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peste des petits ruminants

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Datasheet

peste des petits ruminants

Pictures

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PictureTitleCaptionCopyright
Natural case of PPR in a goat, Ghana.  Late-stage infection, ulceration of the hard palate, erosive stomatitis.
TitleSymptoms
CaptionNatural case of PPR in a goat, Ghana. Late-stage infection, ulceration of the hard palate, erosive stomatitis.
CopyrightMax Bonniwell
Natural case of PPR in a goat, Ghana.  Late-stage infection, ulceration of the hard palate, erosive stomatitis.
SymptomsNatural case of PPR in a goat, Ghana. Late-stage infection, ulceration of the hard palate, erosive stomatitis.Max Bonniwell
Natural case of PPR in a goat, Ghana.  Mucopurulent nasal and ocular discharge.
TitleSymptoms
CaptionNatural case of PPR in a goat, Ghana. Mucopurulent nasal and ocular discharge.
CopyrightMax Bonniwell
Natural case of PPR in a goat, Ghana.  Mucopurulent nasal and ocular discharge.
SymptomsNatural case of PPR in a goat, Ghana. Mucopurulent nasal and ocular discharge.Max Bonniwell
Natural case of PPR in a goat, Ghana.  Evidence of 'zebra striping' in intestine on necropsy examination.
TitlePathology
CaptionNatural case of PPR in a goat, Ghana. Evidence of 'zebra striping' in intestine on necropsy examination.
CopyrightMax Bonniwell
Natural case of PPR in a goat, Ghana.  Evidence of 'zebra striping' in intestine on necropsy examination.
PathologyNatural case of PPR in a goat, Ghana. Evidence of 'zebra striping' in intestine on necropsy examination.Max Bonniwell
PPR in a goat, Nigeria.  Multi-nucleate giant cell in the lung (original magnification x400).
TitleHistopathology
CaptionPPR in a goat, Nigeria. Multi-nucleate giant cell in the lung (original magnification x400).
CopyrightA.C. Rowland
PPR in a goat, Nigeria.  Multi-nucleate giant cell in the lung (original magnification x400).
HistopathologyPPR in a goat, Nigeria. Multi-nucleate giant cell in the lung (original magnification x400).A.C. Rowland
Dried exudate on the muzzle and around the eye resulting from rhinitis and conjunctivitis.
TitleExternal symptoms
CaptionDried exudate on the muzzle and around the eye resulting from rhinitis and conjunctivitis.
Copyright©USDA-2002/Foreign Animal Diseases Training Set/USDA-Animal and Plant Health Inspection Service (APHIS)
Dried exudate on the muzzle and around the eye resulting from rhinitis and conjunctivitis.
External symptomsDried exudate on the muzzle and around the eye resulting from rhinitis and conjunctivitis.©USDA-2002/Foreign Animal Diseases Training Set/USDA-Animal and Plant Health Inspection Service (APHIS)
Necrosis of the epithelium (whitish areas) on the tongue and pharynx.
TitlePathology
CaptionNecrosis of the epithelium (whitish areas) on the tongue and pharynx.
Copyright©USDA-2002/Foreign Animal Diseases Training Set/USDA-Animal and Plant Health Inspection Service (APHIS)
Necrosis of the epithelium (whitish areas) on the tongue and pharynx.
PathologyNecrosis of the epithelium (whitish areas) on the tongue and pharynx.©USDA-2002/Foreign Animal Diseases Training Set/USDA-Animal and Plant Health Inspection Service (APHIS)

Identity

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Preferred Scientific Name

  • peste des petits ruminants

International Common Names

  • English: goat plague; pest of sheep and goats; pest of small ruminants; pneumoenteritis complex; pseudorinderpest of small ruminants; stomatitis-pneumoenteritis syndrome

Local Common Names

  • Nigeria: kata

French acronym

  • PPR

Overview

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The disease was first described by workers in the Côté d’Ivoire (Gargadennec and Lalanne, 1942), and thereafter in other parts of West Africa in the 1950s and 1960s. It is now recognized to be distributed from Tibet through the Middle East, and through most of Africa, From East to West, and from North Africa (Algeria, Tunisia, Morocco) south as far as Tanzania. The similarity in clinical signs to that of rinderpest in cattle probably accounts for the number of reports of rinderpest in small ruminants from some countries, and delayed the recognition of the disease as a distinct entity in India until the early 1990s. The infective agent was first considered a variant of rinderpest virus adapted to small ruminants, but was later shown to be antigenically (Gibbs et al., 1979) and genetically distinct (Diallo et al., 1989). Although it had been previously proposed that PPR virus (PPRV) emerged from rinderpest virus (RPV) more recently than RPV diverged from measles virus and canine distemper virus, comparison of gene sequences suggest PPRV is no more related to RPV than to non-ruminant morbilliviruses (Das et al., 2000; Baron, 2011). Since PPRV isolates of West African, Middle Eastern and south Asian origin comprise distinct genetic groups, it is likely that the infections have circulated largely independently for long periods in each area.

The disease is recognized by the World Organisation for Animal Health (in French the Office International des Epizooties and still abbreviated as OIE) as a notifiable disease on account of the high mortality and morbidity, and rapidity of spread by contagion. Recognition of PPR as a problem has increased in the 1990s, partly as a result of surveillance activities of the global rinderpest eradication programme (GREP), but also because of the capacity of the infection to invade disease-free countries. The presence of infection restricts international trade in livestock and livestock products from infected countries, and is usually associated with ongoing severe losses where conditions exist that support epidemic spread among susceptible breeds, such as the incursions of infection into 'marginal' zones for persistence of infection such as humid zones of West Africa. Under such conditions there is a high social impact of disease, since small ruminants often represent a readily convertible currency in smallholder agriculture. Control by vaccination is merited in many endemic countries, and the benefit-to-cost ratio is usually high. The disease was also important as a complication in the eradication of rinderpest, since PPRV can infect cattle and the resultant antibodies must be distinguished from those elicited by rinderpest. The use of rinderpest vaccine to protect against PPR is no longer permitted now that rinderpest has been eradicated, to avoid the possibility of RP antibody detection in cattle or small ruminants. An attenuated strain of PPRV for use as a vaccine was developed in the late 1980’s (Diallo et al., 1989b) and is in wide use.

