Selected content from the Animal Health and Production Compendium (© CAB International 2013). Distributed under license by African Union – Interafrican Bureau for Animal Resources.
Whilst this information is provided by experts, we advise that users seek veterinary advice where appropriate and check OIE manuals for recent changes to regulations, diagnostic tests, vaccines and treatments.
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Identity Pathogen/s Overview Distribution Distribution Map for Africa Distribution Table for Africa Host Animals Systems Affected Epidemiology Diagnosis Disease Course Disease Treatment Table Disease Treatment Vaccines Prevention and Control References Links to Websites OIE Reference Experts and Laboratories Images
Preferred Scientific Name
foot-and-mouth disease in pigs
International Common Names
foot and mouth, foot and mouth disease in ruminants and pigs - exotic
aftosa, fiebre aftosa
foot-and-mouth disease virus
Foot-and-mouth disease (FMD) is a highly contagious viral disease of cloven footed animals (artiodactyls), characterised by fever, vesicles on the buccal mucosa and feet and sudden death in the young of susceptible species. FMD is caused by an aphthovirus, an RNA virus with a positive-sense single-stranded genome, in the family Picornaviridae. There are seven serotypes of FMD virus, namely O, A, C, ASIA 1, SAT (South African Territories) 1, SAT 2, and SAT 3. Domestic cattle, pigs, sheep, goats, buffalo and all species of wild ruminant and pig are susceptible. FMD is an OIE (Office International des Epizooties) List disease, and is probably the most important constraint to trade in live animals and their products (Kitching, 1998).
The distribution section contains data from OIE's World Animal Health Information Database (WAHID) on disease occurrence. Please see the AHPC library for further information on this disease from OIE, including the International Animal Health Code and the Manual of Standards for Diagnostic Tests and Vaccines. Also see the website: www.oie.int.
FMD is endemic in Africa, most of Asia, the Middle East and parts of South America. Analysis of outbreak data over a number of years has demonstrated the global clustering of FMD viruses and identified 7 virus pools, where multiple serotypes occur but within which are topotypes that remain mostly confined to that pool (Hammond et al., 2011). The World Reference Laboratory for FMD (WRLFMD®) have defined 3 pools covering Europe, the Middle-East and Asia containing serotypes O, A and Asia 1, 3 pools covering Africa containing serotypes O, A, and SATs 1, 2 & 3 and 1 pool covering the Americas containing serotypes O and A. This distribution enables a regional approach to be taken to assist global control of FMD. An increased regional knowledge of FMD outbreaks and identification of these within particular reservoirs or pools of FMD activity can greatly assist globally informed regional FMD control programmes. It also follows that if vaccination is to be a major tool for control, each pool could benefit from investigation into the use of tailored or more specific vaccines relevant to the topotypes present in that pool, rather than a continued reliance on the currently more widely available vaccines.
Over recent years there has been a notable increase in the incidence of FMD outbreaks reported in Asia and the Middle East and a concurrent spread of the serotypes O (Pan-Asia 2 strain) and A (Iran 05 strain). In 2010-2011 Japan, Republic of Korea and Bulgaria all suffered type O FMD outbreaks, losing their status as countries listed by OIE as FMD-free without vaccination. In 2012 Japan and Bulgaria regained their status as free without vaccination but the Republic of Korea has embarked on a prolonged programme of vaccination.
Current trends show that globally the serotype most commonly identified is type O, with more than 80% of isolates characterized by the OIE/FAO FMD reference laboratory network in 2010-2011 being of this serotype (Hammond, 2012). However, in 2011-2012 there has been a marked increase in the number of reports of serotypes Asia 1 in pool 3 and in early 2012 a rapid spread of SAT 2 through North Africa into Libya and Egypt and on into the Middle East to the Palestine Autonomous Territories. In 2012 so far WRLFMD® have observed that more than 25% of samples tested were found to be type Asia 1 and 14% to be SAT 2 (Hammond et al., 2012).
