ORIGINAL_ARTICLE
Persistent bovine viral diarrhea virus (BVDV) infection in cattle herds
Bovine viral diarrhea virus (BVDV) is a significant pathogen associated with gastrointestinal, respiratory, and reproductive diseases of cattle worldwide. It causes continuous economic losses to the cattle industry primarily due to decreased reproductive performance. The ability of virus to cross the placenta during early pregnancy can result in the birth of persistently infected (PI) calves. Persistently infected animals are generally much more efficient transmitters of BVDV than transiently or acutely infected animals because they are capable of shedding large quantities of virus throughout their lives and are considered the primary reservoirs for BVDV. Due to the nature of viral infections, there is no treatment to fully cure an animal of a viral infection. All control programs which are in use in many countries of the world, mainly depend upon the detection of PI animals, eliminating them and preventing their return into the herds. Detection of PI animals at early stage, particularly soon after birth is of significant benefit to implement BVDV control programs. Available diagnostic tests such as virus isolation (VI), immunohistochemistry (IHC), Antigen-Capture ELISA (ACE), and reverse transcriptase polymerase chain reaction (RT-PCR) are used for detection of PI cattle. Each method to detect BVDV has advantages, disadvantages, and applicability for different diagnostic situations. The reliability of diagnostic tests is optimized by choosing the appropriate sampling strategy on the basis of animal age.
https://ijvr.shirazu.ac.ir/article_4190_c437d6dbd58fdae6d2b09acbd83dde18.pdf
2017-09-01
154
163
10.22099/ijvr.2017.4190
Antigen-Capture ELISA
BVD
Immunohistochemistry
Persistent infection
RT-PCR
A.
Khodakaram-Tafti
tafti@shirazu.ac.ir
1
Department of Pathobiology, School of Veterinary Medicine, Shiraz University, Shiraz, Iran
LEAD_AUTHOR
GH.
Farjanikish
2
Department of Pathobiology, School of Veterinary Medicine, Lorestan University, Khorramabad, Iran
AUTHOR
Baker, JC (1987). The clinical manifestations of BVD infection. Vet. Clin. North Am.: Food Anim. Pract., 11: 425-445.
1
Baule, C; Kulcsar, G; Belak, K; Albert, M; Mittelholzer, C; Soos, T; Kucsera, L andBelak, S (2001). Pathogenesis of primary respiratory disease induced by isolates from a new genetic cluster of bovine viral diarrhea virus type I. J. Clin. Microbiol., 39: 146-153.
2
Bedekovic, T; Lemo, N; Lojki, I; Beck, A; Lojkić, M and Madić, J (2011). Implementation of immuno-histochemistry on frozen ear notch tissue samples in diagnosis of bovine viral diarrhea virus in persistently infected cattle. Acta Vet. Scand., 53: 65-72.
3
Belak, S and Ballagi-Pordany, A (1993). Experiences on the application of the polymerase chain reaction in a diagnostic laboratory. Mol. Cell. Prob., 7: 241-248.
4
Bezek, DM; Grohn, YT and Dubovi, EJ (1994). Effect of acute infection with noncytopathic or cytopathic bovine viral diarrhea virus isolates on bovine platelets. Am. J. Vet. Res., 55: 1115-1119.
5
Bielanski, A; Algire, J; Lalonde, A and Nadin-Davis, S (2009). Transmission of bovine viral diarrhea virus (BVDV) via in vitro-fertilized embryos to recipients, but not to their offspring. Theriogenology. 71: 499-508.
6
Birk, AV; Dubovi, EJ; Cohen-Gould, L; Donis, R and Szeto, HH (2008). Cytoplasmic vacuolization responses to cytopathic bovine viral diarrhoea virus. Virus Res., 132: 76-85.
7
Bolin, SR and Grooms, DL (2004). Origination and consequences of bovine viral diarrhea virus diversity. Vet. Clin. North Am.: Food Anim. Pract., 20: 51-68.
8
Bolin, SR; McClurkin, AW; Cutlip, RC andCoria, MF (1985). Severe clinical disease induced in cattle persistently infected with noncytopathic bovine viral diarrhea virus by superinfection with cytopathic bovine viral diarrhea virus. Am. J. Vet. Res., 46: 573-576.
9
Brinkhof, J; Zimmer, G and Westenbrink, F (1996). Comparative study on four enzyme-linked immunosorbent assays and a cultivation assay for the detection of antigens associated with the bovine viral diarrhoea virus in persistently infected cattle. Vet. Microbiol., 50: 1-6.
10
Brock, KV (2003). The persistence of bovine viral diarrhea virus. Biologicals. 31: 133-135.
11
Brock, KV (2004). The many faces of bovine viral diarrhoea virus. Vet. Clin. North Am.: Food Anim. Pract., 20: 1-3.
12
Brodersen, BW (2004). Immunohistochemistry used as a screening method for persistent bovine viral diarrhea virus infection. Vet. Clin. North Am.: Food Anim. Pract., 20: 85-94.
13
Brownlie, J (1990). Pathogenesis of mucosal disease and molecular aspects of bovine virus diarrhea virus. Vet. Microbiol., 23: 371-382.
14
Bruschke, CJM; Haghparast, A; Hoek, A; Rutten, VP; Wentink, GH; Van Rijn, PA and Van Oirschot, JT (1998). The immune response of cattle persistently infected with non-cytopathic BVDV after superinfection with antigenetically semi-homologous cytopathic BVDV. Vet. Immunol. Immunopathol., 62: 37-50.
15
Campbell, JR (2004). Effect of bovine viral diarrhea virus in the feedlot. Vet. Clin. North Am.: Food Anim. Pract., 20: 39-50.
16
Carlsson, U (1991). Border disease in sheep caused by transmission of virus from cattle persistently infected with bovine virus diarrhoea virus. Vet. Rec., 128: 145-147.
17
Carlsson, U and Belak, K (1994). Border disease virus transmitted to sheep and cattle by a persistently infected ewe: epidemiology and control. Acta Vet. Scand., 35: 79-88.
18
Chase, CC; Elmowalid, G and Yousif, AA (2004). The immune response to bovine viral diarrhea virus: a constantly changing picture. Vet. Clin. North Am.: Food Anim. Pract., 20: 95-114.
19
Cornish, TE; Olphen, AL; Cavender, JL; Edwards, JM; Jaeger, PL; Vieyra, LL; Woodard, LF; Miller, DR and O’Toole, D (2005). Comparison of ear notch immuno-histochemistry, ear notch antigen-capture ELISA, and buffy coat virus isolation for detection of calves persistently infected with bovine viral diarrhea virus. J. Vet. Diag. Investig., 17: 110-117.
20
Dabak, M; Karapinar, T; Gulacti, I; Bulut, H; Kizil, O and Aydin, S (2007). Hemorrhagic syndrome-like disease in calves with bovine viral diarrhea and mucosal disease complex. J. Vet. Intern. Med., 21: 514-518.
21
Deregt, D and Loewen, KG (1995). Bovine viral diarrhea virus: biotypes and disease. Can. Vet. J., 36: 371-378.
22
Deregt, D; Tessaro, SV; Baxi, MK; Berezowski, J; Ellis, JA; Wu, JT and Gilbert, SA (2005). Isolation of bovine viral diarrhoea viruses from bison. Vet. Rec., 157: 448-450.
23
Drew, TW; Yapp, F and Paton, DJ (1999). The detection of bovine viral diarrhoea virus in bulk milk samples by use of a singletube RT-PCR. Vet. Microbiol., 64: 145-154.
24
Edmondson, MA; Givens, MD; Walz, PH; Gard, JA; Stringfellow, DA and Carson, RL (2007). Comparison of tests for detection of bovine viral diarrhea virus in diagnostic samples. J. Vet. Diagn. Invest., 19: 376-381.
25
Evermann, JF and Ridpath, JF (2002). Clinical and epidemiologic observations of bovine viral diarrhea virus in the northwestern United States. Vet. Microbiol., 89: 129-139.
26
Ezanno, P; Fourichon, C and Seegers, H (2008). Influence of herd structure and type of virus introduction on the spread of bovine viral diarrhoea virus (BVDV) within a dairy herd. Vet. Res., 39: 39.
27
Falcone, E; Tollis, M and Conti, G (1999). Bovine viral diarrhea disease associated with a contaminated vaccine. Vaccine. 18: 387-388.
28
Farjanikish, GH; Khodakaram-Tafti, A and Mohammadi, A (2013). Serological survey of bovine viral diarrhea virus by antigen capture ELISA in dairy herds in Fars Province, Iran. Bulg. J. Vet. Med., 16: 217-222.
29
Fenton, A; Nettleton, PF; Entrican, G; Herring, JA; Malloy, C; Greig, A and Low, JC (1991). Identification of cattle infected with bovine virus diarrhoea virus using a monoclonal antibody capture ELISA. Arch. Virol., 3: 169-174.
30
Fray, MD; Paton, DJ and Alenius, S (2000). The effects of bovine viral diarrhoea virus on cattle reproduction in relation to disease control. Anim. Reprod. Sci., 2: 615-627.
31
Frey, HR; Flebbe, U and Liess, B (1996). Prevalence and clinical symptoms of persistent BVD-virus infection in cattle herds of Lower Saxony. Praktischer Tierarzt., 14: 14-18.
32
Fulton, RW; Johnson, BJ; Briggs, RE; Ridpath, JF; Saliki, JT; Confer, AW; Burge, LJ; Step, DL; Walker, DA and Payton, ME (2006). Challenge with bovine viral diarrhea virus by exposure to persistently infected calves: protection by vaccination and negative results of antigen testing in nonvaccinated acutely infected calves. Can. J. Vet. Res., 70: 121-127.
33
Givens, MD; Heath, AM; Brock, KV; Brodersen, BW; Carson, RL and Stringfellow, DA (2003). Detection of bovine viral diarrhea virus in semen obtained after inoculation of seronegative postpubertal bulls. Am. J. Vet. Res., 64: 428-434.
34
Goyal, SM (2005). Diagnosis. In: Goyal, SM and Ridpath, JF (Eds.), Bovine viral diarrhea virus: diagnosis, management, and control. (1st Edn.), Ames, IA, Blackwell Publishing. PP: 197-208.
35
Grooms, DL (2004). Reproductive consequences of infection with bovine viral diarrhea virus. Vet. Clin. Food Anim., 20: 5-19.
36
Grooms, DL and Keilen, ED (2002). Screening of neonatal calves for persistent infection with bovine viral diarrhea virus by immunohistochemistry on skin biopsy samples. Clin. Diagn. Lab Immunol., 9: 898-900.
37
Gunn, GJ; Sattkamp, HW; Humphry, RW and Stott, AW (2005). Assessing economic and social pressure for the control of bovine viral diarrhoea virus. Prev. Vet. Med., 72: 149-162.
38
Hilbe, M; Arquint, A; Schaller, P; Zlinszky, K; Braun, U; Peterhans, E and Ehrensperger, F (2007b). Immuno-histochemical diagnosis of persistent infection with Bovine Viral Diarrhea Virus (BVDV) on skin biopsies. Schw. Arch. Tierh., 149: 337-344.
39
Hilbe, M; Stalder, H; Peterhans, E; Haessig, M; Nussbaumer, M; Egli, C; Schelp, C; Zlinszky, K and Ehrensperger, F (2007a). Comparison of five diagnostic methods for detecting bovine viral diarrhea virus infection in calves. J. Vet. Diagn. Invest., 19: 28-34.
40
Hill, FI; Reichel, MP; McCoy, RJ and Tisdall, DJ (2007). Evaluation of two commercial enzyme – linked immuno-sorbent assays for detection of bovine viral diarrhoea virus in serum and skin biopsies of cattle. New Zealand Vet. J., 55: 45-48.
41
Houe, H (1995). Epidemiology of bovine viral diarrhea virus. Vet. Clin. North Am.: Food Anim. Pract., 11: 521-547.
42
Houe, H (1999). Epidemiological features and economical importance of bovine virus diarrhoea virus (BVDV) infections. Vet. Microbiol., 64: 89-107.
43
Kelling, CL (2004). Evolution of bovine viral diarrhea virus vaccines. Vet. Clin. Food Anim. Pract., 20: 115-129.
44
Kennedy, JA (2006). Diagnostic efficacy of a reverse transcriptase-polymerase chain reaction assay to screen cattle for persistent bovine viral diarrhea virus infection. J. Am. Vet. Med. Assoc., 229: 1472-1474.
45
Kennedy, JA; Mortimer, RG and Powers, B (2006). Reverse transcription-polymerase chain reaction on pooled samples to detect bovine viral diarrhea virus by using fresh ear-notch-sample supernatants. J. Vet. Diagn. Invest., 18: 89-93.
46
Khodakaram-Tafti, A and Ikede, BO (2005). A retrospective study of sporadic bovine abortions, stillbirths, and neonatal abnormalities in Atlantic Canada, from 1990 to 2001.Can. Vet. J., 46: 635-637.
47
Khodakaram-Tafti, A and Miller, L (2006). The comparative evaluation of cellular localization of viral antigens with microscopic changes in the ileum of cattle infected with bovine viral diarrhea. Comp. Clin. Pathol., 15: 90-93.
48
Khodakaram-Tafti, A; Mohammadi, A and Farjanikish, GH (2015). Histopathological and immuno-histochemical findings from bovine viral diarrhea virus infection in cattle. Onl. J. Vet. Res., 19: 317-321.
49
Khodakaram-Tafti, A; Mohammadi, A and Farjanikish, GH (2016). Molecular characterization and phylogenetic analysis of bovine viral diarrhea virus in dairy herds of Fars province, Iran. Iran. J. Vet. Res., 17: 89-97.
50
Kuhne, S; Schroeder, C; Holmquist, G; Wolf, G; Horner, S; Brem, G and Ballagi, A (2005). Detection of bovine viral diarrhoea virus infected cattle testing tissue samples derived from ear tagging using an Erns capture ELISA. J. Vet. Med. B. Infect. Dis. Vet. Public Health. 52: 272-277.
51
Kümmerer, BM; Tautz, N; Becher, P; Thiel, H and Meyers, G (2000). The genetic basis for cytopathogenicity of Pestiviruses. Vet. Microbiol., 77: 117-128.
52
Lamm, CG; Broaddus, CC and Holyoak, GR (2009). Distribution of bovine viral diarrhea virus antigen in aborted fetal and neonatal goats by immunohistochemistry. Vet Pathol., 46: 54-58.
53
Larson, RL; Groteloescher, DM; Brock, KV; Hunsaker, BD; Smith, RA; MacGregor, DS and Daragatz, DA (2004). Bovine Viral Diarrhea (BVD): review for beef cattle veterinarians. Bov. Pract., 38: 93-102.
