Upload
yongchang
View
216
Download
0
Embed Size (px)
Citation preview
Recombinant influenza A H3N2 viruses with mutations of HAtransmembrane cysteines exhibited altered virologicalcharacteristics
Jianqiang Zhou • Shun Xu • Jun Ma •
Wen Lei • Kang Liu • Qiliang Liu • Yida Ren •
Chunyi Xue • Yongchang Cao
Received: 2 September 2013 / Accepted: 6 November 2013
� Springer Science+Business Media New York 2013
Abstract Influenza A H3N2 virus as the cause of 1968
pandemic has since been circulating in human and swine.
Our earlier study has shown that mutations of one or two
cysteines in the transmembrane domain of H3 hemagglu-
tinin (HA) affected the thermal stability and fusion activity
of recombinant HA proteins. Here, we report the successful
generation of three recombinant H3N2 mutant viruses
(C540S, C544L, and 2C/SL) with mutations of one or two
transmembrane cysteines of HA in the background of
A/swine/Guangdong/01/98 [H3N2] using reverse genetics,
indicating that the mutated cysteines were not essential for
virus assembly and growth. Further characterization
revealed that recombinant H3N2 mutant viruses exhibited
larger plaque sizes, increased growth rate in cells,
enhanced fusion activity, reduced thermal and acidic
resistances, and increased virulence in embryonated eggs.
These results demonstrated that the transmembrane cyste-
ines (C540 and C544) in H3 HA have profound effects on
the virological features of H3N2 viruses.
Keywords Influenza virus � Hemagglutinin �Transmembrane domain � Cysteine � Reverse genetics
Introduction
In the twentieth century, there were three influenza pan-
demics caused by influenza A viruses, including the 1918
H1N1 virus, the 1957 H2N2 virus, and the 1968 H3N2
virus [1–3]. Since 1968, H3N2 virus has caused the global
persistence of influenza virus circulating in human and
swine population [4–6]. Influenza A viruses contain eight
segments of single-stranded, negative-sense RNA that
encode for more than 11 proteins [7, 8] including hemag-
glutinin (HA). The HA gene is a genetic determinant of
pathogenicity, whose introduction and adaptation from an
animal host to humans contributed to these pandemics.
HA is a spike glycoprotein present on the viral mem-
brane and recognized as the major surface antigen. HA
initiates viral infection by binding to sialylated cell surface
receptors, undergoes endocytosis, and mediates the fusion
of the viral and endosomal membranes, allowing viral
RNAs to enter the cytoplasm [9, 10]. HA is present as a
homotrimer, and each monomer contains a long ectodo-
main, a transmembrane (TM) domain, and a short cyto-
plasmic domain. HA monomer is synthesized as a single
polypeptide, HA0, and cleaved into the disulfide-linked
polypeptides, HA1 and HA2 [11–13].
Previous studies have indicated that HA TM domain
plays roles in viral entry, HA-mediated membrane fusion,
and HA apical sorting [14, 15]. When HA TM domain was
substituted with a glycosylphosphatidylinositol (GPI)
anchor, the expressed GPI-anchored HA in cells could
support only hemifusion to target membranes at low pH
[15, 16], implying a role for the TM domain in transi-
tioning membrane hemifusion to full fusion. When the TM
domain was replaced by the TM domain of the fusogenic
glycoprotein F of Sendai virus, the fusion activity of the
chimeric protein was not altered [17]. On the other hand, a
Electronic supplementary material The online version of thisarticle (doi:10.1007/s11262-013-1011-2) contains supplementarymaterial, which is available to authorized users.
J. Zhou � S. Xu � J. Ma � W. Lei � K. Liu � Q. Liu � Y. Ren �C. Xue � Y. Cao (&)
State Key Laboratory of Biocontrol, Life Sciences School,
Guangzhou Higher Education Mega Center, Sun Yat-sen
University, Guangzhou 510006, People’s Republic of China
e-mail: [email protected]
123
Virus Genes
DOI 10.1007/s11262-013-1011-2
mutational study demonstrated a stringent TM domain
length requirement for supporting full membrane fusion
[18], strongly suggesting that the TM domain needed to
span both inner and outer leaflets to fulfill its function. In
addition, it has been found that the residues within HA TM
domain are important for raft association as sequence
substitutions in the TM domain ablated HA association
with rafts (nonraft HA) [19].
HA protein of H3N2 virus among 16 subtypes of
influenza A viruses is the only one containing two cysteine
residues (C540 and C544) in its TM domain [20–22]. Our
earlier study has shown that mutations of one or two of
these two cysteines affected the thermal stability and fusion
activity of recombinant H3 HA proteins [20]. The enticing
and necessary question was what effects of the incorpora-
tion of these recombinant mutant HAs would be on the
recombinant H3N2 viruses. In this study, we generated
three recombinant H3N2 mutant viruses (wildtype, C540S,
C544L, and 2C/SL) carrying mutations of one or two TM
cysteines (C540 and C544) in the HA TM domain and one
wildtype (WT) recombinant H3N2 virus in the background
of A/swine/Guangdong/01/98 [H3N2] using reverse
genetics. The results showed that the mutations affected
various characteristics of the recombinant H3N2 viruses
including growth rate, fusion activity, thermal and acidic
resistances, and infectivity and virulence in embryonated
eggs.
