Morphogenesis of the foetal membranes and placentation in ...
Elucidation of Nipah virus morphogenesis and replication using ultrastructural and molecular...
Transcript of Elucidation of Nipah virus morphogenesis and replication using ultrastructural and molecular...
Elucidation of Nipah virus morphogenesis and replication usingultrastructural and molecular approaches
Cynthia S. Goldsmith a,*, Toni Whistler a, Pierre E. Rollin a, Thomas G. Ksiazek a,Paul A. Rota a, William J. Bellini a, Peter Daszak a,1, K.T. Wong b, Wun-Ju Shieh a,
Sherif R. Zaki a
a Division of Viral and Rickettsial Diseases, National Center for Infectious Diseases, Centers for Disease Control and Prevention, Mailstop G30, 1600
Clifton Road NE, Atlanta, GA 30333, USAb University of Malaysia, Kuala Lumpur, Malaysia
Received 8 September 2002; received in revised form 18 November 2002; accepted 18 November 2002
Abstract
Nipah virus, which was first recognized during an outbreak of encephalitis with high mortality in Peninsular Malaysia during
1998�/1999, is most closely related to Hendra virus, another emergent paramyxovirus first recognized in Australia in 1994. We have
studied the morphologic features of Nipah virus in infected Vero E6 cells and human brain by using standard and immunogold
electron microscopy and ultrastructural in situ hybridization. Nipah virions are enveloped particles composed of a tangle of
filamentous nucleocapsids and measured as large as 1900 nm in diameter. The nucleocapsids measured up to 1.67 mm in length and
had the herringbone structure characteristic for paramyxoviruses. Cellular infection was associated with multinucleation,
intracytoplasmic nucleocapsid inclusions (NCIs), and long cytoplasmic tubules. Previously undescribed for other members of the
family Paramyxoviridae , infected cells also contained an inclusion formed of reticular structures. Ultrastructural ISH studies suggest
these inclusions play an important role in the transcription process.
Published by Elsevier Science B.V.
Keywords: Nipah virus; Electron microscopy; Paramyxoviridae ; Henipavirus; In situ hybridization; Replication complex; Zoonotic; Encephalitis;
Ultrastructure; Immunogold labeling
1. Introduction
An increase in cases of acute febrile encephalitis
occurred in Peninsular Malaysia between September
1998 and May 1999, with a similar illness being reported
in Singapore in March 1999. Most cases occurred in
males who had been exposed to pigs, including abattoir
workers, and over 100 deaths were reported. The illness
was characterized by fever and headache, followed by
drowsiness and disorientation; in severe cases, seizures
and coma occurred within 24�/48 h. Concurrently, there
was an increase in illness among pigs in the same region
(Centers for Disease Control and Prevention, 1999a,b).
The etiologic agent for both human and swine diseases,
now known as Nipah virus, was isolated from cere-
brospinal fluid from human patients and identified as
belonging to the family Paramyxoviridae (Chua et al.,
1999, 2000).
Members of the family Paramyxoviridae are nonseg-
mented, negative-stranded RNA viruses composed of
helical nucleocapsids enclosed within an envelope to
form roughly spherical, pleomorphic virus particles
(Lamb and Kolakofsky, 2001). Within the family
Paramyxoviridae , there are two subfamilies, the Para-
myxovirinae and Pneumovirinae . The subfamily Para-
myxovirinae has been divided into three genera:
Rubulavirus (prototype, mumps virus), Respirovirus
(prototype, human parainfluenza virus 1), and Morbil-
livirus (prototype, measles virus). An additional fourth
* Corresponding author. Tel.: �/1-404-639-3306; fax: �/1-404-639-
1377.
E-mail address: [email protected] (C.S. Goldsmith).1 Current address: Consortium for Conservation Medicine,
Lamont-Doherty Earth Observatory, 61 Route 9W, Palisades, NY
10964-8000, USA.