Please see the AHPC library for further information from OIE on this disease, including the International Animal Health Code and the Manual of Standards for Diagnostic Tests and Vaccines. Also see the website: www.oie.int.

Host Animals

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Animal nameContextLife stageSystem
Bos indicus (zebu)Domesticated hostCattle & Buffaloes: All Stages
Bubalus bubalis (Asian water buffalo)
Camelus dromedarius (dromedary camel)
Capra hircus (goats)Domesticated host, Wild hostSheep & Goats: All Stages
Ovis aries (sheep)Domesticated host, Wild hostSheep & Goats: All Stages

Hosts/Species Affected

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Disease occurs in goats and sheep, and has been recognized in wild ungulates from families of Gazellinae (Dorcas gazelle), Caprinae (Nubian ibex and Laristan sheep) and Hippotraginae (gemsbok) and other wild sheep/goats (Baron, 2011). Experimentally, severe disease also occurs in white-tailed deer. Cattle undergo mainly subclinical reactions, and pigs develop a viraemia. PPRV has been detected in diseased camels (Roger et al., 2001; Khalafalla et al., 2010; Kwiatek et al., 2011). West African Dwarf goats are more susceptible than European breeds (Scott, 1990), and sheep and goats of the Sahelian zones are more resistant than dwarf types from humid zones to the south (Bourdin, 1983). Seasonality in breeding, in marketing and in crop production all appear related to disease occurrence. In arid and semi-arid zones, surplus animals are sold during the dry season, which may lead to spread of infection into other areas, especially if sale occurs via markets. In humid zones, sale of surplus animals may occur at the start of the rains, with tethering of animals to avoid crop damage. Both sale of animals and close housing/tethering can increase risk of transmission if virus is introduced. The wet season can also predispose to secondary bacterial infections, exacerbating the viral pneumonia.

Systems Affected

Top of page digestive diseases of large ruminants
digestive diseases of small ruminants
respiratory diseases of large ruminants
respiratory diseases of small ruminants
skin and ocular diseases of large ruminants
skin and ocular diseases of small ruminants

Distribution

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The disease is recognized to be distributed from Tibet through the Middle East, and through most of Africa, From East to West, and from North Africa (Algeria, Tunisia, Morocco) south as far as Tanzania. For current information on disease incidence, see OIE's WAHID database.

The development of tests for the confirmation of the agent and the differentiation from rinderpest was only achieved in the late 1980s, and recent recognition of the infection in many African and Asian countries can be attributed to availability of methods for specific detection of virus and antibodies. However, given the rapidity of spread of epidemics and the lack of a carrier state, it is likely that infection is not maintained in some areas because of inadequate supply of susceptible animals and some incursions of disease appear self-limiting. Presence of infection in a country in one year does not imply endemic infection. However, the risk of trans-boundary spread of this disease is high because sheep and goats are easily transported and trade across borders is difficult to control. Recent extension of infection into China and a number of countries in Africa previously free of the disease (e.g. Kenya, Tanzania and several countries north of the Sahara) highlights the risk to previously free areas.

The number of countries in Africa reporting peste des petits ruminants (PPR) outbreaks to the African Union - Interafrican Bureau for Animal Resources (AU-IBAR; AU-IBAR, 2011)  has increased from 19 in 2008 to 20 in 2009, 25 in 2010 and 27 in 2011 as shown in the table below. Although the west, central and eastern Africa regions are regarded largely as endemic foci for PPR, the disease has been showing geographical advances towards the southern and northern regions of Africa; with Tanzania (2008) and Zambia (2010) in the south and Algeria (2011) in the north becoming the most recently affected countries on the continent. 

Out of the 27 countries that reported the disease in 2011, the majority also recorded the disease during the past three years. In total, 1185 epidemiological units were affected by PPR in 27 countries causing 101,016 cases and 62,388 deaths with a case fatality rate of 61.8%. The top three countries with highest number of outbreaks in descending order are Benin (285), Ghana (184) and Nigeria (126), all in West Africa.

Country

Outbreaks

Cases

Deaths

Slaughtered

Destroyed

Benin

285

12,559

3248

2516

14

Burkina Faso

7

745

270

0

0

Cameroon

19

315

102

12

0

CAR

34

2734

1571

0

16

Chad

19

425

252

21

26

Congo

37

1651

889

5

2

 DRC

70

62,635

49,121

16,237

1

Cote d'Ivoire

28

1283

513

112

21

Ethiopia

111

2113

527

62

50

Gabon

1

50

50

0

0

Gambia

2

20

15

2

20

Ghana

184

2319

823

87

22

Guinea

24

542

321

40

3

Guinea-Bissau

13

316

238

13

0

Liberia

1

 

87

0

0

Mali

3

272

76

14

0

Mauritania

6

82

3

0

0

Niger

16

990

523

 

2

Nigeria

126

5610

1533

688

17

Senegal

5

102

68

18

0

Sierra Leone

12

486

255

0

8

Somalia

20

352

148

28

10

Sudan

30

1367

585

0

0

Tanzania

2

28

23

 

38

Togo

101

2467

980

92

1

Tunisia

25

178

22

0

1199

Uganda

4

1,375

145

0

0

Total (27)

1185

101,016

62,388

19,947

1450

 There appears to be no defined temporal trend for the appearance of the disease as it occurs virtually uniformly throughout the year.

Distribution Table

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The distribution in this summary table is based on all the information available. When several references are cited, they may give conflicting information on the status. Further details may be available for individual references in the Distribution Table Details section which can be selected by going to Generate Report.

