Comparative histopathological and immunological study of two field strains of chicken anemia virus
© Rimondi et al.; licensee BioMed Central Ltd. 2014
Received: 28 May 2014
Accepted: 24 September 2014
Published: 8 October 2014
Infection of poultry with chicken anemia virus (CAV) is implicated in several field problems in broiler flocks due to the immunosuppression generated and, consequently, the increased susceptibility to secondary infections. Recently, we have reported an increased occurrence of clinical cases caused by CAV strains distantly related to those commonly used for vaccination. In order to understand the behavior of two Argentinean CAV strains (CAV-10 and CAV-18) in two-week-old chickens, an immune and histopathological study was performed. Neither mortality nor clinical signs were observed in the infected or control groups. Thymus lobes from chickens infected with both CAV viruses were smaller compared to the negative control group. At 14 days post-infection (dpi), only chickens inoculated with CAV-10 show a severe depletion of lymphocytes in the thymus cortex and in follicles from the bursa of Fabricius. Also thymopoiesis disorders, such as reduction in the percentage of total DP (CD4 + CD8α+) thymocytes and alteration in the percentages of DP subpopulations, were more important in animals inoculated with the CAV-10 than the CAV-18 strain. In addition, only animals infected with CAV-10 show a decrease in CD8αβ splenocytes. Altogether our results show that, although both Argentinean CAV strains produce subclinical infections in chickens causing immunosuppression at 14 dpi, they might differ in their in vivo pathogenicity.
Chicken anemia virus (CAV) is a closed circular negative single-stranded DNA virus  from the Circoviridae family that belongs to the Gyrovirus genus . The virus genome encodes a polycistronic mRNA from which three viral proteins are translated ,: ORF1 encodes VP1, the only capsid protein; ORF2 encodes VP2, a scaffold protein which allows the proper folding of VP1 ,; and ORF3 encodes VP3, which is known as an apoptin that induces apoptosis of thymocytes after in vivo infection and apoptosis of transformed avian cell lines after in vitro infection ,.
Worldwide, CAV causes considerable economic losses in the poultry industry because it is responsible for a clinical disease with high mortality characterized by anemia, haemorrhages and atrophy of the thymus and bone marrow in young chicks . Infection of chickens older than two weeks of age, although considered subclinical, also has immunosuppressive effects with important consequences on growth and profitability of poultry -. Markowsky-Grimsrud and Schat  have demonstrated that experimental infection with CAV also impairs the generation of pathogen-specific cytotoxic T lymphocytes (CTL) that may have important implications for adaptive cell-mediated immunity to several secondary pathogens. This was also observed by other authors that reported secondary infections with other viruses, bacteria, parasites and/or fungi ,-.
Experimental infection of chickens with CAV induced a substantial but transient decrease in some immunological parameters corresponding to a generalized lymphocytopenia in the thymus, bursa and spleen -, with a peak at 14 days post-inoculation (dpi) and complete recovery at 28 dpi. These observations were observed in 1 or 14-day-old inoculated chickens ,. While there is a consensus on the idea that absolute numbers of thymic lymphocytes dramatically decrease during the period of transient leukopenia -, the selective alterations in the percentages of T lymphocyte subpopulations in the spleen during the acute phase is still under discussion. Coud et al.  showed a greater depletion of CTL than T-helper lymphocytes (ThL) in the spleen at 14 dpi, while Hu et al.  showed no selective decrease of ThL or CTL by flow cytometric analysis of CD4+ and CD8+ subpopulations. On the contrary, Vaziry et al.  showed a reduction in the percentage of CD4+ splenocytes only at 7 and 28 dpv, with a simultaneous increase in the percentages of CD8+ cells. It is noteworthy that most experimental infections with CAV have been done with reference strains such as CIA-1 or Cux-1 -; therefore, knowledge of the pathogenicity of CAV field strains remains poor and needs to be studied more.