Materials and methods
Cells and viruses
Human embryonic kidney cells (293T) and MDCK cells
were cultured in Dulbecco’s modified Eagle’s medium
(DMEM; Invitrogen) supplemented with 10 % fetal bovine
serum (FBS; Invitrogen), GlutaMAX (200 mM; Invitro-
gen), penicillin (100 units/ml), and streptomycin (100 lg/ml)
in an atmosphere of 5 % CO2 at 37 �C.
The H3N2 strain (A/swine/Guangdong/01/98 [H3N2])
was isolated in Guangdong province, China in 1998; the
nucleotide sequences are available from GenBank under
accession numbers FJ830852.1–FJ830859.1.
The handling of experiments with live viruses was
conducted in a biosafety 2 plus facility under the guidelines
issued by China authority.
Plasmids and constructs
The eight genome-sense (pHH21) plasmids (a gift from Y.
Kawaoka, University of Wisconsin-Madison) and four
protein-expressing (pcDNA3.0) plasmids used to generate
influenza virus by reverse genetics have been described
previously [23–25]. For rescue of recombinant H3N2
viruses, eight genome-sense plasmids together with
expression plasmids encoding the RNP complex (pcDNA–
PB1, pcDNA–PB2, pcDNA–PA, and pcDNA–NP) were
transfected into 293T cells using Lipofectamine2000
(Invitrogen). The transfected cell culture supernatant was
collected at 48–60 h post-transfection and used to passage
onto MDCK cells or 10-days-old embryonated chicken
eggs for the propagation of the recombinant viruses. Virus
production was monitored by hemagglutination titer.
To generate pHH21 encoding the mutant HAs (C540S,
C544L, and 2C/SL), the pHH21 vector encoding WT HA
was subjected to site-directed mutagenesis using the
Stratagene Quick-Change mutagenesis kit (Stratagene, La
Jolla, CA, USA). Primers used in the generation of these
constructs were as follows: 50GATTTCCTTTGCCAT AT
CAAGCTTTTTGCTTTGTGTTG30 [forward (fo)] and
50CAACACAAAGCAA AAAGCTTGATATGGCAAAG
GAAATC30 [reverse (re)] for exchange of cysteine at
position 540; 50CATATCATGCTTTTTGCTTCTTGTTG
TTTTGCTGGGGTTC30 (fo) and 50GAACCCCAGCAAA
ACAACAAGAAGCAAAAAGCATGATATG30 (re) for
exchange of cysteine at position 544; 50CATATCAAGCT
TTTTGCTTCTTGTT GTTTTGCTGGGGTTC30 (fo) and
50GAACCCCAGCAAAACAACAAGAAGCA AAAAGC
TTGATATG30 (re) for exchange of cysteines at position
540 and 544 (the mutation sites are indicated by the
underlined characters).
The recombinant mutant viruses were generated as
described above and the entire genome of the recombinant
viruses was confirmed by sequencing.
Virus growth and plaque assay
MDCK cells were grown in 24-well plates and inoculated
in triplicate with viruses at a multiplicity of infection
(MOI) of 0.001 per well in phosphate-buffered saline
(PBS) containing 0.2 % BSA for 1 h. Unbound viruses
were washed away, and 0.5 ml serum-free medium con-
taining 0.2 % BSA and 2 lg/ml TPCK-trypsin was added
to each well. The supernatants were collected every 12 h
until 72 h post-infection. The viral titers in the supernatants
were determined by plaque assay on MDCK cells.
For plaque assays, MDCK cells in 6-well plates were
infected with serial tenfold dilutions of the recovered
viruses for 1 h at 37 �C. After washing, the media in the
dish were then replaced with MEM-1 % agarose containing
2 lg/ml of trypsin. Plaques were formed by incubation for
3 days at 37 �C. Cells were stained with 0.01 % neutral red
and the formed plaques were photographed.
Virus Genes
123
Virus purification, immunoblotting, and electron
microscopy
The WT and mutant viruses were propagated in embryonated
eggs and purified by centrifugation on 20–60 % sucrose
density gradients [26]. Purified virions were boiled for 5 min
at 100 �C in the loading buffer (50 mM Tris, 100 mM
dithiothreitol, 2 % SDS, 0.1 % bromophenol blue, and 10 %
glycerol). And viral proteins were separated by 10 % SDS
polyacrylamide gel electrophoresis. After that proteins were
transferred to polyvinylidene fluoride membrane (Millipore,
Billerica, MA). Membranes were blocked in 3 % BSA and
then incubated with mouse sera against virus A/swine/GD/
01/98 (1:3,000) for 2 h, followed by incubation with horse-
radish peroxidase-conjugated secondary antibody for 1 h.
Proteins were detected with the commercial ECL kit
(Pierce). The intensity of each band was quantified using
GeneTools software (SynGene).
The procedure of the negative staining of purified viri-
ons was done as described [27]. In brief, purified recom-
binant viruses were attached onto parlodion-coated nickel
grids for 2 min. And the virions were stained by the
phosphotungstic acid buffer for 2 min. The shape of the
viruses was photographed by the JEOL JEM-100 CX-II
electron microscope.