54
Letellier, C; Kerkhofs, P; Wellemans, G and Vanopdenbosch, E (1999). Detection and genotyping of bovine diarrhea virus by reverse transcription-polymerase chain amplification of the 5' untranslated region. Vet. Microbiol., 64: 155-167.
55
Liebler-Tenorio, EM; Kenklies, S; Greiser-Wilke, I; Makoschey, B and Pohlenz, JF (2006). Incidence of BVDV1 and BVDV2 infections in cattle submitted for necropsy in Northern Germany. J. Vet. Med. B. Infect. Dis. Vet. Public Health. 53: 363-369.
56
Lindberg, AL (2003). Bovine viral diarrhea virus infections and its control. A review. Vet. Q., 25: 1-16.
57
Lindberg, A; Brownlie, J; Gunn, GJ; Houe, H; Moennig, V; Saatkamp, HW; Sandvik, T and Valle, PS (2006). The control of bovine viral diarrhoea virus in Europe: today and in the future. Rev. Sci. Tech., 25: 961-979.
58
Lindberg, A and Houe, H (2005). Characteristics in the epidemiology of bovine viral diarrhea virus (BVDV) of relevance to control. Prev. Vet. Med., 15: 55-73.
59
Loneragan, GH; Thomson, DU; Montgomery, DL; Mason, GL and Larson, RL (2005). Prevalence, outcome, and health consequences associated with persistent infection with bovine viral diarrhea virus in feedlot cattle. J. Am. Vet. Med. Assoc., 15: 595-601.
60
Lùken, T (1995). Ruminant Pestivirus infections in animals other than cattle and sheep. Vet. Clin. North Am.: Food Anim. Pract., 11: 597-614.
61
Lunardi, M; Headley, SA; Lisboa, JA; Amude, AM and Alfieri, AA (2008). Outbreak of acute bovine viral diarrhea in Brazilian beef cattle: clinicopathological findings and molecular characterization of a wild-type BVDV strain subtype 1b. Res. Vet. Sci., 85: 599-604.
62
Luzzago, C; Bandi, C; Bronzo, V; Ruffo, G and Zecconi, A (2001). Distribution pattern of bovine viral diarrhoea virus strains in intensive cattle herds in Italy. Vet. Microbiol., 26: 265-274.
63
Luzzago, C; Frigerio, M; Tolari, F; Mazzei, M; Salvadori, C; Del Piero, F and Arispici, M (2006). Indirect immuno-histochemistry on skin biopsy for the detection of persistently infected cattle with bovine viral diarrhoea virus in Italian dairy herds. New Microbiol., 29: 127-131.
64
Moennig, V; Houe, H and Lindberg, A (2005). BVD control in Europe: current status and perspectives. Anim. Health Res. Rev., 6: 63-74.
65
Munoz-Zanzi, CA; Johnson, WO; Thurmond, MC and Hietala, SK (2000). Pooled sample testing as a herd-screening tool for detection of bovine viral diarrhea virus persistently infected cattle. J. Vet. Diagn. Invest., 12: 195-203.
66
Neill, JD; Ridpath, JF; Lange, A and Zuerner, RL (2008). Bovine viral diarrhoea virus infection alters global transcription profiles in bovine endothelial cells. Dev. Biol., 132: 93-98.
67
Nelson, DD; Duprau, JL; Wolff, PL and Evermann, JF (2015). Persistent bovine viral diarrhea virus infection in domestic and wild small ruminants and camelids including the mountain goat (Oreamnos americanus). Front Microbiol., 6: 1415-1422.
68
Niskanen, R and Lindberg, A (2003). Transmission of bovine viral diarrhoea virus by unhygienic vaccination procedures, ambient air, and from contaminated pens. Vet. J., 165: 125-130.
69
Niskanen, R; Lindberg, A; Larsson, B and Alenius, S (2000). Lack of virus transmission from bovine viral diarrhoea virus infected calves to susceptible peers. Acta Vet. Scand., 41: 93-99.
70
Niskanen, R; Lindberg, A and Traven, M (2002). Failure to spread bovine virus diarrhea virus infection from primarily infected calves despite concurrent infection with bovine coronavirus. Vet. J., 163: 251-529.
71
Njaa, BL; Clark, FG; Janzen, E; Ellis, JA and Haines, DM (2000). Diagnosis of persistent bovine viral diarrhea virus infection by immunohistochemical staining of formalin-fixed skin biopsy specimens. J. Vet. Diag. Invest., 12: 393-399.
72
Odeon, AC; Risatti, G; Kaiser, GG; Leunda, MR; Odriozola, E; Campero, CM and Donis, RO (2003). Bovine viral diarrhea virus genomic associations in mucosal disease, enteritis and generalized dermatitis outbreaks in Argentina. Vet. Microbiol., 17: 133-144.
73
Pacheco, JM and Lager, I (2003). Indirect method ELISA for the detection of antibodies against bovine diarrhea virus in bovine serum. Rev. Argentin. Microbiol., 35: 19-23.
74
Palfi, V; Houe, H and Philipsen, J (1993). Studies on the decline of bovine virus diarrhoea virus (BVDV) antibodies and detectability of BVDV in persistently infected calves. Acta Vet. Scand., 34: 105-107.
75
Paton, DJ; Carlsson, U; Lowings, JP; Sands, JJ; VilceÃk, S and Alenius, S (1995). Identification of herdspecific bovine viral diarrhoea virus isolates from infected cattle and sheep. Vet. Microbiol., 43: 283-294.
76
Pellerin, C; Vandenhurk, J; Lecomte, J and Tijssen, P (1994). Identification of a new group of bovine viral diarrhea virus strains associated with severe outbreaks and high mortalities. Virology. 203: 260-268.
77
Peterhans, E; Jungi, TW and Schweizer, M (2003). BVDV and innate immunity. Biologicals. 31: 107-112.
78
Renshaw, RW; Ray, R and Dubovi, EJ (2000). Comparison of virus isolation and reverse transcription polymerase chain reaction assay for detection of bovine viral diarrhea virus in bulk milk tank samples. J. Vet. Diagn. Invest., 12: 184-186.
79
Ridpath, JF (2005). Classification and molecular biology. In: Goyal, SM and Ridpath, JF (Eds.), Bovine viral diarrhea virus: diagnosis, management, and control. (1st Edn.), Ames, Iowa, Blackwell Publishing. PP: 65-80.
80
Ridpath, JF (2010). Bovine viral diarrhea virus: global status. Vet. Clin. North Am.: Food Anim. Pract., 26: 105-121.
81
Ridpath, JF; Fulton, RW; Kirkland, PD and Neill, JD (2010). Prevalence and antigenic differences observed between bovine viral diarrhea virus subgenotypes isolated from cattle in Australia and feedlots in the southwestern United States. J. Vet. Diagn. Invest., 22: 184-191.
82
Saliki, JT and Dubovi, EJ (2004). Laboratory diagnosis of bovine viral diarrhea virus infections. Vet. Clin. North Am.: Food Anim. Pract., 20: 69-83.
83
Saliki, JT; Huchzermeir, R and Dubovi, EJ (2000). Evaluation of a new sandwich ELISA kit that uses serum for detection of cattle persistently infected with BVD virus. Ann. N. Y. Acad. Sci., 916: 358-363.
84
Sandvik, T (2005). Selection and use of laboratory diagnostic assays in BVD control programmes. Preven. Vet. Med., 72: 3-16.
85
Schirrmeier, H; Strebelow, G; Depner, K; Hoffmann, B and Beer, M (2004). Genetic and antigenic characterization of an atypical Pestivirus isolate, a putative member of a novel Pestivirus species. J. Gen. Virol., 85: 3647-3652.
86
Schlafer, DH; Gillespie, JH; Foote, RH; Quick, S; Pennow, NN; Dougherty, EP; Schiff, EI; Allen, SE; Powers, PA and Hall, CE (1990). Experimental transmission of bovine viral diseases by insemination with contaminated semen or during embryo transfer. Deutsche Tierärzt. Wochensch., 97: 68-72.
87
Schweizer, M; Matzener, P; Pfaffen, G; Stalder, H and Peterhans, E (2006). "Self" and "Nonself" manipulation of interferon defense during persistent infection: bovine viral diarrhea virus resists alpha/beta interferon without blocking antiviral activity against unrelated viruses replicating in its host cells. J. Virol., 80: 6926-6935.
88
Shannon, AD; Richards, SG; Kirkland, PD and Moyle, A (1991). An antigen-capture ELISA detects Pestivirus antigens in blood and tissues of immunotolerant carrier cattle. J. Virol. Method., 34: 1-12.
89
Smirnova, NP; Bielefeldt-Ohmann, H; Van Campen, H; Austin, KJ; Han, H; Montgomery, DL; Shoemaker, ML; van Olphen, AL and Hansen, TR (2008). Acute noncytopathic bovine viral diarrhea virus infection induces pronounced type I interferon response in pregnant cows and foetuses. Virus Res., 132: 49-58.
90
Smith, DR and Grotelueschen, DM (2004). Biosecurity and biocontainment of bovine viral diarrhea virus. Vet. Clin. North Am.: Food Anim. Pract., 20: 131-149.
91
Smith, RL; Sanderson, MW; Walz, PH and Givens, MD (2008). Sensitivity of polymerase chain reaction for detection of bovine viral diarrhea virus in pooled serum samples and use of pooled polymerase chain reaction to determine prevalence of bovine viral diarrhea virus in auction market cattle. J. Vet. Diagn. Invest., 20: 75-78.
92
Stokstad, M; Niskanen, R; Lindberg, A; Thoren, P; Belak, S; Alenius, S and Loken, T (2003). Experimental infection of cows with bovine viral diarrhoea virus in early pregnancy – findings in serum and foetal fluids. J. Vet. Med., 50: 424-429.
93
Stringfellow, DA; Riddell, KP; Givens, MD; Galik, PK; Sullivan, E; Dykstra, CC; Robl, J and Kasinathan, P (2005). Bovine viral diarrhea virus (BVDV) in cell lines used for somatic cell cloning. Theriogenology. 63: 1004-1013.
94
Swasdipan, S; McGowan, M; Phillips, N and Bielefeldt-Ohmann, H (2002). Pathogenesis of transplacental virus infection: Pestivirus replication in the placenta and fetus following respiratory infection. Microb. Pathog., 32: 49-60.
95
Taghipour Bazargani, T; Khodakaram-Tafti, A; Mousakhani, F and Nekouie Jahromi, OA (2011). Occurrence of congenital tremor in Holstein calves due to infection with BVDV in two industrial dairies from Tehran and Kerman Provinces (case report). Sci. Res. Iranian Vet. J., 7: 92-96.
96
Tajima, M; Ohsaki, T; Okazawa, M and Yasutomi, I (2008). Availability of oral swab sample for the detection of bovine viral diarrhea virus (BVDV) gene from the cattle persistently infected with BVDV. Jpn. J. Vet. Res., 56: 3-8.
97
Talafha, AQ; Hirche, SM; Ababneh, MM; Al-Majali, AM and Ababneh, MM (2009). Prevalence and risk factors associated with bovine viral diarrhea virus infection in dairy herds in Jordan. Trop. Anim. Health Prod., 41: 499-506.
98
Tautz, N and Thiel, HJ (2003). Cytopathogenicity of Pestiviruses: cleavage of bovine viral diarrhoea virus NS2-3 has to occur at a defined position to allow viral replication. Arch. Virol., 148: 1405-1412.
99
Terpstra, C and Wensvoort, G (1988). Natural infections of pigs with bovine viral diarrhoea virus associated with signs resembling swine fever. Res. Vet. Sci., 45: 137-142.
100
Thur, B; Zlinszky, K and Ehrensperger, F (1996). Immuno-histochemical detection of bovine viral diarrhea virus in skin biopsies: a reliable and fast diagnostic tool. Zentral Veterin., 43: 163-166.
101
Uzal, FA; Plattner, BL and Hostetter, JM (2016). Alimentary system in pathology of domestic animals. In: Maxie, MG (Ed.), Jubb, Keneddy and Palmers pathology of domestic animals. (6th Edn.), Vol. 2, St. Louis, Missouri, Academic Press Inc., PP: 122-130.
102
Van Campen, H (2010). Epidemiology and control of BVD in the U.S. Vet. Microbiol., 14: 94-98.
103
Vilcek, S and Nettleton, PF (2006). Pestiviruses in wild animals. Vet. Microbiol., 116: 1-12.
104
Vilcek, S; Paton, DJ; Rowe, LW and Anderson, EC (2001). Typing of Pestiviruses from eland in Zimbabwe. J. Wildl. Dis., 36: 165-168.
105
Voges, H; Horner, GW; Rowe, S and Wellenberg, GJ (1998). Persistent bovine Pestivirus infection localized in the testes of an immuno-competent, non-viraemic bull. Vet. Microbiol., 61: 165-175.
106
Wilhelmsen, CL; Bolin, SR; Ridpath, JF; Cheville, NF and Kluge, JP (1991). Lesions and localization of viral antigen in tissues of cattle with experimentally induced or naturally acquired mucosal disease, or with naturally acquired chronic bovine viral diarrhea. Am. J. Vet. Res., 52: 269-275.
107
Wittum, TE; Grotelueschen, DM and Brock, KV (2001). Persistent bovine viral diarrhoea virus infection in U.S. beef herds. Prev. Vet. Med., 49: 83-94.
108
Youngl, NJ; Thomas, CJ; Collins, ME and Brownlie, J (2006). Real-time RT-PCR detection of bovine viral diarrhoea virus in whole blood using an external RNA reference. J. Virol. Methods. 138: 218-222.
109
Zimmer, GM; Van Maanen, C; De Goey, I; Brinkhof, J and Wentink, GH (2004). The effect of maternal antibodies on the detection of bovine virus diarrhoea virus in peripheral blood samples. Vet. Microbiol., 100: 145-149.