In 2009, our group reported the circulation of CAV affecting both broilers and layers in commercial flocks in Argentina . Sequence analysis of predicted VP1 peptides showed that most of the Argentinean viruses have a glutamine residue at positions 139 and 144, suggesting that these viruses might have a reduced spread in an avian lymphoblastoid cell line (MDCC-MSB1) compared with Cux-1 . We showed that the circulation of CAV in commercial poultry in Argentina clearly affect their immune status through a subclinical infection . Therefore, it would be important to broaden and deepen our knowledge about the effect of subclinical experimental infections with Argentinean CAV strains in chickens, moreover considering the high frequency of clinical cases and despite the fact that vaccination against CAV is common in breeder flocks in Argentina.
The present study addresses the effect of subclinical infection with two Argentinean CAV strains at 14 dpi. We studied the percentage of T-lymphocyte subpopulations in the thymus and spleen, and the histopathological changes produced in the thymus and bursa of Fabricius by both viruses. In addition, this paper contains the first two complete genome sequences of CAV published from Argentinean field strains and the first report of the behaviour of these viruses in vivo.
Materials and methods
Amplification and sequencing of the CAV genome
Sequences of the primers used to obtain the complete genome sequence of CAV strains
PCR products were purified with a QIAquick PCR purification kit (Qiagen) and sequencing was performed using the BigDye Terminator v3.1 Cycle Sequencing Kit on an ABI PRISM 3700 DNA Analyzer (Applied Biosystems) according to the manufacturer’s instructions. Sequences were carried out with the same amplification primers and internal primers CAV1, CAV2, CAV-VP1-A fw, CAV-VP1-A rev, CAV-VP1-B fw and CAV-VP1-B rev previously described ,. Six new additional internal primers were designed to obtain the complete CAV genome through overlapping fragments: CAV-Genome Fw, CAV-Genome Rv, CAV-VP2 Fw, CAV-VP3 Rv, CAV-Sec1 Rv and CAV-Sec4 Fw (Table 1).
The consensus amino acid and nucleotide sequences for both CAV genomes were generated using Megalign (DNASTAR, Madison, WI, USA). Sequences were assembled and edited with Lasergene 8.1 (DNASTAR); BioEdit 7 was used for alignment and residue analysis.
Chickens and housing
Specific-pathogen-free (SPF) White Leghorn embryonated eggs free of CAV antibodies were purchased (Rosenbusch S.A. CABA, Argentina), incubated and hatched in an automatic incubator (Yonar, CABA, Argentina) under appropriate conditions, and randomly separated into three groups of 6 chickens. Groups were housed separately in sterilized isolators for chickens under negative pressure conditions (Allentown CH8ISOL) with food and water ad libitum throughout the experimental period. Animal care and experimental procedures were performed in accordance with the approved protocols of the National Institute of Agricultural Technology Ethics Committee (INTA, Argentina).
Viruses and inocula
The Argentinean CAV-10 and CAV-18 viruses were obtained from commercial broilers in 2007 with increase of mortality, gangrenous dermatitis and thymus and bursa atrophy . These strains were unable to be grown in MDCC-MSB1 cells. Therefore, under our experimental conditions, inocula were adjusted to 106 copies of CAV DNA per animal for comparative analyses of our results. Argentinean CAV viruses were propagated in chickens and CAV inocula were prepared from thymus samples as previously described . Next, DNA was obtained with the QIAamp DNA Mini Kit (Qiagen Inc.Valencia, CA, USA) according to the manufacturer’s instructions, and the number of CAV genomes contained in each inoculum was determined by SYBR Green-based real-time quantitative PCR (RT-qPCR). Values were converted to number of copies of CAV DNA per μL of inoculum. Finally, the inocula were adjusted to 1 × 106 copies of CAV DNA/200 μL.
Quantitative Real Time PCR
SYBR Green-based quantitative real-time PCR (RT-qPCR) was used to determine the number of copies of the CAV genome in inocula.
Primers used in quantitative real time PCR to detect and quantify chicken anemia virus DNA
CAV-Real Time Fw
CAV-Real Time Rv
The cycling parameters consisted of the following steps: 95°C hold for 10 min, followed by 40 cycles consisting of denaturation at 95°C for 15 s and annealing/extension at 50°C for 1 min, and finally adding a dissociation melting curve analysis.
