Neuraminidase-deficient Sendai virus HN mutants provide protection from homologous superinfection
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- A. Baumann, C. & J. Neubert, W. Arch Virol (2010) 155: 217. doi:10.1007/s00705-009-0567-6
Binding of hemagglutinin-neuraminidase proteins (HN) to sialylated receptors initiates the infection process of several paramyxoviruses, whereas later in the viral life cycle, the neuramindase (NA) activity of newly synthesized HN destroys all receptors. Prior to NA action, expressed HN has to bind the receptor. To evaluate this HN–receptor complex with respect to receptor inactivation, three temperature-sensitive Sendai virus HN mutants carrying amino acid exchanges at positions 262, 264 and/or 461 were created that uncoupled NA activity from receptor binding at 39°C. Interestingly, at elevated temperature, when there is no detectable neuramindase activity, all infected cells are protected against homologous superinfection. Mutated HN protein on the cell surface is mainly bound to sialylated cell-surface components but can be released by treatment with NA. Thus, continuous binding to HN already inactivates the receptors quantitatively. Furthermore, mutant HN bound to receptors is prevented from being incorporated into virus particles in the absence of NA. It is shown here for the first time that during paramyxoviral infection, quantitative receptor inactivation already occurs due to binding of receptors to expressed HN protein without involvement of NA and is independent of NA activity of viral progeny. NA subsequently functions in the release of HN from the complex, coupled with desialysation of receptors. These findings could have implications for further antiviral drug development.
Hemagglutinin-neuraminidase glycoproteins (HN) in the envelope of several paramyxoviruses initiate the infection process by binding to cellular receptors. Later in the viral life cycle, HN expressed on the cell surface is thought to cause destruction of the receptor, thereby preventing re-infection by viral progeny and also homologous superinfection . Both HN functions are based on its affinity for sialylated receptors [6, 42]. Diverse sialic-acid-containing cell-surface components have been characterized [9, 19, 37], and structural studies on HN from NDV, hPIV3 and SV5 suggest that one structurally flexible sialic-acid-recognition site of HN switches between a binding and a catalytic function [4, 16, 43]. This concept of a bifunctional HN site is further supported by work showing that both functions could be simultaneously reduced or even abolished through the binding of monoclonal antibodies or neuraminidase (NA) inhibitors [12, 28, 41]. Using hemadsorption assays, it has been shown that mutated HN, generated in transduced cells, shows both reduced NA and reduced receptor-binding activity [3, 13]. Hence, it seems that HN mutations induce a defect in both functions simultaneously and that generation of an HN protein that possess functional receptor-binding activity but lacks NA activity should not be possible.
Until now, a possible participation of the receptor-binding function in the process of receptor destruction could not be examined using live virus. In earlier studies on cell lines persistently infected with Sendai virus (SeV) [14, 40], we demonstrated protection against homologous superinfection, although hemadsorption specific for HN on the cell surface was reduced by 50% . In parallel, a strong decrease in NA activity was detectable through the inability to release hemagglutinated erythrocytes at 37°C from virus–erythrocyte complexes. Based on these findings, we hypothesized that viruses from persistent infections could contain an HN with uncoupled receptor-binding and receptor-destroying functions: HN bound to receptors would not be released for binding another substrate as long as NA is not active and—as a consequence—incorporation of HN into viral progeny could be hindered. If the same mechanism would also apply to wild-type (wt) infections, such findings could be relevant for further development of antiviral drugs, which are currently mainly focused on neuraminidase inhibition. However, in wild-type infections, both processes occur very quickly due to the high efficiency of NA and therefore could not be investigated separately so far.
We decided to test our hypothesis under natural conditions by infecting cells with SeV mutants carrying selected mutations in the HN gene suspected to be responsible for NA deficiencies. A 30% reduced NA activity was reported for SeV Enders strain mutant ts 271, which has amino acid exchanges at positions 262, 264 and 461 [29, 30] compared to Enders wt, but this mutant is no longer available. Compared to Sendai strain Fushimi HN, the Enders HN shows a reduction in NA activity of 35% [8, 39] due to the aa exchange E461K; therefore, we decided to create mutants based on the Fushimi backbone.