110
ORIGINAL_ARTICLE
Evaluation of amprolium and toltrazuril efficacy in controlling natural intestinal rabbit coccidiosis
This trial was undertaken with the objective to evaluate the efficacy of amprolium, toltrazuril and their combination in rabbits naturally infected with Eimeria species (32 × 103 ± 4.63 oocysts per gram (OPG) of faeces). Thirty-six rabbits (11 weeks old with average body weight (BW) 2000 ± 75 g), were randomly allocated into six groups (six kits each), namely, negative untreated and was retained as negative control (group 1), infected and kept untreated (group 2), treated with single oral dose of amprolium at 50 mg/kg BW for 5 days (group 3), received toltrazuril at 5 mg/kg BW for 2 days (group 4), treated orally with toltrazuril at 2.5 mg/kg BW, two doses with 5 day interval (group 5) and given oral doses of both amprolium and toltrazuril at 50 mg and 5 mg/kg BW (group 6), respectively. Clinical signs, mortalities, production data (feed consumption, feed conversion rate, BW, body weight gain (BWG), and performance index (PI)), OPG of faeces and the percentage of OPG reduction were recorded. The results indicated that both toltrazuril, amprolium and their concurrent use significantly (P<0.05) reduced OPG and effectively controlled coccidiosis related mortality, fully abolished the clinical signs, improved feed consumption, BW, weight gain and feed conversion rate. From the observations of the present study it can be concluded that the oral administration of both drugs and their combined use ameliorated the adverse impacts of intestinal coccidiosis in rabbits as therapeutic, but the concurrent use of both drugs was more superior.
https://ijvr.shirazu.ac.ir/article_4217_f5d52727892ca2e24897d1f43c1562fd.pdf
2017-09-01
164
169
10.22099/ijvr.2017.4217
Amprolium
Coccidiosis
Egypt
Rabbit
Toltrazuril
A.
El-Ghoneimy
1
Department of Pharmacology, Faculty of Veterinary Medicine, South Valley University, Qena, Egypt
AUTHOR
I.
El-Shahawy
dr.ismail_para@yahoo.com
2
Department of Parasitology, Faculty of Veterinary Medicine, South Valley University, Qena, Egypt
LEAD_AUTHOR
Abakar, AD; Seri, HI; Ismail, AA and Musa, HH (2005). Comparative efficacy of selected anticoccidial drug in Ambarorow sheep naturally infected with enteric coccidia in South Darfur, Sudan. Sudan J. Vet. Res., 20: 61-67.
1
Al-Quraishy, S (2012). Exogenous and endogenous stages of Eimeria perforans naturally infected domestic rabbit (Oryctolagus cuniculus) in Saudi Arabia: light microscopic study. Saudi J. Biol. Sci., 19: 31-34. doi: 10.1016/j.sjbs. 2011.09.003.
2
Balicka-Ramisz, A (1999). The usefulness of Baycox (Bayer) for coccidiosis control of lambs. Wiad. Parazytol., 45: 187-191.
3
Borenstein, M; Rothstein, H and Cohen, J (1997). Sample power: release 1.00. Chicago, IL: SPSS Inc.
4
Dowling, L (1992). Ionophore toxicity in chickens: a review of pathology and diagnosis. Avian Pathol., 21: 355-368.
5
Eckert, J; Taylor, M; Catchpole, J; Licois, D; Coudert, P and Bucklar, H (1995). Identification of Eimeria species and strains. Morphological characteristics of oocysts. In: Eckert, J; Braun, R; Shirley, MW and Coudert, P (Eds.), Biotechnology: Guidelines on Techniques in Coccidiosis Research. Office for Official Publications of the European Communities. Luxembourg. PP: 113-116.
6
González-Redondo, P; Finzi, A; Negretti, P and Micci, M (2008). Incidence of coccidiosis in different rabbit keeping systems. Arq. Bras. Med. Vet. Zootec., 60: 1267-1270.
7
Graat, EAM; Kooij, E; Frankena, K; Henken, AM; Smeets, JFM and Hekerman, MTJ (1998). Quantifying risk factors of coccidiosis in broilers using on-farm data based on a veterinary practice. Prev. Vet. Med., 33: 297-308.
8
Grèes, V; Voza, T; Chabaud, A and Landau, I (2003). Coccidiosis of the wild rabbit (Oryctolagus cuniculus) in France. Parasite. 10: 51-57.
9
Greuel, E and Ruhrmann, U (1986). Effectiveness of various dosage concentrations and administration times of Baycox® medication in experimental chicken coccidiosis in caged conditions. Dtsch. Tierztl. Wochenschr., 93: 29-33.
10
Grief, G (2000). Immunity to coccidiosis after treatment with toltrazuril. Parasitol. Res., 86: 787-790.
11
Hauptman, K; Tichy, F and Knotek, Z (2001). Clinical diagnostics of hepatopathies in small mammals: evaluation of importance of individual methods. Acta Vet. Brno., 70: 297-11. doi: 10.2754/avb200170030297.
12
Iqbal, A; Tariq, KA; Wazir, VS and Singh, R (2013). Antiparasitic efficacy of Artemisia absinthium toltrazuril and amprolium against intestinal coccidiosis in goats. J. Parasit. Dis., 37: 88-93.
13
Jithendran, KP and Bhat, TK (1996). Subclinical coccidiosis of Angora rabbits, a field survey in Himachal Pradesh, India. World Rabbit Sci., 4: 29-32.
14
McDougald, LR and Reid, WM (1997). Coccidiosis. In: Calnek, BW (Ed.), Diseases of poultry. (10th Edn.), USA, IowaStateUniversity, Press Ames. PP: 865-883.
15
Mehlhorn, H; Ortmann-Falkenstein, G and Haberkorn, A (1984). The effects of sym. Triazinones on developmental stages of Eimeria tenella, E. maxima and E. acervulina: a light and electron microscopical study. Z. Parasitenkd., 70: 173-182.
16
Morand-Fehr, P; Richard, A; Tessier, J and Hervieu, J (2002). Effects of decoquinate on the growth and milk performance of young female goats. Small Rumin. Res., 45: 109-114.
17
Moskey, HE and Harwood, PD (1941). Methods of evaluating the efficacy of antihelmintics. Am. J. Vet. Res., 2: 55-59.
18
Mukiibi-Muka, G; Otim, MO; Musisi, G; Illango, J; Galiwango, T and Olaho-Mukani, W (2001). Com-parative study on the efficacy of Diclazuril and Amprolium in naturally infected broilers in Uganda. Rev. Elev. Med. Vet. Pays Trop., 54: 33-35.
19
Mundt, HC; Daugschies, A; Uebe, F and Rinke, M (2003). Efficacy of toltrazuril against artificial infections with Eimeria bovis in calves. Parasitol. Res., 3: S166-S167. doi: 10.1007/s00436-003-0929-z.
20
North, MO (1984). Commercial chicken production manual. 3rd Edn., California, USA, AVI Publishing Company. P: 710.
21
Oncel, T; Gulegen, E; Senlik, B and Bakirci, S (2011). Intestinal coccidiosis in angora rabbits (Oryctolagus cuniculus) caused by Eimeria intestinalis, Eimeria perforans and Eimeria coecicola. YYU Veteriner. Fakultesi. Dergisi., 22: 27-29.
22
Paklandl, M (2009). Coccidia of rabbit: a review. Folia Parasitol., 56: 153-166.
23
Peek, HW and Landman, WJM (2003). Resistance to anticoccidial drugs of Dutch avian Eimeria spp. field isolates originating from 1996, 1999 and 2001. Avian Pathol., 32: 391-401.
24
Peeters, JE and Geeroms, R (1986). Efficacy of toltrazuril against intestinal and hepatic coccidiosis in rabbits. Vet. Parasitol., 22: 21-35.
25
Pritchard, MH and Kruse, GO (1982). The collection and preservation of animal parasites. Technical Bulletin No. 1. The Harold W. Manter Laboratory, University of Nebraska Press. PP: 120-141.
26
Redrobe, SP; Gakos, G; Elliot, SC; Saunders, R; Martin, S and Morgan, ER (2010). Comparison of toltrazuril and sulphadimethoxine in the treatment of intestinal coccidiosis in pet rabbits. Vet. Rec., 167: 287-290. doi: 10.1136/vr. c3453.
27
Shameem, H; Devada, K and Mammen, AJ (2011). Clinico-pathological effects of intestinal coccidiosis in rabbits. Indian J. Vet. Pathol., 35: 215-216.
28
Singla, LD; Juyal, PD and Sandhu, BS (2000). Pathology and therapy in naturally Eimeria stiedae infected rabbits. J. Protozool. Res., 10: 185-191.
29
Svensson, C (1998). Prevention of Eimeria alabamensis coccidiosis by along-acting baquiloprim/sulphadimidine bolus. Vet. Parasitol., 74: 143-152.
30
Taylor, MA; Coop, RL and Wall, RL (2007). Veterinary parasitology. 3rd Edn., Oxford, UK, Blackwell Publishing. PP: 1385-1398.
31
Zulpo, DL; Peretti, J; Ono, LM; Longhi, E; Oliveira, MR; Guimaraes, IG; Headley, SA; Junior, J and Garcia, JL (2007). Pathogenicity and histopathological, observations of commercial broiler chicks experimentally infected with isolates of Eimeria tenella, E. acervulina and E. maxima. Semin: Ciênc. Agrár., 28: 97-104.
32
ORIGINAL_ARTICLE
Hypervitaminosis D3 in broiler chicks: histopathological, immunomodulatory and immunohistochemical approach
The present study was undertaken to investigate the toxic effects of higher doses (1,00,000 IU i.e. 2.5 mg/kg body weight (BW)) of vitamin D3, concomitantly with bacterial endotoxins (lipopolysaccharides: LPS) to study the immunomodulatory potential of vitamin D3 in IBL-80 broiler chicks. The chicks were divided into four groups [group I (NSS), group II (LPS), group III (Vit. D3 + NSS), and group IV (Vit. D3 + LPS)] containing eight chicks in each group, treated accordingly for 21 days. Birds were kept under close observation for apparent clinical signs and symptoms. Clinically, vitamin D3 treated chicks were dull, off feed, showed polydipsia, polyuria, watery faeces, rigidity of limbs, severe dehydration, weakness and significant progressive emaciation. Grossly, the bones were soft whereas most organs revealed congestion and hemorrhages in visceral organs. Histopathologically, renal tubular epithelium showed coagulative necrosis and metastatic calcification. The lung parenchyma and bronchi showed hemorrhages, congestion with diffuse heterophilic cell infiltration in inter-alveolar septa and infiltration of heterophils in alveoli along with proteinacious fluid in LPS treated chicks of treatment group, suggesting immunomodulatory action of vitamin D3. Vitamin D3 treated chicks showed strong expression of Calbindin D28k in intestine and kidney but weak expression in lung, which can be linked to nephrocalcinosis seen in kidney and from its prospective role in cellular calcium homeostasis.
https://ijvr.shirazu.ac.ir/article_4218_8f6cd677af94e1fedc248508dcec6654.pdf
2017-09-01
170
176
10.22099/ijvr.2017.4218
Broiler chick
Calbindin D28K
Cholecalciferol
Immunomodulation
LPS
R.
Kumar
rahulpoultrypatho@gmail.com
1
MVSc Scholar in Veterinary Pathology, Department of Veterinary Pathology, Guru Angad Dev Veterinary and Animal Sciences University, Ludhiana-141004, Punjab, India
LEAD_AUTHOR
R. S.
Brar
2
Department of Veterinary Pathology, Guru Angad Dev Veterinary and Animal Sciences University, Ludhiana-141004, Punjab, India
AUTHOR
H. S.
Banga
3
Department of Veterinary Pathology, Guru Angad Dev Veterinary and Animal Sciences University, Ludhiana-141004, Punjab, India
AUTHOR
Abbas, AK; Lichtman, AH and Pober, JS (1997). Cytokines. In Cellular and molecular immunology. (3rd Edn.), Philadelphia, W. B. Saunders. PP: 250-276.
1
Baker, DH; Biehl, RR and Emmert, JL (1998). Vitamin D3 requirement of young chicks receiving diets varying in calcium and available phosphorus. Bri. Poult. Sci., 39: 413-417.
2
Beasley, VR (1999). Veterinary toxicology. International Veterinary Information Service (www.ivis.org), Ithaca, New York.
3
Braun, U; Diener, M; Camezind, D; Fluckiger, R and Thoma, R (2000). Enzooticcalcinosis in goats caused by golden oat grass (Trisetum flavescens). Vet Rec., 5: 161-162.
4
Christakos, S; Brunette, MG and Norman, AW (1981). Localization of immunoreactive vitamin D-dependent calcium binding protein in chick nephron. Endocrinology. 109: 322-324.
5
Driver, JP; Pesti, GM; Bakalli, RI and Edwards, JrHM (2005). Calcium requirements of the modern broiler chicken as influenced by dietary protein and age. Poult. Sci., 84: 1629-1639.
6
Edwards, HM and Sorensen, UP (1987). Effect of short fasts on the development of tibial dyschondroplasia in chickens. J. Nutr., 117: 194-200.
7
Harrington, DD and Page, EH (1983). Acute vitamin D3 toxicosis in horses: case reports and experimental studies of comparative toxicity of vitamins D2 and D3. J. Am. Vet. Med. Assoc., 182: 1358-1369.
8
Hass, GM; Trueheart, RE; Taylor, CB and Stumpe, M (1958). An experimental histologic study of hyper-vitaminosis D. Am. J. Pathol., 34: 395-431.
9
Hunt, RD; Garcia, FG and Walsh, RJ (1972). A comparison of the toxicity of ergocalciferol and cholecalciferol in Rhesus monkeys (Macaca mulatta). J. Nutr., 102: 975-986.
10
Jande, SS; Maler, L and Lawson, DEM (1981b). Immunohistochemical mapping of vitamin D-dependent calcium-binding protein in brain. Nature. 294: 765-770.
11
Jande, SS; Tolnai, S and Lawson, DEM (1981a). Immunohistochemical localization of vitamin D-dependant calcium binding protein in duodenum, kidney, uterus and cerebellum of chickens. Histochemtry. 71: 99-116.
12
Jubb, KVF and Kennedy, PC (1970). Theosteo-dystrophy of poisoning by vitamin D. In: Jubb, KVF and Carleton, P, Pathology of domestic animals. (2nd Edn.), Vol. 1, New York, Academic Press. PP: 40-43.
13
Kaneko, JJ; Harvey, JW and Bruss, ML (2008). In avian clinical biochemistry, Chapter 28. In: Kaneko, JJ; Harvey, JW and Bruss, ML (Eds.), Clinical biochemistry of domestic animals. (6th Edn.), San Diego, Academic Press Inc., P: 861.
14
Kasim, S; Blake, BL and Fan, X (2006). The role of dopamine receptors in the neurobehavioral syndrome provoked by activation of L-type calcium channels in rodents. Dev. Neurosci., 28: 505-517.
15
Kirui, NA; Weisbrode, SE and Kindig, OR (1981). The role of dietary calcium on the development of soft tissue mineralization due to 1,25-dihydroxyvitamin D3 intoxi-cation in rats. Virchows Archives. Cell Pathol., 37: 251-263.
16
Korver, D (2005). Research, analytical techniques and practical experiences using HyDTM. In: Arkansas Nutrition Conference, Arkansas. P: 12.