Continent/Country/RegionDistributionLast ReportedOriginFirst ReportedInvasiveReferenceNotes

Asia

AfghanistanPresentOIE, 2009
ArmeniaDisease not reportedOIE, 2009
AzerbaijanDisease never reportedOIE, 2009
BahrainDisease not reportedOIE, 2009
BangladeshPresentOIE, 2009
BhutanDisease never reportedOIE, 2009
Brunei DarussalamDisease not reportedOIE Handistatus, 2005
CambodiaNo information availableOIE, 2009
ChinaPresentOIE, 2009
-Hong KongDisease never reportedOIE, 2009
Georgia (Republic of)Disease never reportedOIE Handistatus, 2005
IndiaRestricted distributionOIE, 2009
IndonesiaDisease never reportedOIE, 2009
IranPresentOIE, 2009
IraqPresentNULLOIE, 2001a; OIE, 2009
IsraelDisease not reported200602OIE, 2003; OIE, 2009
JapanDisease never reportedOIE, 2009
JordanDisease not reportedOIE, 2009
KazakhstanDisease not reportedOIE, 2009
Korea, DPRDisease not reportedOIE Handistatus, 2005
Korea, Republic ofDisease never reportedOIE, 2009
KuwaitPresentOIE, 2009
KyrgyzstanDisease never reportedOIE, 2009
LaosDisease never reportedOIE, 2009
LebanonAbsent, reported but not confirmedOIE, 2009
MalaysiaDisease never reportedOIE, 2009
-Peninsular MalaysiaDisease never reportedOIE Handistatus, 2005
-SabahDisease never reportedOIE Handistatus, 2005
-SarawakDisease never reportedOIE Handistatus, 2005
MongoliaDisease never reportedOIE, 2009
MyanmarDisease never reportedOIE, 2009
NepalPresentOIE, 2009
OmanPresentOIE, 2009
PakistanRestricted distributionOIE, 2009
PhilippinesDisease never reportedOIE, 2009
QatarNo information availableOIE, 2009
Saudi ArabiaPresentOIE, 2009
SingaporeDisease never reportedOIE, 2009
Sri LankaDisease never reportedOIE, 2009
SyriaDisease not reportedOIE, 2009; OIE, 2009
SyriaPresentOIE, 2009; OIE, 2009
TaiwanDisease never reportedOIE Handistatus, 2005
TajikistanDisease not reportedOIE, 2009
ThailandDisease never reportedOIE, 2009
TurkeyPresentOIE, 2009
TurkmenistanDisease never reportedOIE Handistatus, 2005
United Arab EmiratesPresentNULLOIE, 2001a; OIE, 2009
UzbekistanDisease never reportedOIE Handistatus, 2005
VietnamDisease never reportedOIE, 2009
YemenPresentOIE, 2009

Africa

AlgeriaLast reported2012OIE, 2012
AngolaUnconfirmed recordOIE, 2012
BeninPresentOIE, 2012
BotswanaDisease never reportedOIE, 2012
Burkina FasoPresentOIE, 2012
BurundiDisease not reportedOIE Handistatus, 2005
CameroonOIE Handistatus, 2005
Cape VerdeDisease never reportedOIE Handistatus, 2005
Central African RepublicReported present or known to be presentOIE Handistatus, 2005
ChadNo information availableOIE, 2009
CongoPresentOIE, 2009
Congo Democratic RepublicReported present or known to be presentOIE Handistatus, 2005
Côte d'IvoireReported present or known to be presentNativeOIE, 2004; OIE Handistatus, 2005
DjiboutiDisease not reportedOIE, 2009
EgyptDisease not reportedOIE, 2009
EritreaPresentOIE, 2009
EthiopiaPresentOIE, 2009
GabonDisease not reportedOIE, 2009
GambiaPresentOIE, 2012
GhanaPresentOIE, 2012
GuineaPresentOIE, 2012
Guinea-BissauPresentAU-IBAR, 2011
KenyaPresentOIE, 2012
LesothoDisease never reportedOIE, 2012
LibyaDisease never reportedOIE, 2012
MadagascarDisease never reportedOIE, 2012
MalawiDisease never reportedOIE, 2012
MaliPresentOIE, 2001a; OIE, 2009; AU-IBAR, 2011
MauritaniaRestricted distributionOIE, 2012
MauritiusDisease never reportedOIE, 2009
MoroccoPresentOIE, 2012
MozambiqueDisease never reportedOIE, 2012
NamibiaDisease never reportedOIE, 2012
NigerRestricted distributionOIE, 2012
NigeriaPresentOIE, 2012
RéunionDisease never reportedOIE Handistatus, 2005
RwandaOIE, 2012
Sao Tome and PrincipeDisease not reportedOIE Handistatus, 2005
SenegalPresentOIE, 2012
SeychellesDisease not reportedOIE Handistatus, 2005
Sierra LeonePresentOIE, 2012
SomaliaPresentOIE, 2012
South AfricaDisease never reportedOIE, 2012
SudanPresentOIE, 2012
SwazilandDisease never reportedOIE, 2012
TanzaniaPresentOIE, 2012
TogoPresentOIE, 2012
TunisiaPresentOIE, 2012
UgandaPresentOIE, 2012
ZambiaPresentAU-IBAR, 2011
ZimbabweDisease never reportedOIE, 2012

North America

BermudaDisease not reportedOIE Handistatus, 2005
CanadaDisease never reportedOIE, 2009
GreenlandDisease never reportedOIE, 2009
MexicoDisease never reportedOIE, 2009
USADisease never reportedOIE, 2009

Central America and Caribbean

BarbadosDisease never reportedOIE Handistatus, 2005
BelizeDisease never reportedOIE, 2009
British Virgin IslandsDisease never reportedOIE Handistatus, 2005
Cayman IslandsDisease never reportedOIE Handistatus, 2005
Costa RicaDisease never reportedOIE, 2009
CubaDisease never reportedOIE, 2009
CuraçaoDisease not reportedOIE Handistatus, 2005
DominicaDisease not reportedOIE Handistatus, 2005
Dominican RepublicDisease never reportedOIE, 2009
El SalvadorDisease never reportedOIE, 2009
GuadeloupeDisease never reportedOIE, 2009
GuatemalaDisease never reportedOIE, 2009
HaitiDisease never reportedOIE, 2009
HondurasDisease never reportedOIE, 2009
JamaicaNo information availableOIE, 2009
MartiniqueDisease never reportedOIE, 2009
NicaraguaDisease never reportedOIE, 2009
PanamaDisease never reportedOIE, 2009
Saint Kitts and NevisDisease never reportedOIE Handistatus, 2005
Saint Vincent and the GrenadinesDisease never reportedOIE Handistatus, 2005
Trinidad and TobagoDisease never reportedOIE Handistatus, 2005