Virus resistance assays
In the thermal resistance assay, the viruses with the same HA
titers were incubated at a temperature ranging from 48 to
60 �C for 30 min in a Peltier Gradient Thermal Cycler (Bio-
Rad, Richmond, CA); then the HA titers were measured. In
the acidic resistance assay, the viruses with the same PFUs
were incubated in an acidic buffer (10 mM HEPES, 10 mM
MES in PBS) at pH 7.4, 5.2, or 5.0 at 37 �C for 30 min; then
the solutions were adjusted to pH 7.0; then MDCK cells were
infected with the recombinant viruses in 24-well plates at a
MOI of 2; mock-infected wells were negative controls. After
30 min of adsorption at 37 �C, cells were washed three times
with PBS and replaced with the serum-free medium con-
taining 2 lg/ml TPCK-trypsin. The infected plates were
fixed with 4 % paraformaldehyde at 5 h post-infection for
15 min at room temperature and permeabilized with 0.2 %
Triton X-100 in PBS for 15 min followed by staining using
the FITC-labeled mAb against NP (Abcam, Cambridge,
UK). Images were observed under the Zeiss Observer Z1
inverted fluorescence microscope.
Virus–cell fusion assay
The virus–cell fusion assay has been described [28]. In
brief, the WT and mutant viruses were standardized to HA
256 units and incubated with chicken red blood cells
(RBC) (2 % RBC concentration) on ice for 10 min. Then
the pH was lowered from 5.8 to 4.6 by addition of the
sodium citrate buffer. After incubation at room temperature
for 30 min, the chicken RBC were removed by centrifu-
gation (3,000 rpm for 3 min) and supernatants were
transferred to an ELISA plate for determination of NADPH
content by optical density measurement (340 nm) with a
Bio-Tek (Bio-Tek Instruments, Inc., Winooski, VT, USA)
ELISA plate reader. NADPH was present in the superna-
tant as a function of fusion-induced red blood cell lysis.
Baseline NADPH activity values were derived from sam-
ples without viruses that underwent identical treatment.
Characterization of recombinant viruses
in embryonated chicken eggs
According to the standard protocol [29], 9 or 10-days-old
specific-pathogen-free (SPF) embryonated eggs were
inoculated with a series of tenfold dilution of recombinant
virus stocks, respectively. All recombinant virus stocks had
a titer of 5 9 106 pfu per ml. The dilutions of 100, 10-1,
10-2, 10-3, and 10-4 for assaying 50 % egg lethal doses
(ELD50). And the samples of every dilution were tested for
the infection rate and mortality in the following 5 days.
Values of ELD50 were calculated by the Reed–Muench
method [30].
HA receptor-binding assay in MDCK cells
As previously described [31, 32], HA receptor-binding
affinity of recombinant viruses was determined using
MDCK cells. MDCK cells in 24-well plates were inoculated
with the four recombinant viruses at a MOI of 1.0 for 30 min.
The infected cells were washed three times with PBS and
incubated at 33 �C for 6 h with the medium containing
1 lg/ml TPCK-trypsin. The inoculated plates were then
fixed with 1 % paraformaldehyde, permeabilized with 0.2 %
Triton X-100 in PBS, and stained with anti-NP monoclonal
antibodies. The cell images were captured by the Zeiss Observer
Z1 inverted fluorescence microscope and the percentage of
infected cells was analyzed by the Image-Pro Plus software
(Media Cybernetics, Silver Springs, MD, USA).
Ethics statement
The viruses propagation studies in embryonated eggs were
approved by the Institutional Animal Care and Use Com-
mittee of Sun Yat-sen University and the Institutional
Animal Ethics Committee of Sun Yat-sen University
(Permit Number: IACUC-2012-0701). Research was con-
ducted in compliance with guidelines of the Ordinance on
Laboratory Animals Management set by the State Scien-
tific and Technological Commission of China.
Virus Genes
123
Statistical analysis
Data are presented as mean ± SEM from at least three
independent experiments. All statistical analysis was done
using OriginPro 8 SR3 (Origin Lab Corp.). The differences
between groups were determined by the Student’s t test with
two-tailed t test when only two groups were compared. When
more than two groups were compared, they were analyzed by
one-way analysis of variance (ANOVA). Differences were
considered statistically significant at P \ 0.05.
Results
Generation of recombinant WT and mutant influenza
H3N2 viruses (C540S, C544L, and 2C/SL)
Our earlier study has demonstrated that the two cysteines
(C540 and C544) in H3 HA TM domain affected the
thermal stability and fusion activity of H3 HA proteins
[20]. Since serine (S) at position 540 and leucine (L) at
position 544 are common in most of the subtypes including
H1, H5, and H9, the two cysteines (C540 and C544) in the
H3 HA TM were mutated into serine or leucine individu-
ally (C540S and C544L) or in combination (2C/SL)
(Fig. 1). The eight genomic segments from A/swine/
Guangdong/01/98 (H3N2) were cloned and the HA was
mutated using site-directed mutagenesis. To facilitate the
recovery of mutant viruses, we used a well-characterized
reverse genetics system in which 293T cells and MDCK
cells were co-cultured and transfected with eight genome-
encoding plasmids and four protein (PB1, PB2, PA, and
NP)-expressing plasmids [24, 33]. The authenticity of the
recombinant viruses was confirmed by sequencing all
genome segments (data not shown). The generated
recombinant viruses showed the typical phenotype of
influenza viruses with surface spikes under electron
microscope (Fig. 2a). As showed in Fig. 2c, the recombi-
nant viruses produced the plaques with different sizes; the
cysteines mutant viruses formed larger plaques than the
WT virus, especially the C540S and 2C/SL mutants. The
results taken together indicated that the mutations
introduced into the TM domain did not impede the
assembly and propagation of recombinant H3N2 viruses.