17
Long, GG (1984). Acute toxicosis in swine associated with excessive dietary intake of vitamin D. JAVMA. 184: 164-170.
18
Lorenzoni, AG; Erf, GF; Rath, NC and Wideman, RFJr (2008). Cellular component of lavage fluid from broilers with normal versus aerosol-primed airways. Poult. Sci., 88: 303-308.
19
Machlin, LJ (1984). Handbook of vitamins. Marcel Dekker, Inc., New York, Meric, SM (1995). In: Ettinger, SJ and Feldman, EC (Eds.), Textbook of internal medicine. (6th Edn.), Philadelphia, Saunders. PP: 159-163.
20
Metz, AL; Walser, MM and Olsen, WC (1985). The interaction of dietary vitamin A and vitamin D related to skeletal development in the turkey poult. J. Nutr., 115: 929-935.
21
Morita, T; Awakura, T; Shimada, A; Umemura, T; Nagai, T and Haruna, A (1995). Vitamin D toxicosis in cats: natural outbreak and experimental study. J. Vet. Med. Sci., 57: 831-837.
22
Morrissey, RL; Cohn, RM; Empson Jr, RN; Greene, HL; Taunton, OD and Ziporin, ZZ (1977). Relative toxicity and metabolic effects of cholecalciferol and 25-hydroxycholecalciferol in chicks. J. Nutr., 107: 1027-1034.
23
Morrow, C (2001). Cholecalciferol poisoning. J. Vet. Med., 12: 905-911.
24
Mulligan, RM and Stricker, FL (1948). Metastatic calcifi-cation produced in dogs by hypervitaminosis D and haliphagia. Am. J. Pathol., 24: 451-473.
25
Nain, S; Laarveld, B; Wojnarowicz, C and Olkowski, AA (2007). Excessive dietary vitamin D supplementation as a risk factor for sudden death syndrome in fast growing commercial broilers. Comp. Biochem. Physiol. A MolIntegr. Physiol., 148: 828-833.
26
Norman, AW (1985). The vitamin D endocrine system. Physiologist. 28: 219-232.
27
Price, PA; Buckley, JR and William, MK (2001). The amino bisphosphonate ibandronate prevents vitamin D induced calcification of arteries, cartilage, lungs and kidneys in rats. J. Nutr., 131: 2910-2915.
28
Radostits, OM; Gay, CC; Blood, DC and Hinchcliff, KW (2000). Veterinary medicine - A textbook of the diseases of cattle, sheep, pigs, goats and horses. 9th Edn., PP: 561, 563, 1543, 1642. Book Power (formerly ELST), UK.
29
Rennie, JS and Whitehead, CC (1996). Effectiveness of dietary25-and1-hydroxy colecalciferol in combating tibialdyschondroplasia in broiler chickens. Bri. Poult. Sci., 37: 413-421.
30
Roberson, RJ; Swecker, WS and Hullender, LL (2000). Hypercalcemia and hypervitaminosis D in two lambs. J. Am. Vet. Med. Assoc., 216: 1115-1118.
31
Roeder, DJ; Lei, M and Morrison, DC (1989). Endotoxic-lipopolysaccharide-specific binding protein on lymphoid cells of various animal species: association with endotoxin susceptibility. Infect. Immun., 57: 1054-1058.
32
Roth, J; Thorens, B; Hunziker, W and Norman, AW (1981). Vitamin D-dependent calcium binding protein: immunocytochemical localization in chick kidney. Science. 214: 197-200.
33
Sandhu, HS and Brar, RS (2009). Textbook of veterinary toxicology. 2nd Edn., Ludhiana, Kalyani Publishers. P: 245.
34
Scott, ML; Austic, RE and Cries, CL (1978). Hyper-vitaminosis D. In: Hofsted, MS; Calnek, BW; Helmboldt, CF; Reid, WM and Yoder, HWJr (Eds.), Diseases of poultry. (6th Edn.), Ames, IA, IowaStateUniversity Press. P: 58.
35
Stevenson, RG; Palmer, NC and Finley, GG (1976). Hypervitaminosis D in rabbits. Can. Vet. J., 17: 54-57.
36
Taylor, AN; Mcintosh, JE and Bourdeau, JE (1982). Immunocytochemical localization of vitamin D-dependent calcium-binding protein in renal tubules of rabbit, rat, and chick. Kidney Int., 21: 765-773.
37
Yarger, JG; Saunders, CA; McNaughton, JL; Quarles, CL; Hollis, BW and Gray, RW (1995a). Comparison of dietary 25-hydroxycholecalciferol and cholecalciferolin broiler chickens. Poult. Sci., 74: 1159-1167.
38
ORIGINAL_ARTICLE
Prevalence of Campylobacter jejuni and Campylobacter coli in captive wildlife species of India
Campylobacteriosis is an important zoonotic disease and the prevalence of Campylobacter is largely unknown in the wildlife of India. A total of 370 samples, comprising of 314 fresh faecal samples from apparently healthy captive wild animals and birds, 30 stool swabs from animal care takers and 26 samples of the animals’ food and water were collected from G. B. Pant High Altitude Zoo, Nainital, Kanpur Zoo, Wildlife Park, IVRI and the Post Graduate Research Institute in Animal Sciences (PGRIAS), Chennai, Tamilnadu from August 2014 to May 2015. Samples were processed for cultural isolation, direct PCR and multiplex PCR for species confirmation. To decipher the genetic diversity, the 16S rRNA gene was amplified, sequenced and analyzed. Based on isolation, the overall occurrence rate of Campylobacter spp. was 0.8% (3/370), being 2.94% (3/102) for captive wild birds. Three Campylobacter jejuni were isolated from silver pheasants, lady amherest pheasants and saras cranes. Direct PCR assay showed the overall occurrence rate of Campylobacter spp. to be 4.77% (15/315), being 1.58% (2/126) for captive wild ruminants, 5.81% (5/86) for non-ruminants and 7.84% (8/102) for birds. All the isolates were identified as C. jejuni.
https://ijvr.shirazu.ac.ir/article_4219_0cbde722b6a9d4068dd543ab11427276.pdf
2017-09-01
177
182
10.22099/ijvr.2017.4219
Campylobacter coli
Campylobacter jejuni
Captive wildlife
India
Zoo
A. A.
Prince Milton
1
Division of Veterinary Public Health, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
AUTHOR
R. K.
Agarwal
grace_bly@yahoo.com
2
Division of Bacteriology and Mycology, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
LEAD_AUTHOR
G. B.
Priya
3
Division of Bacteriology and Mycology, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
AUTHOR
M.
Saminathan
4
Division of Pathology, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
AUTHOR
M.
Aravind
5
Department of Veterinary Parasitology, Madras Veterinary College, TANUVAS, Chennai-600007, Tamilnadu, India
AUTHOR
A.
Reddy
6
Division of Veterinary Public Health, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
AUTHOR
C. K.
Athira
7
Division of Veterinary Public Health, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
AUTHOR
P.
Anjay
8
Division of Veterinary Public Health, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
AUTHOR
T. P.
Ramees
9
Division of Veterinary Public Health, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
AUTHOR
K.
Dhama
10
Division of Pathology, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
AUTHOR
A. K.
Sharma
11
Division of Pathology, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
AUTHOR
A.
Kumar
12
Division of Veterinary Public Health, ICAR-Indian Veterinary Research Institute, Izatnagar, Bareilly-243 122, Uttar Pradesh, India
AUTHOR
Adesiyun, AA; Caeser, K and Inder, L (1998b). Prevalence of Salmonella and Campylobacter infections in animals at Emperor Valley Zoo, Trinidad, American Association of Zoo Veterinarians. J. Zoo Wildl. Med., 29: 237-239.
1
Adesiyun, AA; Seepersadsingh, N; Inder, L and Caesar, K (1998a). Some bacterial enteropathogens in wildlife and racing pigeons from Trinidad. J. Wildl. Dis., 34: 73-80.
2
Bengis, RG; Leighton, FA; Fischer, JR; Artois, M; Morner, T and Tate, CM (2004). The role of wildlife in emerging and re-emerging zoonoses. Rev. Sci. Tech., 23: 497-511.
3
Broman, T; Waldenstrom, J; Dahlgren, D; Carlsson, I; Eliasson, I and Olsen, B (2004). Diversities and similarities in PFGE profiles of Campylobacter jejuni isolated from migrating birds and humans. J. Appl. Microbiol., 96: 834-843.
4
Cody, AJ; McCarthy, ND; Bray, JE; Wimalarathna, HM; Colles, FM; Jansen van Rensburg, MJ; Dingle, KE; Waldenstrom, J and Maiden, MC (2015). Wild bird associated Campylobacter jejuni isolates are a consistent source of human disease, in Oxfordshire, United Kingdom. Environ. Microbiol. Rep., 7: 782-788. Colles, FM; Ali, JS; Sheppard, SK; McCarthy, ND and Maiden, MCJ (2011).Campylobacter populations in wild and domesticated Mallard ducks (Anas platyrhynchos).Environ. Microbiol. Rep., 3: 574-580.
5
Colles, FM; Dingle, KE; Cody, AJ and Maiden, MC (2008). Comparison of Campylobacter populations in wild geese with those in starlings and free range poultry on the same farm. Appl. Environ. Microbiol., 74: 3583-3590.
6
Dhama, K; Karthik, K; Chakraborty, S; Tiwari, R and Kapoor, S (2013). Wildlife: a hidden warehouse of zoonosis - a review. Int. J. Curr. Res., 5: 1866-1879.
7
Haagsma, JA; Siersema, PD; De Wit, NJ and Havelaar, AH (2010). Disease burden of post-infectious irritable bowel syndrome in the Netherlands. Epidemiol. Infect., 138: 1650-1656.
8
Hald, B; Skov, MN; Nielsen, EM; Rahbek, C; Madsen, JJ; Waino, M; Chriél, M;Nordentoft, S; Baggesen, DL and Madsen, M (2016). Camylobacter jejuni and Campylo-bacter coli in wild birds on Danish livestock farms. Acta Vet. Scand., 58: 11.
9
Hoar, BM; Whiteside, DP; Ward, L; Inglis, DG and Morck, DW (2007). Evaluation of the enteric microflora of captive whooping cranes (Grus americana) and sandhill cranes (Grus canadensis). Zoo Biol., 26: 141-153.
10
Hollamby, S; Sikarskie, JG and Stuht, J (2003). Survey of peafowl (Pavo cristatus) for potential pathogens at three Michigan zoos. J. Zoo Wildl. Med., 34: 375-379.
11
ISO 1072-1:2006. Microbiology of food and animal feeding stuffs- Horizontal method for detection and enumeration of Campylobacter spp. Part 1: Detection method.
12
Ito, K; Kubokura, Y; Kaneko, K; Totake, Y and Ogawa, M (1988). Occurrence of Campylobacter jejuni in free-living wild birds from Japan. J. Wildl. Dis., 24: 467-470.
13
Kapperud, G; Espeland, G; Wahl, E; Walde, A; Herikstad, H; Gustavsen, S; Tveit, I; Natas, O; Bevanger, L and Digranes, A (2003). Factors associated with increased and decreased risk of Campylobacter infection: a prospective case-control study in Norway. Am. J. Epidemiol., 158: 234-242.
14
Kapperud, G and Rosef, O (1983). Avian wildlife reservoir of Campylobacter fetus subsp. jejuni, Yersinia sp., and Salmonella sp. in Norway. Appl. Environ. Microbiol., 45: 375-380.
15
Keller, JI; Shriver, WG; Waldenström, J; Griekspoor, P and Olsen, B (2011). Prevalence of Campylobacter in wild birds of the Mid-Atlantic region, USA. J. Wildl. Dis., 47: 750-754.
16
Klena, JD; Parker, CT; Knibb, K; Ibbitt, JC; Devane, PM; Horn, ST and Konkel, ME (2004). Differentiation of Campylobacter coli, Campylobacter jejuni, Campylobacter lari, and Campylobacter upsaliensis by a multiplex PCR developed from the nucleotide sequence of the lipid A gene lpxA. J. Clin. Microbiol., 42: 5549-5557.
17
Koga, T; Aoki, W; Mizuno, T; Wakazono, K; Ohno, J; Nakai, T; Nomiya, T; Fujii, M; Fusegawa, K; Kinoshita, K; Hamada, T and Ikeda, Y (2015). Antimicrobial resistance in Campylobacter coli and Campylobacter jejuni in cynomolgus monkeys (Macaca fascicularis) and eradication regimens. J. Microbiol. Immunol. Infect., 50: 75-82.
18
Ling, YE; Saleha, AA and Jalila, A (2012). Detection of Campylobacter and Salmonella in ostrich. J. Vet. Malaysia. 24: 6-8.
19
Linton, D; Lawson, AJ; Owen, RJ and Stanley, J (1997). PCR detection, identification to species level, and fingerprinting of Campylobacter jejuni and Campylobacter coli direct from diarrheic samples. J. Clin. Microbiol., 35: 2568-2572.
20
Marin, C; Palomeque, M; Marco-Jiménez, F and Vega, S (2014). Wild griffon vultures (Gyps fulvus) as a source of Salmonella and Campylobacter in eastern Spain. PLoS One., 9: e94191.
21
Mohan, V (2015). Faeco-prevalence of Campylobacter jejuni in urban wild birds and pets in New Zealand. BMC Res. Notes. 8: 1.
22
Rosef, O; Gondrosen, B; Kapperud, G and Underdal, B (1983). Isolation and characterization of Campylobacter jejuni and Campylobacter coli from domestic and wild animals in Norway. Appl. Environ. Microbiol., 46: 855-859.
23
Singh, H; Rathore, RS; Singh, S and Cheema, PS (2011). Comparative analysis of cultural isolation and PCR based assay for detection of Campylobacter jejuni in food and faecal samples. Braz. J. Microbiol., 42: 181-186.
24
Sippy, R; Sandoval-Green, CM; Sahin, O; Plummer, P; Fairbanks, WS; Zhang, Q and Blanchong, JA (2012). Occurrence and molecular analysis of Campylobacter in wildlife on livestock farms. Vet. Microbiol., 157: 369-375.
25
Stoddard, RA; Gulland, FMD; Atwill, ER; Lawrence, J; Jang, S and Conrad, PA (2005). Salmonella and Campylobacter spp. in northern elephant seals, California. Emerg. Infect. Dis., 11: 1967-1969.
26
Waldenstrom, J; Broman, T; Carlsson, I; Hasselquist, D; Achterberg, RP; Wagenaar, JA and Olsen, B (2002). Prevalence of Campylobacter jejuni, Campylobacter lari, and Campylobacter coli in different ecological guilds and taxa of migrating birds. Appl. Environ. Microbiol., 68: 5911-5917.