The HN mutants examined in the present work possess the amino acid exchanges A262T+G264R+E461K, A262T+E461K or A262T+G264R. Exchanges at positions 262 and 264 are equivalent to those of mutant ts 271, and an exchange at position 461 corresponding to that in the Enders strain should further decrease NA activity. To demonstrate NA-independent receptor inactivation by these mutants specifically, homologous superinfection assays with a Sendai challenge virus carrying an eGFP reporter gene were employed as a very sensitive approach.
The three SeV HN mutants presented here showed a temperature-dependent decrease in NA activity to undetectable levels when the proteins were expressed at elevated temperature. Binding of mutated HN to sialylated receptors of infected cells already prevented homologous superinfection, independent of NA activity.
Materials and methods
Cells and virus infection
LLC-MK2 cells (Rhesus monkey kidney, ATCC no. CCL 7.1) were purchased from Flow Laboratories and were maintained in Dulbecco’s modified Eagle’s medium (DMEM) supplemented with 10% fetal calf serum (FCS).
Cell monolayers were consistently infected with Sendai virus at an m.o.i. of ≥4 to achieve HN synthesis in ≥98% of the cells. Virus adsorption was generally performed at 33°C for 1 h, after which cells were incubated in serum-free DMEM (DMEM−) at the indicated temperatures.
Virus stock and FLAT assay
Virus stocks were prepared by infecting cell monolayers for 46 h at 33°C. Virus particles were activated by cleavage of the F0 protein into F1 and F2 by treatment with acetylated trypsin (4 μg/ml final concentration) for 1 h. Virus stocks were stored in the vapor phase of liquid N2.
Virus titers were determined by the fluorescence-linked antibody titer (FLAT) assay. Cell monolayers (2 × 105 cells) in 24-well plates were infected with ten-fold serially diluted virus suspensions and incubated at 33°C. Two days later, the cells were fixed with methanol. Intracellular viral proteins were detected with monospecific anti-N antibodies generated in our laboratory, followed by incubation with anti-rabbit antibodies labeled with Alexa Fluor 568 fluorescence dye (Molecular Probes). Fluorescent positive cells were counted.
Generation of recombinant Sendai virus (rSeV) HN mutants and rSeV P-EGFP
The construction of the complete cDNA of SeV (Fushimi strain) has been described previously [17, 18]. Mutations in the SeV genome at positions 7,476, 7,482 and 8,073 were generated by using synthetic oligonucleotide primers, the ExSite PCR-based mutagenesis kit (Stratagene, La Jolla), the fusion PCR technique and standard cloning techniques . The presence of the desired mutations in the three different HN mutants was confirmed by nucleotide sequencing. Details of the stepwise generation of the mutated genomic cDNA can be obtained from the authors on request.
Generation of rSeV P-eGFP, which has the enhanced green fluorescent protein (eGFP) gene inserted after the P gene, has been described previously . Rescue of the recombinant SeV HN mutants was performed with MVA-T7 vaccinia virus as described previously [18, 33, 36].
Generation of recombinant measles virus P-DsRed
The construction and generation of the recombinant measles virus P-DsRed (Schwarz strain, Mérieux™) with a Discosoma red (DsRed) gene inserted after the P gene was performed essentially as described previously .
Western blot analysis of cellular and viral proteins
Cell infection was performed in T75 Roux bottles (6 × 106 cells) as described above. After incubation for 47 h, the culture medium was collected for virus purification. Supernatants of infected cells were clarified from cell debris by centrifugation at 700g, and virus particles were pelleted at 30,000 rpm. (154,000g). The virus pellet was solubilized in RIPA buffer, and the protein concentration was determined. Infected cell monolayers were washed and collected in DMEM−. The cells were lysed in RIPA buffer , and DNA was disrupted by sonification (LKB Instruments). The protein concentration of each sample was determined by the Lowry technique .
Cellular and viral proteins were analyzed by western blot after separation on a 10% sodium dodecyl sulfate polyacrylamide gel. The proteins were transferred to an Immobilon-PVDF membrane (Millipore) by electroblotting in Tris–glycine buffer (20 mM Tris–HCl, pH 8.8, 150 mM glycine) at 400 mA for 6.5 h. The membranes were blocked with Roti-Block (Carl Roth GmbH), a polymer-based blocking reagent, and then incubated for 1 h in HN- or N-protein-specific antibodies, which were generated in our laboratory. The blot was rinsed with TBST (10 mM Tris–HCl, pH 8.8, 150 mM NaCl, 0.05% Tween 20) and incubated with peroxidase-conjugated anti-mouse or anti-rabbit antibody (Dako) diluted in TBST. ECL western blotting reagents (Amersham Biosciences) were used for chemiluminescence detection.
