Search tips
Search criteria 


Logo of jvirolPermissionsJournals.ASM.orgJournalJV ArticleJournal InfoAuthorsReviewers
J Virol. 2010 September; 84(17): 8607–8616.
Published online 2010 June 30. doi:  10.1128/JVI.00159-10
PMCID: PMC2918990

Adaptation of Pandemic H1N1 Influenza Viruses in Mice[down-pointing small open triangle]


The molecular mechanism by which pandemic 2009 influenza A viruses were able to sufficiently adapt to humans is largely unknown. Subsequent human infections with novel H1N1 influenza viruses prompted an investigation of the molecular determinants of the host range and pathogenicity of pandemic influenza viruses in mammals. To address this problem, we assessed the genetic basis for increased virulence of A/CA/04/09 (H1N1) and A/TN/1-560/09 (H1N1) isolates, which are not lethal for mice, in a new mammalian host by promoting their mouse adaptation. The resulting mouse lung-adapted variants showed significantly enhanced growth characteristics in eggs, extended extrapulmonary tissue tropism, and pathogenicity in mice. All mouse-adapted viruses except A/TN/1-560/09-MA2 grew faster and to higher titers in cells than the original strains. We found that 10 amino acid changes in the ribonucleoprotein (RNP) complex (PB2 E158G/A, PA L295P, NP D101G, and NP H289Y) and hemagglutinin (HA) glycoprotein (K119N, G155E, S183P, R221K, and D222G) controlled enhanced mouse virulence of pandemic isolates. HA mutations acquired during adaptation affected viral receptor specificity by enhancing binding to α2,3 together with decreasing binding to α2,6 sialyl receptors. PB2 E158G/A and PA L295P amino acid substitutions were responsible for the significant enhancement of transcription and replication activity of the mouse-adapted H1N1 variants. Taken together, our findings suggest that changes optimizing receptor specificity and interaction of viral polymerase components with host cellular factors are the major mechanisms that contribute to the optimal competitive advantage of pandemic influenza viruses in mice. These modulators of virulence, therefore, may have been the driving components of early evolution, which paved the way for novel 2009 viruses in mammals.

In early April 2009, a new H1N1 influenza virus with a previously uncharacterized constellation of eight genes (10) was first detected in humans (5). Since then, this newly emerged influenza virus has spread worldwide to 214 countries (more than 503,536 cases [51]) by human-to-human transmission and prompted the World Health Organization to raise the worldwide pandemic alert to phase 6 (52). Sequence analysis of pandemic 2009 isolates revealed the absence of markers associated with high pathogenicity in avian and mammalian species, such as a multibasic hemagglutinin (HA) cleavage site (49) or lysine at position 627 of the PB2 protein (39, 44). Thus, the molecular mechanism by which pandemic 2009 influenza A viruses were able to sufficiently adapt to humans remains unknown. Subsequent human infections with novel H1N1 influenza viruses prompted an investigation of the genetic basis that determines pandemic influenza virus host range and pathogenicity in mammals.

Mice have been shown to be a good mammalian model for studying influenza virus pathogenicity and host range restriction mechanisms (48). Mice are not naturally infected with human or other strains of influenza virus, but most strains can be experimentally adapted for mouse virulence by serial lung-to-lung passages (15, 34). It is assumed that mouse adaptation results in the acquisition of functions that are critical determinants of virulence. Mouse-adapted influenza virus mutants usually induce pathology in the bronchi or lungs of infected animals (15, 34, 54). Such mutants possess an increased ability to infect alveolar cells, thereby initiating alveolitis, and can cause lethal pneumonitis (34, 54). In addition, all epithelial cells of the bronchi and alveoli are susceptible to infection with fully adapted strains (14, 26). The lung pathology induced by the mouse-adapted viruses shows considerable similarities to that of human influenzal pneumonia (45); thus, the changes that occur in the virus during mouse adaptation may provide insight into factors that affect the development of lung infection in humans.

Several factors that affect influenza virus host range and virulence in mice have been identified. Influenza virus hemagglutinin (HA) is a primary determinant for mouse lung virulence (2, 11, 12, 23, 41, 42). However, seven other genes have also been implicated (3, 4, 21-23, 25, 30, 37, 40, 42, 43, 53-55). For example, studies of the mouse lung-adapted A/FM/1/47 (H1N1) influenza virus revealed that, in addition to the HA protein, the M gene has the capacity to control virus virulence and growth (42). The polymerase basic 2 (PB2) protein is another influenza virus subunit that has been shown to modulate virus virulence and host range in mice (8, 25, 39, 40, 44). PB1, recently identified PB1-F2, and polymerase acidic (PA) proteins have also been implicated in mouse lung virulence but have shown no evidence of having acquired mutations during adaptation (4, 7, 23, 37, 43, 46, 53, 55). Other studies have suggested that nonstructural 1 (NS1) protein function is essential for avoidance of an innate cellular immune response against the virus and may be crucial for influenza virus pathogenicity (21, 22).

Although most studies conducted to date have focused on H1, H2, H3, H5, H7, and H9 HA subtypes of influenza viruses, no mouse adaptation experiments on pandemic 2009 H1N1 isolates have yet been reported. We, therefore, investigated the adaptation of two pandemic isolates, A/CA/04/09 (H1N1) and A/TN/1-560/09 (H1N1), which are not lethal for mice, to a new mammalian host. We used wild-type and mouse-adapted variants to identify molecular determinants of this host adaptation and enhanced virulence in mammals. Our findings suggest that multiple sequence changes within HA and the ribonucleoprotein (RNP) complex of pandemic 2009 influenza A viruses contribute to their adaptation and increased virulence in mice.


Viruses and cells.

The pandemic H1N1 influenza viruses A/CA/04/09 and A/TN/1-560/09 were obtained from the World Health Organization collaborating laboratories. Stock viruses were grown in the allantoic cavities of 10-day-old chicken eggs for 48 h at 37°C, and aliquots were stored at −70°C until used. In vitro experiments with pandemic H1N1 influenza viruses were conducted in a biosafety level 2+ containment facility approved by the U.S. Department of Agriculture.

Madin-Darby canine kidney (MDCK) and human embryonic kidney (293T) cells were obtained from the American Type Culture Collection (Manassas, VA) and maintained as previously described (19).

Adaptation of H1N1 influenza viruses in mice.

Four mouse-adapted variants of A/CA/04/09 (H1N1) and A/TN/1-560/09 (H1N1) viruses, A/CA/04/09-MA1, A/CA/04/09-MA2, A/TN/1-560/09-MA1, and A/TN/1-560/09-MA2 (MA for mouse adapted), were derived in 2 parallel, independent series of sequential lung-to-lung passages, as described previously (2). Briefly, female 6-week-old BALB/c mice (Jackson Laboratories, Bar Harbor, ME) were inoculated intranasally under light isoflurane anesthesia with 50 μl of allantoic fluid containing wild-type H1N1 virus. Lungs were harvested after 2 days and homogenized, and 50 μl of the centrifuged homogenate was used as the inoculum for the next passage. After a total of 9 passages, virus present in the lung homogenate was cloned once by plaque purification in MDCK cells, and the cloned virus was passaged once in the allantoic cavities of 10-day-old chicken eggs for 48 h at 37°C to prepare a virus stock. All animal use was conducted under applicable laws and guidelines, with prior approval of the St. Jude Children's Research Hospital Animal Care and Use Committee.