Virus Research 92 (2003) 89�/98
www.elsevier.com/locate/virusres
0168-1702/02/$ - see front matter. Published by Elsevier Science B.V.
doi:10.1016/S0168-1702(02)00323-4
genus, Henipavirus, has been proposed recently, with
Hendra virus as the prototype virus, and Nipah virus as
the second member (Mayo, 2002). Hendra virus was
first recognized in 1994 during an outbreak of severerespiratory illness in horses and humans that occurred in
Queensland, Australia (Murray et al., 1995). Serologic,
molecular, and immunohistochemical methodologies
developed to detect Hendra virus were instrumental in
the rapid identification of Nipah virus.
In this study, we have examined the morphogenesis of
Nipah virus in cell culture and in the human central
nervous system by using standard thin section, negativestain, and immunogold ultrastructural techniques. An
ultrastructural in situ hybridization (ISH) assay to
Nipah virus was also developed to study the cellular
localization of viral messenger and genomic RNA
(genRNA). Although Nipah virus shares many of its
morphologic features with other members of the family
Paramyxoviridae , the combined ultrastructural and
molecular tools used in this study also allowed identi-fication of several novel features of this newly recog-
nized virus.
2. Methods
2.1. Virus isolation and cell infections
Nipah virus was isolated at the Department ofMedical Microbiology, University Hospital (Kuala
Lumpur, Malaysia) and at the Centers for Disease
Control and Prevention (CDC; Atlanta, GA), by
cocultivation of patient cerebrospinal fluid with Vero
E6 cells (Chua et al., 1999, 2000). Virus was grown
within the Biosafety Level 4 laboratory at CDC in Vero
E6 cells (ATCC CRLI586) with Basal Eagle’s medium
supplemented with 10% fetal bovine serum, 2 mMglutamine, 100 mg/ml streptomycin, and 100 U/ml
penicillin (Life Technologies). Harvesting of infected
and uninfected cells occurred at 35 and 50 h postinocu-
lation.
2.2. Standard EM
Infected and uninfected Vero E6 cells and formalin-fixed brain tissues were washed in 0.1 M phosphate
buffer, pH 7.3, fixed in buffered 2.5% glutaraldehyde,
gamma-irradiated (2�/106 rad) on ice, and stored in
phosphate buffer. Specimens were post-fixed in 1%
buffered osmium tetroxide, stained in 4% uranyl acetate,
dehydrated through a graded series of alcohols and
propylene oxide, and embedded in a mixture of Epon-
substitute and Araldite (Mollenhauer, 1964). Thinsections were stained with 4% uranyl acetate and
Reynold’s lead citrate. For negative stain preparations,
supernatants from infected cultures were gamma-irra-
diated, banded on a 30% sucrose cushion, and concen-
trated at 100 000�/g for 2 h. Pellets were resuspended in
small amounts of dH2O or 2.5% buffered glutaralde-
hyde. Copper mesh grids coated with formvar andcarbon (Electron Microscopy Sciences) were glow-dis-
charged and placed on drops of the specimen for 10 min,
then dried, and stained with 2% phosphotungstic acid,
pH 5.7.
2.3. Immunogold electron microscopy (IEM)
For thin section preparations, infected and uninfected
Vero E6 cells were fixed in phosphate-buffered 1.5%paraformaldehyde and 0.025% glutaraldehyde, gamma-
irradiated, dehydrated in alcohols, and embedded in LR
White resin (London Resin Company). Formalin-fixed
brain tissues were also dehydrated in alcohols and
embedded in LR White resin. For negative stain
preparations, supernatants from infected and uninfected
cells were gamma-irradiated, banded and concentrated,
and resuspended in dH2O or 2% buffered paraformal-dehyde.
