Download Sporadic amyotrophic lateral sclerosis: A hypothesis of persistent

Survey
yes no Was this document useful for you?
   Thank you for your participation!

* Your assessment is very important for improving the workof artificial intelligence, which forms the content of this project

Document related concepts

Orthohantavirus wikipedia , lookup

Hepatitis C wikipedia , lookup

Influenza A virus wikipedia , lookup

Canine parvovirus wikipedia , lookup

Canine distemper wikipedia , lookup

Neonatal infection wikipedia , lookup

Marburg virus disease wikipedia , lookup

Henipavirus wikipedia , lookup

Human cytomegalovirus wikipedia , lookup

Lymphocytic choriomeningitis wikipedia , lookup

Hepatitis B wikipedia , lookup

Transcript
Amyotrophic Lateral Sclerosis. 2005; 6: 77–87
REVIEW ARTICLE
Sporadic amyotrophic lateral sclerosis: A hypothesis of persistent (nonlytic) enteroviral infection
JOHN RAVITS
Neurology Section, Virginia Mason Medical Center and Neurogenomics Laboratory, Benaroya Research Institute of Virginia
Mason, Seattle, USA
Abstract
Because of recently reported reverse transcriptase polymerase chain reaction evidence of enterovirus in sporadic
amyotrophic lateral sclerosis (SALS) and because of newly available anti-enteroviral drugs binding enteroviral capsids, it is
reasonable to re-formulate an enteroviral hypothesis of SALS using recent advances in molecular virology. Viral persistence
is non-lytic and non-cytopathic infection that evades host’s immune surveillance. Enteroviruses are known to cause
persistent as well as lytic infection both in vitro and in vivo. Both virion as well as host factors modulate between persistent
and lytic infection. Apoptosis, or programmed cell death, is a process of active non-necrotic cell death. It has complex
interplay with viruses and may be either promoted or opposed by them. Apoptosis is a major factor in motor neuron death in
SALS. Viral tropism is the process by which viruses select and propagate to target cells. It is controlled by capsid
conformation and surface receptors on host cells. Enteroviruses have a region on their capsids known as the canyon which
docks on such receptors. Docking induces conformational changes of the capsid and genome release. Poliovirus, tropic for
motor neurons, docks on the poliovirus receptor, about which much is known. The virus penetrates the motor system
focally after crossing either the blood-muscle or the blood-brain barriers. It propagates bidirectionally along axons and
synapses to contiguous motor neurons, upper as well as lower, which sequester infection and create avenues for spread over
long distances. If chronic and persistent rather than acute and lytic, such viruses trafficking in a finite system of non-dividing
cells and inducing apoptosis would cause cell death that summates linearly rather than exponentially. Taken together, these
explain signature clinical features of SALS — focal onset weakness, contiguous or regional spread of weakness, confinement
to upper and lower motor neurons, and linear rates of progression. The hypothesis predicts the following testable
investigations: 1) viral detection may be possible by applying amplification technology to optimally acquired nervous tissue
processed by laser microdissection; 2) genetic susceptibility factors such as cell surface receptor polymorphisms may
combine with sporadic exposure and chance penetration of the motor system in SALS; 3) a transgenic animal model might
be created by inserting such genetic factors into an animal host and inoculating intramuscularly rather than intracerebrally
biochemical fractions of SALS motor neurons at vulnerable periods in the developmental life cycle of the transgenic host;
and 4) continual long-term administration of anti-enteroviral agents called capsid-binding compounds which stabilize
capsids and prevent genome release might be efficacious.
Key words: Amyotrophic lateral sclerosis, enterovirus, persistent viral infection, apoptosis, poliovirus receptor, capsid binding
compounds
Introduction
‘‘We believe that a number of current diseases
affecting differentiated systems like the nervous…system yet of unknown etiology may
likely be caused by infectious agents like
viruses which have evolved to persist and
replicate in differentiated cells without causing
lysis of the cell they infect. With the availability
of highly sensitive molecular techniques to
identify limited amounts of materials, this
hypothesis can be adequately tested in the
coming decades. From the evidence that is
evolving, it is likely that the study of such
persistent viruses will dominate virology in the
twenty-first century.’’
J.C. de la Torre and M.B.A. Oldstone, 1996 (1)
A viral cause of sporadic amyotrophic lateral
sclerosis (SALS) has been hypothesized for decades
(reviewed in 2)(3–18). Enteroviruses (Figure 1)
have led the candidate viruses because of the tropism
of poliovirus, an enterovirus subtype, for motor
neurons (19–27). Retroviruses are also candidates
Correspondence: J. Ravits, Neurology Section, Virginia Mason Medical Center and Neurogenomics Laboratory, Benaroya Research Institute, PO Box 900,
1100 Ninth Avenue, Seattle, WA 98111, USA. E-mail: [email protected]
(Received 18 May 2004; accepted 11 November 2004)
ISSN 1466-0822 print/ISSN 1471-180X online # 2005 Taylor & Francis Group Ltd
DOI: 10.1080/14660820510027026
78
J. Ravits
Figure 1. Structure of the poliovirion. A complete capsid
structure of virulent poliovirus type 1 [PV1(M)] illustrated as a
water-accessible molecular surface. One of the 12 pentameric
subunits of the capsid and its five constituent triangular
pseudoprotomeric subunits are illustrated. The 5x and 3x labels
indicate the locations of the five-fold and the three-fold axes of
this pentamer. The two-fold axes occur at the intersection of the
three adjacent pentamers. The central pseudoprotomer illustrates
the subunit geometry of viral capsid proteins VP1, VP2, and
VP3(ii). The biologically relevant protomer (to viral assembly) is
pear-shaped and consists of VP1, VP2, and VP3(i). The internal
VP4 protein is not visible from the surface. The canyon’s north
wall (A), south wall (C), and bottom (B) are indicated. The major
poliovirus antigenic sites are labeled Ia, Ib, II, and III on an
adjacent pseudoprotomer. [Reproduced with permission from
Harber J, Bernhardt G, Lu H, et al: Canyon Rim Residues,
Including Antigenic Determinants, Modulate Serotype-Specific
Binding of Polioviruses to Mutants of the Poliovirus Receptor.
Virology 1995;214:559–70 (reference 20).]
(1,50–55). Host as well as viral factors are significant
since some viruses cause lytic infection in one cell
line and persistent infection in others. Time of
infection is also significant since infection causes
lytic infection at one time in the life of the host and
persistent infection at another. Viruses escape
immune surveillance to persist in host cells through
a
number
of
strategies
(1,51–53,56–58).
Enteroviruses can cause persistent as well as lytic
infections (reviewed in 59) (60,61). Polioviruses, in
particular, can cause persisting infection (25,62–77).
The central nervous system (CNS) is a unique
compartment for persisting infection (53,78–80): it