South America

ArgentinaDisease never reportedOIE, 2009
BoliviaDisease never reportedOIE, 2009
BrazilDisease never reportedOIE, 2009
ChileDisease never reportedOIE, 2009
ColombiaDisease never reportedOIE, 2009
EcuadorDisease never reportedOIE, 2009
Falkland IslandsDisease never reportedOIE Handistatus, 2005
French GuianaDisease never reportedOIE, 2009
GuyanaDisease never reportedOIE Handistatus, 2005
ParaguayDisease never reportedOIE Handistatus, 2005
PeruDisease never reportedOIE, 2009
UruguayDisease never reportedOIE, 2009
VenezuelaDisease never reportedOIE, 2009

Europe

AlbaniaDisease never reportedOIE, 2009
AndorraDisease never reportedOIE Handistatus, 2005
AustriaDisease never reportedOIE, 2009
BelarusDisease never reportedOIE, 2009
BelgiumDisease never reportedOIE, 2009
Bosnia-HercegovinaDisease never reportedOIE Handistatus, 2005
BulgariaDisease never reportedOIE, 2009
CroatiaDisease never reportedOIE, 2009
CyprusDisease never reportedOIE, 2009
Czech RepublicDisease never reportedOIE, 2009
DenmarkDisease never reportedOIE, 2009
EstoniaDisease never reportedOIE, 2009
FinlandDisease never reportedOIE, 2009
FranceDisease never reportedOIE, 2009
GermanyDisease never reportedOIE, 2009
GreeceDisease never reportedOIE, 2009
HungaryDisease never reportedOIE, 2009
IcelandDisease never reportedOIE, 2009
IrelandDisease never reportedOIE, 2009
Isle of Man (UK)Disease never reportedOIE Handistatus, 2005
ItalyDisease never reportedOIE, 2009
JerseyDisease never reportedOIE Handistatus, 2005
LatviaDisease never reportedOIE, 2009
LiechtensteinDisease never reportedOIE, 2009
LithuaniaDisease never reportedOIE, 2009
LuxembourgDisease never reportedOIE, 2009
MacedoniaDisease never reportedOIE, 2009
MaltaDisease never reportedOIE, 2009
MoldovaDisease never reportedOIE Handistatus, 2005
MontenegroDisease never reportedOIE, 2009
NetherlandsDisease never reportedOIE, 2009
NorwayDisease never reportedOIE, 2009
PolandDisease never reportedOIE, 2009
PortugalDisease never reportedOIE, 2009
RomaniaDisease never reportedOIE, 2009
Russian FederationDisease never reportedOIE, 2009
SerbiaDisease never reportedOIE, 2009
SlovakiaDisease never reportedOIE, 2009
SloveniaDisease never reportedOIE, 2009
SpainDisease never reportedOIE, 2009
SwedenDisease never reportedOIE, 2009
SwitzerlandDisease never reportedOIE, 2009
UKDisease never reportedOIE, 2009
-Northern IrelandDisease never reportedOIE Handistatus, 2005
UkraineDisease never reportedOIE, 2009
Yugoslavia (former)Disease never reportedOIE Handistatus, 2005
Yugoslavia (Serbia and Montenegro)Disease never reportedOIE Handistatus, 2005

Oceania

AustraliaDisease never reportedOIE, 2009
French PolynesiaDisease never reportedOIE, 2009
New CaledoniaDisease never reportedOIE, 2009
New ZealandDisease never reportedOIE, 2009
SamoaDisease never reportedOIE Handistatus, 2005
VanuatuDisease never reportedOIE Handistatus, 2005
Wallis and Futuna IslandsNo information availableOIE Handistatus, 2005

Pathology

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The carcass is usually dehydrated, and soiled with faeces. The peri-orbital and perinasal areas are usually encrusted with muco-purulent discharges. The erosions and ulcerations in the mouth and throat are usually prominent, as is the presence of the secondary broncho-pneumonia. The underlying primary viral pneumonia may be less obvious but is manifested by areas of level red consolidation (Rowland et al., 1969). 'Zebra striping' in the colon may also be seen, and lympadenopathy.

The most important histopathological indicator of PPRV is the presence of multi-nucleated giant cells containing intra-nuclear and intra-cytoplasmic inclusions. Multi-nucleated giant cells (syncytia) are most readily detected in the lungs, but also occur in bronchial, alveolar and ileal epithelium.

Diagnosis

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Clinical Diagnosis


A manual on the diagnosis of PPR has been produced (FAO, 1998). Suspicion of PPR would be raised by signs of stomatitis – or pneumonitis, with enteritis in several animals. A high mortality and morbidity rate would be expected in outbreaks occurring in non-endemic areas, or where outbreaks have not occurred for some time and animals are not vaccinated. The occurrence of both stomatitis, with erosions/ulcerations of epithelial surfaces in the oral cavity, together with diarrhoea, occurs in few other single diseases of sheep and goats. In an outbreak situation, early signs of infection, such as oculo-nasal discharges and fever, would be expected for in-contact animals, if some of the group have reached the late stage of the disease or have died. In most countries PPR is a notifiable disease and the authorities require to be informed if the infection is suspected. Given the infectivity of individual animals, immediate actions or advice to community leaders to contain movement of in-contact animals are important to reduce local spread while investigations are proceeding.


Differential Diagnosis


Other conditions to be considered are: contagious caprine pleuropneumonia, bluetongue, pasteurellosis, contagious ecthyma, foot-and-mouth disease, heartwater, coccidiosis, mineral poisoning.