For immunogold procedures, all specimens were
placed on nickel mesh grids. The wash buffer, also
used for dilution of the antibodies, consisted of 0.01 M
phosphate-buffered saline (PBS), 1% bovine serum
albumin, 0.2% Tween-20, and 0.1% Triton-X. Grids
were sequentially placed on drops of 0.05% ovalbumin
in PBS, followed by drops of wash buffer containing 1%normal goat serum. Next, specimens were allowed to
react with appropriate dilutions of HMAF raised
against Hendra virus or Nipah virus; these antibodies
are known to cross-react with either virus. After several
washes, the specimens were reacted with goat anti-
mouse conjugated to colloidal gold particles (Jackson
ImmunoReagents; Electron Microscopy Sciences) di-
luted in wash buffer with 1% fish gelatin added, andthen rinsed several times in wash buffer and then water.
Negative stain preparations were stained with 2%
phosphotungstic acid, pH 5.7, and sections were stained
with 1% osmium tetroxide and 4% uranyl acetate.
Uninfected Vero E6 cells were used as negative controls,
and an unrelated HMAF was reacted with Nipah-
infected cells to check for non-specific staining. All
antibodies were pre-absorbed against uninfected VeroE6 cells prior to their use (Goldsmith et al., 1995).
2.4. Ultrastructural in situ hybridization (ISH)
Reverse transcription-polymerase chain reaction pro-
ducts from portions of nucleoprotein (N), glycoprotein
(G) or fusion protein (F) genes of Nipah virus were
cloned into the dual promoter plasmid pCRII (Invitro-gen) (Table 1). Riboprobes used for ISH were generated
from the linearized plasmid, using the appropriate RNA
polymerase and incorporating either digoxigenin-11-
C.S. Goldsmith et al. / Virus Research 92 (2003) 89�/9890
dUTP or biotin-11-dUTP (RNA Labeling Kit, Roche
Molecular Biochemicals). Optimal lengths of riboprobes
were determined in pilot experiments and found to be in
the range of 200�/400 bases. Both positive- and negative-
sense riboprobes were generated to detect viral genRNA
and messenger RNA (mRNA), respectively. The nega-
tive-sense riboprobe would also hybridize with the anti-
genomic RNA template. Nipah virus probes were
pooled into positive- or negative-sense cocktails to
increase sensitivity.
Several pretreatment methodologies were evaluated in
order to permeabilize the ribonucleoprotein complex
and increase the efficiency of nucleic acid detection.
Pretreatment solutions used included 0.5�/5 N NaOH, 1
N HCl, 1�/10% Triton-X 100, Proteinase K (100 mg/ml),
1�/Citra (Biogenix), 0.01 M EDTA, 10% sodium
periodate, 1% IGEPAL, 0.005% saponin, and 0.05 M
glycine.Sections of LR White-embedded specimens placed on
nickel mesh grids were first floated onto drops of 2�/
standard saline citrate (SSC: 1�/SSC contains 0.15 M
sodium chloride, 0.015 M sodium citrate). Grids were
then prehybridized at room temperature for 30 min in
hybridization buffer (Roche Molecular Biochemicals)
containing 50% formamide, washed in 4�/SSC and
blotted dry. Hybridization cocktail was prepared by
adding riboprobes to hybridization buffer at a final
concentration of 1 ng/ml per probe. The mix was
denatured at 95 8C for 5 min and immediately trans-
ferred onto ice. Sections were allowed to hybridize on
drops of cocktail in a moist, closed chamber at 37 8Covernight. The grids were washed in 6�/SSC for 10 min
at room temperature, followed by two washes in 2�/
SSC containing 50% formamide at 44 8C for 5 and then
20 min. Two final 2�/SSC washes and a water rinse
were performed at room temperature. Immunogold
detection of the digoxigenin and biotin markers was
performed as described above by using either sheep anti-
digoxigenin or goat anti-biotin conjugated to colloidal
gold (Electron Microscopy Sciences).
Negative controls for Nipah virus experiments in-
cluded hybridizations using Nipah virus probes with
uninfected and Hendra virus-infected Vero E6 cells.
Hendra virus probes and an irrelevant riboprobe of
similar length, GC content, and concentration as the
Nipah virus riboprobe pool were hybridized with Nipah
virus-infected cells as additional controls. The specificityof hybridization was also confirmed by application of
RNAse just prior to hybridization in some instances.