Cysteine mutations did not significantly alter the viral
protein compositions of virions
The four recombinant H3N2 viruses (WT, C540S, C544L,
and 2C/SL) were propagated in embryonated eggs and
purified. The viral proteins of all four purified virions were
separated on reduced SDS-PAGE gel, and the separated
proteins were blotted by the sera from whole inactivated
H3N2 virus-immunized mice (Fig. 2b). The results showed
that HA1, HA2, NP, and M1 proteins were present and
their individual expression levels were comparable in all
four recombinant viruses (Fig. S1), demonstrating that the
mutations of cysteines in H3 HA TM did not significantly
alter the viral protein compositions of the virions.
Recombinant mutant viruses (C540S, C544L,
and 2C/SL) had increased growth rate
We next analyzed the growth rate of four recombinant
viruses by infecting MDCK cells with viruses at a low
multiplicity of infection (MOI of 0.001) and measured the
titers of plaque-forming units (pfu) at 0, 12, 24, 36, 48, 60,
and 72 h after infection. The results showed that the pfu
titers of all three recombinant mutant viruses were higher
than that of the recombinant WT virus (Fig. 3). In partic-
ular, the pfu titers of C540S, C544L, and 2C/SL mutant
viruses at 48 h were significantly higher than that of WT
virus (P \ 0.05), while the pfu titer of C544L mutant virus
at 48 h was lower than that of C540S and 2C/SL mutant
viruses but higher than that of WT virus (about twofold
increase) at the 48 h post-infection. In summary, C540S,
C544L, and 2C/SL recombinant viruses showed increased
growth rates in MDCK cells.
Recombinant mutant viruses showed increased fusion
activity
We next investigated the fusion activities of all four
recombinant viruses using virus-induced erythrocyte
Fig. 1 Schematic diagram of
WT and mutant HAs. The
nomenclature of the
recombinant viruses is shown
on the left
Virus Genes
123
hemolysis assay [28]. When all four recombinant viruses
were subjected to the virus-induced erythrocyte hemolysis
assay at a pH range of 4.6, 4.8, 5.0, 5.2, 5.4, 5.6 and 5.8, the
mutant viruses (C540S, C544L, and 2C/SL) showed sig-
nificant higher fusion activity than that of WT virus in the
pH range from 4.6 to 5.0 (P \ 0.01) (Fig. 4). The data
indicated that there was no difference in the HA activation
pH between the mutants and WT virus; instead, the dif-
ference was the extent of membrane fusion. These results
were in line with our earlier study [20], validating the
usefulness of using recombinant HA proteins to study the
HA functions.
Fig. 2 Verification of the
recombinant viruses.
a Negatively stained purified
influenza virions. Images are at
980,000 (Bar 200 nm.).
b Western blot analysis of SDS-
PAGE separated viral
polypeptides. Blots were probed
with antiserum for A/swine/GD/
98. The recombinant viruses
were grown in embryonated
eggs and purified through
sucrose gradients. c Plaque
phenotypes of recombinant
viruses. MDCK cell monolayers
were inoculated with viruses
and subsequently covered with
an agarose-containing medium
overlay. After 3 days of
incubation, plaques were
visualized by staining with
neutral red
Fig. 3 Growth curves of
recombinant H3N2 viruses.
Monolayers of MDCK cells
were inoculated at a MOI of
0.001. The amount of infectious
viruses in the supernatants
harvested at the indicated times
was determined by plaque
assay. Error bars represent the
standard deviation from
triplicate experiments. *on WT
means P \ 0.05, compared with
all mutant viruses
Virus Genes
123
Recombinant mutant viruses exhibited reduced thermal
and acidic resistances
We then used the thermal resistance assay [34] to examine
the thermal resistance of recombinant viruses at the tem-
perature range of 48, 50, 52, 54, 56, 58, and 60 �C. The
temperature range was chosen after our preliminary studies
showed that all four recombinant viruses had similar
thermal resistance below 50 �C and retained no HA titers
over 60 �C. All four recombinant viruses with the same HA
titers were incubated at the designated temperatures for
30 min, and their HA titers were measured after cooling to
room temperature. The results showed that all four
recombinant viruses started to lose their HA titers from
50 �C, and gradually to completely lose their HA titers at
60 �C (Fig. 5). More importantly, the three recombinant
mutant viruses (C540S, C544L, and 2C/SL) lost signifi-
cantly more HA titers than the WT recombinant virus at 56
and 58 �C (P \ 0.05), indicating that the recombinant
mutant viruses had reduced thermal resistances (Fig. 5).
