomes were detected in the blood of all falcons from 3 dpi onwards, with Ct values ranging from 19.94 to 34.78. Viremia ceased in most of the survivors on 6-14 dpi (all except F36), while it persisted in the fatally affected falcons until death. Virus was successfully re-isolated and titrated from blood taken on 3 and 6 dpi (yielding titers in the range of 101.75-106.5 TCID 50/mL respectively). First, WNV-specific neutralizing antibodies were detected on 3 dpi (F36, F55) or 6 dpi (F13, F24, F27, F43), respectively, and ranged from 1:10 to 1:80. However, two of the eight falcons which did not survive the WNV challenge did not develop a neutralizing antibody response (F42, F51). In the survivors (F13, F24, F36, F43), the antibody titers increased to a maximum of 1:1280 at the end of the observation period.
In oral and cloacal swabs and in blood taken from birds of group A, viral genomes were only detectable between 3 dpi and 8 dpi. A solitary positive result in one bird (F28, Ct value of 32.82 at 14 dpi), which was negative by qRT-PCR at all other time points, may be due to an artifact. Virus re-isolations from blood were successful in all birds on 3 dpi (101.75-105 TCID 50/mL) and in two birds (F25, F26) also from samples taken at 6 dpi (102.5 and 103.5 TCID50/mL). Antibody titers from 1:15 to 1:320 were detectable in one bird (F30) from 3 dpi and in three birds from 6 dpi onwards, increasing to a maximum of 1:5120 during the trial. However, in the two birds from this group which eventually died, antibody titers remained low (1:40) after challenge (F26) or disappeared (F29) after being low (1:10) before challenge.
In group B, animal viral genomes were detected in pharyngeal swabs up to 10 dpi and in cloacal swabs of two birds (F34, F35) even until 19-21 dpi. Birds were viremic on 3 and 6 dpi, but not at later time points. Virus titers in blood on 3 dpi were 101.75-103 TCID50/mL. Initial antibody titers on 6 dpi ranged from 1:60 to 1:640 and rose to maximum titers of 1:2560 at the end of the study.
In group C, viral genomes were detected in oral and pharyngeal swabs and in blood up to 14 dpi. One bird (F54) shed virus orally until 21 dpi. Blood Ct values were in the range of 21.40 to 34.5. Virus re-isolations were successful from blood samples taken from three birds on 3 dpi (titers 101.75-102.75 TCID50/mL), but not from blood samples taken at later time points. Antibody titers were detected in two falcons (F52 and F53) already by 3 dpi and in all falcons on 6 dpi. One of these falcons (F52) carried already antibodies on 0 dpi as a result of the vaccination. Initially ranging from 1:10 to 1:480, antibody titers increased to maximum titers 1:7680 and lasted until to the end of the study.
In group D, viral genomes were detected in pharyngeal swabs beginning at 3 dpi until the end of the observation period and until 14 dpi in cloacal swabs and blood. Virus re-isolations were successful in two birds (F60, F59) on 3 dpi with 101.83 TCID50/mL and 102.75 TCID50/mL, respectively, and additionally in one of these birds on 6 dpi (102 TCID50/mL). Antibody titers in four birds ranged from 1:10 to 1:20 on 3 dpi; however, antibodies were present on 0 dpi in two of these birds (F57, F58). The titers increased in all birds, up to maximum levels of 1:3840. One bird (F59) with a low neutralizing antibody titer on 6 dpi (1:20), but without a strong humoral response (maximum titers of 1:320), showed neurological signs and apathy and was eventually euthanized on 18 dpi.
ANOVA demonstrated that oral (p values groups A-D: 0.0006594, 0.000002827, 0.00006856, 0.000122) and cloacal (p values groups A, B, D: 0.0005033, 0.0002035, 0.03737; for group C 0.06771) virus shedding and virus detection in blood (p values groups A-D: 0.001057, 0.000000268, 0.0006269, 0.0005634) were significantly reduced in all groups compared to the control group. However, the duration of oral shedding (p values groups A-D: 0.1013, 0.2041, 0.4702, 0.3014) and viremia (p values groups A-D: 0.1566, 0.09665, 0.4108, 0.4108) was not significantly different, as determined by the Wilcoxon rank sum test.
Post mortem examination, histopathology and immunohistochemistry
A summary of the pathological and immunohistochemical findings is provided in Table 1.
The gross-pathology, histopathology and IHC of the non-vaccinated positive controls (group E) were previously described . Briefly, the most consistent finding associated with WNV infection was a non-suppurative (meningo)-encephalitis (4/8) and an acute or subacute, lymphohistiocytic, necrotizing myocarditis (5/8). A moderate, non-suppurative, necrotizing arteritis was seen in the spleen of one bird only (F24). Virus antigens were detected by IHC in brains, hearts and spleens and at injection sites of the fatally diseased animals (4/8), whereas challenge survivors displayed only scant (2/8) or no (2/8) WNV antigen staining.