Serotype C has not been reported since 2004 where it was detected in Brazil and Kenya. However, it may still be present in regions where surveillance is minimal or not possible due to difficult or restricted access. The SAT serotypes have never established outside of Africa, although in 2000, SAT 2 was found in Saudi Arabia and in 2012 spread from Egypt to Palestine Autonomous Territories.
The World Reference Laboratory for foot and mouth disease (WRLFMD®) located at the renamed Pirbright Institute, UK (formerly The Institute for Animal Health) is responsible for maintaining global surveillance and coordinating the OIE/FAO FMD reference laboratory network. Much of the information generated by WRLFMD® is available on their website located at http://www.pirbright.ac.uk/.
OIE publishes a report each year in which it lists FMD-free countries (see: www.oie.int/en/animal-health-in-the-world/official-disease-status/fmd/list-of-fmd-free-members/).
= Present, no further details = Widespread = Localised
= Confined and subject to quarantine = Occasional or few reports
= Evidence of pathogen = Last reported... = Presence unconfirmed
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 information for individual references may be available in the Animal Health and Production Compendium. A table for worldwide distribution can also be found in the Animal Health and Production Compendium.
|Country||Distribution||Last Reported||Origin||First Reported||Invasive||References||Notes|
|Algeria||Last reported||1999||OIE Handistatus, 2005|
|Angola||Last reported||2001||OIE Handistatus, 2005|
|Benin||Reported present or known to be present||OIE Handistatus, 2005|
|Botswana||Last reported||2003||OIE Handistatus, 2005|
|Burkina Faso||Reported present or known to be present||OIE Handistatus, 2005|
|Burundi||Reported present or known to be present||OIE Handistatus, 2005|
|Cameroon||OIE Handistatus, 2005|
|Cape Verde||Disease never reported||OIE Handistatus, 2005|
|Central African Republic||Reported present or known to be present||OIE Handistatus, 2005|
|Chad||Reported present or known to be present||OIE Handistatus, 2005|
|Congo Democratic Republic||No information available||OIE Handistatus, 2005|
|Côte d'Ivoire||CAB Abstracts data mining||OIE Handistatus, 2005|
|Djibouti||Disease not reported||OIE Handistatus, 2005|
|Egypt||Last reported||2000||OIE Handistatus, 2005|
|Eritrea||Reported present or known to be present||OIE Handistatus, 2005|
|Ethiopia||Reported present or known to be present||OIE Handistatus, 2005|
|Ghana||Reported present or known to be present||OIE Handistatus, 2005|
|Guinea||Last reported||2001||OIE Handistatus, 2005|
|Guinea-Bissau||Disease not reported||OIE Handistatus, 2005|
|Kenya||Reported present or known to be present||OIE Handistatus, 2005|
|Libya||Last reported||2003||Native||OIE, 2004c; OIE Handistatus, 2005|
|Madagascar||Disease never reported||OIE Handistatus, 2005|
|Malawi||OIE Handistatus, 2005|
|Mali||Reported present or known to be present||OIE Handistatus, 2005|
|Mauritius||Disease never reported||OIE Handistatus, 2005|
|Morocco||Last reported||1999||OIE Handistatus, 2005|
|Mozambique||Last reported||2003||OIE Handistatus, 2005|
|Namibia||Last reported||2000||OIE Handistatus, 2005|
|Niger||Reported present or known to be present||OIE Handistatus, 2005|
|Nigeria||Reported present or known to be present||OIE Handistatus, 2005|
|Réunion||Disease never reported||OIE Handistatus, 2005|
|Rwanda||Reported present or known to be present||OIE Handistatus, 2005|
|Sao Tome and Principe||Disease not reported||OIE Handistatus, 2005|
|Senegal||Reported present or known to be present||OIE Handistatus, 2005|
|Seychelles||Disease not reported||OIE Handistatus, 2005|
|Somalia||No information available||OIE Handistatus, 2005|
|South Africa||Reported present or known to be present||OIE Handistatus, 2005|
|Sudan||Reported present or known to be present||OIE Handistatus, 2005|
|Swaziland||Last reported||2001||OIE Handistatus, 2005|
|Tanzania||Reported present or known to be present||OIE Handistatus, 2005|
|Togo||Reported present or known to be present||OIE Handistatus, 2005|
|Tunisia||Last reported||1999||OIE Handistatus, 2005|
|Uganda||Reported present or known to be present||OIE Handistatus, 2005|
|Zambia||Reported present or known to be present||Native||OIE, 2004g; OIE Handistatus, 2005|
|Zimbabwe||Reported present or known to be present||OIE Handistatus, 2005|
|Bos grunniens (yaks)||Domesticated host, Wild host|
|Bos indicus (zebu)||Domesticated host, Wild host|
|Bos mutus (yaks, wild)||Domesticated host, Wild host|