Preparation of standards
A fragment of 75 bp of the CAV genome from Cux-1 vaccine strain was amplified by PCR using the primers described in Table 2 and cloned in pGEM T-Easy vector (Promega Madison, USA) to generate standard curves for the quantitation of number of copies of CAV DNA. Fresh tenfold dilutions were made from the plasmid stocks in distilled water for each PCR run to avoid the problem of plasmid degradation over time in the higher dilutions. Cycle threshold (CT) values were used to plot a standard curve and a range from 101 to 106 copy numbers was represented in each standard curve. The copy number was determined using the conversion factor: 1 ug of a 1-kb DNA = 3.03 pmol ends .
The results from the PCR experiments were analyzed using Sequence Detection Systems v.1.6.3 software. The default settings of the program were used to define both the threshold value and baseline parameters for analysis of the raw data. A standard curve was generated in each assay and used to extrapolate the amounts in the unknown samples.
Six two-week-old chickens were intramuscularly inoculated with 200 μL of CAV-10 or CAV-18 containing 1 × 106 CAV DNA copies. Negative control group (n = 6) was inoculated with 200 μL of phosphate-buffered-saline (PBS). Signs of anorexia, weakness, stunting, cyanosis, petechiae and ecchymoses were looked for everyday in every bird. Fourteen days after inoculation, chickens were bled, euthanized and body, thymus, spleen and bursa of Fabricius were weighed and recorded in all birds. From each animal, the bursa and the first right lobe of the thymus were separated for histopathological evaluation. Fractions of the thymus and spleen were also kept for flow cytometry evaluation.
Samples of the thymus and bursa of Fabricius were collected and immersed into 10% neutral buffered formalin for fixation. Samples were dehydrated and embedded in paraffin wax in the usual manner, sectioned (4 μmthick) and stained with hematoxylin and eosin (HE).
Single cell suspensions from spleens were obtained by direct mechanical disruption in RPMI 1640 through a 40 μm mesh (Cell Strainer, BD). Thymuses were cut into very small pieces and mechanically disrupted by pressing with a syringe plunger, in RPMI 1640. Then, cellular suspensions were passed through a 40 μm mesh (Cell Strainer, BD). Mononuclear cells were isolated from both suspensions by centrifugation over Histopaque density gradient (1.077 g/mL; Sigma, St. Louis, MO, USA) at 400 × g for 30 min and room temperature. Cells were isolated from the interface, washed, and live cells were counted using trypan blue exclusion.
Flow cytometry analysis
Cells were diluted in staining buffer (PBS 1×, 10% FBS, 0.1% Sodium Azide) and 1 × 106 cells per well were transferred into 96 well-plates (V-shape), and washed twice with the same buffer. Staining was performed by resuspending the cellular pellet of each well with 100 μL of staining buffer including different combinations of antibodies, or as single-color stainings for compensation. Cells were incubated at 4°C for 30 min and washed twice with staining buffer by centrifugation at 250 × g for 5 min.
Avian monoclonal antibodies (mAbs) (CD3-SPRD, CD4-FITC, CD8α-PE, CD8α-FITC and CD8α-PE) were purchased from Southern Biotech (Birmingham, AL, USA). Mononuclear cell suspensions from every thymus and spleen were stained with one and two mAb mix, respectively: CD3-SPRD, CD4-FITC and CD8α-PE in tube A (for thymocytes and splenocytes), and CD3-SPRD, CD8α-FITC and CD8β-PE in tube B (splenocytes). All antibodies were titrated in order to determine the optimal staining concentration of each one.
Positive cells were analyzed with a FACS Calibur flow cytometer (BD Biosciences, San Jose, CA, USA) and CellQuest software. Analysis was done on 20 000 events and discrete viable lymphoid cell populations were gated according to the forward/side scatter characteristics. Percentages of different lymphoid cell subpopulations in the thymus and spleen were determined by multiparametric analysis.
Data were tested for normal distribution prior to analysis (Shapiro-Wilk test) using the Statistical Package for the Social Sciences for Windows (SPSS, version 15.0, Chicago, IL, USA). An ANOVA test was used, and a Tukey’s test was applied when differences were detected. Variables that did not fit the ANOVA’s assumptions were analyzed by Kruskall-Wallis and Bonferroni-Dunn post hoc test. P-values of p < 0.05 were considered statistically significant.