One falcon (F29) of group A died 4 dpi and showed a severe, acute, hemorrhagic enteritis with positive antigen staining at the injection site, but without other signs typically associated with WNV infections. In all other birds (4/5) a widely distributed, moderate, acute, non-suppurative (meningo)-encephalitis was diagnosed. Additional findings included an acute to subacute, mild, necrotizing myocarditis (2/5), an acute, mild, necrotizing arteritis in the kidney (2/5), a necrosis of the splenic periarteriolar lymphoid sheaths (PALS) of different degrees with fibrin deposition (4/5), a mild lymphoplasmacellular interstitial nephritis (1/5) and a mild lymphohistiocytic neuritis with axonal degeneration (2/5). The vaccination sites were not altered in any bird of this group. By IHC, scattered antigen was detected at the virus injection sites in three birds (3/5) and in the brains of two birds (2/5) (Figure 11), with one of these (F 26) having antigen in all regions of the brain and additionally in the heart.
One falcon in group B (F35) demonstrated only a slight lymphohistiocytic pancreatitis. All other animals (4/5) demonstrated a mild to moderate, widely distributed, acute, non-suppurative meningoencephalitis. Additionally, a mild, acute, necrotizing myocarditis (2/5), a mild, necrotizing arteritis in the gut connective tissue (1/5), a mild lymphohistiocytic hepatitis (1/5) and neuritis (1/5) were seen. The vaccination site of one animal (1/5) displayed a mild lymphohistiocytic myositis. No WNV antigen was detected by IHC in any bird of this group.
Four birds (4/5) of group C had acute, non-suppurative encephalitis of different degrees, varying from slight lesions (1/4) in the cerebellum/cerebrum to moderate and severe inflammation of all brain areas (1/4) and the meninges (2/4). Additional findings included an acute necrotizing myocarditis (2/5), a mild to moderate, acute, necrotizing arteritis (2/5), a mild lymphohistiocytic neuritis (3/5) and nephritis (1/5). At the vaccination sites, follicular aggregated infiltrations of mononuclear cells with mild lymphocytolysis (2/5) and an acute lymphohistiocytic myositis (1/5) were seen. IHC revealed a mild staining reaction in the spleen or brain and heart, respectively, of two falcons (2/5) (Figure 12), whereas all other birds remained negative.
An acute, non-suppurative meningoencephalitis of varying degrees was observed in all birds from group D (5/5). Additional findings included an acute to subacute, mild to moderate, necrotizing myocarditis (3/5), a mild, acute, necrotizing arteritis (1/5), and a mild, acute to subacute, non-suppurative neuritis (4/5) and nephritis (1/5). The vaccination sites had infiltrations of follicular aggregated mononuclear cells in the connective tissues (1/5) and a granulomatous dermatitis (2/5). In IHC, one bird (F59, Figures 11 and 13) was severely affected in cerebrum (15% positive tissue) and mildly affected in cerebellum and diencephalon. However, IHC results in the spleen and brain of two falcons (F58, F60) were inconclusive.
In general, the occurrence of scattered antigen in neurons, glial cells and cell processes of the brain, in cardiocytes and in single monocytes and fibrocytes at the injection site of vaccinated falcons were similar to findings in the control birds.
Virus loads in organs
The results of qRT-PCR and virology from selected organ samples are summarized in Table 2. In the organs of all falcons of group E viral genomes were detected with lowest Ct values of 16.7 (equivalent to 402 895 copies/mg). All organs of the four fatally affected birds (F27, F42, F51, F55) were qRT-PCR positive, as were 2-5 organs of the four challenge survivors (F13, F24, F36, F43). Accordingly, virus re-isolations were possible from organs of the four deceased birds in most cases (101.75-104.75 TCID50/100 μL). In the four survivors virus isolations were successful only from the brain samples of two birds (F13, F43).
In all birds of group A, viral genomes were detected in the brain and also in the kidneys in four birds. Heart, spleen, liver and lung were negative in the three survivors, but positive in two falcons (F26, F29) which died during the study. In the latter two falcons, viruses could be isolated from all organs (except from heart in F29), but only from brain (100.75-105.75 KID50/100 μL) in two other falcons (F25, F30) and from none of the organs in one falcon (F28).
Brains of three falcons (F31, F32, F34) belonging to group B carried viral genomes and the kidney of one falcon (F32) was also qRT-PCR-positive. None of the other birds and none of the organs were positive by qRT-PCR and virus re-isolation failed in all birds.
In group C, qRT-PCR was positive in three birds (F49, F50, F54) in the brain, but not in other organs. Viral genomes were not detected in any other bird and the virology was negative in all birds for all organs.
Viral genomes were detected in the brain in all birds in group D, in one falcon (F57) additionally in the kidneys and in another falcon (F59) additionally in all other organs. In the latter falcon, which had to be euthanized during the trial, virus re-isolation was successful from the brain with a result of 102.75 TCID50/100 μL, whereas it failed in all other birds of this group in all organs.
Wilcoxon rank sum test revealed that the viral genome detections was significantly reduced in all organs of group B animals (p values of brain, spleen, kidney and heart: 0.01767, 0.02228, 0.009749, 0.008443), in the spleen, kidney and heart of group C animals (p values 0.03582, 0.005709, 0.01536; for brain 0.1286), and in the kidneys of group D animals (p value 0.04762), but not in the spleen, heart and brain of group D birds (p values 0.1726, 0.1187, 0.7262). No significant reduction of viral genome detection in organs was present in group A (p values of brain, spleen, kidney, and heart: 0.5476, 0.6532, 0.5476, and 0.5, respectively).