Infectivity of H1N1 influenza viruses.

The infectivity of wild-type and mouse-adapted H1N1 viruses in MDCK cells was determined by plaque assay and expressed as log10 PFU per milliliter (13). Briefly, confluent MDCK cells were incubated at 37°C for 1 h with 10-fold serial dilutions of virus. The cells were then washed and overlaid with minimal essential medium (MEM) containing 0.3% bovine serum albumin (BSA), 0.9% Bacto agar, and 1 μg/ml l-[tosylamido-2-phenyl]ethylchloromethylketone (TPCK)-treated trypsin. After 3 days of incubation at 37°C, cells were stained with 0.1% crystal violet in 10% formaldehyde solution, and the PFU per milliliter and plaque size were determined using the Finescale comparator (Los Angeles, CA).

The 50% egg infectious dose (EID50) in 10-day-old chicken eggs was determined with 10-fold serial dilutions of virus, incubated for 48 h at 37°C, and calculated by the Reed-Muench method (35).

Replication kinetics.

To determine multistep growth curves, MDCK cells were infected with wild-type and mouse-adapted H1N1 viruses at a multiplicity of infection (MOI) of 0.005 PFU/cell. After incubation, the cells were washed and overlaid with infection medium (MEM with 0.3% BSA and 1 μg/ml TPCK-treated trypsin). Supernatants were collected 12, 24, 36, 48, 60, and 72 h after infection and stored at −70°C for titration by 50% tissue culture infectious dose (TCID50) assay (19).

Pathogenicity and lethality in BALB/c mice.

To determine the 50% mouse lethal dose (MLD50), we anesthetized groups of five female 6-week-old BALB/c mice (Jackson Laboratories, Bar Harbor, ME) with isoflurane and intranasally inoculated them with 50 μl of 10-fold serial dilutions of H1N1 influenza viruses in phosphate-buffered saline (PBS). The MLD50 values were calculated by the Reed-Muench method (35) after a 21-day observation period and expressed in PFU. To monitor survival, we inoculated groups of 13 mice with H1N1 viruses (5,000 PFU/mouse). Animals that showed signs of severe disease and weight loss of >25% were humanely killed. To evaluate the replication kinetics and pathogenicity of H1N1 viruses in vivo, we euthanized three mice on day 3 after inoculation and removed the lungs, brain, spleen, and blood, and the organs were homogenized and suspended in 1 ml of PBS. Virus titers in each of the organ and blood samples were determined by inoculating chicken eggs with serial dilutions of the suspensions. Titers were calculated by the method of Reed and Muench and expressed as mean log10 EID50/ml ± standard deviation (SD). The limit of virus detection was 0.75 log10 EID50/ml. For calculation of the mean, samples with a virus titer of <0.75 log10 EID50/ml were assigned a value of 0.

Assessment of virus pathogenicity in ferrets.

Pathogenicity was tested in 4- to 5-month-old male and female ferrets obtained from Marshall Farms (North Rose, NY). All ferrets were seronegative for influenza A H1N1, H3N2, and H5N1 and influenza B viruses. Groups of three ferrets were inoculated intranasally under light isoflurane anesthesia with 106 EID50 (105.0 to 105.9 PFU/ferret) of H1N1 virus in 1 ml of PBS. Clinical signs of infection, relative inactivity index (36), weight, and temperature were recorded daily. Activity level was assessed by using the following scoring system: 0, alert and playful; 1, alert and playful when stimulated; 2, alert but not playful when stimulated; and 3, neither alert nor playful when stimulated. Body temperature was measured by subcutaneous implantable temperature transponders (Bio Medic Data Systems, Inc.). To monitor virus shedding, nasal washes were collected from ferrets at 3, 5, and 7 days postinoculation (dpi). Virus was titrated in eggs by injecting 0.1 ml of 10-fold serial dilutions of the sample (three eggs per dilution) and expressed as mean log10 EID50/ml ± SD.

RNA isolation, PCR amplification, and sequencing.

Viral RNA was isolated from virus-containing allantoic fluid by using an RNeasy Mini kit (Qiagen, Germantown, MD) according to the manufacturer's protocol. Reverse transcription of viral RNA and subsequent PCR were performed using primers specific for each gene segment, as described previously (17). PCR products were purified with a QIAquick PCR purification kit (Qiagen) according to the manufacturer's protocol. Sequencing was performed by the Hartwell Center for Bioinformatics and Biotechnology at St. Jude Children's Research Hospital. The DNA template was sequenced by using rhodamine or dRhodamine dye terminator cycle sequencing Ready Reaction kits with AmpliTaqDNA polymerase FS (PerkinElmer Applied Biosystems, Waltham, MA) and synthetic oligonucleotides. Samples were analyzed using a PerkinElmer (model 373 or model 377) DNA sequencer. DNA sequences were completed and edited using the Lasergene sequence analysis software package (DNASTAR, Madison, WI).

Hemagglutination inhibition test.

A hemagglutination inhibition (HI) test was performed with 0.5% chicken red blood cells by a standard method (33). We used a panel of 4 monoclonal antibodies (MAbs) to HA of 2 H1 strains: 2 antibodies to A/Swine/AR/2976/02 (H1N2), MAbs H5 and G7, and 2 antibodies to A/Swine/NC/18161/02 (H1N1), MAbs E2 and H7.

Receptor-binding assay.

The binding of wild-type and mouse-adapted H1N1 influenza viruses to fetuin (containing α2,3- and α2,6-linked sialyl receptors) was measured in a direct solid-phase assay using the immobilized virus and horseradish peroxidase-conjugated fetuin, as described previously (9). The affinity of viruses for synthetic 3′- and 6′-sialylglycopolymers obtained by conjugation of a 1-N-glycyl derivative of 3′-sialyllactose (3′SL, “avian-like” α2,3-containing receptor) or 3-aminopropylglycoside of 6′-sialyllactosamine (6′SLN, “human-like” α2,6-containing receptor) with poly(4-phenylacrylate) (1) was measured in a competitive assay based on the inhibition of binding to peroxidase-labeled fetuin (28). Association constant (Kass) values were determined as the sialic acid (Neu5Ac) concentration at the point Amax/2 on Scatchard plots.

Minigenome assay for polymerase activity.