27
Waldenstrom, J; On, SL; Ottvall, R; Hasselquist, D and Olsen, B (2007). Species diversity of Campylobacteria in a wild bird community in Sweden. J. Appl. Microbiol., 102: 424-432.
28
Yogasundram, K; Shane, SM and Harrington, KS (1989). Prevalence of Campylobacter jejuni in selected domestic and wild birds in Louisiana. Avian Dis., 33: 664-667.
29
ORIGINAL_ARTICLE
Comparison of diagnostic tests for the detection of bovine brucellosis in the natural cases of abortion
Rapid and precise diagnosis in natural field cases of bovine abortion caused by Brucella abortus warrants the use of the most sensitive and reliable diagnostic methods. In the present study, bacterial isolation, serology, gross, histopathology, immunohistochemistry and polymerase chain reaction technique(s) were applied. Sero-prevalence studies showed the rate of 28.86% positive cases using the competitive ELISA. Histopathological changes were mainly seen in the placenta, fetal lungs, kidney, liver and spleen. Immunohistochemical (IHC) staining of Brucella spp. was evident as brown, finely granular intracytoplasmic staining in trophoblasts of placental sections and in section(s) of liver, lung, kidney and spleen. Twenty-eight out of the 103 samples (17 from stomach contents, 3 from placental cotyledons, 2 from vaginal discharges and 6 from pooled fetal tissues) produced 193 bp amplicon specific for Brucella genus. Moreover, the species-specific primers amplified a 498 bp amplicon which corresponded to B. abortus. Comparison of diagnostic tests revealed PCR and IHC provide a reliable test for the diagnosis of bovine brucellosis in aborted fetal tissue and placental cotyledons whereas serology is most important for detection of Brucella positive animals in a herd.
https://ijvr.shirazu.ac.ir/article_4220_85116857b52aba83c0b7859ba843dacd.pdf
2017-09-01
183
189
10.22099/ijvr.2017.4220
Abortion
Brucellosis
Immunohistochemistry
Polymerase chain reaction
V.
Mahajan
mahajanv17@gmail.com
1
Department of Animal Disease Research Centre, Guru Angad Dev Veterinary and Animal Sciences University, Ludhiana-141004, Punjab, India
LEAD_AUTHOR
H. S.
Banga
2
Department of Veterinary Pathology, Guru Angad Dev Veterinary and Animal Sciences University, Ludhiana-141004, Punjab, India
AUTHOR
G.
Filia
3
Department of Animal Disease Research Centre, Guru Angad Dev Veterinary and Animal Sciences University, Ludhiana-141004, Punjab, India
AUTHOR
M. P.
Gupta
4
Department of Veterinary and Animal Husbandry Extension, Guru Angad Dev Veterinary and Animal Sciences University, Ludhiana-141004, Punjab, India
AUTHOR
K.
Gupta
5
Department of Veterinary Pathology, Guru Angad Dev Veterinary and Animal Sciences University, Ludhiana-141004, Punjab, India
AUTHOR
Agrawal, R; Kumar, M and Singh, JL (2007). Sero-prevalence of brucellosis in Uttranchal. Indian Vet. J., 84: 204-205.
1
Alton, GG; Jones, LM and Pietz, DE (1975). Laboratory techniques in brucellosis. Monograph Series. World Health Organization, Geneva, Switzerland.
2
Anderson, ML (2007). Infectious causes of bovine abortion during mid to late gestation. Theriogenology. 68: 474-486.
3
Aulakh, HK; Patil, PK; Sharma, S; Kumar, H; Mahajan, V and Sandhu, KS (2008). A study on the epidemiology of bovine brucellosis in Punjab (India) using Milk-ELISA. Acta Vet. Brno., 77: 393-399.
4
Bricker, BJ (2002). PCR as a diagnostic tool for brucellosis. Vet. Microbiol., 90: 435-446.
5
Bricker, BJ and Halling, SM (1994). Differentiation of Brucella abortus bv. 1, 2 and 4, Brucella melitensis, Brucella ovis and Brucella suisbv 1 by PCR. J. Clin. Microbiol., 32: 2660-2666.
6
Cameron, A (1999). Survey Toolbox for Livestock Diseases -A Practical Manual and Software Package for Active Surveillance in Developing Countries. Australian Centre for International Agricultural Research Monograph. P: 330.
7
Chand, P and Sharma, AK (2004). Situation of brucellosis in bovines at organized cattle farms belonging to three different states. J. Immunol. Immunopathol., 6: 11-15.
8
Cortez, A; Scareelli, E; Soares, RM; Heinemann, MB; Sakamoto, SM; Genovez, ME; Ferreira, F and Richtzenhain, LJ (2001). Detection of Brucella DNA from aborted bovine fetuses by polymerase chain reaction. Aust. Vet. J., 79: 500-501.
9
Gall, D and Nielsen, K (2004). Serological diagnosis of bovine brucellosis: a review of test performance and cost comparison. Rev. Sci. Tech. Off. Int. Epiz., 23: 989-1002.
10
Geresu, MA and Kassa, GM (2016). A review on diagnostic methods of brucellosis. J. Veterinar. Sci. Techno., 7: 323.
11
Ilhan, Z; Aksakal, A; Ekin, IH; Gulhan, T; Solmaz, H and Erdenlig, S (2008). Comparison of culture and PCR for the detection of Brucella melitensis in blood and lymphoid tissues of serologically positive and negative slaughtered sheep. Lett. Appl. Microbiol., 46: 301-306.
12
Keid, LB; Soares, RM; Vasconcellos, SA; Chiebao, DP; Megid, J; Salgado, VR and Richtzenhain, LJ (2007). A polymerase chain reaction for the detection of Brucella canis in semen of naturally infected dogs. Theriogenology. 67: 1203-1210.
13
Leal-Klevezas, DS; Martínez-Vázquez, IO; García-Cantu, J; López-Merino, A and Martínez-Soriano, JP (1995). Single-step PCR for detection of Brucella spp. from blood and milk of infected animals. J. Clin. Microbiol., 33: 3087-3090.
14
Leuenberger, R; Boujon, P; Thür, B; Miserez, R; Garin-Bastuji, B; Rüfenacht, J and Stärk, KD (2007). Prevalence of classical swine fever, Aujeszky’s disease and brucellosis in a population of wild boar in Switzerland. Vet. Rec., 160: 362-368.
15
López, A; Hitos, F; Perez, A and Navarro-Fierro, RR (1984). Lung lesions in bovine fetuses aborted by Brucella abortus. Can. J. Comp. Med., 48: 275-277.
16
Luna, LG (1968). Manual of histologic staining methods of the Armed Forces Institute of Pathology. 3rd Edn., New York, McGraw-Hill. PP: 32-39.
17
Meador, VP and Deyoe, BL (1989). Intracellular localization of Brucella abortus in bovine placenta. Vet. Pathol., 26: 513-515.
18
Meador, VP; Deyoe, BL and Cheville, NF (1989). Pathogenesis of Brucella abortus infection of the mammary gland and supramammary lymph node of the goat. Vet. Pathol., 26: 357-368.
19
Meador, VP; Tabatabai, LB; Hagemoser, WA and Deyoe, BL (1986). Identification of Brucella abortus in formalin fixed, paraffin embedded tissues of cows, goats, and mice with an avidin biotin peroxidase complex immuno-enzymatic staining technique. Am. J. Vet. Res., 47: 2147-2150.
20
Muñoz, PM; Marín, CM; Monreal, D; González, D; Garin-Bastuji, B; Díaz, R; Mainar-Jaime, RC; Moriyón, I and Blasco, JM (2005). Efficacy of several serological tests and antigens for diagnosis of bovine brucellosis in the presence of false positive serological results due to Yersinia enterocolitica O: 9. Clin. Diagn. Lab. Immunol., 12: 141-151.
21
Nielsen, K (2002). Diagnosis of brucellosis by serology. Vet. Microbiol., 90: 447-459.
22
Paweska, JT; Potts, AD; Harris, HJ; Smith, SJ; Viljoen, GJ; Dungu, B; Brett, OL; Bubb, M and Prozesky, L (2002). Validation of an indirect enzyme-linked immunosorbent assay for the detection of antibody against Brucella abortus in cattle sera using an automated ELISA workstation. Onderstepoort. J. Vet. Res., 69: 61-77.
23
Pérez, J; Quezada, M; Lopez, J; Casquet, O; Sierra, MA and Martin De Las Mulas, J (1998). Immuno-histochemical detection of Brucella abortus antigens in tissues from aborted bovine fetuses using commercially available polyclonal antibody. J. Vet. Diagn. Invest., 10: 17-21.
24
Poester, FP; Samartino, LE and Lage, AP (2005). Diagnóstico da brucelose bovina. Cad. Téc. Vet. Zootec., 47: 13-29.
25
Rahman, MS; Faruk, MO; Her, M; Kim, JY; Kang, SI and Jung, SC (2011). Prevalence of brucellosis in ruminants in Bangladesh. Vet. Med. Czech., 56: 379-385.
26
Rahman, MA; Islam, MS; Alam, MGS and Shamsuddin, M (1997). Seroprevalence of Brucellosis in the buffalo of a selected area in Bangladesh. Buff. J., 2: 209-214.
27
Richtzenhain, LJ; Cortez, A; Heinemann, MB; Soares, RM; Sakamoto, SM; Vasconcellos, SA; Higa, ZM; Scarcelli, E and Genovez, ME (2002). A multiplex PCR for the detection of Brucella spp. and Leptospira spp. DNA from aborted bovine fetuses. Vet. Microbiol., 87: 139-147.
28
Samartino, LE and Enright, FM (1993). Pathogenesis of abortion of bovine brucellosis. Comp. Immunol. Microbiol. Infect. Dis., 16: 95-101.
29
Sandhu, KS; Filia, G; Sharma, DR; Dhand, NK; Singh, J and Saini, SS (2001). Prevalence of brucellosis among dairy animals of Punjab. Indian J. Comp. Microbiol. Immunol. Infect. Dis., 22: 160-161.
30
Sharma, S; Alka; Mahajan, V; Verma, S; Kaur, K; Meenakshi and Kumar, H (2007). Screening of dairy farms of Punjab (India) for brucellosis and para-tuberculosis. Indian Vet. J., 84: 315-316.
31
Singh, G; Sharma, DR; Sandhu, KS and Dhand, NK (2002). Economic losses occurring due to bovine abortions in Punjab. In: 10th International Congress of Asian-Australasian Association of Animal Production Societies. 23-27 September. Ashoka Hotel, New Delhi. Indian Association of Animal Production and World Buffalo Trust, New Delhi, India.
32
Surucuoglu, S; Sibel, El; Ural, S; Gazi, H; Kurutepe, S; Taskiran, P and Yurtsever, SG (2009). Evaluation of real-time PCR method for rapid diagnosis of brucellosis with different clinical manifestations. Pol. J. Microbiol., 58: 15-19.
33
Zamri-Saad, M and Kamarudin, MI (2016). Control of animal brucellosis: the Malaysian experience. Asian Pac. J. Trop. Med., 9: 1136-1140.
34
ORIGINAL_ARTICLE
Fiber gene based molecular and biological characterization of hydropericardium-hepatitis syndrome associated avian adenoviruses
This study was designed to perform biological and molecular characterization of avian adenoviruses (AAVs) recovered from suspected cases of hydropericardium-hepatitis syndrome (HHS) in commercial poultry. Initially the samples were screened by Agar Gel Precipitation Test (AGPT) for the presence of AAVs followed by its confirmation and typing through polymerase chain reaction (PCR) focusing on already reported serotypes AAV-4, AAV-8 and AAV-10 elsewhere. These PCR-positive samples were further subjected to amplification of fiber gene, followed by conducting restriction fragment length polymorphism (RFLP) using restriction enzyme Alu. The selected isolates were further propagated through cell culture and pathogenic potential of selected isolates was determined by infecting chickens. In this study, out of a total 190 samples, 57.8% of suspected cases were found positive for AAV presence through AGPT while sub-type identification using PCR revealed 46.3% for these viruses belonging to AAV-4, 41.8% to AAV-8 and 11.8% showed co-infection of AAV-4 and AAV-8. AAV-10 was not detected in any of the tested samples. On the basis of RFLP pattern, AAV-4 isolates were further divided into four sub-groups (A-D) while AAV-8 isolates had identical RFLP pattern. To further evaluate the pathogenic potential of these sub-groups of AAV-4 isolates, specific pathogen free (SPF) chicks were challenged with selected isolates belonging to each of the sub-groups, resulting in variable pattern of pathogenicity. It is concluded that any variation in the fiber gene of AAV-4 isolates may affect its pathogenicity and eventually specificity of the vaccines used against such infections. Therefore, regular monitoring of the circulating AAV serotypes may be helpful in understanding the pathogenic potential of emerging AAVs, which may lead to development of more effective response strategies accordingly.
https://ijvr.shirazu.ac.ir/article_4221_ab67457e92bf282d89838c1c34bb276d.pdf
2017-09-01
190
196
10.22099/ijvr.2017.4221
Avian adenoviruses
Inclusion body hepatitis
Hydropericardium-hepatitis syndrome
Hydropericardium syndrome
S.
Yasmeen
1
Mphil in Animal Genomics and Biotechnology, National Reference Lab for Poultry Diseases, Animal Sciences Institute, National Agricultural Research Centre, Islamabad-45500, Pakistan
AUTHOR
N.
Siddique
naila.nrlpd@gmail.com
2
National Reference Lab for Poultry Diseases, Animal Sciences Institute, National Agricultural Research Centre, Islamabad-45500, Pakistan
LEAD_AUTHOR
M.
Athar Abbas
3
National Reference Lab for Poultry Diseases, Animal Sciences Institute, National Agricultural Research Centre, Islamabad-45500, Pakistan
AUTHOR
A.
Ali
4
National Reference Lab for Poultry Diseases, Animal Sciences Institute, National Agricultural Research Centre, Islamabad-45500, Pakistan
AUTHOR
S.
Rafique
5
Ph.D. Scholar, National Reference Lab for Poultry Diseases, Animal Sciences Institute, National Agricultural Research Centre, Islamabad-45500, Pakistan
AUTHOR
F.
Rashid
6
National Reference Lab for Poultry Diseases, Animal Sciences Institute, National Agricultural Research Centre, Islamabad-45500, Pakistan
AUTHOR
A. U.
Shah
7
MSc in Biotechnology, National Reference Lab for Poultry Diseases, Animal Sciences Institute, National Agricultural Research Centre, Islamabad-45500, Pakistan
AUTHOR
F.