Sera were tested by competitive enzyme-linked immunosorbent assay (ELISA) for specific antibodies against CAV according to the manufacturer’s recommendations (Idexx Laboratories, Inc., Westbrook, ME, USA) using 10-fold dilutions of each serum sample.
Nucleotide sequence accession numbers
The nucleotide genome sequence from Argentinean CAV strains obtained in this study are available from GenBank under accession numbers KJ872513 (CAV-10) and KJ872514 (CAV-18).
Characterization of CAV field strains used for experimental infection of chickens
The complete nucleotide genome sequence of CAV-10 and CAV-18 was determined using primers described in Table 1. Both Argentinean CAV genomes are 2298 nt long, and lacked a 21-nt region located within the non-coding, transcription-regulatory region of the genome , that is present in the Cux-1 isolate (M55918). A comparison between the two Argentinean CAV viruses shows 14 individual nucleotide sequence differences dispersed throughout the genome, with three being located in the non-coding region and the rest along ORF1. Nucleotide differences between VP1 from CAV-10 and CAV-18 resulted in only 2 amino acid changes, one Q294H and the other S370T. In addition, both viruses present a glutamine (Q) residue at positions 139 and 144 of VP1.
No mortalities occurred after CAV or PBS inoculation during the experiment. No clinical signs of disease and no differences in body weight were observed between CAV-inoculated and negative control groups.
Analysis of thymic cell subpopulations
Although the comparison of the lymphocyte percentages from each group shows no significant differences in G1, percentages in G2 and G3 were significantly different between groups (Figure 5b). There was a clear and important reduction in the percentages of lymphocytes in G2 from chickens inoculated with Argentinean CAV viruses (p < 0.05). In addition, CAV-10 show a higher reduction of lymphocytes in G2 than CAV-18 (p < 0.05). In contrast, the percentages of lymphocytes in G3 were increased in both CAV inoculated groups (p < 0.05). This increase was higher in thymuses from CAV-10 inoculated chickens with respect to the increase observed in thymuses from CAV-18 inoculated birds (p < 0.05).
Figures 6B and 6C show DP cells from a thymus of the control group in G2 and G3 respectively. Most of the small DP with size and granularity compatible with G2 were in R4, whereas large DP cells from G3 were located in both R4 and R5. In particular, CAV-10 not only reduced (p < 0.05) the percentages of total DP thymocytes in G1, G2 and G3 as CAV-18 (Figure 6J-L), but also altered the percentage of DP thymocytes in R4 and R5 (Figure 6D-I). CAV-10 in particular produced a higher reduction of DP in R4 (in G1, G2 and G3) than CAV-18 (p < 0.05), and a particular significant increase of DP in R5 (G1 and G2) that was not seen in thymuses from CAV-18 inoculated chickens (Figure 6J-L).
Figures 6A, 6D and 6G also show some differences in CD4 + CD8α- and CD4-CD8α + thymocytes in G1 between control, CAV-10 and CAV-18 inoculated groups. Both CAV-inoculated groups appear to have increased their CD4 + CD8α- and CD4-CD8α + subsets when relative percentages were analyzed; however, when the absolute number of CD4 + CD8α- and CD4-CD8α + thymocyte subpopulations were compared between groups, only the number of CD4-CD8α + thymocytes were reduced in thymuses from CAV-10 inoculated chickens (p < 0.05) (Figure 6M).
Analysis of splenic cell subpopulations
Splenic lymphocytes from experimental groups were analyzed in G1 according to forward/side scatter parameters.
Staining with CD3/CD4/CD8α
Staining with CD3/CD8α/CD8α
Complete genome sequencing and comparison of CAV-10 and CAV-18 viruses showed few differences between these two Argentinean strains. Both CAV strains have a deletion that contained a fifth 19-nt repeat, with this region being associated with a better efficiency to replicate in MDCC-MSB1 cell cultures . However, previous reports affirmed that the contribution of this region to the attenuation or pathogenicity of CAV in chickens is still questionable .