We also examined whether the treatment with acidic
solutions prior to infections would affect the infectivity of
the recombinant viruses. All four recombinant viruses with
the same PFUs were treated with a buffer of pH 5.0, 5.2,
and 7.4 at 37 �C for 30 min; and then their infectivity was
tested by infecting MDCK cells. In the pH range tested, pH
5.0 distinguished the WT recombinant virus from all three
recombinant mutant viruses, where only the WT recom-
binant virus retained partial infectivity while all other three
completely lost their infectivity (Fig. 6).
In summary, the mutations of either one or both of the
two TM cysteines rendered the recombinant mutant viruses
with reduced thermal and acidic resistances.
All recombinant viruses shared similar receptor-binding
affinity
We then investigated whether the mutations of the TM
cysteines would affect the receptor-binding affinity of the
recombinant viruses. For assaying the receptor-binding
Fig. 4 Fusion activities of
recombinant H3N2 viruses.
Fusion activity was measured
by the red blood cell fusion
assay. Viruses standardized to
256 HA units were mixed with
2 % chicken red blood cells and
then the buffer was replaced
with the acidic buffer which
varied between 4.6 and 5.8. The
hemolysis representing the
fusion activity was expressed as
the optical density at 340 nm
(OD340) minus the baseline
NADPH value obtained from no
virus treatment condition. Error
bars represent the standard
deviation from triplicate
experiments. At pH 4.6, 4.8, 5.0,
**P \ 0.01, compared with all
mutant viruses
Fig. 5 Thermal resistance of recombinant H3N2 viruses. For four
recombinant viruses, the preparations which had originally 256 HA
units were incubated at indicated temperatures for 30 min in the
thermal cycler. And their HA titers were measured by hemaggluti-
nation. *P \ 0.05, compared with all mutant viruses
Virus Genes
123
affinity, MDCK cells were infected at an MOI of 1.0 with
viruses and immuno-stained with anti-NP monoclonal
antibodies after 6 h [31, 32]. The receptor-binding affini-
ties were presented by the percentage of the infected cells.
The results showed that all four recombinant viruses had
similar receptor-binding affinities (Fig. 7).
Recombinant mutant viruses manifested higher ELD50
titers than recombinant WT virus
We next examined whether the cysteine mutations affected
the pathogenicity of recombinant mutant viruses. The
mouse model has been widely used for assaying the path-
ogenicity of influenza A viruses. However, our preliminary
studies showed that the H3N2 strain used in our study was
poor in infecting mice and the mutants viruses we
constructed cannot also infect mice; thus we examined the
pathogenicity of recombinant viruses in SPF embryonated
chicken eggs by ELD50 assays [35]. The WT, C540S,
C544L, and 2C/SL viruses had the mean titers of ELD50
-1.5, -3, -2.33, and -2.5, respectively (Table 1). The
results showed that all recombinant mutant viruses (C540S,
C544L, and 2C/SL) exhibited enhanced virulence, indi-
cating that the two cysteines in the TM domain are
involved in regulating the virulence of H3N2 influenza
viruses.
Discussion
This study attempted to investigate the relationship of H3
HA TM domain structure and the biological functions of
Fig. 6 Acidic resistance of
recombinant H3N2 viruses.
Virus samples were incubated
with MES buffer at indicated
pH values for 30 min. And then
samples were returned to neutral
pH (7.4) prior to infection at
MOI = 2. The cells were
processed for
immunofluorescence staining
after 5 h of incubation at 37 �C
Fig. 7 HA receptor-binding affinity of recombinant viruses. The
recombinant viruses were adsorbed to MDCK cells at a MOI of 1.0
for 30 min, washed three times with PBS. The cells were then
processed for immunofluorescence staining after 6 h of incubation at
37 �C. The percentage of infected cells (mean ± standard deviation)
indicated in each image is an average of six images
Virus Genes
123
recombinant H3N2 viruses. More specifically, we gener-
ated by reverse genetics four recombinant H3N2 viruses, of
which three contained a H3 HA with mutation of one or
two TM cysteines (C540S, C544L, and 2C/SL); all four
recombinant H3N2 viruses showed the similar viral com-
position, indicating that these two TM cysteines were not
indispensable for the assembly and propagation of H3N2
viruses. Our results showed that while all four recombinant
H3N2 viruses had similar receptor-binding affinity, the
three recombinant mutant viruses manifested different
biological characteristics than the recombinant WT virus,
including different plaque sizes, higher growth rate,
increased fusion activity, reduced thermal and acidic
resistances, and increased EID50 and ELD50 titers.
During membrane fusion, HA forms a helical structure
consisting of its TM and fusion peptide at the end of the
molecule [36]. For influenza virus HA, a TM domain with
]17 amino acids was able to efficiently promote full
fusion in all HAs [18]. Previous work indicated that addi-
tion of palmitic acid to cysteines, which are highly con-
served among the 16 HA subtypes, located in the TM
domain boundary region may regulate the membrane
fusion [37–40]. Our study for the first time provided direct
evidence showing that the TM cysteines (C540 and C544)
contributed to the regulation of fusion activity of H3N2
viruses, reaffirming previous studies on HA molecules [17,
18].
Takeda et al. [19] had studied the effects of the TM
amino acids of HA on the growth of H3N2 viruses in detail
by alanine scanning mutagenesis. They showed that HA
mutants 530–532 and 533–535 had a slower growth rate
and a titer of about 3 logs lower than WT virus [19].