Mehmood
8
Mphil in Microbiology, National Reference Lab for Poultry Diseases, Animal Sciences Institute, National Agricultural Research Centre, Islamabad-45500, Pakistan
AUTHOR
I.
Begum
9
Mphil in Biology, National Reference Lab for Poultry Diseases, Animal Sciences Institute, National Agricultural Research Centre, Islamabad-45500, Pakistan
AUTHOR
T.
Javaid
10
Al-Ferooz Poultry Clinic, Rawalpindi-46000, Pakistan
AUTHOR
S. M. H.
Jaffery
11
Jaffmac Consultant Services, Lahore, Pakistan
AUTHOR
R.
Ali
12
Remount Veterinary and Farms Directorate, GHQ, Rawalpindi, Pakistan
AUTHOR
Kh.
Naeem
13
National Reference Lab for Poultry Diseases, Animal Sciences Institute, National Agricultural Research Centre, Islamabad-45500, Pakistan
AUTHOR
Asrani, RK; Gupta, VK; Sharma, SK; Singh, SP and Katoch, RC (1997). Hydropericardium-hepatopathy syndrome in Asian poultry. Vet. Rec., 141: 271-273.
1
Choi, KS; Kye, SJ; Kim, JY; Jeon, WJ; Lee, EK; Park, KY and Sung, HW (2012). Epidemiological investigation of outbreaks of fowl adenovirus infection in commercial chickens in Korea. Poult. Sci., 91: 2502-2506.
2
Cowen, BS (1992). Inclusion body hepatitis-anaemia and hydropericardium syndromes: aetiology and control. World Poul. Sci. J., 48: 247-254.
3
Crowle, AJ (1973). Immunodiffusion. 2nd Edn., New York, USA, Academic Press. P: 545.
4
Fitzgerald, SD (2013). Adenovirus infections (Introduction). In: Swayne, DE; Glisson, JR; McDougald, LR; Nolan, LK; Suarez, DL and Nair, V (Eds.), Diseases of poultry. (13th Edn.), Ames, Iowa, USA, John Wiley & Sons, Inc., PP: 289-290.
5
Ganesh, K; Suryanarayana, VV and Raghavan, R (2002). Detection of fowl adenovirus associated with hydro-pericardium hepatitis syndrome by a polymerase chain reaction. Vet. Res. Commun., 26: 73-80.
6
Hafez, HM (2011). Avian adenoviruses infections with special attention to inclusion body hepatitis/hydropericardium syndrome and egg drop syndrome. Pak. Vet. J., 31: 85-92.
7
Jaffery, MS (1988). A treatise on Angara disease (hydropericardium-pulmonary oedema-hepatonephritis syndrome). J. Pak. Vet. Med. Assoc., 34: 1-33.
8
Khawaja, DA; Ahmad, S; Rauf, AM; Zulfiqar, M; Mahmood, SM and Hassan, M (1988). Isolation of an adenovirus from hydropericardium syndrome in broiler chicks. Pak. J. Vet. Res., 1: 2-27.
9
Kumar, R; Chandra, R; Shukla, SK; Agrawal, DK and Kumar, M (1997). Hydropericardium syndrome (HPS) in India: a preliminary study on the causative agent and control of the disease by inactivated autogenous vaccine. Trop. Anim. Health. Prod., 29: 158-164.
10
Mase, M; Nakamura, K and Imada, T (2010). Characterization of fowl adenovirus serotype 4 isolated from chickens with hydropericardium syndrome based on analysis of the short fiber protein gene. J. Vet. Diagn. Invest., 22: 218-223.
11
Mazaheri, A; Prusas, C; Voss, M and Hess, M (1998). Some strains of serotype 4 fowl adenoviruses cause inclusion body hepatitis and hydropericardium syndrome in chickens. Avian Pathol., 27: 269-276.
12
Mehmood, MD; Muhammad, K; Rabbani, M; Hanif, A and Hussain, I (2011). In process quality control factors affecting efficacy of hydropericardium syndrome virus vaccine. Pak. J. Zool., 43: 73-77.
13
Naeem, K; Niazi, T; Malik, SA and Cheema, AH (1995a). Immunosuppressive potential and pathogenicity of an avian adenovirus isolate involved in hydropericardium syndrome in broilers. Avian Dis., 39: 723-728.
14
Naeem, K; Rabbani, M; Hussain, M and Cheema, AH (1995b). Development of cell culture vaccine against hydropericardium syndrome in poultry. Pak. Vet. J., 15: 150-151.
15
Reed, LJ and Muench, H (1938). A simple method of estimating fifty percent endpoint. Am. J. Hyg., 27: 937-943.
16
Schat, KA and Sellers, HS (2008). Cell culture methods. In: Dufour-Zavala, L; Swayne, DE; Glisson, JR; Jackwood, MW; Pearson, JE; Reed, WM and Woolcock, PR (Eds.), A laboratory manual for the isolation, identification and characterization of avian pathogens. Jacksonville, FL, USA, American Association of Avian Pathologists. PP: 195-203.
17
Shukla, SK; Chandra, R; Kumar, M and Dixit, PV (1997). Hydropericardium syndrome in India: a report. Ind. J. Anim. Sci., 67: 28-29.
18
Steer, PA; O’Rourke, D; Ghorashi, SA and Noormohammadi, AH (2011). Application of high-resolution melting curve analysis for typing of fowl adenoviruses in field cases of inclusion body hepatitis. Aust. Vet. J., 89: 184-192.
19
Tan, PK; Michou, AI; Bergelson, JM and Cotten, M (2001). Defining CAR as a cellular receptor for the avian adenovirus CELO using a genetic analysis of the two viral fibre proteins. J. Gen. Virol., 82: 1465-1472.
20
Thakor, KB; Dave, CJ; Prajapati, KS; Fefar, DT and Jivani, BM (2012). Molecular charecterization of avian adeno virus causing inclusion body hepatitis-hydropericardium syndrome in broiler chickens of Anand, Gujarat, India. Vet. World. 5: 178-182.
21
ORIGINAL_ARTICLE
Immunopathological evaluation of recombinant mycobacterial antigen Hsp65 expressed in Lactococcus lactis as a novel vaccine candidate
Bovine tuberculosis (TBB) is a zoonotic disease distributed worldwide and is of great importance for public health and the livestock industry. Several experimental vaccines against this disease have been evaluated in recent years, yielding varying results. An example is the Bacillus Calmette-Guérin (BCG) vaccine, which has been used extensively in humans and tested in cattle showing mixed results related to protection (0-80%) against Mycobacterium bovis. In this study, we used the food-grade bacterium Lactococcus lactis as an expression system for production of mycobacterial protein Hsp65. For this purpose, the construction of a replicable plasmid in strain NZ9000 L. lactis (pVElepr) was conducted, which expressed the Mycobacterium leprae Hsp65 antigen, and was recognized by traded anti-Hsp65 antibodies. The strain NZ9000-pVElepr was applied to calves that were negative to tuberculin test and the immune response was monitored. The results showed that immune response was not significantly increased in calves with NZ9000-pVElepr with respect to control groups, and no injury was observed in any lung or lymph of the calves. Finally, this study suggest that the recombinant NZ9000 strain of L. lactis may protect against the development of M. bovis infection, although studies with longer exposure to this pathogen are necessary to conclude the matter.
https://ijvr.shirazu.ac.ir/article_4222_5b66d0e4e0b25c288cf83ca04fa4aad0.pdf
2017-09-01
197
202
10.22099/ijvr.2017.4222
Hsp65
Lactococcus
Mycobacterium leprae
Vaccination
J. C.
Herrera Ramírez
1
Ph.D. Student in Veterinary Sciences, Molecular Biology Laboratory, Veterinary Sciences Research Institute, Autonomous University of Baja California, Mexicali, Baja California, 21388, Mexico
AUTHOR
A. Ch.
De la Mora
2
MSc Student in Veterinary Sciences, Molecular Biology Laboratory, Veterinary Sciences Research Institute, Autonomous University of Baja California, Mexicali, Baja California, 21388, Mexico
AUTHOR
A.
De la Mora Valle
3
MSc, Molecular Biology Laboratory, Veterinary Sciences Research Institute, Autonomous University of Baja California, Mexicali, Baja California, 21388, Mexico
AUTHOR
G.
Lopez-Valencia
4
Molecular Biology Laboratory, Veterinary Sciences Research Institute, Autonomous University of Baja California, Mexicali, Baja California, 21388, Mexico
AUTHOR
R. M. B.
Hurtado
5
Molecular Biology Laboratory, Veterinary Sciences Research Institute, Autonomous University of Baja California, Mexicali, Baja California, 21388, Mexico
AUTHOR
T. B.
Rentería Evangelista
6
Molecular Biology Laboratory, Veterinary Sciences Research Institute, Autonomous University of Baja California, Mexicali, Baja California, 21388, Mexico
AUTHOR
J. L.
Rodríguez Castillo
7
Ph.D. Student in Veterinary Sciences, Molecular Biology Laboratory, Veterinary Sciences Research Institute, Autonomous University of Baja California, Mexicali, Baja California, 21388, Mexico
AUTHOR
A.
Rodríguez Gardea
8
Ph.D. Student in Veterinary Sciences, Molecular Biology Laboratory, Veterinary Sciences Research Institute, Autonomous University of Baja California, Mexicali, Baja California, 21388, Mexico
AUTHOR
S. D.
Gómez Gómez
9
MSc, Molecular Biology Laboratory, Veterinary Sciences Research Institute, Autonomous University of Baja California, Mexicali, Baja California, 21388, Mexico
AUTHOR
G. E.
Medina-Basulto
gerardom@uabc.edu.mx
10
Molecular Biology Laboratory, Veterinary Sciences Research Institute, Autonomous University of Baja California, Mexicali, Baja California, 21388, Mexico
LEAD_AUTHOR
Asociación Médica Mundial (2005). Manual de ética médica.
1
Azevedo, MS; Rocha, CS; Electo, N; Pontes, DS; Molfetta, JB; Goncalves, ED; Azevedo, V; Silva, CL and Miyoshi, A (2012). Cytoplasmic and extracelular expression of pharmaceutical-grade mycobacterial 65-kDa heat shock protein in Lactococcus lactis. J. Genet. Mol. Res., 11: 1146-1157.
2
Bahey-El-Din, M; Gahan, CG and Griffin, BT (2010). Lactococcus lactis as a cell factor for delivery of therapeutic proteins. J. Curr. Gene Ther. 10: 34-45.
3
Bermúdez-Humarán, LG; Langella, P; Miyoshi, A; Gruss, A; Tamez, GR; Montes de Oca-Luna, R and Le, LY (2002). Production of human papillomavirus type 16 E7 protein in Lactococcus lactis. J. App. Environm. Microbiol., 68: 917-922.
4
Bermúdez-Humarán, LG; Pascale, K; Chatel, JM and Langella, P (2011). Lactococci and Lactobacilli as mucosal delivery vectors for therapeutic proteins and DNA vaccines. Microb. Cell Fact. (Suppl. 1), 10: S4.
5
Bolontin, A; Wincker, P; Mauger, S; Jaillon, O; Malarme, K; Weissenbach, J; Ehrlich, SD and Sorokin, A (2001). The complete genome sequence of the lactic acid bacterium Lactococcus lactis spp. lactis IL1403. J. Genome Res. 11: 731-753.
6
Buddle, BM; de Lisle, GW; Pfeiffer, A and Aldwell, FE (1995). Immunological responses and protection against Mycobacterium bovis in calves vaccinated with a low dose of BCG. J. Vaccine. 13: 1123-1130.
7
Buddle, BM; Wedlock, DN; Parlane, NA; Corner, LA; de Lisle, GW and Skinner, MA (2003). Revaccination of neonatal calves with Mycobacterium bovis BCG reduces the level of protection against bovine tuberculosis induced by a single vaccination. J. Infect. Immun., 71: 6411-6419.
8
Cortes-Perez, NG; Bermudez-Humaran, LG; Le, LY; Rodriguez-Padilla, C; Gruss, A; Saucedo-Cárdenas, O; Langella, P and Montes-de-Oca, LR (2003). Mice immunization with live lactococci displaying a surface anchored HPV-16 E7 oncoprotein. FEMS Microbiol. Lett., 229: 37-42.
9
Dieye, Y; Usai, S; Clier, F; Gruss, A and Piard, JC (2001). Design of a protein-targeting system for lactic acid bacteria. J. Bacteriol., 183: 4157-4166.
10
Laemmli, UK (1970). Cleavage of structural proteins during the assembly of the head of bacteriophage T4. J. Nature. 227: 680-685.
11
Lei, H; Sheng, Z; Ding, Q; Chen, J; Wei, X; Lam, DMK and Xu, Y (2011). Evaluation of oral immunization with recombinant avian influenza virus HA1 displayed on the Lactococcus lactis surface and combined with the mucosal adjuvant cholera toxin subunit B. Clin. Vaccine Immunol., 18: 1046-1051.
12
Lima, KM; Dos Santos, SA; Santos, RR; Brandâo, IT; Rodrigues, JM and Silva, CL (2003). Efficacy of DNA-hsp65 vaccination for tuberculosis varies with method of DNA introduction in vivo. J. Vaccine. 22: 49-56.
13
Lopez-Valencia, G; Renteria-Evangelista, T; Williams, JJ; Licea-Navarro, A; Mora-Valle, A and Medina-Basulto, G (2009). Field evaluation of the protective efficacy of Mycobacterium bovis BCG vaccine against bovine tuberculosis. J. Res. Vet. Sci., 88: 44-49.
14
Lowrie, DB (2006). DNA vaccines for therapy of tuberculosis: where are we now? J. Vaccine. 24: 1983-1989.
15
Lowrie, DB; Tascon, RE; Bonato, VL; Lima, VM; Faccioli, LH; Stravropoulos, E; Colston, MJ; Hewinson, RG; Moelling, K and Silva, CL (1999). Therapy of tuberculosis in mice by DNA vaccination. J. Nature. 400: 269-271.
16
Lyashchenko, K; Whelan, OA; Greenwald, R; Pollock, JM; Andersen, P; Hewinson, RG and Vordermeier, HM (2004). Association of tuberculin-boosted antibody responses with pathology and cell-mediated immunity in cattle vaccinated with Mycobacterium bovis BCG and infected with M. bovis. J. Infect. Immun., 72: 2462-2467.
17
Martínez-Vidal, C; Hori, S; De la Mora, A; Bermúdez, RM; Rentería, TB; López, G; Galván, LJ and Medina, GE (2011). VNTR for genotyping of Mycobacterium bovis isolates from cattle slaughtered in Baja California, Mexico. J. Rev. Mex. Cienc. Pecu., 2: 393-401.