Bluetongue infection occurs in many countries that are endemic or at-risk from PPR incursion. It can give rise to a muco-purulent discharge and high morbidity and mortality rate in susceptible sheep, but usually less so in goats. It does not usually result in a severe enteritis, although loose stools may occur, or erosions/ulcerations of epithelial surfaces. Bluetongue usually gives rise to visible signs of haemorrhage on the coronary band of the foot, in contrast to PPR.

Foot-and-mouth disease affects other stock as well as sheep and goats; cattle in the region would be expected to show more severe signs than sheep or goats. On occasion though, the disease is more severe in the latter, and cattle may be absent. However, the enteritis usually present in PPR is not seen in FMD.

The lesions of orf (contagious ecthyma) and sheep and goat pox differ in distribution to that of PPR, but animals recovering from PPR may develop proliferative growths on the lips resembling orf, and the virus may be involved in the pathogenesis of the condition. Contagious caprine pleuropneumonia occurs in many similar countries to PPR but does not usually give a high mortality in sheep, or have an accompanying severe enteritis. Heartwater can give a high mortality rate in susecptible breeds, but without a stomatitis.


Laboratory Diagnosis


Detection of the virus


PPRV is present at a high concentration in secretions and tissue samples in the early stages of the disease, but rapidly becomes difficult to detect after development of antibody responses. Collection of specimens from animals which have a serous ocular-nasal discharge and fever is preferable compared to later-stage signs of necrotic stomatitis-enteritis. The Manual of Standards of the Office International des Epizooties (OIE, 2008) gives a description of the recommended samples to be collected. In live animals, swabs should be made of the conjunctival discharges from the nasal and buccal mucosae. Whole blood should be collected in anticoagulant for virus isolation, polymerase chain reaction (PCR) and haematology. From the necropsy examination of two to three animals, lymph nodes, especially the mesenteric and bronchial nodes, lungs, spleen and intestinal mucosae should also be collected aseptically, chilled on ice and transported under refrigeration. Fragments of organs collected for histopathology are placed in 10% formalin. At the end of the outbreak, blood can be collected for serological diagnosis. The priority is therefore to collect suitable specimens from early cases, after discussion with the national veterinary laboratory and Government officers of the country concerned as to their capability and preferred system for laboratory confirmation. Post-mortem examination of carcasses can be valuable, particularly in wildlife and in situations where samples cannot be kept in suitable conditions during transport to the laboratory, with a view to collection of specimens for detection of multi-nucleated giant cells by histopathology. Infection can be confirmed by identification of the agent with specific tests. Detection of a rise in titre of antibody could also be used, with paired samples collected 14-21 days apart.

Several methods for detection of virus are recognized by the Office International des Epizooties (OIE, 2008). Of these, agar gel immuno-diffusion (AGID) and counter-immuno-electrophoresis (CIEP) are relatively simple and suitable for small-scale field centres and simple laboratories. The latter gives a faster result than the former, enabling detection in less than 2 hours. Antigen-capture ELISA using monoclonal antibodies is sensitive and specific (Libeau et al., 1994). The availability of the ELISA as a kit has undoubtedly assisted countries in the detection of PPR epidemics, and provides a standardised test. Molecular tests using gene probes have been superseded by PCR-based tests (Forsyth and Barrett, 1995), and these in turn have been superseded by real-time or quantitative PCR-based tests (Bao et al., 2008; Kwiatek et al., 2010; Batten et al., 2011). PCR is extremely sensitive and specific, and may be of advantage in testing tissues where virus cannot be detected by other means, including specimens for histopathology. However, the time taken to extract RNA, and undertake the RT-PCR is usually longer than that needed for CIEP, and higher technical standards are required to avoid false-positive reactions. Other tests have been described, including simple staining methods for detecting syncitia in conjunctival cells collected onto glass slides which are suitable for simple field use (Sumption et al., 1998), and monoclonal-based staining of such cells, or infected cells in histopathological sections (Saliki et al., 1994).

The OIE Manual (OIE, 2008) recommends efforts are made to isolate the virus from outbreaks of disease, and this is particularly relevant, although more difficult, in countries where it is suspected for the first time. The FAO (Food and Agriculture Organization of the United Nations) Reference Laboratories for PPR are given on the OIE website, and are currently at CIRAD-EMVT, Montpellier, France or the Institute for Animal Health, Pirbright, Surrey, UK; either laboratory can advise on the use of various techniques for virus identification in field samples.


Serological tests

Antibodies are strongly induced by infection, and become detectable from the diarrheic stage onwards. The prescribed test for international trade (that which is accepted as a basis for the veterinary certification of animals as having evidence of presence or absence of antibodies) is virus neutralisation (VNT; OIE, 2008). Since there is cross-neutralisation between antibodies to PPR and RPV, a positive VNT result to PPR virus used to need to be compared to the titre obtained with RPV. The OIE considered that a serum is considered to be positive for PPR when the neutralisation titre is at least two-fold higher for PPR than for rinderpest. Since the eradication of RPV, this comparison is not required and indeed continued use of RPV in laboratories is strongly discouraged. Virus neutralisation tests involve use of live virus and cell cultures, and therefore require well-equipped laboratories and biosecurity to prevent escape of virus. VNT is therefore mainly restricted to laboratories with sufficient expertise and through-put of samples to justify the investment involved. The development of competition ELISA (C-ELISA) tests using monoclonal antibodies to either H (Anderson and McKay, 1994) or N (Libeau et al., 1995) antigens has extended the access to serological tests, and proved valuable in investigation of PPR epidemiology in the field. The tests are sensitive and specific. Kits are available from international organizations (IAEA, Vienna) and from the World Reference Laboratories for PPR in France, and the Institute for Animal Health in Pirbright, UK. Haemagglutination inhibition tests for antibody have also been described with good correlation with VNT (Raj et al., 2000).