|Bos taurus (cattle)||Domesticated host, Wild host|
|Bubalus bubalis (buffalo)||Domesticated host, Wild host|
|Camelus bactrianus (Bactrian camel)||Domesticated host, Wild host|
|Capra hircus (goats)||Domesticated host, Wild host|
|Lama glama (llamas)||Domesticated host, Wild host|
|Lama pacos (alpacas)||Domesticated host, Wild host|
|Ovis aries (sheep)||Domesticated host, Wild host|
|Ruminantia||Domesticated host, Wild host|
|Sus scrofa (pigs)||Domesticated host, Wild host|
Blood and Circulatory System - Pigs
Digestive - Pigs
Skin - Pigs
Foot-and-mouth disease (FMD) is one of the most contagious of animal diseases. Cattle are the most susceptible of the domesticated species to FMDV, as little as 10 tissue culture infectious doses are required to establish infection by inhalation. Cattle are therefore the principal indicators of the disease. Pigs are important amplifiers because their capacity to excrete large quantities of virus (Sellers et al., 1971). Sheep are maintenance hosts since they can display very slight symptoms (Sellers et al., 1971).
The most common method of spread is by the movement of infected animals; however, FMD may also spread in products from infected animals (such as milk, semen and meat), by movement of people, vehicles or articles contaminated with virus from infected animals; or as an aerosol. The FMD virus is very susceptible to acid (pH 9) conditions, and the lactic acid in the meat of slaughtered animals that has been kept for 24 h at 4ºC to 'set' will kill the virus; but the virus will survive in the bone marrow and glands in which the pH remains close to neutral. With some strains the main means of transmission is as an aerosol, and infected animals, particularly pigs, can produce large amounts of virus in their breath, depending on the strain of virus - pigs may produce up to log10 8.6 TCID50 (tissue culture infectious doses) per day, and cattle and sheep, up to log10 5.2 TCID50 per day. Under the right weather conditions, an aerosol of infectious virus can spread as a discrete plume over considerable distances, having been recorded to have spread 250 km from France to southern England in 1981 (these outbreaks were quickly eliminated); over land, the plume is more likely to be disrupted, and spread in excess of 16 km is unlikely. The distance over which the virus can travel by the airborne route varies with virus strain and host species (Alexandersen and Donaldson, 2002). Cattle and sheep may be infected with as little as 20 TCID50 of virus by the respiratory route, while pigs require greater amounts (800 TCID50, but depends on strain of virus). All species are considerably less susceptible to infection by the oral route. FMD virus will quickly die at relative humidity below 60% RH, and is very susceptible to drying in the environment. At neutral pH and moist conditions, the virus can persist for a few weeks in contaminated premises or pasture (Donaldson, 1979; Donaldson, 1987).
FMDV infection of susceptible animals in the field occurs primarily through the upper respiratory tract by inhalation of airborne virus from an infected animal (Burrows et al., 1981; Donaldson et al., 1989; Eskildsen, 1969). Aerosol transmission usually occurs with animals in close proximity. However, there is circumstantial evidence that animals may be infected from several yards to many miles downwind from a source of infection (Hyslop, 1965; Sangar, 1979). The oesophageal-pharyngeal (OP) fluid, respiratory aerosols, saliva, vaginal and tracheal mucus, faeces, milk, and semen of infected animals may contain virus before appearance of clinical signs and lesions of the disease. Whilst lesions are present, FMDV is also present in the epithelium and vesicular fluids. Therefore, the disease may spread rapidly by movement of infected animals. Pigs do not become carriers. Other species after clinical signs may become persistently infected for variable periods (between 6 and 36 months in cattle, 4-9 months in sheep and goats and in the African Buffalo for at least 5 years) (Burrows et al., 1981, 1966; Prato-Murphy, 1994; Straver et al., 1970; Terpstra et al., 1990; Bekkum et al., 1960). Reports of field outbreaks indicate that convalescent cattle may transmit the disease when introduced into a FMD-free herd (Sangar, 1979). The role of carrier animals in the transmission has never been demonstrated experimentally in cattle and sheep. There is only one study that shows transmission of virus from carrier buffaloes to cattle under field conditions (Dawe et al., 1994; Hedger et al., 1985).