18
Mustafa, AS; Lundin, KEA; Meloen, RH; Shinnick, TM and Oftung, F (1999). Identification of promiscuous epitopes from the mycobacterial 65-kilodalton heat shock protein recognized by human CD4+ T cells of the Mycobacterium leprae memory repertoire. Infect. Immun., 67: 5683-5689.
19
NOM-031-ZOO-1995 (NORMA, Oficial Mexicana). Campaña nacional contra la tuberculosis bovina (Mycobacterium bovis).
20
Nouaille, S; Ribeiro, LA; Miyoshi, A; Pontes, D; Le, LY; Oliveira, SC; Langella, P and Azevedo, V (2003). Heterologous protein production and delivery systems for Lactococcus lactis. J. Genet. Mol. Res., 2: 102-111.
21
Sambrook, J and Russell, DW (2001). Molecular cloning a laboratory manual. 3rd Edn., New York, USA, Cold Spring Harbor Laboratory Press. PP: 15.35.
22
Santos, PD; Pacheco, AMS; Chatel, JM; Langella, P; Azevedo, V and Miyoshi, A (2011). Lactoccocus lactis as a live vector: heterologous protein production and DNA delivery systems. J. Protein Expr. Purif., 79: 165-175.
23
Thoen, CO; Steele, JH and Gilsdorf, MJ (2006). Mycobacterium bovis infection in animals and humans. 2nd Edn., Iowa, USA, Blackwell Publishing. PP: 34-49.
24
ORIGINAL_ARTICLE
Cumulus cell expansion and ultrastructural changes in in vitro matured bovine oocytes under heat stress
Cumulus-oocyte complexes (COCs) from cows were matured under normal (38.5°C) and elevated temperatures (41°C) simulating heat stress and their maturation was assessed based on measurement of cumulus expansion in both groups. There was a significant reduction (P<0.01) in maturation rate in the heat stressed oocytes. The ultrastructural events associated with in vitro oocyte maturation and changes associated with elevated temperature were also studied by transmission electron microscopy (TEM). Normal maturation cellular events were marked by migration of Golgi and mitochondria from the cortical regions, and conversely by a migration of cortical granules from the inner regions to a sub-perivitelline zone. Heat stressed oocytes (41°C) were not only marked by a reduction in rate and less cumulus cell expansion, but also by a reduction in cortical granule migration. The mitochondria appeared swollen with cristolysis. Ribosomal disruption and an abundance of free ribosomes were also seen. Changes in the cumulus cells include nuclear chromatin margination, condensation and karyolysis, formation of nuclear and cell membrane blebs, and typical membrane bound vesicles enclosing cell fragments indistinguishable from apoptosis. Evidently, heat stress can be associated with reduced cytoplasmic events of oocyte maturation, thereby decreasing the oocyte competence and can be associated with apoptosis of the cumulus cells and therefore compromise the survival of the oocyte itself.
https://ijvr.shirazu.ac.ir/article_4223_5bdec55e1f952a2068c40a81aaf62244.pdf
2017-09-01
203
207
10.22099/ijvr.2017.4223
Bovine
Heat stress
IVM
Oocyte
TEM
J. A.
Ahmed
jafrinahmed@rediffmail.com
1
Division of Veterinary Physiology and Biochemistry, Faculty of Veterinary Sciences & Animal Husbandry, Sher-e-Kashmir University of Agricultural Sciences & Technology-Jammu, RS Pura-181102, Jammu & Kashmir, India
LEAD_AUTHOR
N.
Nashiruddullah
2
Division of Veterinary Pathology, Faculty of Veterinary Sciences & Animal Husbandry, Sher-e-Kashmir University of Agricultural Sciences & Technology-Jammu, RS Pura-181102, Jammu & Kashmir, India
AUTHOR
D.
Dutta
3
Department of Veterinary Physiology, College of Veterinary Science, Assam Agricultural University, Guwahati-781022, Assam, India
AUTHOR
R. K.
Biswas
4
Department of Animal Reproduction, Gynaecology and Obstetrics, College of Veterinary Science, Assam Agricultural University, Guwahati-781022, Assam, India
AUTHOR
P.
Borah
5
State Biotech Hub, College of Veterinary Science, Assam Agricultural University, Guwahati-781022, Assam, India
AUTHOR
Ahmed, JA; Dutta, D and Nashiruddullah, N (2016). Comparative efficacy of antioxidant retinol, melatonin, and zinc during in vitro maturation of bovine oocytes under induced heat stress. Turk. J. Vet. Anim. Sci., 40: 365-373.
1
Cetica, PD; Pintos, LN; Dalvit, GC and Beconi, MT (2001). Antioxidant enzyme activity and oxidative stress in bovine oocyte in vitro maturation. IUBMB Life. 51: 57-64.
2
Ealy, AD; Howell, JL; Monterroso, VH; Aréchiga, CF and Hansen, PJ (1995). Developmental changes in sensitivity of bovine embryos to heat shock and use of antioxidants as thermoprotectants. J. Anim. Sci., 73: 1401-1407.
3
Edwards, JL and Hansen, PJ (1996). Elevated temperature increases heat shock protein 70 synthesis in bovine two-cell embryos and compromises function of maturing oocyte. Biol. Reprod., 55: 340-346.
4
Edwards, JL; Saxton, AN; Lawrence, JL; Payton, RR and Dunlap, JR (2005). Exposure to a physiologically relevant elevated temperature hastens in vitro maturation of bovine oocytes. J. Diary Sci., 88: 4326-4333.
5
Ferreira, EM; Vireque, AA; Adona, PR; Meirelles, FV; Ferriani, RA and Navarro, PA (2009). Cytoplasmic maturation of bovine oocytes: structural and biochemical modifications and acquisition of developmental com-petence. Theriogenology. 71: 836-848.
6
Hansen, PJ (2013). Cellular and molecular basis of therapies to ameliorate effects of heat stress on embryonic development in cattle. Anim. Reprod., 10: 322-333.
7
Hosoe, M and Shioya, Y (1997). Distribution of cortical granules in bovine oocytes classified by cumulus complex. Zygote. 5: 371-376.
8
Hyttel, P; Fair, T; Callesen, H and Greve, T (1997). Oocyte growth, capacitation and final maturation in cattle. Theriogenology. 47: 23-32.
9
Jainudeen, MR; Wahid, H and Hafez, ESE (2008). Ovulation induction, embryo production and transfer. In: Hafez, ESE and Hafez, B (Eds.), Reproduction in farm animals. (7th Edn.), Blackwell Publishing. P: 418.
10
Ju, JC; Jiang, S; Tseng, JK; Parks, JE and Yang, X (2005). Heat shock reduces developmental competence and alters spindle configuration of bovine oocytes. Theriogenology. 64: 1677-1689.
11
Ju, JC and Tseng, JK (2004). Nuclear and cytoskeletal alterations of in vitro matured porcine oocytes under hyperthermia. Mol. Reprod. Dev., 68: 125-133.
12
Krisher, RL and Bavister, BD (1998). Responses of oocytes and embryos to the culture environment. Theriogenology. 49: 103-114.
13
Lawrence, JL; Payton, RR; Godkin, JD; Saxton, AM; Schrick, FN and Edwards, JL (2004). Retinol improves development of bovine oocytes compromised by heat stress during maturation. J. Dairy Sci., 87: 2449-2454.
14
Maya-Soriano, MJ (2012). Heat stress and antioxidant agents: effects on gamete development. Ph.D. Dissertation, Universtat Autonoma de Barcelona (Autonomous University of Barcelona), Spain. PP: 41-47.
15
Nabenishi, H; Ohta, H; Nishimoto, T; Morita, T; Ashizawa, K and Tsuzuki, Y (2012a). The effects of cysteine addition during in vitro maturation on the developmental competence, ROS, GSH and apoptosis level of bovine oocytes exposed to heat stress. Zygote. 20: 249-259.
16
Nabenishi, H; Takagi, S; Kamata, H; Nishimoto, T; Morita, T; Ashizawa, K and Tsuzuki, Y (2012b). The role of mitochondrial transition pores on bovine oocyte competence after heat stress, as determined by effects of cyclosporin A. Mol. Reprod. Dev., 79: 31-40.
17
Qu, P; Tian, W; Li, T; Jiang, Z; Gao, S; Tian, Z and Wang, M (2009). Development competence and ultrastructural changes of heat-stressed mouse early blastocysts produced in vitro. Curr. Zool., 55: 61-66.
18
Rivera, RM; Kelly, KL; Erdos, GW and Hansen, PJ (2004). Reorganization of microfilaments and microtubules by thermal stress in two-cell bovine embryos. Biol. Reprod., 70: 1852-1862.
19
Roth, Z and Hansen, PJ (2004). Involvement of apoptosis in disruption of developmental competence of bovine oocytes by heat shock during maturation. Biol. Reprod., 71: 1898-1906.
20
Roth, Z and Hansen, PJ (2005). Disruption of nuclear maturation and rearrangement of cytoskeletal elements in bovine oocytes exposed to heat shock during maturation. Reproduction. 129: 235-244.
21
Schrock, GE; Saxton, AM; Shrick, FN and Edwards, JL (2007). Early in vitro fertilization improves development of bovine ova heat stressed during in vitro maturation. J. Dairy Sci., 90: 4297-4303.
22
Soto, P and Smith, LC (2009). BH4 peptide derived from Bcl-xL and Bax-inhibitor peptide suppresses apoptotic mitochondrial changes in heat stressed bovine oocytes. Mol. Reprod. Dev., 76: 637-646.
23
Stojkovic, M; Machado, SA; Stojkovic, P; Zakhartchenko, V; Hutzler, P; Goncalves, PB and Wolf, E (2001). Mitochondrial distribution and adenosine triphosphate content of bovine oocytes before and after in vitro maturation: correlation with morphological criteria and developmental capacity after in vitro fertilization and culture. Biol. Reprod., 64: 904-909.
24
Tanghe, S; Van Soom, A; Nauwynck, H; Coryn, M and DeKruif, A (2002). Minireview: functions of the cumulus oophorus during oocyte maturation, ovulation, and fertilization. Mol. Reprod. Dev., 61: 414-424.
25
Warnes, GM; Moor, RM and Johnson, MH (1977). Changes in protein synthesis during maturation of sheep oocytes in vivo and in vitro. J. Reprod. Fertil., 49: 331-335.
26
ORIGINAL_ARTICLE
Molecular detection of virulence genes and multi-drug resistance patterns in Escherichia coli (STEC) in clinical bovine mastitis: Alborz province, Iran
The aim of this study was to identify virulence genes and antimicrobial resistance of Escherichia coli isolated from bovine clinical mastitis in dairy herds in Iran. Sampling was done from 86 inflamed quarters of dairy cows in 8 commercial farms of Alborz province, Iran in summer 2015. Shiga toxin-producing E. coli (STEC) virulence genes were detected by multiplex PCR and multi-drug resistance profiles were confirmed using disk diffusion method. Among 60 E. coli isolated from examined samples, 13 (21.6%) of them were STEC. The results of PCR assay showed that eaeA gene was carried by 4 (30.8%) of STEC isolates. Although stx1 in combination with eaeA gene was detected from 7 (53.8%) of STEC isolates, stx1 and stx2 genes were detected from only 1 (7.7%) of the examined samples. The result of the disk diffusion method showed that all E. coli isolates were resistant to penicillin, tylosin, oxytetracycline, erythromycin, ampicillin, streptomycin and neomycin. However all isolates were susceptible to enrofloxacin. Therefore, according to the results establishing a regular monitoring system for identification of cases with clinical mastitis and conducting antibiotic sensitivity tests are recommended.
https://ijvr.shirazu.ac.ir/article_4224_c9d31c857d0adeaf66fbfc0f0e12ba28.pdf
2017-09-01
208
211
10.22099/ijvr.2017.4224
Antimicrobial resistance
Clinical mastitis
E. coli
STEC
Virulence factors
M.
Tavakoli
1
Department of Microbiology, College of Veterinary Medicine, Karaj Branch, Islamic Azad University, Karaj, Iran
AUTHOR
H.
Pourtaghi
hadi.pourtaghi1@gmail.com
2
Department of Microbiology, College of Veterinary Medicine, Karaj Branch, Islamic Azad University, Karaj, Iran
LEAD_AUTHOR
Beutin, L; Krause, G; Zimmermann, S; Kaulfuss, S and Gleier, K (2004). Characterization of Shiga toxin-producing Escherichia coli strains isolated from human patients in Germany over a 3-year period. J. Clin. Microbiol., 42: 1099-1108.
1
Bradley, AJ and Green, MJ (2001). Etiology of clinical mastitis in six somerset dairy herds. Vet. Rec., 148: 683-686.
2
CLSI (2008). Performance and standards for antimicrobial disk diffusion and dilution susceptibility tests for bacteria isolated from animals; approved standards. 3rd Ed., Vol. 28, M31-A3. Clinical and Laboratory Standard Institute, Wayne, Pennsylvania, USA.
3
Dubravka, M; Bojana, P; Maja, V; Dalibor, T and Vladimir, P (2015). Investigation of biofilm formation and phylogenetic typing of Escherichia coli stains isolated from milk of cows with mastitis. Acta Vet. Beograd., 65: 202-216.
4
Frank, SM; Bosworth, BT and Moon, HW (1998). Multiplex PCR for enterotoxigenic, attaching and effacing, and Shiga toxin-producing Escherichia coli strains from calves. J. Clin. Microbiol., 36: 1795-1797.
5
Guler, L and Gündüz, K (2007). Virulence properties of Escherichia coli isolated from clinical bovine mastitis. Turk. J. Vet. Anim. Sci., 31: 361-365.
6
Kobori, D; Rigobelo, EC; Macedo, C; Marin, JM and Avila, FA (2004). Virulence properties of Shiga toxin-producing Escherichia coli isolated from cases of bovine mastitis in Brazil. Rev. Elev. Med. Vet. Pays. Trop., 57: 15-20.
7
Mansouri-Najand, L and Khalili, M (2007). Detection of Shiga-like toxigenic Escherichia coli from raw milk cheeses produced in Kerman-Iran. Veterinarski. Arhiv., 77: 515-522.
8
Momtaz, H (2010). Investigation of virulence factors in Escherichia coli isolated from clinical and subclinical bovine mastitis. Bulg. J. Vet. Med., 13: 122-126.
9
Momtaz, H; Dehkordi, SF; Taktaz, T; Rezvani, A and Yarali, S (2012). Shiga toxin-producing Escherichia coli isolated from bovine mastitic milk: serogroups, virulence factors, and antibiotic resistance properties. Sci. World J., 2012: 618709.