is relatively isolated from the immune system by the
blood-brain barrier, its neurons have relative
absence of major histocompatibility-complex molecules fundamental to invoking immunologic
response (81,82), its cells are static and cannot be
overgrown by replacements, and its extensive networks of axons and dendrites create avenues for
sequestering and spreading infection over long
distances. SALS is fundamentally a disease of the
CNS — all motor neurons reside inside the CNS
compartment and only axons of the lower motor
neurons extend outside it. SALS, traditionally
regarded as a disease in which inflammation and
immune response are absent, in fact has subtle
responses (reviewed in 83) (84–90).
Viral-associated apoptosis
because motor neuron syndromes are associated
with both HIV and HTLV1 retroviral subtypes (28–
38). Amplification technologies, polymerase chain
reaction (PCR) (39,40) and reverse transcriptase
polymerase chain reaction (RT-PCR) (41–43) have
reinvigorated the search. To date, three studies from
two laboratories have reported evidence of enterovirus in nervous systems of patients dying from
SALS using RT-PCR (44–46) and three studies
from three laboratories, two of them recent, have
reported negative results with this technique (47–
49). With the availability of highly effective antienteroviral therapy (i.e., [(oxazolylphenoxy)alkyl]isoxazole capsid-binding compounds), the hypothesis
remains significant.
Apoptosis, or programmed cell death, is a process of
active non-necrotic cell death. It has a complex
interplay with viruses and may be either promoted or
opposed by them (91–99). Very little is known about
this interplay; one example is the Sindbus virus that
induces an encephalitis and hind limb paralysis in
mice by apoptosis (100,101). Another example is the
poliovirus, which can either induce or oppose
apoptosis depending on viral properties and host
cell factors (102–106). One function of apoptosis is
regulation of embryonic development (107–109). In
embryonic development, 50% or more of motor
neurons are eliminated by apoptosis, underlining
motor neurons’ intrinsic apoptotic capability (110).
Based on biochemical (111–115), and morphologic
(114) evidence, apoptosis is now thought to be a
major factor in cell death in SALS (reviewed in 116
and 117). The interplay of viruses and apoptosis in
the nervous system has been speculated but never
proven to be important in neural degeneration
(96,109,118–120).
Viral persistence (non-lytic infection) and the
privilege of the CNS
Cell surface receptors, viral tropism, and viral
sequestration
Viral persistence is non-lytic and non-cytopathic
infection that evades host’s immune surveillance
Viral tropism is the process by which viruses select
and propagate to targets cells (reviewed historically
Persistent enteroviral infection in ALS
in 121). It is controlled by capsid conformation
and receptors on the cell’s surface. Models are the
pircornaviruses (122–124), especially polioviruses,
tropic for motor neurons (reviewed in 125)
(19,22,23,126). Key to poliovirus’s tropism is the
poliovirus receptor (PVR) (127–133). PVR is a cellsurface sialylated glycoprotein belonging to the
immunoglobulin superfamily and has three extracellular immunoglobulin-like domains, a transmembrane domain and a cytoplasmic tail. Its gene maps
to chromosome 19q 13.1–13.2. The cellular function of PVR is unknown. It is found only in primate
cell lines. A transgenic mouse model expressing
human PVR has susceptibility to poliovirus infection
when it otherwise has none. This has allowed
significant evaluation of PVR’s molecular biology
(134). PVR underlies both viral selection and
infection— PVR protruding from the cell surface
fits into a depression on the surface of the virion
capsid known as the canyon, a depression located
just below the five-fold axis of symmetry on the
north face of the icosahedal structure (Figure 2).
This induces conformational changes in the capsid
leading to destabilization, uncoating and RNA
release (132,133,135–138). Since PVR is distributed
in cell lines not infected by the virus, other factors
are important in its tropism for and sequestration in
the motor system (139–145).
Focal access and contiguous viral propagation
One of the best-understood and most relevant
models of viral propagation is again the poliovirus
(reviewed in 125) (146–148). Extensive clinical
(149–157) and experimental (146,149,150,157–
162) observations indicate poliovirus penetrates the
motor system either from the periphery or from the
CNS. From the periphery, it establishes a focal nidus
in muscle by first crossing the blood-muscle barrier
and then travels retrograde along motor neurons to
invade the motor system (163). From the CNS, it
first crosses the blood-brain barrier then invades the
motor system. Once inside motor neurons, poliovirus propagation is trans-neuronal to contiguous
motor neurons, either horizontal between neighboring neurons or trans-synaptic between upper and
lower motor neurons. Both axonal and transsynaptic transmissions are bidirectional: antegrade
or retrograde along axons and orthodromic or
antidromic across synapses. Axonal transmission is
probably through fast transport systems (161).
Motor neurons create avenues for spreading over
long distances infection already sequestered by
its unique tropism. Thus, poliovirus infection
begins focally and spreads contiguously to
infect the entire motor system, upper as well
as lower motor neurons, a feature known from
early pathologic studies of acute lytic polio (21–
23,149).
79
Figure 2. Locations of human PVR (hPVR) binding mutations on
the poliovirus capsid and a virus-receptor model. (a) Stereo view
showing details of the five-fold depression, referred to as the
canyon. The axes of icosahedral symmetry are labeled around a
single representative of the 60 triangular pseudoprotomeric facets.
The view is seen along the icosahedral two-fold axes of symmetry
looking down upon the canyon area. Residues exchanged in the
antigenic hybrids (NAgI and NAgII) are represented in magenta
color, while the amino acid substitutions resulting from sitedirected mutagenesis are colored in cyan. The sphingosine
molecule occupying the hydrophobic pocket of the viral capsid
protein VP1 protein is shown in yellow. (b) Stereo view of the
same area as that shown in (a) except that the view is
perpendicular to the axes of the icosahedral five- and two-fold
symmetry. (c) A poliovirus receptor modeled after the CD4
molecule is docked into the canyon. Orientation is the same as
that in (b). Domain 1, an immunoglobulin V-like domain (gold)
enters the canyon. The smaller domain 2, an immunoglobulin Clike domain, is colored green and sits above the surface of the
virion. It is possible that domain 1 contacts residues of the north
wall (nearest NAgI) and south wall (the NAgII face) simultaneously based on spatial considerations alone. Also, binding of the
receptor to the canyon rim regions does not necessarily involve
contacts of the receptor to the bottom of the canyon. [Reproduced
with permission from Harber J, Bernhardt G, Lu H, et al. Canyon
Rim Residues, Including Antigenic Determinants, Modulate
Serotype-Specific Binding of Polioviruses to Mutants of the