This was done by incubation of the grids in a solution
containing 100 mg/ml DNAse-free RNAse (Roche
Molecular Biochemicals) in 2�/SSC for 1 h in a humid
chamber at 37 8C. Sections were then thoroughly rinsed
in PBS, post-fixed in 4% paraformaldehyde for 5 min,
and equilibrated to 2�/SSC prior to hybridization.
2.5. Multiple labeling
For double-label experiments to detect both genRNA
and mRNA on a single section, the positive- and
negative-sense riboprobes were added sequentially to
avoid self-annealing of probes. Therefore, hybridization
and washes were performed in two rounds, the first with
the genomic riboprobe pool, and then repeated using a
differently labeled messenger riboprobe pool. In double-
label experiments to detect nucleic acid and proteinwithin a single section, ISH was conducted first and the
sections were rinsed in distilled water, followed by the
HMAF binding steps of the immunogold protocol. Last,
to detect riboprobes and HMAF, grids were processed
for gold labeling as described above, using an appro-
priate combination (anti-digoxigenin, anti-biotin, or
anti-mouse) of colloidal gold-conjugated antibodies.
These antibodies were tagged with varying sizes ofcolloidal gold (from 5 to 18 nm) to allow for differential
localization.
3. Results
3.1. Morphologic characteristics of Nipah virus in cell
culture
The morphologic features of Nipah virus isolates were
similar to those of other members of the family
Paramyxoviridae , subfamily Paramyxovirinae . In both
thin section and negative stain preparations, extracel-lular virions appeared as tangled collections of filamen-
tous, helical nucleocapsids surrounded by the viral
envelope (Fig. 1A, B). Particles were pleomorphic and
varied greatly in size (Fig. 1C), averaging about 500 nm
in diameter (range, 180�/1900 nm). Negative stain
electron microscopy (EM) revealed nucleocapsids with
the typical herringbone appearance that is characteristic
for paramyxoviruses (Fig. 1D). These measured anaverage of 21 nm in diameter with a 5 nm periodicity,
and up to 1.67 mm in length. In thin section prepara-
tions, nucleocapsids averaged 18 nm in diameter, and
Table 1
Riboprobes used for ISH studies of Nipah and Hendra viruses
Virus, GenBank accession
no., gene
Nucleotide posi-
tions
Riboprobe size (nu-
cleotides)
Nipah-AF212302
Nucleocapsid 1292�/1515 223
Glycoprotein 8943�/9333 390
Fusion 6654�/6954 300
Hendra-AFO17149
Nucleocapsid 1292�/1515 223
C.S. Goldsmith et al. / Virus Research 92 (2003) 89�/98 91
spikes along the viral envelope, when seen, measured 12
nm in length (Fig. 1E).
When thin sections of infected Vero E6 cells were
examined, the cytopathic effect observed included the
formation of massive multinucleate giant cells (Fig. 2A),
vacuolation, and apoptotic features as evidenced by
condensed and fragmented nuclei. Within the cytoplasm
of infected cells, inclusions were formed by accumula-
Fig. 1. Morphologic features of Nipah virus particles grown in Vero E6 cells. (A) In thin section preparations, extracellular particles consist of a
compact tangle of filamentous nucleocapsids enclosed within the virus envelope. Note that some nucleocapsids are arranged transversely or
tangentially along the virus envelope. (B) Negative staining of particles revealed a dense accumulation of filamentous nucleocapsids within the
envelope. A few spikes (arrow) are seen along the surface. (C) Aggregation of extracellular particles, with a variety of shapes and sizes. At times, the
virus envelope appears detached from the nucleocapsid core (arrow). Long tubules (arrowhead) are also apparent within some particles (see Fig. 5D).
Immunogold labeling of negative stain preparation of Nipah virus nucleocapsid, using HMAF and 12 nm colloidal gold. Note the herringbone
appearance of the helical nucleocapsid, characteristic for paramyxoviruses. (E) Prominent spikes on the envelope (arrowhead) were seen only
occasionally for Nipah virus particles. Bars, 100 nm.