In many areas reservoir hosts are important factors in the epidemiology of foot-and-mouth disease. The African buffalo maintains the SAT serotype (in particular SAT1 and 3) in those countries which have a wild buffalo population, and there are many examples of transmission direct to cattle (Bastos et al., 1999) or transmission to impala, which then infect cattle (Bastos et al., 2000). Very little is known about the involvement of Indian buffalo in the epidemiology of FMD, although they will develop clinical disease and transmit infection to cattle. Other wild ruminants, such as deer, are susceptible to FMD, but usually as the recipient of FMD virus from cattle; there are no examples of FMD being maintained in a wild ruminant population other than in African buffalo.
Indirect transmission of infection is important because the virus can retain infectivity for a considerable time in the environment (Cottral 1969). The virus is inactivated in the meat of carcasses that undergo the normal post-slaughter acidification processes, but it persists for a very long time in frozen or chilled lymph nodes, bone marrow and residual blood clots. It also retains infectivity in uncooked, salted and cured meats, and unpasteurized milks (Cottral, 1969).
Higher titres of virus are required in all species to cause disease by ingestion. The virus may also gain entrance and establish the initial infection through abrasions in the mucous membranes or skin (Sellers, 1971; Sutmoller, 1976). Infection is also possible through the skin from a local trauma or abrasions.
Transmission is possible through artificial insemination, and contaminated embryos. However, embryo transplantation using properly collected and washed embryos does not constitute a risk (Sutmoller, 1976).
Transmission via arthropod or parasite vectors is possible, but is not considered important.
Generally, all susceptible animals in an exposed herd develop infection but under some circumstances, the incidence of disease is considerably less than 100%. Young animals are usually more susceptible than adults, unless protected by maternal antibodies arising from previous infection or vaccination. The climate may affect the spread of the virus. Hot, dry weather may slow the spread of epidemics.
Clinical signs and lesions
In pigs, clinical signs include fever, inappetance and reluctance to move. Vesicles may occur, particularly on the feet (coronets, interdigital skin) and may cause lameness. They may lead to separation of the keratinized layers of the hoof from the corium. Also, vesicles can develop on the snout and, in a lower frequency, on the tongue. Sows often develop vesicles on their teats. Pregnant sows may abort. The mortality may be high in sucking piglets.
FMD is indistinguishable from other vesicular viral diseases (vesicular stomatitis, swine vesicular disease, vesicular exanthema) and should be confirmed or excluded using suitable tests. Also, differential diagnoses should include rinderpest, mucosal disease, bovine viral diarrhoea, infectious bovine rhinotracheitis, bluetongue, bovine mamillitis and bovine papular stomatitis.
The best samples are epithelium of the vesicles from the mouth or foot, and vesicular fluid from the unruptured vesicles. Epithelium samples of between 1 and 2 cm² are satisfactory. Epithelial samples should be placed in a transport medium that maintains a pH 7.2-7.4 and is kept cool.
From ruminants, oesophageal-pharyngeal fluid (OPF) should be collected using a probang cup. The OPF should be diluted with buffer phosphate.
FMD virus causes an acute disease in over 70 species of cloven-hoofed animals but primarily it is the disease in farmed livestock such as cattle, sheep, goats, pigs and buffalo that requires laboratory diagnosis and confirmation. The disease is associated with the development of vesicles on epithelial surfaces of the mouth and feet and infection also generates a transient viraemia in infected animals that typically lasts for approximately five days (Alexandersen et al., 2003).