Poliovirus Receptor. Virology 1995;214:559–70 (reference 20).]
Viral etio-pathogenesis of SALS
Cardinal clinical features of SALS are focal onset,
regional or contiguous spread, confinement to upper
and lower motor neurons, relatively linear progression for each patient, but highly variable among
different patients. These are readily explained by
persistent viral infection. Persistent infection is nonlytic and non-cytopathic. Viral properties, host
susceptibility factors and time of exposure may all
80
J. Ravits
be important factors in its establishment. Tropism
for motor neurons, controlled by viral capsid conformation and host cell-surface receptors, ensures
infection selects motor neurons and stays sequestered. Infection may gain access either after penetrating the blood-muscle barrier or the blood-brain
barrier. Once inside, it spreads contiguously. Horizontal propagation includes crossing the midline at
spinal and brainstem levels because of relative
proximity of anterior horns and brainstem nuclei.
Vertical or trans-synaptic propagation causes a jump
between lower and upper motor neurons, the latter
leading to propagation over long distances. Because
infection is persistent and propagation through the
motor system is successive, progression is linear
rather than accelerating. Because of variation of
biologic factors such as viral load, viral virulence and
host cell factors, progression rates are highly variable
among different host patients. As infection propagates, it switches on apoptosis, a capability well
established in motor neurons and known to have
complex interplay with viruses. Since motor neurons
are limited in number and non-dividing, cell death
summates. This is manifested clinically as progressive muscle weakness that begins focally, spreads
regionally, and progresses linearly. Thus, SALS is
reminiscent of the description the Icelandic veterinarian Bjorn Sigurdsson employed of Visna-Maedi
disease in sheep, the original ‘slow virus’ and one
of the first descriptions of what was later found to
be a retroviral disease: ‘acute disease in slow
motion’! (164).
Implications for therapy
Capsid-binding compounds
The capsid binding compounds [(oxazolylphenoxy)alkyl]isoxazoles, have been designed for treatment
of enteroviral and picornavirus infections (165–172).
These compounds bind in the hydrophobic pocket
situated at the base of the canyon site on the north
face of the virion icosahedral capsid where cellular
receptors interact. This binding raises the floor of
the canyon and alters the virion’s ability to attach
and bind to receptors, thus inhibiting disassembly
and RNA release (Figure 3). Since these drugs act
on the virion’s capsid and not its RNA genome, they
block viral propagation – once virus has released
RNA and infected a cell, capsid-binding drugs
would have little effect. Therefore, for them to be
effective in SALS, assuming the viral pathogenesis, a
constant level of drug would have to be present in
the body over months or years and it would be
controlling rather than curative treatment. Since the
hydrophobic pocket has unique topology not found
in other classes of proteins, the compounds are viral
specific and have minimal host toxicity (166). One of
these compounds, VP 63843 (PleconarilH), is well
tolerated, well absorbed after oral administration,
Figure 3. Diagrammatic view of picornavirus with enlargement of one icosahedral asymmetric unit showing the outline of the canyon and
the entrance to the antiviral-binding pocket. The protomeric assembly unit (which differs from the geometric definition of the asymmetric
unit) is shown in heavy outline on the icosahedron. [Reproduced with permission from Oliveira MA, Rossmann MG, et al. The structure of
human rhinovirus 16. Structure1993;1:51–68 (reference 170).]
Semi-nested in 2
centers
has few side-effects, little toxicity, and crosses readily
into the central nervous system and into gray matter
(173,174). Anecdotal evidence of benefit in one
SALS patient has been reported (175).
Other therapeutic strategies
Other specific anti-picornavirus therapy includes
inhibitors of 3C protease and recombinant soluble
intercellular adhesion molecules (reviewed in 176).
Interferons are potent mediators resisting enteroviruses (165). Cells exposed to enteroviruses
increase production of interferon through an intracellular cascade and this increases resistance to
infection. Alpha interferon, a potent inhibitor of
enteroviral infection, may be even more effective
when combined with capsid-binding compounds
(177). Therapeutic strategies to alter apoptosis pathways are in early stages of development (reviewed in
178) (179–182). Strategies combining antiviral and
anti-apoptotic with current anti-neuroexcitatory
therapies may be effective. Vaccination is now
conceivable to prevent chronic viral infections (183).
1
1
Nested, in situ
RT-PCR
Semi-nested for
echovirus 7
Nested
1
1 or 2
Nested
1–4 (usu. 1 or 2)
Positive 8/10 (72%) SALS & 1/2
(50%) FALS, Negative 0/6 (0%) controls
Negative 0/28 (0%) SALS
Negative 0/6 (0%) controls
Positive 15/17 (88%) SALS
Negative 1/29 (3%) controls
Negative for echo 7 0/20 (0%) SALS
spinal cords and 0/10 (0%) cortex
Positive 3/5 (60%) SALS
Positive 2/14 (14%) controls
Negative 24/24 (100%) ALS
Negative 17/17 (100%) controls
Positive 5/5 (100%) positive controls
Nested
1
Spinal cord
Archived tissue
Archived tissue
Uncertain
Uncertain
Retrospective
Retrospective
Prospective
Prospective
(2 Centers)
Frozen
Archived tissue
Retrospective
Frozen
Spinal cord and
cortex
Spinal cord
Spinal cord, brain
stem, and cortex
Spinal cord
Archived tissue
Retrospective
Woodall, 1994
(ref44)
Swanson, 1994
(ref47)
Berger, 2000
(ref45)
Walker, 2001
(ref48)
Giraud, 2001
(ref46)
Nix, 2004
(ref49)
Collection method
Formalin-fixed, paraffin
embedded
Formalin-fixed, paraffin
embedded (one frozen)
Formalin-fixed, paraffin
embedded
Frozen
Spinal cord
RT-PCR Method
81
Predictions
Prospective or
retrospective
Study
Table I. Summary of RT-PCR studies and methodologies.
Fixative
Neuraxis Level
Sample sites
Results
Persistent enteroviral infection in ALS
The hypothesis predicts the following: 1) viral
presence either may be detectable only using highly
sensitive techniques on optimally procured and
processed nervous system tissue. Laser microdissection is a new technology that allows isolation of cells
and thus overcomes problems of sampling; 2) host
genomic factors such as cell surface receptors or host
immune factors may be important susceptibility
factors that permit establishment of persistent
infection; 3) disease may depend on the chance
concurrence of these genetic susceptibility factors,
sporadic infection, motor system penetration provided through the blood-muscle barrier breakdown
(from exercise, trauma or other factors), and
possibly vulnerable times in the host’s development;
4) an animal model might be created by inserting
genetic susceptibility factors such as cell surface
receptors into a transgenic animal and inoculating with extract from frozen motor neurons –
intramuscular inoculation may allow better entry to
the motor system than intracerebral inoculation;
controlling times of exposure may be important;