Cells grown on glass slides were infected for 24 h at 33 or 39°C. The cells were incubated with anti-HN monoclonal antibody S2, courteously provided by Portner et al. . It was added to the living cells for 1 h at room temperature. After washing the cell monolayers, the cells were fixed for 10 min with 100% methanol. HN protein-antibody complexes were made visible by incubation in anti-mouse Alexa Fluor 568-conjugated antibody (Molecular Probes) for 1 h. Cells were photographed at 200× magnification.
Erythrocyte binding assay and treatment of infected cells with Vibrio cholerae neuraminidase (V.C. NA)
Erythrocytes of type O were freshly obtained from human blood. Cells were seeded in 24-well plates with 1.6 × 105 cells/well and incubated for 1 day at 37°C. Subsequently, the cell monolayers were infected for 24 h as described above. Hemadsorption activity (HAd) was determined using a 0.5% erythrocyte suspension in serum-free medium. After washing the cells, erythrocytes were added in DMEM− for 1 h at 4°C. Unbound erythrocytes were removed by washing, and the percentage of hemadsorption-positive cells was determined. Alternatively, the hemoglobin content of bound erythrocytes was determined: Erythrocytes were eluted by treatment for 2 h at 37°C with 1 mU of V.C. NA (Sigma), pelleted and lysed in 50 mM NH4Cl. The lysate was clarified by centrifugation, and the absorbance of the hemoglobin was measured at 450 nm using a microtiter plate reader (Dynatech MR7000).
V.C. NA treatment was performed 23 h after cell infection at the temperature used for production of HN proteins. The monolayer was washed with DMEM−, and 10 mU of V.C. NA was added in 250 μl DMEM− for 1 h. HAd activity was determined after removing the enzyme.
Detection of neuraminidase activity by substrate cleavage
Assays were performed in T12.5 Roux bottles (1 × 106 cells). Monolayers were infected as described above. Cells were washed and subsequently incubated in 0.4 ml colorless Medium 199 (Gibco-Invitrogen) without FCS. NAe substrate X-Neu5Ac (5-bromo-4-chloro-3-indolyl α-d-N-acetylneuraminic acid, 0.2 μmol) (Sigma)  was added for 1 h at the indicated infection temperatures. Afterward, the supernatant was centrifuged through an Ultrafree-MC centrifugal filter unit (Millipore) for 2 min at 8,000g (Beckman centrifuge), and the flow-through was transferred to a polystyrol cuvette. NA activity converted X-Neu5Ac to the blue pigment 5,5′-dibromo-4,4′-dichloro indigo, which was quantified 24 h later at 660 nm in a spectrophotometer (Beckman).
Assays were performed in T25 Roux bottles (2 × 106 cells). Primary infection was carried out as described above. The infected cells were washed 24 h later with DMEM−. Homologous superinfection was initiated by adding rSeV P-eGFP  at an m.o.i. of ≥4. Measles virus P-DsRed at an m.o.i. of ≥2 was used for heterologous superinfection. The challenge virus was allowed to adsorb for 1 h at the temperatures used for primary infection. Cells were inspected for eGFP or DsRed after 2 and 3 days, respectively.
Production of SeV HN mutants and characterization of the expressed HN proteins
In the next step, the stable and efficient expression of mutant HN proteins in infected cells at 33 and 39°C was analyzed. Infections were generally performed using an m.o.i. of ≥4, virus particles were adsorbed at 33°C, and cells were incubated at 33 or 39°C. HN in cell extracts prepared 46 h later were analyzed by immunoblot detection. Using a small amount of cell extract (5 μg) resulted in clear HN signals with all three mutants at both temperatures without detection of degradation products (Fig. 1a). In contrast to our efficient HN synthesis, in transduced cells, in which the HN expression was restricted, either due to a small number of transfected cells and/or a generally low level of expression, 250 μg of cell extract or immunoprecipitation of radioactively labeled proteins was required for detection [10, 13]. Next, mutant HN expressed on the cell surface was detected in situ by cell-surface immunofluorescence. Incubation with the primary antibody was carried out before cell fixation. In this way, the undesired permeabilization of cell membranes, which could lead to binding of intracellular HN protein to the antibody, was definitely prevented . Transport to the cell surface was independent of incubation temperature, since mutated HN were clearly detectable at 33 and 39°C (Fig. 1c). HN signals on the cell surface were more regularly distributed compared to the signals of cytoplasmic proteins. Unimpaired expression of mutant HN and transport to the cell surface were important prerequisites for investigating HN–receptor complexes.