List of Symptoms/Signs

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SignLife StagesType
Digestive Signs / Anorexia, loss or decreased appetite, not nursing, off feed Sign
Digestive Signs / Bloody stools, faeces, haematochezia Sign
Digestive Signs / Congestion oral mucous membranes, erythema, redness oral mucosa Sign
Digestive Signs / Diarrhoea Sheep & Goats:All Stages Diagnosis
Digestive Signs / Excessive salivation, frothing at the mouth, ptyalism Sheep & Goats:All Stages Sign
Digestive Signs / Mucous, mucoid stools, faeces Sign
Digestive Signs / Oral mucosal ulcers, vesicles, plaques, pustules, erosions, tears Sheep & Goats:All Stages Diagnosis
Digestive Signs / Tongue ulcers, vesicles, erosions, sores, blisters, cuts, tears Sign
General Signs / Dehydration Sheep & Goats:All Stages Sign
General Signs / Fever, pyrexia, hyperthermia Sheep & Goats:All Stages Sign
General Signs / Generalized weakness, paresis, paralysis Sign
General Signs / Inability to stand, downer, prostration Sign
General Signs / Sweating excessively, hyperhidrosis Sign
General Signs / Tenesmus, straining, dyschezia Sheep & Goats:All Stages Sign
General Signs / Underweight, poor condition, thin, emaciated, unthriftiness, ill thrift Sign
General Signs / Weight loss Sign
Nervous Signs / Dullness, depression, lethargy, depressed, lethargic, listless Sign
Ophthalmology Signs / Chemosis, conjunctival, scleral edema, swelling Sign
Ophthalmology Signs / Conjunctival, scleral, redness Sign
Ophthalmology Signs / Corneal edema, opacity Sign
Ophthalmology Signs / Lacrimation, tearing, serous ocular discharge, watery eyes Sheep & Goats:All Stages Diagnosis
Ophthalmology Signs / Purulent discharge from eye Sign
Pain / Discomfort Signs / Mouth, oral mucosal or tongue pain Sheep & Goats:All Stages Sign
Reproductive Signs / Abortion or weak newborns, stillbirth Sheep & Goats:All Stages Sign
Reproductive Signs / Agalactia, decreased, absent milk production Sign
Reproductive Signs / Papule, pustule, vesicle, ulcer penis or prepuce Sign
Reproductive Signs / Vaginal or cervical ulcers, vesicles, erosions, tears, papules, pustules Sign
Respiratory Signs / Abnormal breath odor, foul odor mouth Sheep & Goats:All Stages Sign
Respiratory Signs / Abnormal breathing sounds of the upper airway, airflow obstruction, stertor, snoring Sign
Respiratory Signs / Abnormal lung or pleural sounds, rales, crackles, wheezes, friction rubs Sign
Respiratory Signs / Coughing, coughs Sheep & Goats:All Stages Sign
Respiratory Signs / Dull areas on percussion of chest, thorax Sheep & Goats:All Stages Sign
Respiratory Signs / Dyspnea, difficult, open mouth breathing, grunt, gasping Sign
Respiratory Signs / Epistaxis, nosebleed, nasal haemorrhage, bleeding Sign
Respiratory Signs / Increased respiratory rate, polypnea, tachypnea, hyperpnea Sheep & Goats:All Stages Sign
Respiratory Signs / Mucoid nasal discharge, serous, watery Sheep & Goats:All Stages Diagnosis
Respiratory Signs / Purulent nasal discharge Sheep & Goats:All Stages Diagnosis
Respiratory Signs / Sneezing, sneeze Sheep & Goats:All Stages Sign
Skin / Integumentary Signs / Skin crusts, scabs Sign

Disease Course

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The pathogenesis has been little studied but what we do know shows it to be essentially similar to rinderpest virus, with infection occurring via aerosols, or ingestion by nuzzling or licking, with entry through the oropharynx and subsequent multiplication in the draining lymph nodes, and thereafter in lymph nodes through the body. Virus is then released which enters the circulation and is transported to the epithelium, where it multiplies in susceptible cells, resulting in the development of lesions and disease signs associated with damage to these sites (Rossiter and Taylor, 1993).

The course of infection is swift, with an incubation period of 2 to 6 days, with death usually occurring within 14 days of infection, 5 to 7 days after onset of pyrexia. The course of infection is development of fever, followed by ocular and nasal discharges and later erosions of the epithelial surfaces of the mouth and/or gums and onset of diarrhoea. Death occurs by dehydration, complicated by pneumonia.

The first signs are of fever, with a serous nasal discharge, followed within hours by depression. Pale areas of necrosis become visible on the gums, which develop into erosions develop in the mucous membranes lining the upper alimentary, upper respiratory and uro-genital tracts 1 to 2 days after onset of fever. Salivation becomes profuse, and the nasal discharge becomes muco-purulent and may block the nostrils, and muco-purulent ocular secretions may mat the eyelids together. Ulceration of the lesions in the alimentary tract contributes to a debilitating diarrhoea, and rapid loss of condition. Pneumonia commonly occurs, with frequent secondary infections with Pasteurella, and other latent infections including Mycoplasma capri, adenoviruses, orf virus and dermatophilosis. The condition is rapidly debilitating and death may rapidly occur after development of the diarrhoea/pneumonia. Affected animals have an exceptionally miserable appearance, and recovery is slow, often accompanied by growths on the lips, attributed to recrudescence of orf virus and/or exacerbation of Dermatophilus congolense infection (Scott, 1990).

Epidemiology

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PPRV has a direct life cycle, maintained by infected animal to susceptible animal transmission, without involvement of carrier animals or vectors. The underlying requirement is a regular supply of susceptible hosts plus sufficient animal movement to allow mixing of the population (Rossiter and Taylor, 1993). Risk factors include unconfined husbandry, whether in urban or rural settings. The population size required to maintain infection is not known, but small populations probably cannot maintain infection for long and, therefore, given the rapid population turnover of small ruminants, disease associated with re-introduction can be severe. Severe epidemics probably reflect introduction of virus into areas with mainly susceptible populations and breeds, rather than endemic presence of infection throughout the year (Rossiter and Taylor, 1993). Re-introduction of infection at intervals appear frequently related to livestock movement into areas, for example introduction for slaughter at festivals (Bonniwell, 1980). There is one serotype of virus, and immunity is long-lasting, probably life-long. Because colostral antibody protects young animals, in endemic areas most disease occurs in animals after waning of colostral immunity, from 4 months to 2 years of age, with protection of animals which have had previous exposure. Serological studies indicate that many, if not most, infections are subclinical or insufficiently severe to attract attention, and this may be related to breed resistance. Mortality rate in areas considered endemic may be in the region of 4-5% whereas rates from 20% to 90% in outbreaks have frequently been reported under epidemic conditions (Rossiter and Taylor, 1993). Climate appears to play a role in increasing the severity of disease, via secondary infections exacerbating the infection of the lung, but also affects the migration of pastoralist flocks in response to rainfall and drought and the resultant exposure to infection.