5) continual long-term administration of capsidbinding compounds such as VP 63843 (PleconarilH)
that readily penetrate the CNS may be efficacious.
Recent investigations of persisting enteroviral
detection
Signal-to-noise ratio of persisting enteroviral infection in motor neurons would be infinitesimal due to
low viral copy, small virion size, small viral genome
(7.4 kB), high host nucleic acid noise level from
82
J. Ravits
within the motor neuron, and high host nucleic acid
noise level from the surrounding tissue. RT-PCR is
able to amplify signal billion-fold or more and
enteroviral RT-PCR has extremely high sensitivity
and specificity (42,184–187). RT-PCR detection of
low-copy persisting viral genome is more complex
than lytic infection (188,189). Six RT-PCR studies
searching enteroviruses have been completed: three
studies from two laboratories are positive (44–46)
and three studies from three laboratories are negative
(47–49). The methodological issues and results are
summarized in Table I. Problems for most of these
studies variously include: 1) retrospective testing of
archived specimens; 2) collection, fixation and
storage not specifically designed for nucleic acid
preservation and PCR technology; 3) random,
limited and non-selective tissue sampling; 4) testing
tissue homogenates with little or no information
about the neuropathologic status of motor neuron
degeneration in the tested tissue (190); 5) different
RT-PCR methods including simple, nested and seminested amplification, different primers and different
sensitivities (190); and 6) lack of internal controls
such as housekeeping genes or validation studies with
positive controls for establishing sensitivities (190).
Interestingly, the best-designed studies have been
negative (48,49), but they have been performed on
frozen tissue, and the more problematically designed
studies have tended to be positive, but they have been
performed on formalin-fixed tissue. Thus, the possiblity remains that formalin fixation may better
preserve viral signal or better deliver it to RT-PCR
than freezing. RT-PCR can be performed on formalin-fixed, paraffin-embedded archived tissue (191–
197) and recent protocols for spinal cord samples
have been published (198). Sample size may also be
important and paradoxically less tissue may be more
likely to reveal persisting virus than larger samples,
possibly because of increased noise and inhibitor
factors (199–201). Clearly, the most significant limit
to detection of enterovirus in ALS is the severe
reduction of the targets of investigation, motor
neurons, due to elimination by the disease and the
marked variation of regional topography of pathology
along the neuraxis. Use of laser-based tissue microdissection that is able to isolate, collect, and
standardize specific cells such as motor neurons will
resolve these methodologic problems (202,203).
Note
*
The ratio of diameters of enterovirus (30 nm) to motor
neurons (30–120 mm) is 1 to 1000–4000 and the corresponding ratio of volumes is ,1 to 109.
References
1. de la Torre JC, Oldstone MBA. Anatomy of viral persistence: mechanisms of persistence and associated disease.
Adv Virus Research. 1996;46:311–43.
2. Salazar-Gureso EF, Roos RP. Amyotrophic lateral sclerosis
and viruses. Clin Neurosci. 1995;3:360–7.
3. Rowland LP, Shneider NA. Amyotrophic lateral sclerosis.
NEJM. 2001;344:1688–700.
4. Viola M, Myers J, Gramm K, Gibbs JC Jr, Roos RP. Failure
to detect poliovirus genetic information in amyotrophic
lateral sclerosis. Ann Neurol. 1979;5:402–3.
5. Cremer N, Oshiro L, Norris F. Cultures of tissues from
patients with amyotrophic lateral sclerosis. Arch Neurol.
1973;29:331–3.
6. Muller WK, Schaltenbrtand G. Attempts to reproduce
amyotrophic lateral sclerosis in laboratory animals by
inoculation of Schu virus isolated from patient with apparent
amyotrophic lateral sclerosis. J Neurol. 1979;220:1–19.
7. Norris FJ Jr. Current status of the search for virus in
amyotrophic lateral sclerosis. Neuro Neuro Psychiatr.
1977;18(Suppl. 2–3): 443–54.
8. Weiner LP, Stohlman SA, Davis R. Attempts to demonstrate
virus in amyotrophic lateral sclerosis. Neurology. 1980;30:
1319–22.
9. Gibbs CJ, Gajdusek DC. An update on long-term in vivo
and in vitro studies designed to identify a virus as the cause
of amyotrophic lateral sclerosis, Parkinsonism dementia and
Parkinson’s disease. In: Rowland LP, editor. Human Motor
Neuron Diseases. New York: Raven Press; 1982. pp 343–53.
10. Fallis RJ, Weiner LP. Further studies in search of a virus in
amyotrophic lateral sclerosis. In: Rowland LP, editor.
Human Motor Neuron Diseases. New York: Raven Press;
1982. pp 355–61.
11. Kennedy PGE. On the possible role of viruses in the
eetiology of motor neuron disease: a review. J Royal Soc
Med. 1990;83:784–7.
12. Jubelt B. Viruses and motor neuron diseases. Adv Neurol.
1991;56:463–72.
13. Fraser H, Behan W, Chree A, Crossland G, Behan P. Mouse
inoculation studies reveal no transmissible agent in amyotrophic lateral sclerosis. Brain Pathology. 1996;6:89–100.
14. Miller J, Guntaka RM, Myers J. Amyotrophic lateral
sclerosis. Search for poliovirus by nucleic acid hybridization.
Neurology. 1980;30:884–6.
15. Kohne DE, Gibbs CJ, White L, Tracy SM, Meinke W,
Smith RA. Virus detection by nucleic acid hybridization
examination of normal and ALS tissues for the presence of
poliovirus. J Gen Virol. 1981;56:223–33.
16. Brachic M, Smith RA, Gibbs CJ, Garruto RM,
Tourtellotte WW, Cash E. Detection of picornavirus
sequences in nervous tissue of amyotrophic lateral sclerosis
and control patients. Ann Neurol. 1985;18:337–43.
17. Love S. The search for a transmissible agent in ALS. Brain
Pathol. 1996;6:99–100.
18. Muir P, Nicholson F, Spencer GT, Ajetunmobi JF,
Starkey WG, Khan M, et al. Enterovirus infection of the
central nervous system of humans: lack of association with
chronic neurological disease. J Gen Virol. 1996;77:1469–76.
19. Muir P, van Loon AM. Enterovirus infections of the central
nervous system. Intervirology. 1997;40:153–66.
20. Harber J, Bernhardt G, Lu H, Sgro JY, Wimmer E. Canyon
rim residues, including antigenic determinants, modulate
serotype-specific binding of polioviruses to mutants of the
poliovirus receptor. Virology. 1995;214:559–70.
21. Bodian D. Histopathologic basis of clinical findings in
poliomyelitis. Am J Med. 1949;6:563–78.
22. Sabin AB, Ward R. The natural history of human
poliomyelitis. I. Distribution of virus in nervous and nonnervous tissues. J Exp Med. 1941;73:771–93.
23. Johnson RT. Selective vulnerability of neural cells to viral
infections. In: Rowland LP, editor. Human Motor Neuron
Diseases. New York: Raven Press; 1982. pp 331–7.
24. Salazar-Grueso EF, Cashmann NR, Maselli R, Roos RP.
Upper motor neuron findings in patients with antecedent
poliomyelitis. Neurology. 1987;37(Suppl1): 215.
Persistent enteroviral infection in ALS
25. Melchers W, de Villser M, Jongen P, van Loon A,
Nibbeling R, Oostvogel P, et al. The postpolio syndrome:
no evidence for poliovirus persistence. Ann Neurol.
1992;32:728–32.
26. Dalakas MC, Illa I. Post-polio syndrome: concepts in
clinical diagnosis, pathogenesis and etiology. Adv Neurol.
1991;56:495–511.
27. Giraud P, Kopp N, Lina B, Chazot G. La sclérose latérale