Tests that exploit these clinical windows in an infected animal form the basis of laboratory approaches currently used to diagnose FMD. These assays aim to detect FMDV in epithelium and fluid from vesicles, as well as in blood and swabs from mucosal surfaces (oral and nasal swabs). In addition, FMDV-specific antibody responses in exposed animals can be detected using serological assays.
Most commonly diagnosis is by observation of clinical signs (see Disease Course) and the subsequent isolation of live virus on tissue culture coupled with the identification of viral antigen by ELISA or viral nucleic acid by reverse transcription polymerase chain reaction (RT-PCR). Increase of specific antibody may also be used to indicate recovery from infection. Amplification of specific nucleic acid sequences using RT-PCR is now widely used for the laboratory detection of FMDV. These molecular assays are suitable for the diverse range of different samples that might be submitted for laboratory investigation (tissues, blood, swabs, oesophageal or pharyngeal (OP) scrapings, faecal samples and milk). Over the past 15 years, improvements have been made to RT-PCR protocols used for the detection of FMDV and real-time RT-PCR (rRT-PCR) assays have now largely replaced agarose gel based assay formats. These more rapid fluorescence-based approaches are highly sensitive enabling simultaneous amplification and quantification of FMDV specific nucleic acid sequences. In addition to enhanced sensitivity, the benefits of these closed-tube rRT-PCR assays over conventional endpoint detection methods include a reduced risk of cross-contamination, their large dynamic range, an ability to be scaled up for high-throughput applications and the potential for accurate target quantification. Several assays have been developed to detect FMDV that use 5'-nuclease assay (TaqMan®) system to detect PCR amplicons (Callahan et al., 2002; Oem et al., 2005; Reid et al., 2002). Other formats exploited for FMDV-specific rRT-PCR assays include the use of modified minor groove binder (MGB) probes (McKillen et al., 2011; Moniwa et al., 2007), hybridisation probes (Moonen et al., 2003), Primer-probe energy transfer (PriProET: Rasmussen et al., 2003) and RT-linear-after-the-exponential PCR (LATE PCR: Reid et al., 2010). In order to minimise human operator errors and increase assay throughput, these assays can be automated using robots for nucleic acid extraction (Moonen et al., 2003). Together with the implementation of quality control systems, these improvements have increased the acceptance of the rRT-PCR assays for routine diagnostic purposes.
More recently, lateral-flow devices (LFDs, also referred to as immuno-chromatographic strip tests or point of care tests) have been developed for the detection of FMD viral antigen. These simple-to-use and rapid tests utilise FMDV specific antibody reagents (normally monoclonal antibodies) in a format similar to the sandwich capture ELISA used for laboratory diagnosis. Positive test signal is generated by the diffusion of coloured, antibody-coated latex beads or colloidal gold particles through a membrane towards an immobilising band of trapping antibody. An LFD has been developed for the detection of all seven FMDV serotypes which uses a pan-serotypic monoclonal antibody (Ferris et al., 2009). In addition, sample preparation in field conditions can be achieved using simple disposable tissue homogenizers for preparing epithelial suspensions. In terms of diagnostic sensitivity and specificity, the overall performance of this LFD is similar to laboratory-based antigen ELISA, although the diagnostic sensitivity of the current test is lower for SAT 2 field strains (Ferris et al., 2009) and a separate Sat 2 LFD has been developed for this reason.
Epithelium from ruptured lesions is the most suitable sample to collect for diagnosis. This should be placed in 50% PBS-Glycerol plus antibiotics at neutral pH, and kept at 4°C or -20°C until submission to a laboratory capable of carrying out FMD diagnosis. This is usually the national laboratory, but samples may also be sent to the World Reference Laboratory for FMD at the Pirbright Institute (formerly The Institute for Animal health) Pirbright, UK. If submitting to the World Reference Laboratory, it is necessary to first contact for submission requirements (www.pirbright.ac.uk, Fax 00441483232621). The sample is prepared at the laboratory as a 10% suspension and inoculated onto a susceptible cell culture.