C.S. Goldsmith et al. / Virus Research 92 (2003) 89�/9892
tions of viral nucleocapsids surrounded by ill-defined,
‘fuzzy’ electron-dense material. Inclusions could become
quite large, at times filling most of the cytoplasm (Fig.
2A). As with other members of the family Paramyx-
oviridae , nucleocapsids accumulated and became closely
aligned along the plasma membrane as particles pre-
pared to bud (Fig. 3A). Viral budding was associated
with darkening at the plasma membrane, where nucleo-
capsids were variously oriented. Occasionally, budding
profiles had very organized (fingerprint-like) arrange-
ments of nucleocapsids as they juxtaposed along the
viral envelope (Fig. 3B).
Fig. 2. (A) Multinucleate giant cell with a large NCI (*) measuring almost 25 mm across and filling most of the cytoplasm. (B) Enlargement of area at
arrow in A, showing a typical NCI (*) and a separate RI (encompassed by arrowheads) composed of a network of membrane-like structures. Nu,
nucleus; RER, rough endoplasmic reticulum. Bars: (A) 1 mm; (B) 100 nm.
Fig. 3. Budding particles. (A) Nipah virus nucleocapsids (arrow) become tightly aligned along the plasma membrane as particle prepares to bud. (B)
Rigid positioning of nucleocapsids sometimes formed fingerprint-like structures. Bars, 100 nm.
C.S. Goldsmith et al. / Virus Research 92 (2003) 89�/98 93
Additional noteworthy features were associated with
Nipah virus-infected cells. First, an unusual cytoplasmicinclusion was found, composed of a network of mem-
brane-like reticular structures (Fig. 2B, Fig. 4A). These
were formed by open and closed ring-like structures,
which averaged 38 nm in diameter, and were observed in
close proximity to, and at times connected with, rough
endoplasmic reticulum membranes. This reticular inclu-
sion (RI) was morphologically distinct from the typical
nucleocapsid inclusions (NCIs) and absent from unin-fected Vero E6 cells (Fig. 4B), and its viral origin
became evident after ISH labeling experiments (see
below). Second, also found within the periphery of
Nipah virus-infected cells were long cytoplasmic tubules,
30�/45 nm in diameter (Fig. 5). These occasionally were
continuous with the plasma membrane or were incor-
porated into virus particles (Fig. 1C).
3.2. Localization of viral proteins, messenger RNA, and
genomic RNA
In both thin section and negative stain preparations,immunogold EM (IEM) labeling employed anti-Nipah
or anti-Hendra hyperimmune mouse ascitic fluid
(HMAF). Negative stain preparations showed gold label
on the naked nucleocapsids (Fig. 1D) and lightly
along the fringe of viral glycoproteins. In thin section
preparations, label was evident on nucleocapsids in
inclusions and within particles (Fig. 6A, B). A less-
intense label was also observed over the RIs
(Fig. 6A) and the long cytoplasmic tubules. No IEM
labeling was observed by reacting anti-Nipah or anti-
Hendra HMAFs with uninfected Vero E6 cells, or by
reacting an unrelated HMAF with Nipah virus-infected
cells.
In contrast, ultrastructural ISH using positive- or
negative-sense riboprobes, or a combination of both,
revealed localization of genRNA, anti-genomic RNA
template, and mRNA almost exclusively over the RIs
(Fig. 7A�/C). Only rarely was signal associated with the
NCIs, despite several attempts to ‘open up’ the RNA-
protein complex. ISH label was detected in only some of
the virus particles, and in these cases signal was seen in
association with the RIs.
Results of double-label experiments where both
protein and either mRNA or genRNA were detected
(IEM/ISH experiments) underscored the finding that
viral nucleic acids were found almost exclusively in the
RIs, whereas viral antigens were seen in both NCIs and
RIs (Fig. 7D).