Subconfluent monolayers of 293T cells (7.5 × 105 cells in 35-mm dishes) were transfected with a luciferase reporter plasmid (enhanced green fluorescent protein [EGFP] open reading frame in pHW72-EGFP substituted with a firefly luciferase gene [16, 38]) and a mix of PB2, PB1, PA, and NP plasmids (wild type or mutated) in quantities of 1, 1, 1, and 2 μg, respectively. Plasmid pGL4.75[hRluc/CMV] vector, which expresses Renilla luciferase (Promega, Madison, WI), was used as an internal control for the dual luciferase assay. As a negative control, 293T cells were transfected with the same plasmids, with the exception of the NP expression plasmid. After 24 h, cell extracts were harvested and lysed, and luciferase levels were assayed with a dual luciferase assay system (Promega, Madison, WI) and a BD Monolight 3010 luminometer (BD Biosciences, San Diego, CA). Experiments were performed in triplicate.

Protein gel electrophoresis and Western blot analysis.

Subconfluent monolayers of 293T cells were transfected the same way as described for the minigenome assay (see above). After 24 h, the cells were harvested and whole-cell extracts were prepared by lysis in radioimmunoprecipitation assay (RIPA) buffer (50 mM Tris-HCl, pH 8.0, 150 mM NaCl, 1.0% Igepal, 0.5% sodium deoxycholate, and 0.1% sodium dodecyl sulfate [SDS] [Sigma-Aldrich, St. Louis, MO]) and protease inhibitors (Pierce, Rockford, IL) on ice for 20 min. Extracts were centrifuged (15,700 × g, 15 min, 4°C), and the supernatants were collected. Proteins from cell extracts were denatured by heating at 100°C for 5 min in 2× SDS-polyacrylamide gel electrophoresis (SDS-PAGE) sample buffer and were then separated by SDS-PAGE. For Western blot analysis, the proteins were transferred to a nitrocellulose membrane, which was then probed with specific primary antibodies and peroxidase-labeled secondary antibody. Equal loading of wells was confirmed by Western blotting with a mouse monoclonal primary antibody against the cellular protein β-actin. The blots were analyzed by chemiluminescence and exposed to X-ray film.

Statistical analysis.

Virus yields in vitro and in vivo, plaque size, mean days to death, weight changes of mice, virus titers in the internal organs (lungs, brain, and spleen) and blood of mice, binding to sialyl receptors, and polymerase activities of RNP complexes of wild-type and mouse-adapted H1N1 influenza viruses were compared by analysis of variance (ANOVA). The probability of survival of infected mice was estimated by the Kaplan-Meier method (47). Weight changes and nasal wash titers of ferrets inoculated with wild-type or mouse-adapted viruses were compared by an unpaired, two-tailed t test. A probability value of 0.05 was prospectively chosen to indicate that the findings were not the result of chance alone.


Adaptation of pandemic H1N1 influenza viruses in mice.

Recent studies have shown that the novel 2009 A (H1N1) human influenza viruses are almost avirulent for mice (MLD50 of ≥106 PFU for A/CA/04/09) (20, 27). To increase the virulence of pandemic H1N1 isolates in mice, we produced mouse-adapted variants of A/CA/04/09 (H1N1) and A/TN/1-560/09 (H1N1) strains (two for each virus) by serial lung-to-lung passages, beginning with intranasal inoculation of 106.2 and 105.2 EID50 of virus per mouse, respectively. Nine subsequent passages involved the inoculation of diluted lung extracts, constituting dosages of ~103 to 106 EID50/mouse (data not shown). Survival of infected animals and virus titers of lung homogenates were assayed after each passage. Wild-type A/CA/04/09 (H1N1) and A/TN/1-560/09 (H1N1) influenza viruses generated virus titers of 6.8 and 5.8 log10 EID50/ml of lung homogenates, respectively. However, after 4 to 5 passages, virus titers increased to 7.5 to 8.2 log10 EID50/ml (data not shown). After 6 to 8 passages, mice showed a continuous trend of weight loss and commenced dying at 6 or 7 dpi, indicating that virus populations of mouse-adapted variants of pandemic H1N1 isolates had acquired mutations that profoundly affect virulence.

Growth characteristics of mouse-adapted H1N1 viruses in vitro.

We studied the growth of A/CA/04/09-MA1, A/CA/04/09-MA2, A/TN/1-560/09-MA1, and A/TN/1-560/09-MA2 variants both in eggs and in MDCK cells. The mouse-adapted variants grew to significantly higher titers in eggs than their respective wild-type viruses (P < 0.05) (Table (Table1).1). Comparison of virus yields of mouse-adapted variants indicated that A/CA/04/09-MA1 and A/TN/1-560/09-MA1 grew better than their respective MA2 clones (P < 0.05). The yields of the mouse-adapted viruses in cell culture were 1.6 to 2.2 logs higher than that of their parental wild-type strains, with the exception that A/TN/1-560/09-MA2 replicated to significantly lower titers than did either A/TN/1-560/09 or A/TN/1-560/09-MA1 (P < 0.05). All H1N1 viruses formed homogeneous small plaques (diameter, 0.2 to 0.6 mm) in MDCK cells, although the A/CA/04/09-MA1 plaques were larger than the wild-type A/CA/04/09 plaques (P < 0.05) (Table (Table11).

Growth characteristics of wild-type and mouse-adapted H1N1 influenza virusesd

To further evaluate the replicative ability of the mouse-adapted H1N1 viruses, we assayed their virus yields in comparison with those of the respective wild-type strains after multiple replication cycles in MDCK cells (Fig. 1A and B). Both mouse-adapted variants A/CA/04/09-MA1 and A/CA/04/09-MA2 grew faster and to significantly higher titers than the A/CA/04/09 strain in cell culture (Fig. (Fig.1A).1A). However, we observed significant differences in growth rates between A/TN/1-560/09-MA1 and A/TN/1-560/09-MA2 variants at almost all postinfection time points (Fig. (Fig.1B).1B). The replication ability of A/TN/1-560/09-MA1 was significantly higher than that of the wild-type virus at 24, 48, 60, and 72 h after infection (>1.5 to 3 logs, P < 0.05). In contrast, the yield of A/TN/1-560/09-MA2 was only approximately 0.1 to 16% that of A/TN/1-560/09 at all time intervals except 24 h after infection, when the mouse-adapted virus reached titers comparable to those of the wild-type strain in MDCK cells (Fig. (Fig.1B).1B). Taken together, our findings showed that mouse adaptation of pandemic H1N1 influenza viruses selected variants with increased replicative fitness in eggs, MDCK cells, or both in vitro systems.

FIG. 1.
Multistep growth curves of wild-type A/CA/04/09 (H1N1) (A) and A/TN/1-560/09 (H1N1) (B) viruses and their respective mouse-adapted variants in MDCK cells. Confluent MDCK cells were infected with H1N1 viruses at an MOI of 0.005 PFU/cell. Virus yields (log ...

Pathogenicity and lethality of mouse-adapted H1N1 viruses in vivo.