The virus will infect a range of ruminant hosts, but appears to cause disease in only goats, sheep, certain antelope species and occasionally water buffalo (Govindarajan et al, 1997). The virus will infect cattle and pigs, but subclinically; potentially these species might be involved in transmission between small-ruminant populations, although evidence that this is important in the field is lacking. Infection of cattle with PPRV protects against rinderpest virus, and the exposure rates of cattle in West Africa to PPRV may have contributed to a failure to induce antibodies to RPV after vaccination (Anderson and McKay, 1994), and also to the rapidity of eradication efforts against RPV in this region. In the same way, antibodies to RPV can protect sheep/goats from PPRV (Taylor, 1979), and it is possible that the recent rapid spread of PPR may be due to the eradication of RP and the cessation of vaccination against this disease. Antibodies to RPV can be distinguished from those to PPRV in cattle by use of monoclonal antibody based tests. PPR virus isolates differ in their pathogenicity for each host, with some strains resulting in more disease in sheep than goats. However, the outcome of infection is also markedly affected by animal breed, with some breeds from Sahelian countries showing marked resistance in contrast to those of West African humid zones (Bourdin, 1983).

Impact: Economic

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The annual toll of infection in Nigeria in 1976 was US$1.5 million (Hamdy et al., 1976). The disease contributes to loss of the live export trade in sheep and goats because PPR is a list A disease; however, in most countries where it occurs other list A diseases would also require to be eradicated or controlled before PPRV was the limiting constraint to trade. Stem (1993) estimated a US$24 million return on an investment of US$2 million in PPR control in Niger over a 5-year period. Awa et al. (2000) also indicated benefit-to-cost ratios of 2.26 to 4.23 for a PPR vaccination and strategic anthelminthic programme in Cameroon.

Zoonoses and Food Safety

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PPR virus has not been shown to present any risk to human health. However, the carcasses of animals suffering from PPR are unlikely to provide good-quality meat and should be buried or destroyed by heat.

Disease Treatment

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There is no treatment for PPRV infection itself, but antibiotics may be given to prevent secondary infections and other treatments given to alleviate the clinical signs.

Chloramphenicol 10 ml/kg body weight, penicillin 10,000 IU/kg, streptomycin 10 mg/kg, each given intramuscularly for 5 days), intestinal sedatives (Entero Sediv, 20 ml/kg for 4 days orally) and fluid therapy (Pedialyte, 30 ml/kg, for 4 days subcutaneously) were used to treat pneumonia, diarrhoea and restore body fluid ionic balance (Wosu, 1989).

Prevention and Control

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Immunization and Vaccines

A live, attenuated strain (PPRV Nigeria 75/1) of the PPR virus has been developed for use as a vaccine and provides protection for over 3 years (Diallo et al., 1989b). Other attenuated strains of PPRV have been developed in India (for review, see Sen et al., 2010). These vaccines have superseded the use of an attenuated rinderpest vaccine, whose use is no longer permitted following the eradication of RPV. Previous trials (usually with RP vaccine) reported reduction in mortality, particularly in weaned young stock, and positive benefit-to-cost ratios. A reduction in mortality of 24% was reported in Nigeria compared to controls, for a combined vaccination and dipping programme (Reynolds and Francis, 1988). In Cameroon, a benefit to cost ratio of between 2.26 and 4.23 was reported for goats and sheep through use of PPR vaccination and strategic anthelminthic treatment (Awa et al., 2000). In Niger, Stem (1993) estimated an internal rate of return of 900% for a PPRV vaccination programme over 5 years.

Husbandry methods and good practice

Risk factors for occurrence of disease are the purchase of animals from markets, and free-range husbandry of animals, when PPRV is known to be present in the region. In Oman, animals under controlled grazing (e.g. fenced or paddocked) were at lower risk than free-ranging urban livestock (Taylor et al., 1990).

Local Control

Movement control, at the level of total standstill of livestock movements and banning of markets may be effective if enforceable and short-lasting in duration, since the incubation period is short. However, an effective quarantine of affected and in-contact animals for one month after the recovery of the last clinically affected case has been recommended (Rossiter and Taylor, 1993). These measures may be accompanied by a slaughter policy of animals on infected and in-contact premises, in addition to the ban on livestock movements, if the aim is rapid eradication. Measures that negatively affect livelihoods will be unpopular and difficult to enforce unless accompanied by incentives, and have rarely been implemented by authorities.

National and International Control Policy

PPR is a list A disease of the OIE, and thus member states are required to inform the OIE of the occurrence of the disease in their territory. The OIE publishes recommendations for zoo-sanitary conditions and certification of trade in animals and livestock products from countries which are not recognized as having freedom from PPR disease (OIE, 2011). The OIE recommends sanitary prophylaxis (movement control, quarantine of infected premises, with slaughter of infected animals and in-contacts) when the disease appears in previously PPR-free countries. The use of a stamping-out policy, involving slaughter of infecteds and in-contact animals on infected premises, can lead to a reduced period of time elapsing after the last case of disease has been reported before the country is internationally recognized as free of PPR.

The Animal Health Code of the OIE (OIE, 2011) considers:

  • the period for quarantine purposes, ('incubation period') for the peste des petits ruminants (PPR) to be 21 days.
  • A country may be considered free from PPR when it has been shown that PPR has not been present for at least the past 3 years.
  • Or, this period shall be 6 months after the slaughter of the last affected animal for countries in which a stamping-out policy is practised with or without vaccination against PPR.