Interestingly, the HA mutant 539–541 was the only one
showing higher growth rate than WT virus. This strongly
corroborated our results showing that C540S mutant virus
had the higher growth rate than WT virus (Fig. 3), because
the mutant 539–541 in Takeda et al. [19] had the C540
residue changed to alanine. In addition, the positions of the
amino acids in the TM might affect their contributions to
the growth rate. In Takeda et al. [19], different mutants had
different growth rates. Our results also supported this point
by showing that C540S and C544L mutants had different
growth rates. Furthermore, the reasons for the increased
growth rates for C540S, C544L, and 2C/SL mutant H3N2
viruses might be their increased fusion activity. A number
of previous studies reported that the elevated fusion
activity could enhance the virus growth [41–44]. In the
present study, the growth rates of the mutant H3N2 viruses
were correlated with their fusion activities (Figs. 3, 4). This
adds another support for the relationship between the virus
growth rate and their fusion activity.
Previous studies have demonstrated that the conforma-
tional changes of HA proteins might affect the thermal
resistances of influenza viruses [34, 45], and that elevated
pH for membrane fusion could change the stability of the
viruses [42, 44–46]. The results in our study showed that
the recombinant WT H3N2 viruses were more resistant to
elevated temperature exposure or acidic treatment than the
mutant viruses (Figs. 5, 6), indicating that the TM cyste-
ines might contribute to the conformational stability of H3
HA proteins in H3N2 viruses. In addition, for the para-
myxoviruses, the fusion protein activation involves cyto-
plasmic tails signaling to the ectodomain [47, 48] and TM
domain can affect ectodomain stability [49–51]. The HA
TM domain can probably modulate the membrane fusion
by the inside-out signaling. Our results provided a plausible
explanation for the previous studies showing that the TM
domain of the H3N2 strain A/X-31 exhibited a strong
potential for the stable oligomers [52, 53] and more tightly
associated within trimers [54].
The recombinant mutant H3N2 viruses exhibited
increased infectivity and virulence in the embryonated
eggs; this is to the best of our knowledge the first time a
study showing that mutations of one or two TM cysteines
in the H3 HA could increase the infectivity and virulence
of H3N2 viruses. These results should not be surprising
since these recombinant mutants H3N2 viruses have been
shown to have increased growth rate and fusion activity.
Even though we made a strong case for arguing that there is
a causal relationship between the increased infectivity and
virulence and the increased growth rate and fusion activity,
further studies are needed to establish such a relationship.
In summary, our results have demonstrated that muta-
tions of one or two cysteines in the TM domain of H3 HA
protein could alter many characteristics of recombinant
mutant H3N2 viruses including plaque size, increased
growth rate, fusion activity, reduced thermal and acidic
resistances. This study has important practical applications,
for example, the recombinant mutant H3N2 viruses with
increased growth rate could be developed to improve
H3N2 influenza vaccine production. Furthermore, it would
be interesting to know whether an insertion of the corre-
sponding TM cysteines into the TM domains of other
subtype HA proteins could decrease the infectivity and
virulence of the resultant recombinant viruses; for example,
if the infectivity and virulence of H5N1 viruses could be
reduced by such insertions in their HA proteins, it might
Table 1 Pathogenicity of recombinant H3N2 viruses in eggs
Virus Log10 ELD50
rH3N2/A/swine/GD/01/98-HA-WT -1.5
rH3N2/A/swine/GD/01/98-HA-C540S -3
rH3N2/A/swine/GD/01/98-HA-C544L -2.33
rH3N2/A/swine/GD/01/98-HA-2C/SL -2.5
Virus Genes
123
facilitate the development of vaccines against H5N1
viruses.
Acknowledgments This work was supported by grants from the
State Key Laboratory of Biocontrol at Sun Yat-sen University. We
thank George D. Liu for critical review and revision of the manuscript
and Professor A.D. Osterhaus of Erasmus University Medical Center,
Rotterdam and Professor Y. Kawaoka of University of Wisconsin-
Madison for offering the plasmids.
References
1. K. Stohr, Lancet Infect. Dis 2, 517 (2002)
2. M.R. Sandbulte, K.B. Westgeest, J. Gao, X. Xu, A.I. Klimov,
C.A. Russell, D.F. Burke, D.J. Smith, R.A. Fouchier, M.C. Ei-
chelberger, Proc. Natl. Acad. Sci. USA 108, 20748–20753 (2011)
3. J.C. Krause, T. Tsibane, T.M. Tumpey, C.J. Huffman, R. Albr-
echt, D.L. Blum, I. Ramos, A. Fernandez-Sesma, K.M. Edwards,
A. Garcia-Sastre, C.F. Basler, J.E. Crowe Jr, J. Virol. 86,
6334–6340 (2012)
4. C.A. Russell, T.C. Jones, I.G. Barr, N.J. Cox, R.J. Garten, V.
Gregory, I.D. Gust, A.W. Hampson, A.J. Hay, A.C. Hurt, J.C. de
Jong, A. Kelso, A.I. Klimov, T. Kageyama, N. Komadina, A.S.
Lapedes, Y.P. Lin, A. Mosterin, M. Obuchi, T. Odagiri, A.D.
Osterhaus, G.F. Rimmelzwaan, M.W. Shaw, E. Skepner, K.