Using a BALB/c mouse model, we compared the virulence of generated mouse-adapted variants with that of the original A/CA/04/09 (H1N1) and A/TN/1-560/09 (H1N1) strains. We observed that all mouse-adapted clones were significantly more virulent for mice than their respective wild-type viruses (~103- to 104-fold decrease in MLD50 values) (Table (Table2).2). Furthermore, for a given dose of virus (5,000 PFU), all mice infected with either mouse-adapted isolate exhibited clinical signs of disease, including decreased activity, huddling, hunched posture, and ruffled fur. Mice in these groups lost weight progressively, and all died between 5 and 10 dpi (Fig. 2A and B). We also observed a significant difference in time to death of mice infected with A/CA/04/09-MA1 versus A/CA/04/09-MA2 (P < 0.05). In contrast, no morbidity or mortality was observed in mice infected with either parental wild-type virus (Table (Table22 and Fig. Fig.22).

FIG. 2.
Survival of BALB/c mice infected with 5,000 PFU/mouse (each in 50 μl) of wild-type A/CA/04/09, A/CA/04/09-MA1, or A/CA/04/09-MA2 virus (A) and wild-type A/TN/1-560/09, A/TN/1-560/09-MA1, or A/TN/1-560/09-MA2 virus (B).
Pathogenicity of wild-type and mouse-adapted H1N1 influenza viruses in BALB/c micea

To determine whether the different levels of virulence of wild-type and mouse-adapted H1N1 influenza viruses were related to a difference in ability to replicate in mouse organs, groups of 3 BALB/c mice were inoculated intranasally with 5,000 PFU of either virus, and virus replication in the lungs, brains, spleens, and blood of infected animals was determined 3 dpi. Wild-type A/CA/04/09 (H1N1) and A/TN/1-560/09 (H1N1) viruses replicated efficiently in mouse lungs (~6.2 log10 EID50/ml) without prior host adaptation and did not spread to other organs tested (<0.75 log10 EID50/ml) (Table (Table2).2). These data were in good agreement with previous reports (20, 27). In contrast, all mouse-adapted H1N1 variants replicated to significantly higher titers in the lungs (up to 8.4 log10 EID50/ml, P < 0.05) (Table (Table2).2). The virus was also detected in the brains (3.0 to 3.6 log10 EID50/ml), spleens (3.8 to 4.4 log10 EID50/ml), and blood (4.9 to 5.4 log10 EID50/ml) of mice 3 dpi, indicating that mouse-adapted H1N1 viruses had gained the ability to replicate in other organs as well as in the lungs.

To determine whether mouse adaptation of pandemic H1N1 isolates resulted in the selection of influenza viruses with increased virulence in other animal models in which influenza virus pathogenesis closely resembles that in humans, we characterized the pathogenicity of the generated mouse-adapted viruses in ferrets. Four groups of three ferrets each were inoculated with 106 EID50 of A/CA/04/09-MA1 or A/TN/1-560/09-MA1 virus, which exhibited better viral growth either in vitro or in mice, or their parental wild-type strains (Table (Table3).3). Both original wild-type viruses caused mild clinical disease signs without marked changes in body temperature. The mean maximum weight loss was ~6 to 9%, similar to that observed by other groups (20, 27, 29). No significant differences between wild-type and mouse-adapted variants were seen either in clinical features of infection or in virus titers in nasal washes 3 and 5 dpi in a ferret animal model (Table (Table3).3). Therefore, our findings showed that changes acquired during mouse adaptation were host specific and did not markedly affect the pathogenesis of pandemic H1N1 influenza viruses in ferrets.

Pathogenicity of wild-type and mouse-adapted H1N1 influenza viruses in ferrets

Sequence analysis.

To understand the molecular basis for the increased virulence acquired by pandemic H1N1 viruses during mouse adaptation, the complete genomes of the wild-type and mouse-adapted counterparts were sequenced. Sequence analysis mapped the acquired mutations to HA, NP, and polymerase proteins (Table (Table4).4). A total of 10 amino acid substitutions affecting 3 or 4 viral proteins were involved in adaptation of the pandemic A/CA/04/09 (H1N1) or A/TN/1-560/09 (H1N1) strain to mice, respectively; however, undetected genetic changes that might have occurred after a single passage in chicken eggs could not be excluded. Interestingly, the A/TN/1-560/09-MA1 variant had an adaptive change, K119N, in the HA protein (H1 numbering used throughout the text) leading to acquisition of the potential glycosylation site (Table (Table44).

Amino acid substitutions identified in mouse-adapted H1N1 influenza viruses

To investigate whether the amino acid changes observed in mouse-adapted H1N1 variants generated in this study might occur in other pandemic 2009 A (H1N1) isolates, we analyzed the H1N1 sequences deposited in the Influenza Research Database (data were obtained from the National Institute of Allergy and Infectious Diseases database available online at The mouse-adapted viruses were found to share common residues with novel H1N1 isolates in PA (295P) and HA (222G) proteins (Table (Table4).4). In fact, all pandemic H1N1 viruses possess proline at residue 295 in PA, and leucine at this position is unique to the original wild-type A/TN/1-560/09 strain. Furthermore, the mutation D222G was found in the HA protein of 1% of contemporary H1N1 isolates. However, the other eight amino acid substitutions acquired during mouse adaptation (E158G/A in PB2; K119N, G155E, S183P, and R221K in HA; and D101G and H289Y in NP [Table [Table4])4]) were not present in any H1N1 strains examined (0% or <0.1%).

Effect of HA amino acid substitutions on antigenic and receptor specificity.

To test whether in the course of mouse lung adaptation the pandemic H1N1 viruses changed their antigenic specificity due to acquired HA mutations, we determined the antigenic properties of wild-type and mouse-adapted H1N1 variants in an HI test using postinfection goat and ferret antisera and MAbs raised against a selection of currently circulating human, pandemic, and swine H1 isolates (Table (Table5).5). We observed that the original A/CA/04/09 (H1N1) and A/TN/1-560/09 (H1N1) strains did not react with the postinfection ferret antisera or MAbs raised against contemporary human or swine H1 viruses, which was in good agreement with previous findings (10, 20). The results of the HI assay showed that the mouse-adapted A/CA/04/09-MA1 and A/CA/04/09-MA2 clones had a reduced ability to react with ferret antisera raised against the parental strains (4- to 8-fold differences), whereas A/TN/1-560/09-MA1 and A/TN/1-560/09-MA2 reacted more strongly with the same antisera. Additionally, mouse-adapted H1N1 variants exhibited a change in reactivity with E2 and H7 MAbs (Table (Table55).