Primary bovine thyroid cells are the most sensitive indicator of virus presence, but lamb kidney may also be used. If the sample is fresh, and there are likely to be high levels of viral antigen present, the suspension may be used directly in an ELISA, which will also indicate the serotype. Virus recovered from tissue culture should also be typed by ELISA. Once isolated, the virus can be sequenced, if not locally, then at the World Reference Laboratory, to provide epidemiological data as to its likely origin, by comparison with other sequences in the Reference Laboratory database. It can also be used to help identify the most relevant vaccine strain to help control the outbreak by antigenic comparisons with existing vaccine strains (Kitching et al., 1989).
Serology for FMD virus antibodies is by ELISA (liquid phase blocking) (Hamblin et al., 1987), solid phase competition ELISA (Paiba et al., 2004) and non structural protein (NSP) antibody ELISA. The 'gold standard' test is still considered to be the virus neutralisation test (VNT), however, this test requires the use of tissue culture facilities and the handling of live FMD virus which may not be possible in some laboratories. The ELISA's can give false positives which should be confirmed by VNT. The LPB and SPC ELISA's and VNT are serotype specific, but several ELISAs for detecting antibodies to the NSP's such as 3ABC have been developed which are non-serotype specific and some are now commercially available The NSP antibody tests do have the advantage of allowing the distinction of antibodies produced following infection and those induced by vaccination (Clavijo et al., 2004) and can be used for surveillance and demonstration of disease freedom. FMD vaccines are inactivated and, although they may contain some non-structural protein (particularly 3D), the antibody response to these proteins is much lower than following an infection.
The NSP tests are recommended by the OIE to support declaration of freedom from infection after emergency vaccination. Extensive validation of NSP tests has been carried out and demonstrates acceptable accuracy (for example Nanni et al., 2005; Sørensen et al., 2005; Brocchi et al., 2006); but the existing tests are still considered insufficiently sensitive and specific under field conditions to be used on an individual animal basis, and should be applied at herd level only (Bronsvoort et al., 2004; Brocchi et al., 2006).
The course of foot-and-mouth disease (FMD) is acute. The incubation period is variable and depends mainly on the strain and doses of virus, route of entry, and level of immunity. It may oscillate between 2-3 days and 10-14 days (Salt 1993; Sellers 1969).
The respiratory system is the usual primary site of FMDV infection (Burrows 1981). Early sites of FMDV replication are in the glandular cells of the mucous membrane and associated lymphoid tissues. Within 2-4 h, replicating virus can be detected in the upper respiratory tract secretions.
Following the primary virus replication, FMDV is disseminated to secondary sites that include the epithelial tissues in and around the mouth and feet, mammary glands, glandular organs and other lymphoid nodes, and cardiac muscle. This first stage of the infection is subclinical and large amounts of FMDV are shed in secretions and other body fluids.
After between 72 and 96 h the fever begins. As a result of the infection, the cells of the stratum spinosum of the epithelium vacuolate, swell and burst (Bekkum, 1959; Yilma, 1980). The intercellular fluid coalesces into vesicles. Affected animals show inappetance, lameness and reluctance to move, sudden death due to cardiac failure is common in piglets.
At 5 days post-infection (dpi), the vesicles in the coronets may extend round the top of the hoof so that the horn becomes separate. Vesicles can also appear in lips, tongue and teats. Pregnant sows may abort. Rising serum antibody titre coincides with a precipitous reduction in the titre of virus shed in external body fluids. Resolution is usually complete by 14 dpi. The lesions heal, although secondary bacterial infection can complicate these lesions.
Most excretion of the virus ceases about 4-6 days after the appearance of vesicles. The virus has been detected in the milk and semen of experimentally infected cattle for 23 and 56 days, respectively.
After clinical recovery, up to 60% of ruminant animals may become persistently infected. This persistent infection is established in the pharyngeal and cranial oesophageal tissues. The duration of the carrier state varies with, among other factors, species of animal affected, and strain of virus. The maximum reported carrier periods for different species are in cattle 2.5 years, sheep and goats for up to 9 months, African buffaloes, 5 years or more (Prato Murphy et al., 1994; Salt, 1993). Pigs do not become carriers.