Stohr, M. Tashiro, R.A. Fouchier, D.J. Smith, Science 320,
340–346 (2008)
5. J. Bahl, M.I. Nelson, K.H. Chan, R. Chen, D. Vijaykrishna, R.A.
Halpin, T.B. Stockwell, X. Lin, D.E. Wentworth, E. Ghedin, Y.
Guan, J.S. Peiris, S. Riley, A. Rambaut, E.C. Holmes, G.J. Smith,
Proc. Natl. Acad. Sci. USA 108, 19359–19364 (2011)
6. R.J. Garten, C.T. Davis, C.A. Russell, B. Shu, S. Lindstrom, A.
Balish, W.M. Sessions, X. Xu, E. Skepner, V. Deyde, M. Okomo-
Adhiambo, L. Gubareva, J. Barnes, C.B. Smith, S.L. Emery, M.J.
Hillman, P. Rivailler, J. Smagala, M. de Graaf, D.F. Burke, R.A.
Fouchier, C. Pappas, C.M. Alpuche-Aranda, H. Lopez-Gatell, H.
Olivera, I. Lopez, C.A. Myers, D. Faix, P.J. Blair, C. Yu, K.M.
Keene, P.D. Dotson Jr, D. Boxrud, A.R. Sambol, S.H. Abid, K. St
George, T. Bannerman, A.L. Moore, D.J. Stringer, P. Blevins,
G.J. Demmler-Harrison, M. Ginsberg, P. Kriner, S. Waterman, S.
Smole, H.F. Guevara, E.A. Belongia, P.A. Clark, S.T. Beatrice,
R. Donis, J. Katz, L. Finelli, C.B. Bridges, M. Shaw, D.B.
Jernigan, T.M. Uyeki, D.J. Smith, A.I. Klimov, N.J. Cox, Science
325, 197–201 (2009)
7. R.A. Lamb, R.M. Krug, in Fields Virology, 4th edn., ed. by D.M.
Knipe, P.M. Howley (Lippincott Williams & Wilkins, Philadel-
phia, 2001), pp. 1487–1532
8. M.L. Grantham, W.H. Wu, E.N. Lalime, M.E. Lorenzo, S.L.
Klein, A. Pekosz, J. Virol. 83, 8655–8661 (2009)
9. J.J. Skehel, D.C. Wiley, Annu. Rev. Biochem. 69, 531–569
(2000)
10. H.D. Klenk, R. Rott, Adv. Virus Res. 34, 247–281 (1988)
11. E.J. Schrauwen, T.M. Bestebroer, V.J. Munster, E. de Wit, S.
Herfst, G.F. Rimmelzwaan, A.D. Osterhaus, R.A. Fouchier, J.
Gen. Virol. 92, 1410–1415 (2011)
12. E.J. Schrauwen, S. Herfst, L.M. Leijten, P. van Run, T.M.
Bestebroer, M. Linster, R. Bodewes, J.H. Kreijtz, G.F. Rim-
melzwaan, A.D. Osterhaus, R.A. Fouchier, T. Kuiken, D. van
Riel, J. Virol. 86, 3975–3984 (2012)
13. W.H. Wu, A. Pekosz, J. Virol. 82, 1059–1063 (2008)
14. P. Scheiffele, M.G. Roth, K. Simons, EMBO J. 16, 5501–5508
(1997)
15. G.W. Kemble, T. Danieli, J.M. White, Cell 76, 383–391 (1994)
16. G.B. Melikyan, J.M. White, F.S. Cohen, J. Cell Biol. 131,
679–691 (1995)
17. B. Schroth-Diez, E. Ponimaskin, H. Reverey, M.F. Schmidt, A.
Herrmann, J. Virol. 72, 133–141 (1998)
18. R.T. Armstrong, A.S. Kushnir, J.M. White, J. Cell Biol. 151,
425–437 (2000)
19. M. Takeda, G.P. Leser, C.J. Russell, R.A. Lamb, Proc. Natl.
Acad. Sci. USA 100, 14610–14617 (2003)
20. S. Xu, J. Zhou, K. Liu, Q. Liu, C. Xue, X. Li, J. Zheng, D. Luo,
Y. Cao, Virus Genes 47, 20–26 (2013)
21. E. Nobusawa, T. Aoyama, H. Kato, Y. Suzuki, Y. Tateno, K.
Nakajima, Virology 182, 475–485 (1991)
22. R.D. Tall, M.A. Alonso, M.G. Roth, Traffic 4, 838–849 (2003)
23. G. Neumann, T. Watanabe, H. Ito, S. Watanabe, H. Goto, P. Gao,
M. Hughes, D.R. Perez, R. Donis, E. Hoffmann, G. Hobom, Y.
Kawaoka, Proc. Natl. Acad. Sci. USA 96, 9345–9350 (1999)
24. E. Fodor, L. Devenish, O.G. Engelhardt, P. Palese, G.G.
Brownlee, A. Garcia-Sastre, J. Virol. 73, 9679–9682 (1999)
25. E. Hoffmann, G. Neumann, G. Hobom, R.G. Webster, Y. Ka-
waoka, Virology 267, 310–317 (2000)