Antigenic characterization of wild-type and mouse-adapted H1N1 influenza viruses by hemagglutination inhibition assay

Since one of the mechanisms by which HA mutations may increase virus virulence is by affecting HA affinity to sialyl receptors (48), we next measured the receptor specificity of H1N1 viruses to high-molecular-weight sialic substrates, both natural (fetuin) and synthetic (3′SL and 6′SLN), attached to a polyacrylic carrier (Fig. (Fig.3).3). As shown by the Kass values, pandemic wild-type H1N1 viruses had increased affinity for 6′SLN, whereas the binding to the “avian-type” 3′ substrate was negligible (6, 27). Our results revealed that all mouse-adapted H1N1 viruses showed significantly reduced binding to fetuin and the “human-type” 6′SLN receptor (3- to 33-fold difference, P < 0.01) (Fig. (Fig.3).3). In contrast, the affinity to the 3′ substrate was significantly higher in the mouse-adapted variants than in the respective parental strains, except A/TN/1-560/09-MA2 (P < 0.05). The latter exhibited a moderate decrease in affinity toward the 6′SLN-acrylic polymer from that of the wild-type A/TN/1-560/09 (H1N1) virus (2.4-fold difference) (Fig. (Fig.33).

FIG. 3.
Receptor specificity of wild-type and mouse-adapted H1N1 influenza viruses. Association constants (Kass) of virus complexes with sialylglycopolymers conjugated to fetuin (containing α2,3- and α2,6-linked sialyl receptors), 6′SLN ...

Effect of amino acid substitutions in the RNP complex on protein expression and viral polymerase activity.

To investigate whether the observed mutations in the PB2, PA, and NP proteins of mouse-adapted H1N1 variants changed the total protein expression and/or viral transcription and replication activity, we analyzed reconstituted RNP complexes in 293T cells by Western blotting and a luciferase minigenome assay. Densitometric analysis of protein band intensities showed that the initial expression of all mutant PB2 and NP proteins was 72 to 374% that of the respective wild types, showing that the mutations did not abrogate initial expression levels of these proteins (Fig. 4A and B).

FIG. 4.
Total protein expression and viral polymerase activity of RNP complexes. (A and B) Total expression of wild-type and mutant PB2 and NP proteins of A/CA/04/09 (H1N1) (A) and A/TN/1-560/09 (H1N1) (B) viruses in 293T cells. 293T cells expressing wild-type ...

In the minigenome assay, A/CA/04/09-MA1, carrying PB2 E158G and NP D101G mutations, and A/TN/1-560/09-MA1, carrying PB2 E158A, PA L295P, and NP H289Y mutations, had polymerase activities of ~240 to 250% that of their respective parental viruses (Fig. 4C and D). To assign this increase to single mutations, we examined all possible combinations. We observed that the PB2 E158G amino acid substitution increased polymerase activity of the A/CA/04/09 polymerase complex to ~260%, whereas NP D101G did not (A/CA/04/09-MA2 variant), stressing the importance of the PB2 E158G change for the significant enhancement of transcription and replication activity (Fig. (Fig.4C).4C). Single point mutations PB2 E158A and PA L295P increased polymerase activity of the A/TN/1-560/09 RNP complex to 200% and 125%, respectively, and their combination further enhanced polymerase activity to 240% in an additive manner (Fig. (Fig.4D).4D). In contrast, amino acid change H289Y in the NP protein did not affect enzymatic activity when introduced alone or in any combination tested. Taken together, our findings showed that efficient polymerase activity (2.5-fold increase, P < 0.01) was achieved by PB2 E158G or by the combination of PB2 E158A and PA L295P in the A/CA/04/09 (H1N1) or A/TN/1-560/09 (H1N1) RNP complex, respectively.


Adaptation is believed to be a driving force in evolution, where organisms are selected in nature because of increased fitness conferred by beneficial mutations. Importantly, until now the molecular basis of adaptation of pandemic influenza A viruses to a new host species has been poorly understood. To address this problem, we assessed the genetic basis for increased virulence of novel H1N1 isolates in a new mammalian host by performing mouse adaptation of these isolates.

To reveal the pattern of positively selected mutations, we performed two independent series of sequential lung-to-lung passages of A/CA/04/09 (H1N1) and A/TN/1-560/09 (H1N1) viruses. Therefore, for each pandemic isolate, two mouse-adapted variants were produced and were subjected to sequence analysis to determine whether they shared common mutations. The A/CA/04/09-MA1 and A/CA/04/09-MA2 viruses differed by one amino acid substitution (E158G) in PB2 and possessed 4 amino acid changes in HA and NP proteins in common, indicating positive selection of these four mutations. Sequencing of A/TN/1-560/09-MA1 and A/TN/1-560/09-MA2 revealed that they differed by two mutations in PB2 and HA (E158A and K119N, respectively) and shared three positive mutations in PA, HA, and NP proteins. The positive selection of 7 out of 10 mutations indicated that they confer a replicative advantage; however, there is reason to believe that the remaining three mutations observed in MA1 clones (namely, PB2 E158G/A and HA K119N) were also adaptive, because they occurred independently at the same residue in two pandemic strains and/or were instrumental in adaptation by increasing viral growth in eggs, MDCK cells, and mice (discussed below).

In the present study, we identified five mutations in the HA protein, K119N, G155E, S183P, R221K, and D222G, that partially and most likely independently controlled the virulence of pandemic H1N1 viruses in mice. Further characterization of receptor specificity of generated mouse-adapted variants revealed their enhanced binding abilities to α2,3 together with decreased binding to α2,6 sialic acid-linked receptors. It is likely that the observed changes in receptor specificity contributed not only to the increased initial ability of the virus to infect and spread in the lung bronchiolar epithelium (18, 24) but also to the broader tissue tropism in other major mouse organs, which would facilitate consequent pneumonia, systemic spread, and death of infected animals.

The HA protein is a primary determinant for mouse lung virulence, and a number of studies have shown that increase in virulence could be controlled by the changes in important protein functions due to altered biological properties of the virus (48). The HA molecule mediates the attachment of influenza virus to the host cell sialyloligosaccharide receptor via a receptor binding site, which determines the viral binding specificity (50). HA undergoes the cleavage processing that is essential for infectivity of influenza virus particles (49, 50). This permits fusion of the viral envelope with the secondary endosome, a process activated by conformational changes in HA at the acidified pH (50). Previously, it was shown that one of the common structural mechanisms important for acquisition of mouse virulence could be the loss of glycosylation sites, which, as a consequence, affects the HA receptor binding specificity (30, 48), the pH of HA-catalyzed fusion (4, 42), and/or the ability of mouse serum β inhibitors to inhibit hemagglutination (12, 48). However, these general pathways for adaptation might be achieved not only by the removal of carbohydrate but also by other, yet unidentified structural factors.