WNV infections can lead to subclinical or severe diseases and mortality in falcons [27,30,35,37,51]. Free-ranging birds play a major role in the spread of WNV over large distances [15-17]. In order to protect raptors, vaccines destined for use in horses have recently been tested in falcons . As these show only sub-optimal efficacy, more vaccine candidates were tested in the present study. For this purpose, WNV DNA vaccines were chosen because they had been used in raptors and other avian species with promising results [34,40,45,46]. However, differences in their efficacy were observed for several avian species . Therefore, a species-specific efficacy study was initiated to determine the rates of clinical protection and the reduction of virus shedding, viral load and virus distribution in large falcons.
In contrast to the WNV DNA vaccine used in previous studies in raptors, which coded for prM and E glycoproteins of WNV , in the present study, two DNA vaccines encoding a secreted version of the E protein ectodomain of WNV lineage 1  (WNV-DNA-1) and 2 (WNV-DNA-2), respectively, were used. Previously, DNA vaccines have been administered intramuscularly into the leg muscles of raptors [34,46]. This administration corresponds to findings in dogs, robins, and crows, where influences of the administration routes on humoral responses were demonstrated. Intramuscular administration induced stronger antibody responses compared to oral or intradermal applications, respectively [40,41,45,57]. However, the pectoral muscle is generally the preferred site for intramuscular drug administration in birds, due to the larger muscle mass and possible rapid drug elimination by a renal portal venous system from the leg muscles. Therefore, the pectoral muscles were preferred for intramuscular injection in the falcons of groups A and B. Moreover, WNV-DNA-1 was administered using EP in two groups (groups C and D) and boosted in the same way (group C) or with recombinant WNV protein subcutaneously (group D) according to successful studies in mice . As EP has only been sparsely reported in avian species  and impairment of heart function by the electric impulses in the adjacent thoracic muscles could not be ruled out, vaccination and EP were applied to the lower leg muscles in these groups.
Overall, the safety and acceptance of both vaccines and the EP were good. There was no alteration in behavior, food uptake, movement or general health condition in any bird. In comparison to previous studies in falcons using a recombinant canarypox vectored WNV vaccine  no remarkable loss of body weight was observed in this study, but there was also local inflammation at the vaccination sites. Two birds in group B developed an edematous/gelatinous texture of pectoral muscle which disappeared after two weeks and could not be confirmed at necropsy. Moreover, mild, non-suppurative myositis and follicular aggregates were seen at the vaccination sites of single birds in groups B, C and D. Two falcons of group D developed a moderate to severe granulomatous dermatitis. Taken together, most alterations were confined to groups which were vaccinated twice and electroporated. Therefore, a reaction to the extended vaccination scheme was suspected, possibly caused by hypersensitivity reactions to the vaccine, the adjuvant or the recombinant protein.
A possible shedding of the WNV vaccine plasmid by immunized birds was investigated by taking cloacal and pharyngeal swabs from all falcons on a weekly basis (data not displayed). The fact that WNV DNA plasmid was not found in any of these swabs highlights the environmental safety of these DNA plasmid vaccines used.
Elicited antibody titers were low in all four vaccination groups and lasted for a maximum of 3 weeks in single individuals. Moreover, many vaccinated birds failed to produce detectable antibody levels, or titers were detectable on single days only but not repeatedly over weeks. These results contrast strongly with DNA vaccination reports in California and Andean condors, where all birds demonstrated increased neutralizing antibody levels in plaque-reduction test 4 wpv . It also lags behind other DNA vaccination studies, where in 15/19 American crows and in 6/9 fish crows, neutralizing antibodies were demonstrated [40,41]. Moreover, antibody levels were low compared to previous studies in large falcons, using formalin-inactivated WNV vaccines and recombinant canarypox live WNV vaccines . However, similar differences have been shown in four penguin species, where higher antibody levels were induced by an inactivated vaccine compared to a DNA vaccine . Low antibody titers had also been reported in red tailed hawks, where only 3/14 birds developed low titers (maximum titers 1:10) 4 wpv following DNA vaccination . Moreover, in 3/3 American robins, no detectable antibody levels have been measured 2 wpv . Thereby, species-specific differences may play a role in humoral response, as previously discussed .
To solve the problem of low immunogenicity of DNA vaccines, strategies such as in-vivo EP have been developed which result in a significant increase in humoral and cellular immune responses . However, antibody responses were not markedly stronger using this approach in the present study. A likely explanation is that DNA vaccination in falcons mainly enhances cellular and/or innate immune mechanisms, as suggested for other species [39,41,52,58,60,61] This might explain the higher survival rates, the lower oral virus shedding and the lower viral organ load in groups C and D compared to group A.
Besides EP, antibody levels were recently further stimulated using recombinant protein DIII in mice . However, this failed in falcons of group D compared to falcons of groups A and C in this study. This might be explained by a possible lower efficacy of the adjuvant ISA 70 in falcons compared to oligonucleotides (ODN 1826), which have been used in the mice . The importance of the adjuvant has been shown in geese, where ISA720 induced significantly higher antibody titers compared to vaccination of the subunit protein antigen without this adjuvant . In contrast, in crows, the adjuvant did not significantly affect the performance of the DNA vaccine .