In addition to the deletion, genome sequencing of CAV-10 and CAV-18 confirmed that both viruses present mutations in the hypervariable region of VP1 that are also associated with a reduced spread in an avian lymphoblastoid cell line (MDCC-MSB1) compared with Cux-1 . However, these authors were unable to demonstrate differences in host pathogenesis in vivo due to differences in this region. On the contrary, Meehan et al.  have shown that this region does not contribute disproportionately to pathogenicity compared to other regions throughout the genome, and that alterations in more than one of the three CAV proteins, as well as in the noncoding region of the genome, may influence pathogenicity.
Despite the eleven nucleotide differences observed along VP1, only two deduced amino acid substitutions were seen in CAV-10 with respect to the CAV-18 virus. To our knowledge, there are still no reports about the plausible role or the way in which these differences may affect the pathogenesis of CAV in the chicken. We believe that this report could be the first approach to evaluate these amino acid differences of VP1 in vivo, moreover taking into account the few nucleotide variations between CAV-10 and CAV-18 observed only in the non-coding region. However, under our experimental conditions we cannot ensure that the same dosage of each isolate was administered in chickens. Therefore, further studies should be performed to calculate infectivity titres of these field strains in vitro to associate genomic differences between Argentinean CAV strains with different pathogenicities in vivo.
In the present study chickens infected either with CAV-10 or CAV-18 did not present clinical signs of disease throughout the experiment. However, both groups inoculated with Argentinean CAV strains experimented a significant reduction of thymus-to-body weight ratios (CAV-10 produced a significantly higher reduction than CAV-18) and thymocyte depletion at 14 dpi. These results suggest that both CAV field strains produce a subclinical infection in 2-week-old birds.
In addition, chickens infected with CAV-10 virus also show histopathological lesions in the thymus and bursa, compatible with those previously reported by Haridy et al.  in subclinical infections with CAV. It is important to mention that these authors infected animals intramuscularly using an isolate that was passaged 10 times in MDCC-MSB1 cells , where mutations could be introduced. By contrast, CAV-18 inoculated chickens did not present obvious morphological changes in the evaluated organs. This might suggest that alteration of functionality was not very strong or that their course was produced in a very short time in this group and, consequently, the morphological changes could not be observed throughout a histopathological study. Therefore, differences in histopathological lesions produced by CAV-10 or CAV-18 in 2-week-old chickens might suggest that CAV-10 is more aggressive than CAV-18 after in vivo infection, at least at this time post-infection.
Flow cytometry analysis of thymocytes in G1, G2 and G3 from CAV-inoculated chickens vs. control group animals suggests that Argentinean CAV strains alter the thymocyte maturation process after 14 dpi.
The most evident variation was the reduction observed in DP thymocytes following CAV inoculation. Similar results were published by Vaziry et al.  and Hu et al. , evaluating the lesions in 1-day-old chicks infected with the CIA-1 strain. In addition, our results clearly demonstrate that there are different stages of maturation of DP cells due to thymopoiesis in the thymus, and that some of these stages could be altered after CAV infection. While DP in R4 significantly decreased after CAV infection, DP in R5 significantly increased. These evident changes in the percentages of DP thymocytes with different CD4 and CD8α surface expression support the idea that Argentinean CAV viruses can alter thymopoiesis. Even more, under our experimental conditions, CAV-10 produced significantly deeper alterations than CAV-18 in thymocyte maturation two weeks after infection.
On the contrary, the reduction in the total number of lymphocytes in thymuses from CAV inoculated chickens observed during the cell isolation procedure, the absence of significant changes in the number of CD4 + CD8α- thymocytes and the slight decrease of CD4-CD8α + cells observed after flow cytometry analysis of the thymic population add to the notion that mature lymphocytes were not recruited into the thymus at 14 dpi with Argentinean CAV strains. These results were in concordance with previous observations by Vaziry et al.  in a subclinical infection with a vaccinal strain.