Due to the lack of suitable recombinant H1N1 viruses carrying the single HA mutations identified here, it is not yet known which substitutions or combinations of substitutions are necessary for affecting the receptor specificity properties of novel H1N1 viruses and, as a consequence, pathogenesis. However, having two mouse-adapted variants, A/TN/1-560/09-MA1 and A/TN/1-560/09-MA2, which differed from each other only by the presence of the K119N HA mutation associated with the acquisition of a potential glycosylation site, made possible the examination of the role of this particular substitution. Whether or not the HA protein of the A/TN/1-560/09-MA1 virus had acquired an oligosaccharide chain, the K119N change located at the outer region of the HA globular head affected the protein structure such that the binding to α2,3 sialyl receptors became possible. The K119N HA mutation was also sufficient to significantly reduce α2,6 binding, compared with the R221K amino acid substitution observed in the A/TN/1-560/09-MA2 variant. Interestingly, our findings also indicated that adaptation of novel H1N1 viruses was accompanied by changes in antigenic reactivity as a result of acquired HA mutations, but not in the elevation of pH for membrane fusion (all H1N1 viruses caused membrane fusion at a pH of ~5.6 [data not shown]). However, it would seem likely that the changes in antigenic specificity were not a result of host-induced modification but rather occurred independently of the selection of variants with increased virulence for mice.

We also observed that mutations at four points of the RNP complex, namely, PB2 E158G/A, PA L295P, NP D101G, and NP H289Y, were involved in the mouse adaptation of pandemic H1N1 isolates. Previous studies have shown that the native RNP is a helical structure formed by the association of multiple monomers of NP protein and a single copy of the RNA-dependent RNA polymerase, a heterotrimer composed by the PB1, PB2, and PA subunits (31, 32). Such RNP complexes are independent molecular machines responsible for transcription and replication of each influenza virus gene in the nucleus of infected cells. Here, we found that, of the four mutations that occurred in the RNP complex during adaptation, only substitutions in the PB2 and PA proteins were sufficient to significantly enhance the transcription and replication activity of polymerase complexes of H1N1 influenza viruses. This characteristic resulted in an increased ability to replicate per se, which likely was necessary for optimized interaction of the viral polymerase with the host proteins and which allowed the virus to circumvent the host defense barriers, facilitating efficient virus spread and replication in the lower respiratory tract. Thus, our findings confirm and underline that host factors are important for the polymerase action of influenza virus (8).

From the analysis of virus yields in eggs and cell culture and survival of mice infected with the A/CA/04/09-MA1 and A/CA/04/09-MA2 viruses, which differed only by the PB2 E158G mutation, we surmised that the acquisition of this particular substitution provided a replicative advantage both in vitro and in vivo that enabled the pandemic H1N1 virus to become more virulent. Importantly, an amino acid change of the same residue (residue 158) occurred in two pandemic strains in two independent experiments, indicating that this event is not a chance of fluctuation; rather, it reflects a specific character of the variation, most likely connected with identifying one of the strong determinants of virulence and replication of pandemic H1N1 viruses in mice. Furthermore, PB2 E158G/A and PA L295P are localized within the PB1-binding site and the near nuclear localization signal, respectively (32); the NP D101G and NP H289Y substitutions are located within the strands of the NP body domain, which interacts with some cellular or viral proteins (31). Therefore, given the locations of the mutations reported here, they appear to implicate the central processes of influenza virus replication and sites of interaction with host and viral components.

In conclusion, in this study, we identified genes that controlled the virulence of pandemic A/CA/04/09 (H1N1) and A/TN/1-560/09 (H1N1) viruses in a mouse animal model, together with their role in mouse pathogenesis. Our findings showed that increased virulence of pandemic 2009 isolates, seen clinically as increased disease, was associated with accelerated viral growth in mammalian cells and extended tissue tropism in vivo. Our results add to the growing body of mutational analysis data defining the structural and functional changes governing new host adaptation, which may provide insights into the development of effective therapeutic intervention strategies. Our findings also suggest that changes optimizing receptor specificity and interaction of viral polymerase components with host cellular factors are the major means of pandemic influenza virus achieving an optimal competitive advantage in a mammalian host. These modulators of virulence, therefore, may have been the driving components of early evolution, which paved the way for pandemic H1N1 influenza A viruses in mammals, including humans.


We thank Jerry R. Aldridge and Ashley Prevost for excellent assistance, Elena A. Govorkova for helpful discussions, Julie Groff for illustrations, and David Galloway for editorial assistance.

This study was supported by the National Institute of Allergy and Infectious Diseases, National Institutes of Health, Department of Health and Human Services, under contract no. HHSN266200700005C, by RAS Presidium grant “Molecular and cell biology,” and by the American Lebanese Syrian Associated Charities (ALSAC).


[down-pointing small open triangle]Published ahead of print on 30 June 2010.