Antibody responses to virus challenge were poor in the deceased or euthanized birds but were good in the surviving control birds. In the vaccinated birds, titers raised from 3 dpi onwards in group B, and even higher in EP groups C and D. Therefore, the first antibodies in vaccinated falcons were demonstrated three days earlier compared to the first antibody detection in 4/8 control birds and unvaccinated large falcons from a previous WNV infection trial . In a study in geese, a humoral response by vaccinated birds was demonstrated by antibodies from day six onwards following live virus challenge . Similar high seroconversion rates following DNA vaccination and challenge have been reported in red-tailed hawks  and crows ; however, in the hawks, seroconversion occurred in 11/14 vaccinated birds only after challenge, underlining the importance of live virus challenge in vaccine evaluation and assessment of clinical protection.
Passage of the challenge virus on Vero E6 cells may have attenuated the virus. However, virus attenuation is very unlikely, as the virus in the present study was taken as an aliquot from the same virus stock and was therefore identical to the WNV which had been used successfully in two previous infectious trials [37,51]. Moreover, similar to the non-vaccinated falcons in previous studies [37,51], the control animals in the present trial demonstrated clinical signs, viremia, virus shedding, organic virus accumulation, and pathological alterations associated to WNV infection.
There are indications that the occurrence of natural WNV infections in captive and free-ranging peregrine falcons is lower than that in gyrfalcons and gyr-hybrid-falcons, despite the opportunity for exposure. Therefore, the use of different falcon species and their hybrids might have limited the evaluation of results. However, there is no valid proof available that susceptibility to WNV varies between falcon species, as this had been stated for other viruses . Moreover, the phylogenetic relationship between most of the falcon species used is so close [63-65] that differences in the immunological reaction to vaccines and virus challenge are unlikely. Accordingly, the results of the present study do not point towards any species susceptibility; however, certain host variability should be taken into account when interpreting results as it is known from other studies using non-standard laboratory animals .
In groups B, C, and D, clinical scores were significantly reduced and survival rates increased compared to the control group, while the survival rate of group A was low (60%). One of the two deceased falcons in group A died, most likely due to hemorrhagic enteritis, but demonstrated no signs typical for a WNV-associated disease in pathology, histopathology and IHC. It is possible that the incubation time of about 4 dpi was too short to develop clear signs of disease. A second falcon in group A and one falcon in group D had to be euthanized before the end of the trial. Interestingly, both animals demonstrated distinct amounts of antigen in the brain and/or heart by IHC, even without pathological alterations. All other vaccinated falcons (17/20) survived the challenge trial without or with mild clinical signs (n = 9), showing moderate to severe signs (clinical score ≥2) temporarily on single days (n = 4) or on 4-12 days (n = 4), respectively. However, in this study, the rate of survivors in groups A and D, but not in groups B and C, is lower compared to robins, where 3/3 vaccinated birds survived a challenge with WNV isolate WN02 for two weeks . Similarly, 9/9 fish crows , 14/14 vaccinated red-tail hawks , and 44/44 geese  were protected from lethal WNV infection; however, in all of these studies, all control and mock birds also survived to the end of the infectious trial. Therefore, evaluation of the true benefits of vaccination in these studies is limited. In addition, the study of viral dissemination or pathological examinations were far less complete in those studies. This was not the case in the present study, where only 50% of the non-vaccinated control falcons survived virus challenge, suffering temporarily from moderate to severe clinical signs. Whether species-specific differences, higher virus infection doses in the present study or a different pathogenicity of the WNV challenge strains used is responsible for this remains unclear, but it highlights the fact that previous studies in other avian species are not directly comparable to the present study.
Independently of the vaccination scheme, almost all animals revealed clear histopathological signs of a mild to severe, non-suppurative (meningo-)encephalitis, which was even accompanied by a mild to moderate, non-suppurative myocarditis and/or arteritis in several falcons. Thereby, vaccination WNV-DNA-1 and WNV-DNA-2 did not prevent the development of pathological lesions; however, individual variability among the birds was high. Besides lesions which are typically associated with WNV infections, several vaccinated and non-vaccinated falcons revealed lymphohistiocytic infiltrations in different tissues. Interestingly, only in three of the surviving birds the WNV antigen was detected in brain, myocardium or spleen, suggesting an early clearance of viral antigen during the progress of disease, as discussed before .
In accordance with previous studies in falcons, viremia levels and virus shedding were high in non-vaccinated control falcons, especially if birds died or had to be euthanized during the trial . In comparison, the levels but not the duration of oral and cloacal (except group C) virus shedding and viremia were significantly reduced in all vaccination groups. However, in the three surviving control birds, viral genome detection was also negative for single days or after 8-14 dpi, respectively. In most falcons, virus shedding extended beyond the viremic period, which has also been reported from other raptor species [46,67]. The reduction of viremia levels is in accordance with other studies. In DNA-vaccinated geese, the virus was absent from the blood; however, oral shedding occurred on 3-6 dpi, suggesting virus replication and the absence of sterile immunity . In absence of mortality in the cited study, viremia during challenge has been used as a surrogate for mortality as known from different animal models for flaviviral diseases [43,68]. In robins  and fish-crows , the viremia level was decreased below the infectious level of mosquitoes, which has been reported to be 105 PFU/mL blood . However, this failed in crows, where viremia levels were decreased from 1010 only to 105 PFU/mL blood . In accordance to previous reports, the results of this study suggest a reduction of the transmission risk through blood sucking mosquitoes from vaccinated birds.