The virus can be recovered intermittently from such animals by oesophageal-pharyngeal (OP) probang collections. The quantity and frequency of virus that can be collected decreases progressively with time.
Vaccinated animals may become infected. Although they are fully protected against clinical disease, they may develop carrier state (Prato Murphy et al., 1994; Salt, 1993).
|Drug||Dosage, administration and withdrawal times||Life stages||Adverse affects||Drug resistance||Type|
|foot-and-mouth disease vaccine||Seek veterinary advice and information from product manufacturer. Use of vaccine may cause international trade restrictions on products. Only oil adjuvanted vaccines should be used in pigs.||All Stages||No||Vaccine|
In recent years there has been a resurgence of interest in treatment as the huge cost of stamping out the disease has become much more expensive where the disease is out of control.
T-705 (favipiravir) is an experimental anti-FMDV drug that has been tested in pigs in Japan with activity and side-effects not fully understood at present (Furuta et al., 2009).
|Vaccine||Dosage, Administration and Withdrawal Times||Life Stages||Adverse Affects|
|foot-and-mouth disease vaccine||Seek veterinary advice and information from product manufacturer. Use of vaccine may cause international trade restrictions on products. Only oil adjuvanted vaccines should be used in pigs.|
Animals in endemic areas may be given some protection with prophylactic vaccination. The seven serotypes of FMD virus are immunologically distinct, and recovery from infection or vaccination with one serotype does not provide protection against the other six. In addition, within each serotype there are a large number of strains representing a spectrum of antigenic characteristics. It is therefore necessary to antigenically match the outbreak strain with a suitable vaccine strain, or even produce a new vaccine strain. Protection with even a closely matched vaccine will only last for approximately 6 months, and in endemic situations it is usually necessary to vaccinate cattle three times yearly, and sheep twice-yearly. Calves from vaccinated cows are protected for up to 4 months by colostral antibody, although this may be for a shorter time depending on the frequency of vaccination. The dose of vaccine varies according to the manufacturer and whether they are able to concentrate the antigen. There are no live vaccines officially in use worldwide. Adjuvant for ruminant FMD vaccines can be either aluminium hydroxide plus saponin or oil; for pigs it must be oil, either as a single or double emulsion. Other control measures should also be used to control outbreaks such as quarantine, disinfection and movement restrictions.
Countries usually free of FMD generally control outbreaks by slaughtering all infected and in-contact animals, and implementing strict movement controls and other zoosanitary measures ('stamping out'). More extensive slaughter policies, including culling of animals on adjacent premises and small ruminants and pigs within 3 km of infected premises, were used during the UK epidemic in 2001. The effectiveness of such pre-emptive slaughter in controlling the spread of infection is controversial. It is important to note that vaccination is now expected to be considered as part of any response to an FMD outbreak in a free country and that those countries which hold FMD antigen banks should be prepared with practical contingency plans for deployment of vaccination should the situation arise.
Most FMD-free countries maintain the option to vaccinate by participating in FMD antigen banks, which they would take advantage of should the slaughter policy prove ineffective. There is still some reluctance to use vaccine because of the possibility that some of the vaccinated cattle that contacted live field virus would become carriers. However, recent scientific advances should allow a more rapid return to FMD-free status. This could be achieved through a combined approach involving improved vaccines and better use of rapid diagnostic tests to detect early infection and persistent infection accurately and competent data management. This is reflected by the increased priority given to vaccination in current FMD contingency plans, such as those of the European Union countries (Laddomada, 2003).
The use of vaccine delays the re-establishment of freedom from FMD status, as it affects international trade (Kitching et al., 1998; Barteling and Vreeswijk, 1991; Kitching, 1992; Kitching and Salt, 1995; Woolhouse et al. 1996; OIE, 1998). This restriction, however, is now less onerous: the OIE reduced the time period for regaining FMD-free status following emergency vaccination from the original 12 to 6 months, provided that non-structural proteins (NSP) tests are used to document that the remaining vaccinated population is free of infection.
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