The Code also recognizes the presence of zones of infection, which shall be considered as infected with PPR until:

  • at least 21 days have elapsed after the confirmation of the last case and the completion of a stamping-out policy and disinfection procedures, or
  • until 6 months have elapsed after the clinical recovery or death of the last affected animal if a stamping-out policy was not practised.

The risk of entry of PPR into PPR-free countries is dealt with mainly by a strict prohibition of the import of live animals, recognizing that the majority of importations of virus have been via entry of live animals. The Animal Health Code of the OIE recognizes that Veterinary Administrations of PPR-free countries may prohibit importation or transit through their territory, from countries considered infected with PPR:

  • of domestic and wild ruminants,

  • semen of ruminants,

  • embryos/ova of ruminants,

  • fresh meat of domestic and wild ruminants,

  • meat products of domestic and wild ruminants that have not been processed to ensure the destruction of the PPR virus,

  • products of animal origin (from ruminants) intended for use in animal feeding or for agricultural or industrial use which have not been processed to ensure the destruction of the PPR virus,

  • products of animal origin (from ruminants)intended for pharmaceutical or surgical use which have not been processed to ensure the destruction of the PPR virus,

  • pathological material and biological products (from ruminants) which have not been processed to ensure the destruction of the PPR virus.

For each of the above, the Animal Health Code recommends the use of sanitary measures, including (where required) laboratory test results, backed by international veterinary certificates to ensure that within the boundary of error associated with test or quarantine procedures, the animals and animal products are free of disease and/or infection at the time of importation. For example, for importation of small ruminants from countries not free of PPR, Veterinary Administrations should require the presentation of an international veterinary certificate attesting that the animals:

  • showed no clinical sign of PPR on the day of shipment;

  • were kept since birth, or for the past 21 days, in an establishmentwhere no case of PPR was officially reported during that period, and that the establishment was not situated in a PPR-infected zone; and/or

  • were kept in a quarantine station for the 21 days prior to shipment;

  • have not been vaccinated against PPR; or were vaccinated against PPR: not less than 15 days and not more than 4 months prior to shipment in the case of animals for breeding or rearing; or not less than 15 days and not more than 12 months prior to shipment in the case of animals for slaughter.

Importing countries may in addition impose additional conditions on the importation, that is, do not allow importation despite these conditions being fulfilled; they might be challenged in international courts, with the OIE acting as independent assessors of the risk involved in the importation.

There is at present no international programme for PPR control; the situation differs in each country according to the level of state subsidy, if any, for disease control programmes and the degree of emphasis on the private sector to undertake vaccination under a demand and supply system. Positive ratios for benefit-to-cost of national programmes have been reported (Stem, 1993) and increase in small-ruminant numbers in Oman was attributed to control of PPR by vaccination (Rossiter and Taylor, 1993). Additional controls on PPRV may be required if the infection adapts to fill the void left by lack of immunity to RP after eradication of rinderpest, since PPRV can infect cattle and in almost all PPR-endemic countries, RP has been present for at least the twentieth century. Morbilliviruses are highly adaptable, and the potential of PPRV to adapt to transmission via cattle requires monitoring, and continued vigilance for RP-like infections after RP eradication.

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Links to Websites

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WebsiteURLComment
CFSPH: Animal Disease Informationhttp://www.cfsph.iastate.edu/DiseaseInfo/index.php"Animal Disease Information" provides links to various information sources, including fact sheets and images, on over 150 animal diseases of international significance.
FAO: Supporting livelihoods and building resilience through Peste des Petits Ruminantshttp://www.fao.org/docrep/017/aq236e/aq236e.pdfFAO. 2013. Supporting livelihoods and building resilience through Peste des Petits Ruminants (PPR) and small ruminant diseases control. Animal Production and Health Position Paper. Rome.
OIE Manual of Diagnostic Tests and Vaccines for Terrestrial Animalshttp://www.oie.int/en/international-standard-setting/terrestrial-manual/access-online/The Manual of Diagnostic Tests and Vaccines for Terrestrial Animals (Terrestrial Manual) aims to facilitate international trade in animals and animal products and to contribute to the improvement of animal health services world-wide. The principal target readership is laboratories carrying out veterinary diagnostic tests and surveillance, plus vaccine manufacturers and regulatory authorities in Member Countries. The objective is to provide internationally agreed diagnostic laboratory methods and requirements for the production and control of vaccines and other biological products.
OIE Technical Disease Cardshttp://www.oie.int/animal-health-in-the-world/technical-disease-cards/An updated compilation of 33 technical disease cards, containing summary information, mainly directed to a specialised scientific audience, including 32 OIE-listed priority diseases. USDA-APHIS (USA) are also credited with contributing to the maintenance of the cards.
OIE Terrestrial Animal Health Codehttp://www.oie.int/en/international-standard-setting/terrestrial-code/access-online/The OIE Terrestrial Animal Health Code sets out standards for the improvement of terrestrial animal health and welfare and veterinary public health worldwide, including through standards for safe international trade in terrestrial animals and their products. The health measures in the Terrestrial Code should be used by the veterinary authorities of importing and exporting countries to provide for early detection, reporting and control agents pathogenic to terrestrial animals and, in the case of zoonoses, for humans, and to prevent their transfer via international trade in terrestrial animals and terrestrial animal products, while avoiding unjustified sanitary barriers to trade.
USAHA: Foreign Animal Diseases. Seventh Editionhttp://www.aphis.usda.gov/emergency_response/downloads/nahems/fad.pdfCopyright © 2008 by United States Animal Health Association ALL RIGHTS RESERVED. Library of Congress Catalogue Number 2008900990 ISBN 978-0-9659583-4-9. Publication with 472pp. aimed at providing information for practitioners within the USA to prevent and or mitigate the incursion of foreign animal diseases into that country. Contains general chapters on surveillance, diagnosis, etc. as well as 48 chapters covering individual diseases, mostly those notifiable to the OIE.

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