High viral organ loads have been reported in falcons infected with WNV lineages 1 and 2 previously , and correspond to findings in the deceased birds of the present study. Compared to the control group, viral load was significantly reduced in most or all organs in groups B and C and in single organs in group D, but not in group A. Similar to 2/4 surviving control birds in group E, virus genome detection was successful from the brain of all birds in group A. Moreover, in birds of group A, the viral genome was detected in kidney, heart, spleen, liver and lung of some falcons, especially in deceased animals. In contrast, the number of falcons with positive virus detection in the brain was reduced in groups B (n = 3) and C (n = 3), but not in group D (n = 5), and positive virus detection from other organs occurred only in one bird of group B and two birds of group D, but not in group C. This reduction of viral organ load corresponds to previous studies in falcons, where inactivated and recombinant vaccines decreased the viral organ load significantly .
In conclusion, the WNV DNA vaccines used in this study induced partial protection against WNV associated diseases and, depending on the route of administration, full protection from death. Interestingly, WNV-DNA-2 provided cross-protection against the WNV lineage 1 strain NY99. A similar cross-protection between different WNV lineages has been reported in horses and mouse studies . Even if sterile immunity was not achieved, in many cases virus shedding, viremia and viral loads in organs were significantly decreased, reducing the risk of disease transmission from vaccinated birds. Although almost all animals developed signs of disease, the survival rate was higher compared to controls. From the practical point of view, the results of WNV-DNA-2, which was injected IM, are promising regarding the attenuation of virus shedding and viremia. Also, EP of DNA led to 100% survival of falcons; however, the set-up and availability of machines for in-vivo EP generally currently limit the extensive use of this technology for DNA-vaccines .
Campbell GL, Marfin AA, Lanciotti RS, Gubler DJ (2002) West Nile virus. Lancet Infect Dis 2:519–529
Bondre VP, Jadi RS, Mishra AC, Yergolkar PN, Arankalle VA (2007) West Nile virus isolates from India: evidence for a distinct genetic lineage. J Gen Virol 88:875–884
Mackenzie JS, Williams DT (2009) The zoonotic flaviviruses of Southern, South-Eastern and Eastern Asia, and Australasia: the potential for emergent viruses. Zoonoses Public Health 56:338–356
Kramer LD, Li J, Shi P-Y (2007) West Nile virus. Lancet Neurol 6:171–181
Kramer LD, Styer LM, Ebel GD (2008) A global perspective on the epidemiology of West Nile virus. Annu Rev Entomol 53:61–81
Calistri P, Giovannini A, Hubalek Z, Ionescu A, Monaco F, Savini G, Lelli R (2010) Epidemiology of West Nile in Europe and in the Mediterranean Basin. Open Virol J 4:29–37
Papa A (2013) West Nile virus infections in humans - focus on Greece. J Clin Virol 58:351–353
Weissenböck H, Hubálek Z, Bakonyi T, Nowotny N (2010) Zoonotic mosquito-borne flaviviruses: worldwide presence of agents with proven pathogenicity and potential candidates of future emerging diseases. Vet Microbiol 140:271–280
Marra PP, Griffing S, Caffrey C, Kilpatrick AM, McLean R, Brand C, Saito EMI, Dupuis AP, Kramer L, Novak R (2004) West Nile virus and wildlife. Bioscience 54:393–402
van der Meulen KM, Pensaert MB, Nauwynck HJ (2005) West Nile virus in the vertebrate world. Arch Virol 150:637–657
McLean RG, Ubico SR, Docherty DE, Hansen WR, Sileo L, McNamara TS (2001) West Nile virus transmission and ecology in birds. Ann N Y Acad Sci 951:54–57
Smithburn KC, Hughes TP, Burke AW, Paul JH (1940) A neurotropic virus isolated from the blood of a native of Uganda. Am J Trop Med Hyg 20:471–492
Bagnarelli P, Marinelli K, Trotta D, Monachetti A, Tavio M, Del Gobbo R, Capobianchi M, Menzo S, Nicoletti L, Magurano F, Varaldo P (2011) Human case of autochthonous West Nile virus lineage 2 infection in Italy, September 2011. Euro Surveill 16:20002
Klenk K, Snow J, Morgan K, Bowen R, Stephens M, Foster F, Gordy P, Beckett S, Komar N, Gubler D, Bunning M (2004) Alligators as West Nile virus amplifiers. Emerg Infect Dis 10:2150–2155
Malkinson M, Banet C (2002) The role of birds in the ecology of West Nile virus in Europe and Africa. Curr. Top. Microbiol Immunol 267:309–322