amotrophique: implication des entérovirus? Rev Neurol.
(Paris). 2000;156:352–6.
28. Harter DH. Viruses other than poliovirus in human
amyotrophic lateral sclerosis. In: Rowland LP, editor.
Human Motor Neuron Diseases. New York: Raven Press;
1982. pp 339–42.
29. Westarp ME, Foring B, Rasmussen H, Schraff S, Mertens T,
Kornhuber HH. Human spuma retrovirus antibodies in
amyotrophic lateral sclerosis. Neuro, Psych, Brain Res.
1992;1:1–4.
30. Westarp ME, Ferrante P, Perron H, Bartmann P,
Kornhuber HH. Sporadic ALS/MND: a global neurodeneration with retroviral involvement? J Neurol Sci.
1995;129(Suppl): 145–7.
31. Rosener M, Hahn H, Kranz M, Heeney J, Rethwilm A.
Absence of serological evidence for foamy virus infection in
patients with amyotrophic lateral sclerosis. J Med Virol.
1996;48:222–6.
32. Andrews WD, Tuke PW, Al-Chalabi A, Gaudin P, Ijaz S,
Parton MJ, Garson JA. Detection of reverse transcriptase
activity in the serum of patients with motor neuron disease.
J Med Virol. 2000;61:527–32.
33. Moulignier A, Moulonguet A, Pialoux G, Rozenbaum W.
Reversible ALS-like disorder in HIV infection. Neurology.
2001;57:995–1001.
34. MacGowan DJ, Scelsa SN, Waldron M. An ALS-like
syndrome with new HIV infection and complete response
to antiretroviral therapy. Neurology. 2001;57:1094–7.
35. Jubelt B, Berger JR. Does viral disease underlie ALS?
Lessons from the AIDS pandemic. Neurology.
2001;57:945–6.
36. Cermelli C, Vinceti M, Beretti F, Pietrini V, Nacci G,
Pietrosemoli P, et al. Risk of sporadic amyotrophic lateral
sclerosis associated with seropositivity for herpesviruses and
echovirus-7. Eur J Epidemiol. 2003;18:123–7.
37. Andrews WE, Al-Chalabi A, Garson JA. Lack of evidence
for HTLV tax-rex DNA in motor neuron disease. J Neurol
Sci. 1997;153:86–90.
38. Sola P, Bedin R, Casoni F, Barozzi P, Mandrioli J, Merelli E.
New insights into the viral theory of amyotrophic lateral
sclerosis: study on the possible role of Kaposi’s sarcomaassociated virus/human herpesvirus 8. Eur Neurol.
2002;47:108–12.
39. Mullis KB, Faloona FA. Specific synthesis of DNA in vitro
via a polymerase-catalysed chain rection. Methods Enzymol.
1987;155:335–50.
40. Saiki R, Gelfand DH, Stoffel S, Scharf SJ, Higuchi R,
Horn GT, et al. Primer-directed enzymatic amplification of
DNA with a thermostable DNA polymerase. Science.
1988;239:487–91.
41. Hyypia T, Auvinen P, Maaronen M. Polymerase chain
reaction for human picornaviruses. J Gen Virol. 1989;70:
3261–8.
42. Rotbart HA. Enzymatic RNA amplification of the enteroviruses. J Clin Microbiol. 1990;28:438–42.
43. Chapman NM, Tracy S, Gauntt CJ, Fortmueller U.
Molecular detection and identification of enteroviruses using
enzymatic amplification and nucleic acid hybridization.
J Clin Microbiol. 1990;28:843–50.
44. Woodall CJ, Riding MH, Graham DI, Clements GB.
Sequences specific for enterovirus detected in spinal cord
from patients with motor neuron disease. Br Med J.
1994;308:1541–3.
83
45. Berger MM, Kopp N, Vital C, Redl B, Aymard M, Lina B.
Detection and cellular localization of enterovirus RNA
sequences in spinal cord of ALS patients. Neurology.
2000;54:20–25.
46. Giraud P, Beaulieux F, Ono S, Shimizu N, Chazot G,
Lina B. Detection of enteroviral sequences from frozen
spinal cord samples of Japanese ALS patients. Neurology.
2001;56:1777–8.
47. Swanson NR, Fox SA, Mastaglia FI. Search for persistent
infection with poliovirus or other enteroviruses in amyotrophic lateral sclerosis. Neuromusc Disord. 1995;5:457–65.
48. Walker MP, Schlaberg R, Hays AP, Bowser R, Lipkin WI.
Absence of echovirus sequences in brain and spinal cord
of amyotrophic lateral sclerosis patients. Ann Neurol.
2001;49:249–53.
49. Nix WA, Berger MM, Oberste MS, Brooks BR, McKennaYasek DM, Brown RH Jr, et al. Failure to detect enterovirus
in the spinal cord of ALS patients using a sensitive RT-PCR
method. Neurology. 2004;62:1372–7.
50. Oldstone MBA. Viruses can cause disease in the absence
of morphological evidence of cell injury: implication for
uncovering new diseases in the future. J Inf Diseases.
1989;159:384–9.
51. Oldstone MB. Viral persistence: mechanisms and consequences. Current Opinion in Microbiolgy. 1998;1:436–41.
52. Ahmed R, Morrison LA, Knipe DM. Viral persistence. In:
Nathanson N, et al., eds, Viral Pathogenesis. Philadelphia:
Lippincott-Raven Publishers; 1997. Chapter 9.
53. Lipton HL, Gilden DH. Viral diseases of the nervous
system: persistent infections. In: Nathanson N, et al., eds,
Viral
Pathogenesis.
Philadelphia:
Lippincott-Raven
Publishers; 1997. Chapter 36, 1997.
54. Ter Meulen V, Carter MJ, Wege H, Watanabe R.
Mechanisms and consequences of virus persistence in the
human nervous system. Ann NY Acad Sci. 1984;436:86–97.
55. Ahmed R, Chen ISY, editors, Persistent Viral Infections.
Chichester: John Wiley & Sons; 1999.
56. Alcami A, Koszinowski UH. Viral mechanisms of immune
evasion. Trends Microbiol. 2000;8:410–8.
57. Mahalingam S, Meanger J, Foster P, Lidbury BA. The viral
manipulation of the host cellular and immune environments
to enhance propagation and survival: a focus on RNA
viruses. J Leukocyte Biology. 2002;72:429–39.
58. Vossen MTM, Westerhout EM, Soöderbert-Nauclér C,
Wiertz EJ. Viral immune evasion: a masterpiece of evolution.
Immunogenetics. 2002;54:527–42.
59. Frisk G. Mechanisms of chronic enteroviral persistence in
tissue. Current Opin Infect Dis. 2001;14:251–6.
60. McKinney RE, Katz SL, Wilfert CM. Chronic enteroviral
meningoencephalitis in agammaglobulinemic patients. Rev
Infects Dis. 1987;9:334–56.
61. Zhang S, Racaneillo VR. Peristent echovirus infection of
mouse cells expressing the viral receptor VLA-2. Virology.
1997;235:293–301.
62. Pavio N, Buc-Caron MH, Colbere-Garpin F. Persistent
poliovirus infection of human fetal brain cells. J Virol.
1996;70:6395–401.
63. Carp RI. Persistent infection of human lymphoid cells
with poliovirus and development of temperature sensitive
mutants. Intervirology. 1981;15:49–56.
64. Lloyd RE, Bovee M. Persistent infection of human
erythroblastoid cells by poliovirus. Virology. 1993;194:
200–9.
65. Colbere-Garapin F, Christodoulou C, Crainic R, Pelletier I.
Persistent poliovirus infection of human neuroblastoma
cells. Proc Natl Acad Sci. USA. 1989;86:7590–4.
66. Borzakian S, Couderc T, Barbier Y, Attal G, Pelletier I,
Colbere-Garapin F. Persistent poliovirus infection: establishment and maintenance involve distinct mechanisms.
Virology. 1992;186:398–408.
84
J. Ravits
67. Pelletier I, Duncan G, Pavio , et al. Molecular mechanisms
of poliovirus persistence: key role of capsid determinants
during the establishment phase. Cell Mol Life Sci.
1998;54:1385–1402.
68. Blondel B, Duncan G, Couderc T, et al. Molecular aspects
of poliovirus biology with a special focus on the interactions
with nerve cells. J NeuroVirol. 1998;4:1–26.
69. Morrison ME, He YJ, Wien MW, Hogle JM, Racaniello VR.
Homolog-scanning mutagenesis reveals poliovirus receptor
residues important for virus binding and replication. J Virol.
1994;68:2578–88.
70. Colbere-Garapin F, Jacques S, Drillet AS, Pavio N,
Couderc T, Blondel B, et al. Poliovirus persistence in
human cells in vitro. Dev Biol. (Basel). 2001;105:99–104.
71. Destombes J, Couderc T, Thiesson D, Girard S, Wilt SG,
Blondel B. Persistent poliovirus infection in mouse motor