26. H. Jin, K. Subbarao, S. Bagai, G.P. Leser, B.R. Murphy, R.A.
Lamb, J. Virol. 70, 1406–1414 (1996)
27. H. Jin, G.P. Leser, J. Zhang, R.A. Lamb, EMBO J 16, 1236–1247
(1997)
28. T.T. Wang, G.S. Tan, R. Hai, N. Pica, E. Petersen, T.M. Moran,
P. Palese, PLoS Pathog. 6, e1000796 (2010)
29. D.E. Swayne, D.A. Halvorson, Influenza in Diseases of Poultry,
11th edn. (Iowa State Press, Iowa City, 2003)
30. A.K. Thakur, W.L. Fezio, Drug Chem. Toxicol. 4, 297–305
(1981)
31. B. Lu, H. Zhou, D. Ye, G. Kemble, H. Jin, J. Virol. 79,
6763–6771 (2005)
32. B. Lu, H. Zhou, W. Chan, G. Kemble, H. Jin, Vaccine 24,
6691–6693 (2006)
33. E. Hoffmann, G. Neumann, Y. Kawaoka, G. Hobom, R.G.
Webster, Proc. Natl. Acad. Sci. USA 97, 6108–6113 (2000)
34. A. Farnsworth, T.D. Cyr, C. Li, J. Wang, X. Li, Vaccine 29,
1529–1533 (2011)
35. H. Sun, P. Jiao, B. Jia, C. Xu, L. Wei, F. Shan, K. Luo, C. Xin, K.
Zhang, M. Liao, Vet. Microbiol. 152, 258–265 (2011)
36. Z.N. Li, B.J. Lee, W.A. Langley, K.C. Bradley, R.J. Russell, D.A.
Steinhauer, J. Virol. 82, 6337–6348 (2008)
37. L.V. Kordyukova, M.V. Serebryakova, L.A. Baratova, M. Veit, J.
Virol. 82, 9288–9292 (2008)
38. B.J. Chen, M. Takeda, R.A. Lamb, J. Virol. 79, 13673–13684
(2005)
39. R. Wagner, A. Herwig, N. Azzouz, H.D. Klenk, J. Virol. 79,
6449–6458 (2005)
40. T. Sakai, R. Ohuchi, M. Ohuchi, J. Virol. 76, 4603–4611 (2002)
41. S. Murakami, T. Horimoto, M. Ito, R. Takano, H. Katsura, M.
Shimojima, Y. Kawaoka, J. Virol. 86, 1405–1410 (2012)
42. M.L. Reed, H.L. Yen, R.M. DuBois, O.A. Bridges, R. Salomon,
R.G. Webster, C.J. Russell, J. Virol. 83, 3568–3580 (2009)
43. M.L. Reed, O.A. Bridges, P. Seiler, J.K. Kim, H.L. Yen, R.
Salomon, E.A. Govorkova, R.G. Webster, C.J. Russell, J. Virol.
84, 1527–1535 (2010)
44. Y.P. Lin, S.A. Wharton, J. Martin, J.J. Skehel, D.C. Wiley, D.A.
Steinhauer, Virology 233, 402–410 (1997)
45. B.M. Krenn, A. Egorov, E. Romanovskaya-Romanko, M. Wol-
schek, S. Nakowitsch, T. Ruthsatz, B. Kiefmann, A. Morokutti, J.
Humer, J. Geiler, J. Cinatl, M. Michaelis, N. Wressnigg, S.
Sturlan, B. Ferko, O.V. Batishchev, A.V. Indenbom, R. Zhu, M.
Kastner, P. Hinterdorfer, O. Kiselev, T. Muster, J. Romanova,
PLoS One 6, e18577 (2011)
Virus Genes
123
46. R.S. Daniels, J.C. Downie, A.J. Hay, M. Knossow, J.J. Skehel,
M.L. Wang, D.C. Wiley, Cell 40, 431–439 (1985)
47. D.L. Waning, C.J. Russell, T.S. Jardetzky, R.A. Lamb, Proc.
Natl. Acad. Sci. USA 101, 9217–9222 (2004)
48. D.L. Waning, A.P. Schmitt, G.P. Leser, R.A. Lamb, J. Virol. 76,
9284–9297 (2002)
49. S. Seth, A.L. Goodman, R.W. Compans, J. Virol. 78, 8513–8523
(2004)
50. M. Li, Z.N. Li, Q. Yao, C. Yang, D.A. Steinhauer, R.W. Com-
pans, J. Virol. 80, 6106–6114 (2006)
51. M.L. Bissonnette, J.E. Donald, W.F. DeGrado, T.S. Jardetzky,
R.A. Lamb, J. Mol. Biol. 386, 14–36 (2009)
52. S.A. Tatulian, L.K. Tamm, Biochemistry 39, 496–507 (2000)
53. L. Godley, J. Pfeifer, D. Steinhauer, B. Ely, G. Shaw, R. Kauf-
mann, E. Suchanek, C. Pabo, J.J. Skehel, D.C. Wiley et al., Cell
68, 635–645 (1992)
54. L.V. Kordyukova, M.V. Serebryakova, A.A. Polyansky, E.A.
Kropotkina, A.V. Alexeevski, M. Veit, R.G. Efremov, I.Y. Fi-
lippova, L.A. Baratova, Biochim. Biophys. Acta 1808,
1843–1854 (2011)
Virus Genes
123