Peterson AT, Vieglais DA, Andreasen JK (2003) Migratory birds modeled as critical transport agents for West Nile virus in North America. Vector Borne Zoonotic Dis 3:27–37
Rappole JH, Derrickson SR, Hubalek Z (2000) Migratory birds and spread of West Nile virus in the Western Hemisphere. Emerg Infect Dis 6:319–328
Austin RJ, Whiting TL, Anderson RA, Drebot MA (2004) An outbreak of West Nile virus-associated disease in domestic geese (Anser anser domesticus) upon initial introduction to a geographic region, with evidence of bird to bird transmission. Can Vet J 45:117–123
Bin H, Grossman Z, Pokamunski S, Malkinson M, Weiss L, Duvdevani P, Banet C, Weisman Y, Annis E, Gandaku D, Yahalom V, Hindyieh M, Shulman L, Mendelson E (2001) West Nile fever in Israel 1999–2000. Ann N Y Acad Sci 951:127–142
Ellis AE, Mead DG, Allison AB, Stallknecht DE, Howerth EW (2007) Pathology and epidemiology of natural West Nile viral infection of raptors in Georgia. J Wildl Dis 43:214–223
Erdelyi K, Ursu K, Ferenczi E, Szeredi L, Ratz F, Skare J, Bakonyi T (2007) Clinical and pathologic features of lineage 2 West Nile virus infections in birds of prey in Hungary. Vector Borne Zoonotic Dis 7:181–188
Fitzgerald SD, Patterson JS, Kiupel M, Simmons HA, Grimes SD, Sarver CF, Fulton RM, Steficek BA, Cooley TM, Massey JP, Sikarskie JG (2003) Clinical and pathologic features of West Nile virus infection in native North American owls (family strigidae). Avian Dis 47:602–610
Gancz AY, Smith DA, Barker IK, Lindsay R, Hunter B (2006) Pathology and tissue distribution of West Nile virus in North American owls (family strigidae). Avian Pathol 35:17–29
Hofle U, Blanco JM, Crespo E, Naranjo V, Jimenez-Clavero MA, Sanchez A, de la Fuente J, Gortazar C (2008) West Nile virus in the endangered Spanish imperial eagle. Vet Microbiol 129:171–178
Ip HS, Van Wettere AJ, McFarlane L, Shearn-Bochsler V, Dickson SL, Baker J, Hatch G, Cavender K, Long R, Bodenstein B (2014) West Nile virus transmission in winter: the 2013 Great Salt Lake bald eagle and eared grebes mortality event. PLoS Curr 6:ecurrents.outbreaks.b0f031fc8db2a827d9da0f30f0766871
Jimenez-Clavero MA, Sotelo E, Fernandez-Pinero J, Llorente F, Blanco JM, Rodriguez-Ramos J, Perez-Ramirez E, Hofle U (2008) West Nile virus in golden eagles, Spain, 2007. Emerg Infect Dis 14:1489–1491
Nemeth N, Gould D, Bowen R, Komar N (2006) Natural and experimental West Nile virus infection in five raptor species. J Wildl Dis 42:1–13
Wunschmann A, Shivers J, Bender J, Carroll L, Fuller S, Saggese M, van Wettere A, Redig P (2004) Pathologic findings in red-tailed hawks (Buteo jamaicensis) and Cooper’s hawks (Accipiter cooper) naturally infected with West Nile virus. Avian Dis 48:570–580
Wunschmann A, Shivers J, Bender J, Carroll L, Fuller S, Saggese M, van Wettere A, Redig P (2005) Pathologic and immunohistochemical findings in goshawks (Accipiter gentilis) and great horned owls (Bubo virginianus) naturally infected with West Nile virus. Avian Dis 49:252–259
Wodak E, Richter S, Bago Z, Revilla-Fernandez S, Weissenbock H, Nowotny N, Winter P (2011) Detection and molecular analysis of West Nile virus infections in birds of prey in the eastern part of Austria in 2008 and 2009. Vet Microbiol 149:358–366
Steele KE, Linn MJ, Schoepp RJ, Komar N, Geisbert TW, Manduca RM, Calle PP, Raphael BL, Clippinger TL, Larsen T, Smith J, Lanciotti RS, Panella NA, McNamara TS (2000) Pathology of fatal West Nile virus infections in native and exotic birds during the 1999 outbreak in New York City, New York. Vet Pathol 37:208–224
D’Agostino JJ, Isaza R (2004) Clinical signs and results of specific diagnostic testing among captive birds housed at zoological institutions and infected with West Nile virus. J Am Vet Med Assoc 224:1640–1643
Wunschmann A, Timurkaan N, Armien AG, Bueno Padilla I, Glaser A, Redig PT (2014) Clinical, pathological, and immunohistochemical findings in bald eagles (Haliaeetus leucocephalus) and golden eagles (Aquila chrysaetos) naturally infected with West Nile virus. J Vet Diagn Invest 26:599–609
Chang GJ, Davis BS, Stringfield C, Lutz C (2007) Prospective immunization of the endangered California condors (Gymnogyps californianus) protects this species from lethal West Nile virus infection. Vaccine 25:2325–2330
Busquets N, Bertran K, Costa TP, Rivas R, de la Fuente JG, Villalba R, Solanes D, Bensaid A, Majo N, Pages N (2012) Experimental West Nile virus infection in Gyr-Saker hybrid falcons. Vector Borne Zoonotic Dis 12:482–489