1. Bovin, N. V., E. Y. Korchagina, T. V. Zemlyanukhina, N. E. Byramova, O. E. Galanina, A. E. Zemlyakov, A. E. Ivanov, V. P. Zubov, and L. V. Mochalova. 1993. Synthesis of polymeric neoglycoconjugates based on N-substituted polyacrylamides. Glycoconj. J. 10:142-151. [PubMed]
2. Brown, E. G. 1990. Increased virulence of a mouse-adapted variant of influenza A/FM/1/47 virus is controlled by mutations in genome segments 4, 5, 7, and 8. J. Virol. 64:4523-4533. [PMC free article] [PubMed]
3. Brown, E. G., and J. E. Bailly. 1999. Genetic analysis of mouse-adapted influenza A virus indentifies roles for the NA, PB1, and PB2 genes in virulence. Virus Res. 61:63-76. [PubMed]
4. Brown, E. G., H. Liu, L. C. Kit, S. Baird, and M. Nesrallah. 2001. Pattern of mutation in the genome of influenza A virus on adaptation to increased virulence in the mouse lung: identification of functional themes. Proc. Natl. Acad. Sci. U. S. A. 98:6883-6888. [PubMed]
5. Centers for Disease Control and Prevention. 2009. Swine influenza A (H1N1) infection in two children—Southern California, March-April 2009. MMWR Morb. Mortal. Wkly. Rep. 58:400-402. [PubMed]
6. Childs, R. A., A. S. Palma, S. Wharton, T. Matrosovich, Y. Liu, W. Chai, M. A. Campanero-Rhodes, Y. Zhang, M. Eickmann, M. Kiso, A. Hay, M. Matrosovich, and T. Feizi. 2009. Receptor-binding specificity of pandemic influenza A (H1N1) 2009 virus determined by carbohydrate microarray. Nat. Biotechnol. 9:797-799. [PubMed]
7. Flehmig, B., A. Vallbracht, and H.-J. Gerth. 1976. Influenza virus: association of mouse-lung virulence with plaque formation in mouse kidney cells. Intervirology 7:201-210. [PubMed]
8. Gabriel, G., B. Dauber, T. Wolff, O. Planz, H.-D. Klenk, and J. Stech. 2005. The viral polymerase mediates adaptation of an avian influenza virus to a mammalian host. Proc. Natl. Acad. Sci. U. S. A. 102:18590-18595. [PubMed]
9. Gambaryan, A. S., and M. N. Matrosovich. 1992. A solid-phase enzyme-linked assay for influenza virus receptor-binding activity. J. Virol. Methods 39:111-123. [PubMed]
10. Garten, R. J., 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. López-Gatell, H. Olivera, I. López, 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, and N. J. Cox. 2009. Antigenic and genetic characteristics of swine-origin 2009 (A) H1N1 influenza viruses circulating in humans. Science 325:197-201. [PMC free article] [PubMed]
11. Gitelman, A. K., N. V. Kaverin, I. G. Kharitonenkov, I. A. Rudneva, and V. N. Zhdanov. 1984. Changes in the antigenic specificity of influenza virus haemagglutinin in the course of adaptation to mice. Virology 134:230-232. [PubMed]
12. Hartley, C. A., P. C. Reading, A. C. Ward, and E. M. Anders. 1997. Changes in the hemagglutinin molecule of influenza type A (H3N2) virus associated with increased virulence for mice. Arch. Virol. 142:75-88. [PubMed]
13. Hayden, F. G., K. M. Cote, and R. G. Douglas. 1980. Plaque inhibition assay for drug susceptibility testing of influenza viruses. Antimicrob. Agents Chemother. 17:865-870. [PMC free article] [PubMed]
14. Hers, J. F., J. Mulder, N. Masurel, L. V. D. Kuip, and D. A. Tyrrell. 1962. Studies on the pathogenesis of influenza virus pneumonia in mice. J. Pathol. Bacteriol. 83:207-217. [PubMed]
15. Hirst, G. K. 1947. Studies on the mechanism of adaptation of influenza virus to mice. J. Exp. Med. 86:357-366. [PMC free article] [PubMed]
16. Hoffmann, E., G. Neumann, G. Hobom, R. G. Webster, and Y. Kawaoka. 2000. “Ambisense” approach for the generation of influenza A virus: vRNA and mRNA synthesis from one template. Virology 267:310-317. [PubMed]
17. Hoffmann, E., J. Stech, Y. Guan, R. G. Webster, and D. R. Perez. 2001. Universal primer set for the full-length amplification of all influenza A viruses. Arch. Virol. 146:2275-2289. [PubMed]
18. Ibricevic, A., A. Pekosz, M. J. Walter, C. Newby, J. T. Battaile, E. G. Brown, M. J. Holtzman, and S. L. Brody. 2006. Influenza virus receptor specificity and cell tropism in mouse and human airway epithelial cells. J. Virol. 80:7469-7480. [PMC free article] [PubMed]
19. Ilyushina, N. A., E. A. Govorkova, T. E. Gray, N. V. Bovin, and R. G. Webster. 2008. A switch to human-like receptor specificity does not affect the neuraminidase-inhibitor susceptibility of influenza A (H5N1) viruses. PLoS Pathog. 4:e1000043. [PMC free article] [PubMed]
20. Itoh, Y., K. Shinya, M. Kiso, T. Watanabe, Y. Sakoda, M. Hatta, Y. Muramoto, D. Tamura, Y. Sakai-Tagawa, T. Noda, S. Sakabe, M. Imai, Y. Hatta, S. Watanabe, C. Li, S. Yamada, K. Fujii, S. Murakami, H. Imai, S. Kakugawa, M. Ito, R. Takano, K. Iwatsuki-Horimoto, M. Shimojima, T. Horimoto, H. Goto, K. Takahashi, A. Makino, H. Ishigaki, M. Nakayama, M. Okamatsu, K. Takahashi, D. Warshauer, P. A. Shult, R. Saito, H. Suzuki, Y. Furuta, M. Yamashita, K. Mitamura, K. Nakano, M. Nakamura, R. Brockman-Schneider, H. Mitamura, M. Yamazaki, N. Sugaya, M. Suresh, M. Ozawa, G. Neumann, J. Gern, H. Kida, K. Ogasawara, and Y. Kawaoka. 2009. In vitro and in vivo characterization of new swine-origin H1N1 influenza viruses. Nature 460:1021-1025. [PMC free article] [PubMed]
21. Jackson, D., M. J. Hossain, D. Hickman, D. R. Perez, and R. A. Lamb. 2008. A new influenza virus virulence determinants: the NS1 protein four C-terminal residues modulate pathogenicity. Proc. Natl. Acad. Sci. U. S. A. 105:4381-4386. [PubMed]
22. Jiao, P., G. Tian, Y. Li, G. Deng, Y. Jiang, C. Liu, W. Liu, Z. Bu, Y. Kawaoka, and H. Chen. 2008. A single-amino-acid substitution in the NS1 protein changes the pathogenicity of H5N1 avian influenza virus in mice. J. Virol. 82:1146-1154. [PMC free article] [PubMed]
23. Kaverin, N. V., N. N. Finskaya, I. A. Rudneva, A. K. Gitelman, I. G. Kahritonenkov, and Y. A. Smirnov. 1989. Studies on the genetic basis of human influenza A virus adaptation to mice: degrees of virulence of reassortants with defined genetic content. Arch. Virol. 105:29-37. [PubMed]
24. Keleta, L., A. Ibricevic, N. V. Bovin, S. L. Brody, and E. G. Brown. 2008. Experimental evolution of human influenza virus H3 hemagglutinin in the mouse lung identifies adaptive regions in HA1 and HA2. J. Virol. 82:11599-11608. [PMC free article] [PubMed]
25. Li, Z., H. Chen, P. Jiao, G. Deng, G. Tian, Y. Li, E. Hoffmann, R. G. Webster, Y. Matsuoka, and K. Yu. 2005. Molecular basis of replication of duck H5N1 influenza viruses in a mammalian mouse model. J. Virol. 79:12058-12064. [PMC free article] [PubMed]