Fig. 4. (A) RI composed of a network of open and closed ring-like structures (arrowheads). Note the continuity between these structures and the
membranes of the rough endoplasmic reticulum (RER). (B) Uninfected Vero E6 cell, showing a comparable area of RER as is shown in Fig. 4A.
Bars, 100 nm.
Fig. 5. Long cytoplasmic tubules (arrowhead), at times continuous with the plasma membrane (arrow), were observed in Nipah virus-infected cells.
Bar, 100 nm.
C.S. Goldsmith et al. / Virus Research 92 (2003) 89�/9894
The specificity of the ISH reactions was also con-
firmed by hybridization with control cells and probes.
Nipah virus probes did not react with uninfected or
Hendra virus-infected Vero E6 cells. No signal was
observed when Nipah virus-infected cells were
hybridized with unrelated or Hendra virus probes.
Finally, pretreatment of Nipah virus-infected cells with
RNAse eliminated the reactivity with homologous
probes.
3.3. Human brain tissue
During ultrastructural examination of central nervous
system tissues from fatal cases of Nipah virus infection,
both the typical viral NCIs and the RIs were recognized
(Fig. 8A, B). Infected cells were generally difficult to
locate and were mostly seen in areas surrounding blood
vessels of the brain stem. Inclusions were seen within
neurons and neuronal processes and occasionally within
Fig. 6. Immunogold labeling, using HMAF. (A) Detection of Nipah virus proteins (12 nm gold) on the NCI (*) and lightly over the RI (arrow) by
using immunolabeling. (B) Localization of Nipah virus proteins (18 nm gold) on nucleocapsids within extracellular virus particles. Bars, 100 nm.
Fig. 7. Localization of Nipah virus RNA by using ultrastructural ISH. (A) Low-power magnification of Nipah virus-infected cell with detection of
genRNA (6 nm gold) over the RI (arrow) but not within the NCI (*). (B) Detection of mRNA (10 nm gold) over the RI. (C) Colocalization of Nipah
virus mRNA (10 nm gold) and genRNA (6 nm gold) over the region of the RI. (D) Detection of Nipah virus genRNA (6 nm gold) in the RI by using
ultrastructural ISH, and of Nipah virus proteins (10 nm gold) on the NCI and lightly over the RI by using immunogold labeling. Bars, 100 nm.
C.S. Goldsmith et al. / Virus Research 92 (2003) 89�/98 95
endothelial cells, and were immunogold-labeled by using
specific antisera (Fig. 8C). No mature virus particles
were identified in the limited number of tissues exam-
ined.
4. Discussion
When an outbreak of severe encephalitis with a high
mortality rate occurred in Malaysia during 1998�/1999,
Japanese encephalitis virus was initially suspected as the
causative agent. Even so, the clinical and epidemiologicfeatures were not consistent with this disease. Ultra-
structural observations of a virus isolated from cerebral
spinal fluids were instrumental in identifying the etiolo-
gic agent as a member of the family Paramyxoviridae .
Serologic, molecular, and immunohistochemical ap-
proaches indicated it was closely related to, but distinct
from, Hendra virus, another recently recognized virus
first detected in Australia in 1994 (Chua et al., 1999,2000; Goldsmith et al., 2000; Wong et al., 2002).
Nipah virus-infected Vero E6 cells had numerous
ultrastructural features in common with other members
of the family Paramyxoviridae , sub-family Paramyx-
ovirinae , including characteristic herringbone-structured
viral nucleocapsids; cytoplasmic NCIs; nucleocapsids
aligned at the plasma membrane during the budding
process; pleomorphic, extracellular particles; and the
formation of multinucleate giant cells (Compans et al.,
1966; Raine et al., 1969; Dubois-Dalcq and Reese, 1975;
Choppin and Compans, 1975; Hyatt and Selleck, 1996;
Hyatt et al., 2001). The typical cytoplasmic NCIs, which
measured up to 28 mm in diameter, displayed strong
immunogold labeling of nucleocapsids when reacted
with HMAF raised against either Nipah or Hendra
viruses. Additional structures present in Nipah virus-
infected cells, which have also been reported for Hendra
virus-infected cells (Hyatt et al., 2001), were long
cytoplasmic tubules that were at times continuous with
the plasma membrane. Of interest were the highly
pleomorphic virions. These measured up to 1900 nm
in diameter, which would allow for the inclusion of
multiple copies of the viral nucleocapsids within a single
particle. Although not a common finding, polyploid
virions have been previously reported for other members
of the family Paramyxoviridae (Rager et al., 2002).