Komar N, Langevin S, Hinten S, Nemeth N, Edwards E, Hettler D, Davis B, Bowen R, Bunning M (2003) Experimental infection of North American birds with the New York 1999 strain of West Nile virus. Emerg Infect Dis 9:311–322
Ziegler U, Angenvoort J, Fischer D, Fast C, Eiden M, Rodriguez AV, Revilla-Fernandez S, Nowotny N, de la Fuente JG, Lierz M, Groschup MH (2013) Pathogenesis of West Nile virus lineage 1 and 2 in experimentally infected large falcons. Vet Microbiol 161:263–273
Okeson DM, Llizo SY, Miller CL, Glaser AL (2007) Antibody response of five bird species after vaccination with a killed West Nile virus vaccine. J Zoo Wildl Med 38:240–244
Davis MR, Langan JN, Johnson YJ, Ritchie BW, Van Bonn W (2008) West Nile virus seroconversion in penguins after vaccination with a killed virus vaccine or a DNA vaccine. J Zoo Wildl Med 39:582–589
Turell MJ, Bunning M, Ludwig GV, Ortman B, Chang J, Speaker T, Spielman A, McLean R, Komar N, Gates R, McNamara T, Creekmore T, Farley L, Mitchell CJ (2003) DNA vaccine for West Nile virus infection in fish crows (Corvus ossifragus). Emerg Infect Dis 9:1077–1081
Bunning ML, Fox PE, Bowen RA, Komar N, Chang GJ, Speaker TJ, Stephens MR, Nemeth N, Panella NA, Langevin SA, Gordy P, Teehee M, Bright PR, Turell MJ (2007) DNA vaccination of the American crow (Corvus brachyrhynchos) provides partial protection against lethal challenge with West Nile virus. Avian Dis 51:573–577
Samina I, Havenga M, Koudstaal W, Khinich Y, Koldijk M, Malkinson M, Simanov M, Perl S, Gijsbers L, Weverling GJ, Uytdehaag F, Goudsmit J (2007) Safety and efficacy in geese of a PER.C6-based inactivated West Nile virus vaccine. Vaccine 25:8338–8345
Jarvi SI, Lieberman MM, Hofmeister E, Nerurkar VR, Wong T, Weeks-Levy C (2008) Protective efficacy of a recombinant subunit West Nile virus vaccine in domestic geese (Anser anser). Vaccine 26:5338–5344
Fassbinder-Orth CA, Hofmeister EK, Weeks-Levy C, Karasov WH (2009) Oral and parenteral immunization of chickens (Gallus gallus) against West Nile virus with recombinant envelope protein. Avian Dis 53:502–509
Kilpatrick AM, Dupuis AP, Chang GJ, Kramer LD (2010) DNA vaccination of American robins (Turdus migratorius) against West Nile virus. Vector Borne Zoonotic Dis 10:377–380
Redig PT, Tully TN, Ritchie BW, Roy AF, Baudena MA, Chang GJ (2011) Effect of West Nile virus DNA-plasmid vaccination on response to live virus challenge in red-tailed hawks (Buteo jamaicensis). Am J Vet Res 72:1065–1070
Wheeler SS, Langevin S, Woods L, Carroll BD, Vickers W, Morrison SA, Chang GJ, Reisen WK, Boyce WM (2011) Efficacy of three vaccines in protecting Western scrub-jays (Aphelocoma californica) from experimental infection with West Nile virus: implications for vaccination of island scrub-jays (Aphelocoma insularis). Vector Borne Zoonotic Dis 11:1069–1080
Samina I, Khinich Y, Simanov M, Malkinson M (2005) An inactivated West Nile virus vaccine for domestic geese-efficacy study and a summary of 4 years of field application. Vaccine 23:4955–4958
Sá e Silva M, Ellis A, Karaca K, Minke J, Nordgren R, Wu S, Swayne DE (2013) Domestic goose as a model for West Nile virus vaccine efficacy. Vaccine 31:1045–1050
Olsen GH, Miller KJ, Docherty DE, Bochsler VS, Sileo L (2009) Pathogenicity of West Nile virus and response to vaccination in sandhill cranes (Grus canadensis) using a killed vaccine. J Zoo Wildl Med 40:263–271
Angenvoort J, Fischer D, Fast C, Ziegler U, Eiden M, Garcia de la Fuente J, Lierz M, Groschup MH (2014) Limited efficacy of West Nile virus vaccines in large falcons (Falco spp.). Vet Res 45:41
Schneeweiss A, Chabierski S, Salomo M, Delaroque N, Al-Robaiy S, Grunwald T, Bürki K, Liebert UG, Ulbert S (2011) A DNA vaccine encoding the E protein of West Nile virus is protective and can be boosted by recombinant domain DIII. Vaccine 29:6352–6357
Lierz M, Korbel R (2012) Anesthesia and analgesia in birds. J Exot Pet Med 21:44–58
Seidowski D, Ziegler U, von Ronn JA, Muller K, Huppop K, Muller T, Freuling C, Muhle RU, Nowotny N, Ulrich RG, Niedrig M, Groschup MH (2010) West Nile virus monitoring of migratory and resident birds in Germany. Vector Borne Zoonotic Dis 10:639–647
Eiden M, Vina-Rodriguez A, Hoffmann B, Ziegler U, Groschup MH (2010) Two new real-time quantitative reverse transcription polymerase chain reaction assays with unique target sites for the specific and sensitive detection of lineages 1 and 2 West Nile virus strains. J Vet Diagn Invest 22:748–753