10
Pourtaghi, H; Dahpahlavan, V and Momtaz, H (2013). Virulence genes in Escherichia coli isolated from calves with diarrhoea in Iran. Com. Clin. Pathol., 12: 513-515.
11
Pourtaghi, H and Sodagari, HR (2016). Antimicrobial resistance of entrotoxigenic and non-entrotoxigenic Escherichia coli isolated from diarrheic calves in Iran. Int. J. Enteric. Pathog., 4: e34557.
12
Rangel, P and Marin, JM (2009). Analysis of Escherichia coli isolated from bovine mastitic milk. Pesq. Vet. Bras., 29: 363-368.
13
Sawant, AA; Hegde, NV; Straley, BA; Donaldson, SC; Love, BC; Knabel, SJ and Jayarao, BM (2007). Antimicrobial-resistant enteric bacteria from dairy cattle. Appl. Environ. Microbiol., 73: 156-163. Seyda, C; Gökçen, D and Ünlü, SM (2014). Detection of several virulence properties, antibiotic resistance and
14
phylogenetic relationship in E. coli isolated from cow mastitis. Acta Vet. Beograd., 64: 413-425.
15
Spnu, M; Kobolkuti, L; Cadar, D; Niculae, M; Bianu, G; Popescu, S and Lukacs, L (2012). Changes in antibiotic resistance indices of animal Escherichia coli strains with number of isolates. Ann. Rom. Soc. Cell. Biol., 17: 361-366.
16
Stephan, R; Schumacher, S; Corti, S; Krause, G; Danuser, J and Beutin, L (2008). Prevalence and characteristics of Shiga toxin producing Escherichia coli in Swiss raw milk cheeses collected at producer level. J. Dairy. Sci., 91: 2561-2565.
17
Vivegnis, J; Lioui, EM; Leclercq, A; Lambert, B and Decallonne, J (1993). Detection of Shiga-like toxin producing Escherichia coli from raw milk cheeses produced in Wallonia. Biotechnol. Agron. Soc. Environ., 3: 159-164.
18
Wenz, JR; Barrington, GM; Garry, FB; Ellis, RP and Magnuson, RJ (2006). Escherichia coli isolates’ serotypes, genotypes, and virulence genes and clinical coliform mastitis severity. J. Dairy. Sci., 89: 3408-3412.
19
ORIGINAL_ARTICLE
Phylogenic analysis of serotype Asia1 foot-and-mouth disease virus from Sulaimani/Iraq using VP1 protein: heterogeneity with vaccine strain As1/Shamir/89
Foot-and-mouth disease virus (FMDV) serotypes O, A and Asia1 are responsible for a significant number of disease outbreaks in Iraq. The current study can be considered as the first molecular characterization of serotype Asia1 in Iraq. The present investigation reports the detection of serotype FMDV Asia1 from local farms in Sulaimani districts in 2012 and 2014 outbreaks. Phylogenetic analysis of the complete VP1 gene has shown that FMDV Asia1 field isolates were under genetic novel variant Sindh-08 (group VII) including PAK/iso/11 and TUR/13 strains. The VP1 protein sequence of circulatory FMDV Asia1 genotype showed heterogeneity of nine amino acid substitutions within the G-H loop with the vaccine strain As1/Shamir/89 (JF739177) that is currently used in vaccination program in Iraq. Our result indicated that differences in VP1 protein at G-H loop of the locally circulated FMDV serotype Asia1 strain may be a reason for current vaccination failure.
https://ijvr.shirazu.ac.ir/article_4226_97fef59715c10306e11d2e1184e11cc8.pdf
2017-09-01
212
215
10.22099/ijvr.2017.4226
Molecular genotyping
Phylogenetic analysis
viral evolution
M. O.
Baba Sheikh
muhamad.omer@ymail.com
1
School of Informatics and Computing, Indiana University-Purdue University, Indianapolis, 46202, India; Department of Molecular Biology, Veterinary Laboratory Center, Sulaimani Veterinary Directorate, Sulaimani, Iraq
LEAD_AUTHOR
P. M. A.
Rashid
2
Department of Molecular Biology, Veterinary Laboratory Center, Sulaimani Veterinary Directorate, Sulaimani, Iraq
AUTHOR
A. S.
Marouf
3
Department of Molecular Biology, Veterinary Laboratory Center, Sulaimani Veterinary Directorate, Sulaimani, Iraq
AUTHOR
Z. H.
Raheem
4
Department of Molecular Biology, Veterinary Laboratory Center, Sulaimani Veterinary Directorate, Sulaimani, Iraq
AUTHOR
S. C.
Janga
5
School of Informatics and Computing, Indiana University-Purdue University, Indianapolis, 46202, India; Center for Computational Biology and Bioinformatics, and Department of Medical and Molecular Genetics, Indiana University School of Medicine, India
AUTHOR
Acharya, R; Fry, E; Stuart, D; Fox, G; Rowlands, D and Brown, F (1989). The three-dimensional structure of foot-and-mouth disease virus at 2.9 Å resolution. Nature. 337: 709-716.
1
Ansell, D; Samuel, A; Carpenter, W and Knowles, N (1994). Genetic relationships between foot-and-mouth disease type Asia 1 viruses. Epidemiol. Infect., 112: 213-224.
2
Carrillo, C; Tulman, E; Delhon, G; Lu, Z; Carreno, A; Vagnozzi, A; Kutish, G and Rock, D (2005). Com-parative genomics of foot-and-mouth disease virus. J. Virol., 79: 6487-6504.
3
Domingo, E; Escarmı́s, C; Baranowski, E; Ruiz-Jarabo, CM; Carrillo, E; Núñez, JI and Sobrino, F (2003). Evolution of foot-and-mouth disease virus. Virus Res., 91: 47-63.
4
El-Kholy, AA; Soliman, HM; Helmy, NA and Rahman, AOA (2007). Genetic identification of the foot-and-mouth disease virus caused 2006 outbreak in Egypt. Arab. J. Biotech., 10: 193-206.
5
Ferris, N and Donaldson, A (1992). The World Reference Laboratory for Foot and Mouth Disease: a review of thirty-three years of activity (1958-1991). Revue Scientifique et Technique (International Office of Epizootics). 11: 657-684.
6
Jamal, SM and Belsham, GJ (2013). Foot-and-mouth disease: past, present and future. Vet. Res., 44: 116.
7
Jamal, SM; Ferrari, G; Ahmed, S; Normann, P and Belsham, GJ (2011). Molecular characterization of serotype Asia-1 foot-and-mouth disease viruses in Pakistan and Afghanistan; emergence of a new genetic group and evidence for a novel recombinant virus. Infect. Genet. Evol., 11: 2049-2062.
8
Jelokhani-Niaraki, S; Esmaelizad, M; Daliri, M; Vaez-Torshizi, R; Kamalzadeh, M and Lotfi, M (2010). Sequence and phylogenetic analysis of the non-structural 3A and 3B protein-coding regions of foot-and-mouth disease virus subtype A Iran 05. J. Vet. Sci., 11: 243-247.
9
Li, P; Lu, Z; Bao, H; Li, D; King, DP; Sun, P; Bai, X; Cao, W; Gubbins, S and Chen, Y (2011). In-vitro and in-vivo phenotype of type Asia 1 foot-and-mouth disease viruses utilizing two non-RGD receptor recognition sites. BMC Microbiol., 11: 154.
10
Logan, D; Abu-Ghazaleh, R; Blakemore, W; Curry, S; Jackson, T; King, A; Lea, S; Lewis, R; Newman, J and Parry, N (1993). Structure of a major immunogenic site on foot-and-mouth disease virus. Nature. 362: 566-568.
11
Rashid, PMA; Marouf, AS; Raheem, ZH and Babashekh, MO (2014). Phylogenic analysis and molecular characterization of Slemani/Kurdistan/2013 foot and mouth disease virus shows circulation of new genotype in Iraq J. Zankoy Sulaimani. Part A. 16: 3.
12
Reid, SM; Ferris, NP; Hutchings, GH; Samuel, AR and Knowles, NJ (2000). Primary diagnosis of foot-and-mouth disease by reverse transcription polymerase chain reaction. J. Virol. Methods. 89: 167-176.
13
Ruiz-Jarabo, CM; Arias, A; Baranowski, E; Escarmís, C and Domingo, E (2000). Memory in viral quasispecies. J. Virol., 74: 3543-3547.
14
Sabar, AA; Al-Banna, AS; Abdul-Rasoul, LM and Abood, BK (2012). Diagnostic study of FMD virus in different area in Iraq. In: Proceeding of the Eleventh Veterinary Scientific Conference. 55.
15
Saeed, A; Khan, QM; Waheed, U; Arshad, M; Asif, M and Farooq, M (2011). RT-PCR evaluation for identification and sequence analysis of foot-and-mouth disease serotype O from 2006 to 2007 in Punjab, Pakistan. Comp. Immunol. Microbiol. Infect. Dis., 34: 95-101.
16
Soleimanjahi, H; Sedeh, FM; Jalilian, A and Mahravani, H (2013). Sequence analysis of the foot and mouth disease virus type O/IRN/2007 VP1 gene from Iranian isolate. Folia Biol. (Praha), 59: 93-98.
17
Tamura, K; Stecher, G; Peterson, D; Filipski, A and Kumar, S (2013). MEGA6: molecular evolutionary genetics analysis version 6.0. Mol. Biol. Evol., 30: 2725-2729.
18
Thompson, JD; Higgins, DG and Gibson, TJ (1994). CLUSTAL W: improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucleic Acids Res., 22: 4673-4680.
19
Zinnah, M; Islam, M; Rahman, M; Hossain, M; Bari, M; Haque, M; Khan, M and Islam, M (2012). Standardization of multiplex reverse transcription-polymerase chain reaction and typing of foot-and-mouth disease virus prevalent in Bangladesh. Bangladesh J. Vet. Med., 8: 149-155.
20
ORIGINAL_ARTICLE
Axial pattern flaps, using the deep circumflex iliac artery, superficial brachial and cranial superficial epigastric direct cutaneous arteries in the dog
Three dogs (Boxer, Labrador Retriever and German Shepherd) between the age of 7-10 years were presented with the history of tumour masses on right caudo-lateral thigh, right cranial forearm and left cranial and caudal thoracic mammary gland region, respectively. Fine needle aspiration cytology of the tumour masses and the sentinel regional lymph nodes were done. Plain radiography was done to rule out distant metastasis. In all the three cases the tumour masses were large in size, firmly adherent to the tissues underneath and sufficient loose skin was not available to close the skin defect following surgery. Hence axial pattern flaps were chosen to close the skin defect, following wide margin excision of tumour masses, leaving 3 cm from all the dimensions including healthy tissue. Deep circumflex iliac axial pattern flap, superficial brachial axial pattern flap and cranial superficial epigastric axial pattern flap were chosen to close the skin defect in case 1, case 2 and case 3, respectively. Post-operatively the dogs were admitted in in-patient unit for 5 days to restrict movement of the dog for immobilization of the flap and for wound dressing. All the cases recovered uneventfully with few complications.
https://ijvr.shirazu.ac.ir/article_4227_7a356f27ff88a2979d0b528e4781104e.pdf
2017-09-01
216
220
10.22099/ijvr.2017.4227
Axial pattern flaps
Canine
Extensive tumours
Histopathology
Reconstruction
M.
Shafiuzama
1
Department of Veterinary Surgery and Radiology, Madras Veterinary College, Tamilnadu Veterinary and Animal Sciences University, TANUVAS, Vepery, Chennai-600007, India
AUTHOR
M. S.
Sabarish Babu
sabanary@gmail.com
2
MVSc Scholar in Veterinary Surgery and Radiology, Department of Veterinary Surgery and Radiology, Madras Veterinary College, Tamilnadu Veterinary and Animal Sciences University, TANUVAS, Vepery, Chennai-600007, India
LEAD_AUTHOR
A.
Mohamed
3
MVSc in Veterinary Surgery and Radiology, Department of Clinics, Madras Veterinary College, Tamilnadu Veterinary and Animal Sciences University, TANUVAS, Vepery, Chennai-600007, India
AUTHOR
P.
Sankar
4
Department of Veterinary Surgery and Radiology, Madras Veterinary College, Tamilnadu Veterinary and Animal Sciences University, TANUVAS, Vepery, Chennai-600007, India
AUTHOR
G. N.
Sindhu
5
MVSc Scholar in Veterinary Surgery, Department of Veterinary Surgery and Radiology, Madras Veterinary College, Tamilnadu Veterinary and Animal Sciences University, TANUVAS, Vepery, Chennai-600007, India
AUTHOR
S.
Hemalatha
6
Department of Veterinary Pathology, Madras Veterinary College, Tamilnadu Veterinary and Animal Sciences University, TANUVAS, Vepery, Chennai-600007, India
AUTHOR
G.
Ravi Sundar
7
Department of Veterinary Surgery and Radiology, Madras Veterinary College, Tamilnadu Veterinary and Animal Sciences University, TANUVAS, Vepery, Chennai-600007, India
AUTHOR
Gregory, C and Gourley, IM (1990). Use of flap and or grafts for repair of skin defects of the distal limb of the dog and cat. Prob. Vet. Med., 2: 424-432.
1
Kirpensteijn, J and Haar, GT (2013). Reconstructive techniques of the neck and trunk. In: Northcott, J and Beynon, P (Eds.), Reconstructive surgery and wound management of the dog and cat. (1st Edn.), London, UK, Manson Publishing. PP: 160-162.
2
Kostolich, M and Pavletic, MM (1987). Axial pattern flap based on the genicular branch of the saphenous artery in the dog. Vet. Surg., 16: 217-222.
3
Pavletic, MM (1980). Caudal superficial epigastric arterial pedicle grafts in the dog. Vet. Surg., 9: 103-107.
4
Pavletic, MM (1991). Pedicle grafts. In: Slatter, DH (Ed.), Textbook of small animal surgery. (2nd Edn.), Philadelphia, W. B. Saunders. PP: 295-325.
5
Pavletic, MM (2010). Axial pattern skin flaps. In: Pavletic, MM (Ed.), Atlas of small animal wound management and reconstructive surgery. (3rd Edn.), Ames, Wiley-Blackwell. PP: 380-384.
6
Smith, MM; Payne, JT; Moon, ML and Freeman, LE (2009). Axial pattern flaps based on the caudal auricular artery in dogs. Am. J. Vet. Res., 52: 922-925.
7
Trevor, PB; Smith, MM; Waldron, DR and Hedlund, CS (1992). Clinical evaluation of axial pattern skin flaps in dogs and cats: 19 cases (1981-1990). J. Am. Vet. Med. Assoc., 4: 608-612.
8