neurons. J Virol. 1997;71:1621–8.
72. Leparc-Goffart I, Julien J, Fuchs F, Janatova I, Aymard M,
Kopecka H. Evidence for the presence of poliovirus genomic
sequences in the CSF of patients with post-polio syndrome.
J Clin Microbiol. 1996;34:2023–6.
73. See DM, Kean KM, Kopecka H. Analysis of the sequence
of a poliovirus type 2-like defective interfering virus from
the cerebrospinal fluid of a patient with post-polio syndrome. Abstract 5th Congres de la Societe Franaise de
Microbiologie, Lille, France, April 28 1998.
74. Julien J, Leparc-Goffart I, Lina B, Fuchs F, Foray S,
Janatova I, et al. Post-polio syndrome: poliovirus persistence
is involved in the pathogenesis. J Neurol. 1999;246:472–6.
75. Leon-Monzon ME, Dalakas MC. Detection of poliovirus
antibodies and poliovirus genome in patients with the postpolio syndrome. Ann NY Acad Sci. 1995;753:208–18.
76. Sharief MK, Hentges R, Ciardi M. Intrathecal immune
response in patients with the post-polio syndrome.
N Engl J Med. 1991;325:749–55.
77. Galbraith DN, Nairn C, Clements GB. Evidence for
enteoviral persistence in humans. J Gen Virology. 1997;78:
307–12.
78. Kristensson K, Norrby E. Persistence of RNA viruses in the
central nervous system. Ann Rev Microbiol. 1986;40:
159–84.
79. Johnson RT. Chronic inflammatory and demyelinating
diseases. In: Viral Infections of the Nervous System (2nd
edn). Philadelphia: Lippincott-Raven Press; 1998. Chapter
10.
80. Coles A, Scolding N. Immune responses and the nervous
system. In: Scolding N, editor. Immunological and Inflammatory Disorders of the Central Nervous System. Oxford:
Butterworth Heinemannn; 1999. Chapter 1. pp 1–20.
81. Jolly E, Mucke L, Oldstone M. Viral persistence in neurons
explained by lack of major histocompatibility class I
expression. Science. 1991;253:1283–5.
82. Perlman S, Wu GF. Selection of and evasion from cytotoxic
T-cell responses in the central nervous system. In:
Buchmeier MJ, Campbell MJ, editors. Neurovirology:
Viruses and the Brain. San Diego: Academic Press; 2001.
pp 219–42.
83. McGeer PL, McGeer EG. Inflammatory processes in
amytrophic lateral sclerosis. Muscle Nerve. 2002;26:
459–70.
84. McGreer PL, Itagaki S, McGreer EG. Expression of
histocompatibility glycoprotein HLA-DR in neurological
disease. Acta Neuropathol. 1988;76:550–7.
85. Troost D, van den Oord JJ, de Jong JM, Swaab DF.
Lymphocytic infiltration in the spinal cord of patients with
amyotrophic lateral sclerosis. Clin Neuropathology. 1989;8:
289–94.
86. Engelhardt JI, Appel SH. IgG reactivity in the spinal cord
and motor neurons in amyotrophic lateral sclerosis. Arch
Neurol. 1990;47:1210–6.
87. Lampson LA, Kushner PD, Sobel RA. Major histocompatibility complex antigen expression in the affected tissues
in amyotrophic lateral sclerosis. Ann Neurol. 1990;28:
365–72.
88. Troost D, Van den Oord JJ, De Jong JMBV. Immunohistochemical characterization of the inflammatory infiltrate
in amyotrophic lateral sclerosis. Neuropath Appl Neurobiol.
1990;16:401–10.
89. Kawamata T, Akiyama H, Yamada T, McGeer PL.
Immunologic reactions in amyotrophic lateral sclerosis brain
and spinal cord tissue. Am J Path. 1992;140:691–707.
90. Engelhardt JI, Tajti J, Appel SH. Lymphocytic infiltrate in
the spinal cord in amyotrophic lateral sclerosis. Arch Neurol.
1993;50:30–6.
91. Roulston A, Marcellus RC, Brapton PE. Viruses and
apoptosis. Annu Rev Microbiol. 1999;53:577–628.
92. O’Brien V. Viruses and apoptosis. J Gen Virol.
1998;79:1833–45.
93. Hardwick JM. Viral-induced apoptosis. Adv Pharmacol.
1997;41:295–336.
94. Young LS, Dawson C, Eliopsulos AG. Viruses and
apoptosis. Br Med Bull. 1997;53:509–21.
95. Shen Y, Shenk TE. Viruses and apoptosis. Curr Opin Genet
Dev. 1995;5:105–11.
96. Allsopp TE, Fazakerley JK. Altruistic cell suicide and the
specialized case of the virus-infected nervous system. Trends
Neurosci. 2000;23:284–90.
97. Thomson BJ. Viruses and apoptosis. Int J Exp Pathol.
2001;82:65–76.
98. Barber GN. Host defense, viruses and apoptosis. Cell Death
Differ. 2001;8:113–26.
99. Fazakerley JK, Allsopp TE. Programmed cell death in virus
infections of the nervous system. Curr Top Microbiol
Immunol. 2001;253:95–119.
100. Ubol S, Tucker PC, Griffin DE, Hardwick JM.
Neurovirulent strains of alphavirus induce apoptosis in
bcl-2-expressing cells: role of a single amino acid change
in the E2 glycoprotein. Proc Natl Acad Sci. USA.
1994;91:5202–6.
101. Levine B, Huang Q, Isaacs JT, Reed JC, Griffin DE,
Hardwick JM. Conversion of lytic to persistent alphavirus
infection
by
bcl-2
cellular
oncogene.
Nature.
1993;361:739–42.
102. Tolskaya EA, Romanova LI, Kolesnikova MS,
Ivannikova TA, Smirnova EA, Raikhlin NT, et al.
Apoptosis-inducing and apoptosis-preventing functions of
poliovirus. J Virol. 1995;69:1181–9.
103. Agol VI, Belov GA, Bienz K, Egger D, Kolesnikova MS,
Raikhlin NT, et al. Two types of death of poliovirus-infected
cells: caspase involvement in the apoptosis but not cytopathic effect. Virology. 1998;252:343–53.
104. Girard S, Couderc T, Destombes J, Thiesson D,
Delpeyroux F, Blondel B. Poliovirus induces apoptosis
in the mouse central nervous system. J Virol.
1999;73:6066–72.
105. Barco A, Feduchi E, Carrssco L. Poliovirus protease 3Cpro
kills cells by apoptosis. Virology. 2000;266:352–60.
106. Goldstaub D, Gradi A, Bercovitch Z, Grosmann Z,
Nophar Y, Luria S, et al. Poliovirus 2A protease induces
apoptotic cell death. Mol Cell Biol. 2000;20:1271–7.
107. Blaschke AJ, Weiner JA, Chun J. Programmed cell death is a
universal feature of embryonic and postnatal neuroproliferative regions throughout the central nervous system.
J Comp Neurol. 1998;396:39–50.
108. Johnson EM, Deckwerth TL. Molecular mechanisms of
developmental neuronal death. Annu Rev Neurosci.
1993;16:31–46.
109. Yuan J, Yankner BA. Apoptosis in the nervous system.
Nature. 2000;407:802–9.
110. Burek MJ, Oppenheim RW. Cellular interactions that
regulate programmed cell death in the developing vertebrate
Persistent enteroviral infection in ALS
111.
112.
113.
114.
115.
116.
117.
118.
119.
120.
121.
122.
123.
124.
125.
126.
127.
128.
129.
130.
131.
132.
nervous system. In: Koliatsos VE, Ratan RR, editors. Cell
death and diseases of the nervous system. New Jersey:
Humana Press Inc; 1999. pp 145–179.
Yoshiyama Y, Yamada T, Asanuma K, Asahi T. Apoptosis
related antigen, Ley and nick-end labeling are positive in
spinal motor neurons in amyotrophic lateral sclerosis. Acta
Neuropathol. 1994;88:207–11.
Troost D, Aten J, Morsink F, de Jong JM. Apoptosis in
amyotrophic lateral sclerosis in not restricted to motor
neurons. Bcl-2 expression is increased in unaffected postcentral gyrus. Neuropath Appl Neurobiol. 1995;21:
498–504.
Mu X, He J, Anderson DW, Trojanowski JQ, Springer JE.
Altered expression of bcl-2 and bax mRNA in amyotrophic
lateral sclerosis spinal cord motor neurons. Ann Neurol.
1996;40:379–86.
Martin LJ. Neuronal death in amyotrophic lateral sclerosis is
apoptosis: possible contribution of a programmed cell death
mechanism. J Neuropathol Exp Neurol. 1999;58:459–71.
Ekegren T, Grundstrom E, Lindholm D, Aquilonius SM.
Up-regulation of Bax protein and increased DNA degradation in ALS spinal cord motor neurons. Acta Neurol Scand.
1999;1000:317–21.
Sathasivam S, Ince PG, Shaw PJ. Apoptosis in amyotrophic