Finally, the alterations in percentages of splenic lymphocyte subpopulations were also analyzed by flow cytometry. There were no differences in mature DP and ThL cells between groups after infection with Argentinean field strains, similar to results previously published by other authors with the CIA-1 vaccinal strain . However, in our experimental infection, CTL cells were statistically reduced in spleens from CAV-10 inoculated chickens. Moreover, staining with CD3, CD8α and CD8β mAb allowed discrimination between CD8+ subsets (CD8αα or CD8αβ) that were affected by CAV inoculation. While our results show no differences in CD8αα cells, significant reduction in percentages of the CD8αβ subpopulation was observed only in CAV-10 inoculated birds. Adair et al.  have demonstrated the presence of infected mature lymphocytes in the spleen after 6 dpi, although the numbers of infected cells as a proportion of the total number recorded was much lower than that in the thymus or bone marrow. Our results, where a significant decrease in splenic CD8αβ lymphocytes was observed at 14 dpi, could be the consequence of the large amount of CAV-infected splenocytes reported by Adair et al. at a previous time post-infection. Altogether, our results suggest that CAV-10 affects splenic lymphocyte subpopulations by a reduction in CD8αβ subset and, consequently, this could alter the host immune response against other secondary pathogens.
In this work we studied the subclinical infection of 2-week-old chickens with two Argentinean CAV field strains, showing some nucleotide differences in their genome sequence. Under our experimental conditions, the results might suggest there are differences in the behavior of CAV-10 and CAV-18 strains in vivo at 14 dpi. Further studies should be done to determine first the viral titer of these CAV field strains and then, to associate nucleotide/amino acidic composition, in VP1 and/or in non-coding region, with differential pathogenicity in chickens.
AR participated in the design of the study and conception, coordinated and carried out the animal studies, the sequence alignment, the cytometry and statistical analysis and drafts the manuscript and revised it critically for important intellectual content. SP carried out the histopathology. VO participated in virus detection, virus sequencing and animal studies. MD participated in animal studies. MPF helped to draft the manuscript. MIC conceived of the study, participated in its design, in animal studies and helped to draft the manuscript. AP conceived of the study, participated in its design, in animal studies and helped to draft the manuscript. AR, SP, VO, MD, MPF, MIC and AP have given final approval of the version to be published.
List of abbreviations
Chicken Anemia Virus
Chicken Anemia Virus, Argentinean strain 10
Chicken Anemia Virus, Argentinean strain 18
Enzyme-Linked ImmunoSorbent Assay
Hematoxylin and eosin stain
Chicken hematopoietic lymphoblast cell line
Open Reading Frame
Polymerase Chain Reaction
Real-time quantitative PCR
The authors thank to Mariela Gammella for acquisition of data by flow cytometry, Juan Manuel Schammas for technical support and María José Gravisaco for interpretation of data. This work was partially supported by the NIAID Center for Research on Influenza Pathogenesis (CRIP) through University of Maryland, College Park, contract no. HHSN266200700010C. This work was also supported by P. E. Enfermedades Infecciosas de las Aves PNSA 1115056 from INTA and by PICT 2008 – 0922 from MINCyT. A. Rimondi is recipient of CONICET fellowship.
- Schat KA: Chicken Infectious Anemia. Diseases of Poultry. Edited by: Saif YM, Barnes HJ, Glisson JR, Fadly AM, McDougald LR, Swayne DE. 2003, Iowa State University Press, Ames, 182-202. 11Google Scholar