Development Core Team R (2011) R: A Language and Environment for Statistical Computing. R Foundation for Statistical Computing, Vienna, Austria
Osorio JE, Tomlinson CC, Frank RS, Haanes EJ, Rushlow K, Haynes JR, Stinchcomb DT (1999) Immunization of dogs and cats with a DNA vaccine against rabies virus. Vaccine 17:1109–1116
Khawaja G, Buronfosse T, Jamard C, Guerret S, Zoulim F, Luxembourg A, Hannaman D, Evans C, Hartmann D, Cova L (2012) Enhanced magnitude and breadth of neutralizing humoral response to a DNA vaccine targeting the DHBV envelope protein delivered by in vivo electroporation. Virology 425:61–69
Li L, Saade F, Petrovsky N (2012) The future of human DNA vaccines. J Biotechnol 162:171–182
Kim S, Li L, McMurtrey CP, Hildebrand WH, Weidanz JA, Gillanders WE, Diamond MS, Hansen TH (2010) Single-chain HLA-A2 MHC trimers that incorporate an immundominant peptide elicit protective T cell immunity against lethal West Nile virus infection. J Immunol 184:4423–4430
Shrestha B, Ng T, Chu H-J, Noll M, Diamond MS (2008) The relative contribution of antibody and CD8+ T cells to vaccine immunity against West Nile encephalitis virus. Vaccine 26:2020–2033
Oaks JL, Schrenzel M, Rideout B, Sandfort C (2005) Isolation and epidemiology of falcon adenovirus. J Clin Microbiol 43:3414–3420
Nittinger F, Gamauf A, Pinsker W, Wink M, Haring E (2007) Phylogeography and population structure of the saker falcon (Falco cherrug) and the influence of hybridization: mitochondrial and microsatellite data. Mol Ecol 16:1497–1517
Nittinger F, Haring E, Pinsker W, Wink M, Gamauf A (2005) Out of Africa? Phylogenetic relationships between Falco biarmicus and the other hierofalcons (aves: falconidae). J Zoolog Syst Evol Res 43:321–331
Wink M, Sauer-Guerth H, Ellis D, Kenward R (2004) Phylogenetic Relationships in the Hierofalco Complex (saker-, gyr-, lanner-, lagger falcon). In: Chancellor R, Meyburg B (eds) Raptors Worldwide. WWGBP/MME, Budapest, Berlin, pp 499–504
Pérez-Ramírez E, Llorente F, Jiménez-Clavero MÁ (2014) Experimental infections of wild birds with West Nile virus. Viruses 6:752–781
Nemeth NM, Hahn DC, Gould DH, Bowen RA (2006) Experimental West Nile virus infection in Eastern screech owls (Megascops asio). Avian Dis 50:252–258
Siger L, Bowen RA, Karaca K, Murray MJ, Gordy PW, Loosmore SM, Audonnet JC, Nordgren RM, Minke JM (2004) Assessment of the efficacy of a single dose of a recombinant vaccine against West Nile virus in response to natural challenge with West Nile virus-infected mosquitoes in horses. Am J Vet Res 65:1459–1462
Turell MJ, O’Guinn ML, Dohm DJ, Jones JW (2001) Vector competence of North American mosquitoes (diptera: culicidae) for West Nile virus. J Med Entomol 38:130–134
Magnusson SE, Karlsson KH, Reimer JM, Corbach-Söhle S, Patel S, Richner JM, Nowotny N, Barzon L, Bengtsson KL, Ulbert S, Diamond MS, Stertman L (2014) Matrix-M™ adjuvanted envelope protein vaccine protects against lethal lineage 1 and 2 West Nile virus infection in mice. Vaccine 32:800–808
This work was funded in part by the EU commission (projects NADIR and EDENext). The German National Academic Foundation funded a scholarship for DF. Roc Falcon S.L., Spain generously provided the falcons for the animal experiment.
The authors declare that they have no competing interests.
The study was designed by ML, UZ and MHG with additional inputs from DF, JA and SU. SC and SU prepared the vaccines and measured plasmid excretion. DF and KM vaccinated, sampled and examined the birds at the breeding center with assistance from SU. JA, DF, UZ, CF and ME carried out the experiments. The results were analyzed by JA, UZ, DF, ML and MHG and the manuscript was written and corrected by DF, JA, CF, KM, UZ, SU, MHG and ML. All authors read and approved the final manuscript.
Dominik Fischer and Joke Angenvoort contributed equally to this work.
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Fischer, D., Angenvoort, J., Ziegler, U. et al. DNA vaccines encoding the envelope protein of West Nile virus lineages 1 or 2 administered intramuscularly, via electroporation and with recombinant virus protein induce partial protection in large falcons (Falco spp.). Vet Res 46, 87 (2015). https://doi.org/10.1186/s13567-015-0220-1
- West Nile Virus
- West Nile Virus Infection
- Cloacal Swab
- West Nile Virus Strain
- Necrotizing Arteritis