lateral sclerosis: a review of the evidence. Neuropathol Appl
Neurobiol. 2001;27:257–74.
Guégan C, Przedborski S. Programmed cell death in amyotrophic lateral sclerosis. J Clin Invest. 2003;111:153–61.
Griffin DE, Hardwick JM. Perspective: virus infections and
the death of neurons. Trends Microbiol. 1999;7:155–60.
Everett H, McFadden G. Apoptosis: an innate immune
response to virus infection. Trends Microbiol. 1999;7:
160–5.
Friedlander RM. Apoptosis and caspases in neurodegenerative diseases. NEJM. 2003;348:1365–75.
Gosztonyi G, Koprowski H. The concept of neurotropism
and selective vulnerability (‘pathoclisis’) in virus infections
of the nervous system: a historical overview. Curr Top
Microbiol Immunol. 2001;253:1–13.
Evans DJ, Almond JW. Cell receptors for picornaviruses as
determinants of cell tropism and pathogenesis. Trends
Microbiol. 1998;6:198–202.
Rossmann MG, Bella J, Kolatkar PR, He Y, Wimmer E,
Kuhn RJ, et al. Cell recognition and entry by rhinoviruses
and enteroviruses. Virology. 2000;269:239–47.
Rossmann MG, He Y, Kuhn RJ. Picornavirus-receptor
interactions. Trends Microbiol. 2002;10:324–31.
Ohka S, Nomoto A. Recent insights into poliovirus
pathogenesis. Trends Microbiology. 2001;9:501–6.
Nomoto A, Koike S, Aoki HJ. Tissue tropism and species
specificity of poliovirus infection. Trends Microbiology.
1994;2:47–51.
Rossmann MG, Bella J, Kolatkar R, He Y, Wimmer E,
Kuhn RJ, et al. Cell recognition and entry by rhinoviruses
and enteroviruses. Virology. 2000;269:239–47.
Belnap DM, McDermott BM Jr, Filman DJ, Cheng N,
Trus BL, Zuccola HJ, et al. Three-dimensional structure of
poliovirus receptor bound to poliovirus. Proc Natl Acad Sci.
2000;97:73–8.
Gromeier M, Lu HH, Bernhardt G, Harber JJ, Bibb JA,
Wimmer E. The human poliovirus receptor: receptor-virus
interaction and parameters of disease specificity. Ann NY
Acad Sci. 1995;753:19–36.
Bernhardt G, Bibb JA, Bradley J, Wimmer E. Molecular
characterization of the cellular receptor for poliovirus.
Virology. 1994;199:105–13.
Racaneillo VR. The poliovirus receptor: a hook or an
unzipper? Structure. 1996;4:769–73.
Solecki D, Gromeier M, Harber J, Bernhardt G, Wimmer E.
Poliovirus and its cellular receptor: a molecular genetic
133.
134.
135.
136.
137.
138.
139.
140.
141.
142.
143.
144.
145.
146.
147.
148.
149.
150.
151.
152.
153.
85
dissection of a virus/receptor affinity interaction. J Mol
Recogn. 1998;11:2–9.
Racaniello VR. Early events in poliovirus infection:
virus-receptor interactions. Poc Natl Acad Sci. USA.
1996;93:11378–81.
Mendelsohn C, Johnson B, Lionetti KA, Nobis P,
Wimmer E, Racaniello VR. Transformation of a human
poliovirus receptor gene into mouse cells. Proc Natl Acad
Sci. USA. 1986;83:7845–9.
Rossman MG. The canyon hypothesis: hiding the host cell
receptor attachment site on a viral surface from immune
surveillance. J Biol Chem. 1989;264:14587–90.
Wien MW, Chow M, Hogle JM. Poliovirus: new insights
from an old paradigm. Structure. 1996;4:763–7.
Belnap DM, McDermott BM, Filman DJ, Cheng N,
Trus BL, Succola HJ, et al. Three-dimensional structure
of poliovirus receptor bound to poliovirus. PNAS.
2000;97:73–8.
He Y, Bowman VD, Mueller S, Bator CM, Bella J, Peng X,
et al. Interaction of the poliovirus receptor with poliovirus.
PNAS. 2000;97:79–84.
Brown RH Jr, Johnson D, Ogonowski M, Weiner HL. Type
1 human poliovirus binds to human synaptosomes. Ann
Neurol. 1987;21:64–70.
Freistadt MF, Kaplan G, Racaniello VR. Heterogeneous
expression of poliovirus receptor-related proteins in human
cells and tissues. Mol Cell Biol. 1990;10:5700–6.
Mendelsohn C, Wimmer E, Racaniello VR. Cellular
receptor for poliovirus: molecular cloning, nucleotide
sequence and expression of a new member of the immunoglobulin suerfamily. Cell. 1989;56:855–65.
Yang WX, Terasaki T, Shiroki K, Ohka S, Aoki J, Tanabe S,
et al. Efficient delivery of circulating poliovirus to the central
nervous system independently of poliovirus receptor.
Virology. 1997;229:
421–8.
Crotty S, Hix L, Sigal LJ, Andino R. Poliovirus pathogenesis
in a new poliovirus receptor transgenic mouse model: agedependent paralysis and a mucosal route of infection. J Gen
Virol. 2002;83:1707–20.
Ida-Hosonuma M, Iwasaki T, Taya C, Sato Y, Li J,
Nagata N. Comparison of neuropathogenicity of poliovirus
in two transgenic mouse strains expressing human poliovirus
receptor with different distribution patterns. J Gen Virol.
2002;83:1095–105.
Andino R, Boddeker N, Silvera D, Gamarnik AV.
Intracellular determinants of picornavirus replication.
Trends Microbiol. 1999;7:76–82.
Jubelt B, Narayan O, Johnson RT. Pathogenesis of human
poliovirus infection in mice. II. Age-dependency of paralysis.
J Neuropathol Exp Neurol. 1980;39:149–59.
Johnson RT. Pathogenesis of poliovirus infections. Ann NY
Acad Sci. 1995;753:361–5.
Johnson RT. Pathogenesis of central nervous system
infections. In: Johnson RT, editor. Viral Infections of the
Nervous System (2nd edn). Philadelphia: Lippincott-Raven;
1998. Chapter 3.
Ren R, Racaniello VR. Poliovirus spreads from muscle to the
central nervous system by neural pathways. J Infect Dis.
1992;166:747–52.
Illa I, Leon-Monzon M, Agboatwalla M, Dure-Samin A,
Dalakas MC. Role of muscle in acute poliomyelitis infection.
Ann NY Acad Sci. 1995;753:58–67.
Gromeier M, Wimmer E. Mechanism of injury-provoked
poliomyelitis. J Virol. 1998;72:5056–60.
Bradford-Hill A, Knowelden J. Inoculation and poliomyelitis: a statistical investigation in England and Wales in 1949.
Br Med J. 1950;2:1–6.
McCloskey BP. The relationship of prophylactic inoculations to the onset of poliomyelitis. Lancet. 1950;2:659–63.
86
J. Ravits
154. Sutter RW, Patriarca PA, Suleiman AJ, Brogan S,
Malankar PG, Cochi SL, et al. Attributable risk of DTP
injection in provoking paralytic poliomyelitis during a large
outbreak in Oman. J Infect Dis. 1992;165:444–9.
155. Strebel PM, Ion-Nedelcu N, Baughman AL, Sutter RW,
Cochi SL. Intramuscular injections within 30 days of
immunization with oral poliovirus vaccine: a risk for
vaccine-associated
paralytic
poliomyelitis.
NEJM.
1995;332:500–6.
156. Nathanson N, Langmuir AD. The Cutter incident: poliomyelitis following formaldehyde inactivated poliovirus vaccination in the United States during the spring of 1955.
Am J Hyg. 1963;78:16–81.
157. Bodian D, Horstmann DH. Polioviruses. In: Horsfall FL,
Tamm I, editors. Viral and rickettsial Infections of man.
Philadelphia: Lippincott; 1965. pp 430–73.
158. Bodian D, Howe HA. The rate of progression of poliomyelitis virus in nerves. Bull Johns Hopkins Hosp. 1941;69:
79–85.
159. Samuel BU, Ponnuraj E, Rajasingh J, John TJ. Experimental
poliomyelitis in bonnet monkey: clinical features, virology
and pathology. In: Brown F, Lewis BP, eds. Poliovirus
attenuation: molecular mechanisms and practical aspects.
Dev Biol Stand. 1993;78:71–8.
160. Leon-Monzon ME, Illa I, Dalakas MC. Expression of
poliovirus receptor in human spinal cord and muscle. Ann
NY Acad Sci. 1995;753:48–57.
161. Ohka S, Yang WX, Terada E, Iwasaki K, Nomoto A.
Retrograde transport of intact poliovirus through the axon
via the fast transport system. Virol. 1998;250:67–75.
162. Ponnuraj EM, John TJ, Levin MJ, Simoes EA. Cell-to-cell
spread of poliovirus in the spinal cord of bonnet monkeys.