- Pringle CR: Virus taxonomy at the XI International Congress of Virology, Sydney, Australia. Arch Virol. 1999, 144: 2065-2070. 10.1007/s007050050728.View ArticlePubMedGoogle Scholar
- Noteborn MHM, Kranenburg O, Zantema A, Koch G, de Boer GF, van der Eb AJ: Transcription of the chicken anemia virus (CAV) genome and synthesis of its 52-kDa protein. Gene. 1992, 118: 267-271. 10.1016/0378-1119(92)90198-X.View ArticlePubMedGoogle Scholar
- Phenix KV, Meehan BM, Todd D, McNulty MS: Transcriptional analysis and genome expression of chicken anaemia virus. J Gen Virol. 1994, 75: 905-909. 10.1099/0022-1317-75-4-905.View ArticlePubMedGoogle Scholar
- Koch G, van Roozelaar DJ, Verschueren CAJ, van der Eb AJ, Noteborn MHM: Immunogenic and protective properties of chicken anaemia virus proteins expressed by baculovirus. Vaccine. 1995, 13: 763-770. 10.1016/0264-410X(94)00034-K.View ArticlePubMedGoogle Scholar
- Noteborn MHM, Verschueren CA, Koch G, van der Eb AJ: Simultaneous expression of recombinant baculovirus-encoded chicken anemia virus (CAV) proteins VP1 and VP2 is required for formation of the CAV-specific neutralizing epitope. J Gen Virol. 1998, 79: 3073-3077.View ArticlePubMedGoogle Scholar
- Noteborn MH, Todd D, Verschueren CA, de Gauw HW, Curran WL, Veldkamp S, Douglas AJ, McNulty MS, van der Eb AJ, Koch G: A single chicken anemia virus protein induces apoptosis. J Virol. 1994, 68: 346-351.PubMed CentralPubMedGoogle Scholar
- Jeurissen SHM, Wagenaar F, Pol JMA, van der Eb AJ, Noteborn MHM: Chicken anemia virus causes apoptosis of thymocytes after in vivo infection and of cell lines after in vitro infection. J Virol. 1992, 66: 7383-7388.PubMed CentralPubMedGoogle Scholar
- McNulty MS: Chicken anemia agent: a review. Avian Pathol. 1991, 20: 187-203. 10.1080/03079459108418756.View ArticlePubMedGoogle Scholar
- McNulty MS, McIlroy SG, Bruce DW, Todd D: Economic effects of subclinical chicken anemia infection in broiler chicks. Avian Dis. 1991, 35: 263-268. 10.2307/1591175.View ArticlePubMedGoogle Scholar
- Toro H, Ramirez AM, Laurenas J: Pathogenicity of chicken anemia virus (isolate 10343) for young and older chickens. Avian Pathol. 1997, 26: 485-499. 10.1080/03079459708419229.View ArticlePubMedGoogle Scholar
- McConnell CD, Adair BM, McNulty MS: Effects of chicken anemia virus on cell-mediated immune function in chickens exposed to the virus by a natural route. Avian Dis. 1993, 37: 366-374. 10.2307/1591660.View ArticlePubMedGoogle Scholar
- Markowski-Grimsrud CJ, Schat KA: Infection with chicken anemia virus impairs the generation of antigen-specific.cytotoxic T lymphocytes. Immunology. 2003, 109: 283-294. 10.1046/j.1365-2567.2003.01643.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Schat KA: Marek’s disease immunosuppression. Marek’s Disease: An Evolving Problem. Edited by: Davison F, Nair V. 2004, Elsevier Academic Press, London, 49-61. 1Google Scholar
- Davidson I, Kedem M, Borochovitz H, Kass N, Ayali G, Hamzani E, Perelman B, Smith B, Perk S: Chicken infectious anemia virus infection in Israeli commercial flocks: virus amplification, clinical signs, performance, and antibody status. Avian Dis. 2004, 48: 108-118. 10.1637/7072.View ArticlePubMedGoogle Scholar
- Zanella A, Dall’Ara P, Lavazza A, Marchi R, Morena MA, Rampin T: Interaction between Marek’s disease virus and chicken infectious anemia virus. Current Progress on Marek’s Disease Research. Edited by: Schat KA, Morgan RM, Parcells MS, Spencer JL. 2001, American Association of Avian Pathologists, Kennett Square, PA, 11-19.Google Scholar
- Taniguchi T, Yuasa M, Maeda M, Horiuchi T: Chronological observations on hemapathological changes in chicks inoculated with chicken anemia agent. Natl Inst Anim Health Q (Tokyo). 1983, 22: 61-69.Google Scholar
- Goryo M, Hatashi S, Yoshizaida K, Umemura T, Itakura C, Yamashiro S: Ultrastructure of the thymus in chickens inoculated with chicken anemia agent (MSB1-TK 5803 strain). Avian Pathol. 1989, 18: 605-617. 10.1080/03079458908418636.View ArticlePubMedGoogle Scholar