The technique of ultrastructural ISH has become a
powerful tool in the EM laboratory (McFadden et al.,
1988; Puvion-Dutilleul and Puvion, 1991; Bienz and
Egger, 1995). In the current study, ISH techniques aided
Fig. 8. Central nervous system of Nipah virus patients. (A) Thin section electron micrograph of human brain tissue, showing Nipah virus NCI
(arrow) within a neuron. (B) Mixed inclusion of virus nucleocapsids (arrow) and reticular membrane-like structures (arrowheads) within a neuronal
process. (C) Antigen-positive staining of virus inclusions, using HMAF and 18 nm colloidal gold. Nu, nucleus; RER, rough endoplasmic reticulum.
Bars: (A) 1 mm; (B, C) 100 nm.
C.S. Goldsmith et al. / Virus Research 92 (2003) 89�/9896
in the recognition of a RI (see Fig. 7) and confirmed its
viral nature. The RIs were also seen in autopsy tissues
from patients infected with Nipah virus, indicating that
this feature may play a significant role in virus replica-tion in vivo. This is, to our knowledge, a previously
undescribed feature for members of the family Para-
myxoviridae .
The long-standing model for paramyxoviruses holds
that viral genRNA remains encapsidated during mRNA
transcription and genome replication (Sedlmeier and
Neubert, 1998). Although ultrastructural ISH did not
detect genRNA in the nucleocapsids, this result may bedue to the tight packaging of the RNA with viral
proteins; similar ISH results have been reported for
other RNA viruses (Troxler et al., 1992; Grief et al.,
1997). Instead, Nipah virus RNAs, along with viral
proteins, were detected within the RIs. These findings
raise the possibility that for Nipah virus, these structures
are central to the transcription process. The RIs may be
analogous to the ‘replication complexes’ that have beenreported for positive-stranded RNA viruses (see Egger
et al., 2000). This term has been used to describe smooth
membrane clusters present within positive-stranded
RNA virus-infected cells (e.g. vesicular rosettes in
poliovirus, double-membrane vesicles in arteriviruses,
and vesiculate inclusions in members of the plant virus
family Comoviridae ; Francki et al., 1985; Pedersen et al.,
1999; Teterina et al., 2001). Ultrastructural ISH andRNA protection assay studies have also shown the
presence of viral RNA associated with these structures
and strongly suggest their integral involvement with
virus RNA initiation and replication (Bienz et al., 1992;
Egger et al., 1996; Grief et al., 1997).
Phylogenetic and serologic data have established that
Nipah and Hendra viruses are sufficiently different from
other members of the subfamily Paramyxovirinae towarrant a new genus, Henipavirus, to include these two
related, recently emergent viruses (Wang et al., 2000;
Harcourt et al., 2001; Mayo, 2002). Here, we report
ultrastructural features of Nipah virus that are also
different from other members of the subfamily Para-
myxovirinae . These include RIs, cytoplasmic tubules, a
longer length of viral nucleocapsid, and the highly
pleomorphic nature of the virus particles. Studies onNipah and Hendra viruses have emphasized the unique
role of traditional EM techniques in the recognition of
emerging pathogens and of the insights into virus
replication gained when molecular techniques are
adapted to ultrastructural studies.
Acknowledgements
We are most thankful to the following people: K.B.
Chua, for initial isolation of Nipah virus; Brian Har-
court, for primer information, virus purification, and
review of the manuscript; Larry Anderson and Brian
Mahy, for guidance; and Claudia Chesley for editorial
review.
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