J Gen Virol. 1998;79:2393–403.
163. Chou SM, Norris FH. Amyotrophic lateral sclerosis: lower
motor neuron disease spreading to upper motor neuron
disease. Muscle & Nerve. 1993;16:864–9.
164. Sigurdsson B. Observations on three slow infections of
sheep: maedi, paratuberculosis, rida, a slow encephalitis of
sheep with general remarks on infections which develop
slowly, and some of their special characteristics. Br Vet J.
1954;110:255–70.
165. O’Connell J, Albin R, Blum D, Grint P, Schwartz J.
Development of antiviral agents for picornavirus infections.
In: Rotbart HA, editor. Human Enteroviral Infections.
Washington DC: American Society for Microbiology;
1995. Chapter 18.
166. Smith TJ, Kremer MJ, Luo M, Vriend G, Arnold E,
Kamer G, et al. The site of attachment in human rhinovirus
14 for antiviral agents that inhibit uncoating. Science.
1986;233:1286–93.
167. Rossmann MG. The structure of antiviral agents that inhibit
uncoating when complexed with viral capsids. Antiviral Res.
1989;11:3–14.
168. Zhang A, Nanni RG, Li T, Arnold GF, Oren DA, JacoboMolina A, et al. Structure determination of antiviral
compound SCH 38057 complexed with human rhinovirus
14. J Mol Biol. 1993;230:857–67.
169. McKinley MA, Fever DC, Rosen MG. Treatment of the
picornavirus common cold by inhibitors of viral uncoating
and attachment. Annu Rev Microbiol. 1992;46:635–45.
170. Oliveira MA, Zhao R, Lee WM, Kremer MJ, Minor I,
Rueckert RR, et al. The structure of human rhinovirus 16.
Structure. 1993;1:51–68.
171. Lewis JK, Bothner B, Smith TJ, Siuzdak G. Antiviral agent
blocks breathing of the common cold virus. Proc Natal Acad
Sci. USA. 1998;95:6774–8.
172. Wang W, Lee WM, Mosser AG, Rueckert RR. WIN 52035dependent human rhinovirus 16: assembly deficiency
caused by mutations near the canyon surface. J Virol.
1998;72:1210–8.
173. Abdel-Rahman SM, Kearns GL. Single oral dose escalation
pharmacokinetics of pleconaril (VP63843) capsules in
adults. J of Clin Pharm. 1999;39:613–8.
174. Kearns GL, Abdel-Rahman SM, James LP, Blowey DL,
Marshall JD, Wells TG, et al. Single-dose pharmacokinetics
of a pleconaril (VP63843) oral solution in children and
adolescents. Antimicrobial Anents and Chemotherapy.
1999;43:634–8.
175. Ansevin CF. Treatment of ALS with pleconaril. Neurology.
2001;56:691–2.
176. McKinlay MA. Recent advances in the treatment of
rhinovirus infections. Current Opinion Pharmacol. 2001;1:
477–81.
177. Okada I, Matsumori A, Matoba Y, Tominaga M, Yamada T,
Kawai C. Combination treatment with ribavirin and
interferon for coxsackievirus B3 replication. J Lab Clin
Med. 1992;120:569–73.
178. Waldmeier PC. Prospects for antiapoptotic drug thereapy
of neurodegenerative diseases. Progress in NeuroPsychopharmacology & Biological Psychiatry. j2003;27:
303–21.
179. Jacobson MD. Anti-apoptosis therapy: a way of treating
neural degeneration? Curr Biol. 1998;8:R418–21.
180. Tatton WG, Chalmers-Redman RM, Ju WY, Wadia J,
Tatton NA. Apoptosis in neural degenerative disorders:
potential for therapy by modifying gene transcription.
J Neural Transm. 1997;49(Suppl): 245–68.
181. Schulz JB, Weller M, Moskowitz MA. Caspases as treatment
targets in stroke and neurodegenerative diseases. Ann
Neurol. 1999;45:421–9.
182. Nicholson DW. From bench to clinic with apoptosis-based
therapeutic agents. Nature. 2000;407:810–6.
183. Vandepapelièr P. Thereapeutic vaccination against chronic
viral infections. Lancet Infectious Diseases. 2002;2:353–67.
184. Rotbart HA. Nucleic acid detection systems for enteroviruses. Clin Microbiol Rev. 1991;4:156–68.
185. Romero JR, Rotbart HA. PCR-based strategies for the
detection of human enteroviruses. In: Ehrlich GD,
Greenberg SJ, editors. PCR-Based Diagnostics in
Infectious Disease. Cambridge, MA: Blackwell Scientific
Publications; 1994. p 341.
186. Romero JR. Reverse transcription-polymerase chain reaction
detection of the enteroviruses: overview and clinical utility in
pediatric enteroviral infections. Archives of Pathology and
Laboratory Medicine. 1999;123:1161–9.
187. Olive DM, Al-Mufti S, Al-Mulla W, Khan MA, Pasca A,
Stanway G, Al-Nakib W. Detection and differentiation of
picornaviruses in clinical samples following genomic amplification. J Gen Virol. 1990;71:2141–7.
188. Gruber AD, Moennig V, Hewicker-Trautwein M,
Trautwein G. Effect of formalin fixation and long-term
storage on the detectability of bovine viral-diarrhoea-virus
(BVDV) RNA in archival brain tissue using polymerase
chain reaction. J Vet Med. 1994;41:654–61.
189. Karlsen F, Kalantari M, Chitemerere M, Johansson B,
Hagmar B. Modifications of human and viral deoxyribonucleic acid by formaldehyde fixation. Lab Investigation.
1994;71:604–11.
190. Jubelt B, Lipton HL. ALS: persistent scientists do not find
persisting enteroviruses (editorial). Neurology. 2004;62:
1250–1.
191. Redline RW, Genest DR, Tycko B. Detection of enteroviral
infection in paraffin-embedded tissue by the RNA polymerase chain reaction technique. Am J Clin Pathol.
1991;96:568–571.
192. Rupp GM, Locker J. Purification and analysis of RNA from
paraffin-embedded tissues. BioTechniques. 1988;6:56–60.
193. Ben-Ezra J, Johnson DA, Rossi J, Cook N, Wu A. Effect of
fixation on the amplification of nucleic acids from paraffinembedded material by the polymerase chain reaction.
J Histochem Cytochem. 1991;39:351–4.
Persistent enteroviral infection in ALS
194. Foss RD, Guha-Thakurta N, Conran RM, Gutman P.
Effects of fixative and fixation time on the extraction and
polymerase chain reaction amplification of RNA from
paraffin-embedded tissue. Comparison of two housekeeping
gene
mRNA
controls.
Diagnostic
Mol
Pathol.
1994;3:148–55.
195. Dakhama A, Macek V, Hogg JC, Hegele RG. Amplification of human ß-actin gene by the reverse transciptasepolymerase chain reaction: implications for assessment of
RNA from formalin-fixed, paraffin-embedded material.
J Histochem Cytochem. 1996;44:1205–7.
196. Coombs NJ, Gough AC, Primrose JN. Optimization
of DNA and RNA extraction from archival formalinfixed tissue. Nucleic Acids Research. 1999;27:
1–3.
197. Masuda N, Ohnishi T, Kawamoto S, Monden M, Okubo K.
Analysis of chemical modification of RNA from formalinfixed samples and optimization of molecular biology
applications for such samples. Nucleic Acids Research.
1999;27:4436–43.
87
198. Beaulieux F, Berger MM, Tcheng R, Giraud P, Lina B.
RNA extaction and RT-PCR procedures adapted for the
detection of enterovirus sequences from fozen and paraffinembedded formalin-fixed spinal cord samples. J Virol
Methods. 2003;107:115–20.
199. Wolk D, Mitchell S, Patel R. Principles of molecular
microbiology testing methods. Infectious Disease Clinics of
North America. 2001;15:1157–1204.
200. Reiss RA, Rutz B. Quality control PCR: a method for
detecting
inhibitors
of
Taq
DNA
polymerase.
BioTechniques. 1999;27:920–6.
201. Konet DS, Mezencio JMS, Babcock G, et al. Inhibitors of
RT-PCR in serum. J Virol Methods. 2000;84:95–8.
202. Simone NL, Bonner RF, Gillespie JW, Emmert-Buck MR,
Liotta LA. Laser-capture microdissection: opening the
microscopic frontier to molecular analysis. Trends Genet.
1998;14:272–6.
203. Eltoum IA, Siegal GP, Frost AR. Microdissection of
histologic sections: past, present, and future. Adv Anat
Path. 2002;9:316–22.