- Coud SS, Lillehoj HS, Rosenberger JK: Immune dysfunction following infection with chicken anemia agent and infectious bursal disease virus. I. kinetic alterations of avian lymphocyte subpopulations. Vet Immunol Immunopathol. 1992, 34: 337-352. 10.1016/0165-2427(92)90174-O.View ArticleGoogle Scholar
- Hu LB, Lucio B, Schat KA: Depletion of CD4+ and CD8+ T lymphocyte subpopulations by CIA-1, a chicken infectious anemia virus. Avian Dis. 1993, 37: 492-500. 10.2307/1591677.View ArticlePubMedGoogle Scholar
- Vaziry A, Silim A, Bleau C, Frenette D, Lamontagne L: Chicken infectious anaemia vaccinal strain persists in the spleen and thymus of young chicks and induces thymic lymphoid cell disorders. Avian Pathol. 2011, 40: 377-385. 10.1080/03079457.2011.586330.View ArticlePubMedGoogle Scholar
- Adair BM, McNeilly F, McConnell CD, McNulty MS: Characterization of surface markers present on cells infected by chicken anemia virus in experimentally infected chickens. Avian Dis. 1993, 37: 943-950. 10.2307/1591898.View ArticlePubMedGoogle Scholar
- Drén CN, Kant A, Van Roozelaar DJ, Hartog L, Noteborn MH, Koch G: Studies on the pathogenesis of chicken infectious anaemia virus infection in six-week-old SPF chickens. Acta Vet Hung. 2000, 48: 455-467.PubMedGoogle Scholar
- Meehan BM, Todd D, Creelan JL, Connor TJ, McNulty MS: Investigation of the attenuation exhibited by a molecularly cloned chicken anemia virus isolate by utilizing a chimeric virus approach. J Virol. 1997, 71: 8362-8367.PubMed CentralPubMedGoogle Scholar
- Craig MI, Rimondi A, Delamer M, Sansalone P, König G, Vagnozzi A, Pereda A: Molecular characterization of chicken infectious anemia virus circulating in Argentina during 2007. Avian Dis. 2009, 53: 331-335. 10.1637/8478-100808-Reg.1.View ArticlePubMedGoogle Scholar
- Renshaw RW, Soiné C, Weinkle T, O’Connell PH, Ohashi K, Watson S, Lucio B, Harrington S, Schat KA: A hypervariable region in VP1 of chicken infectious anemia virus mediates rate of spread and cell tropism in tissue culture. J Virol. 1996, 70: 8872-8878.PubMed CentralPubMedGoogle Scholar
- Van Santen VL, Li L, Hoerr FJ, Lauerman LH: Genetic characterization of chicken anemia virus from commercial broiler chickens in Alabama. Avian Dis. 2001, 45: 373-388. 10.2307/1592977.View ArticlePubMedGoogle Scholar
- Davidson I, Loeb E, Lublin A, Perk S, Shkoda I, Schat KA: Assessment of various criteria to determine the chicken anemia virus pathogenicity in embryonated eggs and in day-old chicks. Curr Trop Virol. 2007, 6: 95-111.Google Scholar
- Technical Reference Promega., [http://www.promega.com/~/media/files/resources/technical%20references/plasmid%20and%20protein%20quantitation.pdf]
- Noteborn MHM, Verscheuren CAJ, Zantema A, Koch G, van der Eb AJ: Identification of the promoter region of chicken anemia virus (CAV) containing a novel enhancer element. Gene. 1994, 150: 313-318. 10.1016/0378-1119(94)90444-8.View ArticlePubMedGoogle Scholar
- Todd D, Connor TJ, Calvert VM, Creelan JL, Meehan BM, McNulty MS: Molecular cloning of an attenuated chicken anaemia virus isolate following repeated cell culture passage. Avian Pathol. 1995, 24: 171-187. 10.1080/03079459508419057.View ArticlePubMedGoogle Scholar
- Haridy M, Sasaki J, Ikezawa M, Okada K, Goryo M: Pathological and immunohistochemical studies of subclinical infection of chicken anemia virus in 4-week-old chickens. J Vet Med Sci. 2012, 74: 757-764. 10.1292/jvms.11-0374.View ArticlePubMedGoogle Scholar
- Goryo M, Sugimura H, Matsumoto S, Umemura T, Itakura C: Isolation of an agent inducing chicken anemia. Avian Pathol. 1985, 14: 483-496. 10.1080/03079458508436251.View ArticlePubMedGoogle Scholar
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