26. Loosli, C. G., S. F. Stinson, D. P. Ryan, M. S. Herweck, J. D. Hardy, and R. Serebrin. 1975. The destruction of type 2 pneumocytes by airborne influenza PR8-A virus; its effect on surfactant and lecithin content of the pneumonic lesions of mice. Chest 67:7S-14S. [PubMed]
27. Maines, T. R., A. Jayaraman, J. A. Belser, D. A. Wadford, C. Pappas, H. Zeng, K. M. Gustin, M. B. Pearce, K. Viswanathan, Z. H. Shriver, R. Raman, N. J. Cox, R. Sasisekharan, J. M. Katz, and T. M. Tumpey. 2009. Transmission and pathogenesis of swine-origin 2009 (A) H1N1 influenza viruses in ferrets and mice. Science 325:484-487. [PMC free article] [PubMed]
28. Matrosovich, M. N., A. S. Gambaryan, A. B. Tuzikov, N. E. Byramova, L. V. Mochalova, A. A. Golbraikh, M. D. Shenderovich, J. Finne, and N. V. Bovin. 1993. Probing of the receptor-binding sites of the H1 and H3 influenza virus hemagglutinins by synthetic and natural sialosides. Virology 196:111-123. [PubMed]
29. Munster, V. J., E. de Wit, J. M. van den Brand, S. Herfst, E. J. Schrauwen, T. M. Bestebroer, D. van de Vijver, C. A. Boucher, M. Koopmans, G. F. Rimmelzwaan, T. Kuiken, A. D. Osterhaus, and R. A. Fouchier. 2009. Pathogenesis and transmission of swine-origin 2009 (A) H1N1 influenza viruses in ferrets. Science 325:481-483. [PubMed]
30. Narasaraju, T., M. K. Sim, H. H. Ng, M. C. Phoon, N. Shanker, S. K. Lal, and V. T. K. Chow. 2009. Adaptation of human influenza H3N2 virus in a mouse pneumonitis model: insights into viral virulence, tissue tropism and host pathogenesis. Microbes Infect. 11:2-11. [PubMed]
31. Ng, A. K., J.-H. Wang, and P.-C. Shaw. 2009. Structure and sequence analysis of influenza A virus nucleoprotein. Sci. China C Life Sci. 52:439-449. [PubMed]
32. Ohtsu, Y., Y. Honda, Y. Sakata, H. Kato, and T. Toyoda. 2002. Fine mapping of the subunit binding sites of influenza virus RNA polymerase. Microbiol. Immunol. 46:167-175. [PubMed]
33. Palmer, D. F., W. R. Dowdle, M. T. Coleman, and G. C. Schild. 1975. Advanced laboratory techniques for influenza diagnosis. U.S. Department of Health, Education, and Welfare, immunology series no. 6. Centers for Disease Control and Prevention, Atlanta, GA.
34. Raut, S., J. Hurd, R. J. Cureton, G. Blandford, and R. B. Heath. 1975. The pathogenesis of infections of the mouse caused by virulent and avirulent variants of an influenza virus. J. Med. Microbiol. 8:127-136. [PubMed]
35. Reed, L. J., and H. Muench. 1938. A simple method for estimating fifty percent endpoints. Am. J. Hyg. (Lond.) 27:493-497.
36. Reuman, P. D., S. Keely, and G. M. Schiff. 1989. Assessment of signs of influenza illness in the ferret model. J. Virol. Methods 24:27-34. [PubMed]
37. Rudneva, I. A., N. V. Kaverin, N. L. Varich, A. K. Gitelman, A. M. Makhov, S. M. Klimenko, and V. M. Zhdanov. 1986. Studies on the genetic determinants of influenza virus pathogenicity for mice with the use of reassortants between mouse-adapted and non-adapted variants of the same virus strain. Arch. Virol. 90:237-248. [PubMed]
38. Salomon, R., J. Franks, E. A. Govorkova, N. A. Ilyushina, H.-L. Yen, D. Post, J. Humberd, M. Trichet, J. E. Rehg, R. Webby, R. G. Webster, and E. Hoffmann. 2006. The polymerase complex genes contribute to the high virulence of the human H5N1 influenza virus isolate A/Vietnam/1203/04. J. Exp. Med. 203:689-697. [PMC free article] [PubMed]
39. Shinya, K., S. Hamm, M. Hatta, H. Ito, T. Ito, and Y. Kawaoka. 2004. PB2 amino acid at position 627 affects replicative efficiency, but not cell tropism, of Hong Kong H5N1 influenza A viruses in mice. Virology 320:258-266. [PubMed]
40. Shinya, K., S. Watanabe, T. Ito, N. Kasai, and Y. Kawaoka. 2007. Adaptation of an H7N7 equine influenza A virus in mice. J. Gen. Virol. 88:547-553. [PubMed]
41. Shulman, J. L. 1983. Virus-determined differences in the pathogenesis of influenza virus infections, p. 305-320. In P. Palese and D. W. Kingsbury (ed.), Genetics of influenza viruses. Springer, New York, NY.
42. Smeenk, C. A., and E. G. Brown. 1994. The influenza virus variant A/FM/1/47-MA possesses single amino acid replacements in the hemagglutinin, controlling virulence, and in the matrix protein, controlling virulence as well as growth. J. Virol. 68:530-534. [PMC free article] [PubMed]
43. Song, M.-S., P. N. Q. Pascua, J. H. Lee, Y. H. Baek, O.-J. Lee, C.-J. Kim, H. Kim, R. J. Webby, R. G. Webster, and Y. K. Choi. 2009. The polymerase acidic protein gene of influenza A virus contributes to pathogenicity in a mouse model. J. Virol. 83:12325-12335. [PMC free article] [PubMed]
44. Subbarao, E. K., W. London, and B. R. Murphy. 1993. A single amino acid in the PB2 gene of influenza A virus is a determinant of host range. J. Virol. 67:1761-1764. [PMC free article] [PubMed]
45. Sweet, C., and H. Smith. 1980. Pathogenicity of influenza virus. Microbiol. Rev. 44:303-330. [PMC free article] [PubMed]
46. Vallbracht, A., C. Scholtissek, B. Flehmig, and H.-J. Gerth. 1980. Recombination of influenza A strains with fowl plague virus can change pneumotropism for mice to a generalized infection with involvement of the central nervous system. Virology 107:452-460. [PubMed]
47. Venables, W. N., and B. D. Ripley. 1997. Modern applied statistics, p. 223-242, 297-321, 345-350. Springer, New York, NY.
48. Ward, A. C. 1997. Virulence of influenza A virus for mouse lung. Virus Genes 14:187-194. [PubMed]
49. Webster, R. G., W. J. Bean, O. T. Gorman, T. M. Chambers, and Y. Kawaoka. 1992. Evolution and ecology of influenza A viruses. Microbiol. Rev. 56:152-179. [PMC free article] [PubMed]
50. Wiley, D. C., and J. J. Skehel. 1987. The structure and function of the hemagglutinin membrane glycoprotein of influenza virus. Annu. Rev. Biochem. 56:365-394. [PubMed]
51. World Health Organization. 30 May 2010, accession date. Pandemic (H1N1) 2009—update 102.
52. World Health Organization. 7 June 2009, accession date. Pandemic (H1N1) 2009.
53. Wu, R., H. Zhang, K. Yang, W. Liang, Z. Xiong, Z. Liu, X. Yang, H. Shao, X. Zheng, M. Chen, and D. Xu. 2009. Multiple amino acid substitutions are involved in the adaptation of H9N2 avian influenza virus to mice. Vet. Microbiol. 138:85-91. [PubMed]
54. Wyde, P. R., R. B. Couch, B. F. Mackler, T. R. Cate, and B. M. Levy. 1977. Effects of low- and high-passage influenza virus infection in normal and nude mice. Infect. Immun. 15:221-229. [PMC free article] [PubMed]
55. Zamarin, D., M. B. Ortigoza, and P. Palese. 2006. Influenza A virus PB1-F2 protein contributes to viral pathogenesis in mice. J. Virol. 80:7976-7983. [PMC free article] [PubMed]

Articles from Journal of Virology are provided here courtesy of American Society for Microbiology (ASM)