Finally, the neuraminidase (NA) activity of mutant HN suspected to be decreased at elevated temperature was measured at 33 and 39°. In comparison to wt infected cells, mutant cells infected at 33°C revealed significantly reduced but clearly detectable neuraminidase. At 39°C, activity was undetectable (Fig. 1b). In this assay, even low levels of sialidase activity should be detectable due to repeated binding and cleavage of the synthetic substrate. However, when the substrate incubation time was extended to 4.75 h, we again failed to detect any enzymatic activity (data not shown). In summary, cytoplasmic mutant HN synthesis and its transport to the cell surface are not impaired and NA activity is undetectable at 39°C, as proposed. Therefore, these virus mutants should be useful tools for investigating possible influences of HN–receptor complexes on receptor inactivation.
Homologous superinfection by challenge virus carrying a reporter gene
HN 262+264+461 and HN 262+461 protein expression induces protection against homologous superinfection
Homologous superinfection assays were employed to test infected but NA-negative cells for presentation and accessibility of functional SeV receptors on the cell surface. LLC-MK2 cells were infected with HN mutants. After 24 h, one set of infected cultures was subjected to hemadsorption tests, the other treated with challenge virus. After incubation with challenge virus for 47 h, there was a lack of eGFP signal, indicating that the cells infected with HN 262+264+461 and HN 262+461 had been able to develop complete protection against homologous superinfection (Fig. 3a). Interestingly, resistance to SeV superinfection could be also demonstrated in cells lacking HAd activity. The rare detection of single cells with very intense fluorescence signals (Fig. 3a, 262+264+461, 33°C) was attributed to cells that remained uninfected by mutant viruses. These strong eGFP-specific signals are comparable to those in cells infected with SeV P-eGFP alone (Fig. 3a, SeV-eGFP infection).
In contrast, only partial protection against superinfection was achieved in cells infected with mutant HN 262+264 (Fig. 3a). Homologous superinfection was identified in only a few cells at 33°C but by most of the cells at 39°C: HN 262+264 was not able to induce a complete and temperature-independent inactivation of receptors. Superinfection was also detectable at an increased m.o.i. of up to 75 as well as after prolonged infection times of up to 48 h before challenge (data not shown). Quantitative protection against homologous superinfection was finally reached when cells infected at 39°C with mutant HN 262+264 were subsequently treated with V.C. NA (Fig. 3a, 262+264+NA). Therefore, superinfection at 39°C can be interpreted as a temperature-sensitive effect on HN 262+264 binding activity.
To exclude any non-specific effects on HN–receptor inactivation due to infection with mutants HN 262+264+461 and HN 262+461, heterologous superinfection assays with recombinant measles virus containing the DsRed reporter gene (P-DsRed) were also performed. As shown with HN 262+461 infected cells, measles challenge virus infection and replication were not impeded (Fig. 3b). Taken together, infection with NA-deficient mutants protects cells against homologous superinfection. Thus, earlier findings obtained with persistently infected cells  could be reproduced by using recombinant virus carrying only two or three defined mutations within the HN gene.
HN–receptor complexes on the surface of mutant infected cells
To test whether the receptor-binding site of HN was blocked by sialylated cell-surface components, the cells were treated with exogenous NA and subsequently tested for HAd activity. Like SeV neuraminidase, V.C. NA preferentially hydrolyzes α (2, 3) linkages of sialic acids . After V.C. NA treatment, erythrocyte binding was greatly enhanced at 39°C on cells infected with either HN mutant 262+264+461 or 262+461, whereas cells infected with HN mutant 262+264 showed a minor effect (Fig. 4a, c). The remaining HAd-negative cells during 262+264 infections might have been due to inefficient extracellular neuraminidase treatment, which is also unable to completely prevent LLC-MK2 cells from being infected with SeV wt (data not shown).
These results now allow an explanation of superinfection protection after infection with NA-deficient HN mutants: Mutant HN protein expressed in increasing amounts binds to receptors, leading to a quantitative formation of the HN–receptor complex and—when this binding persists—to a quantitative inactivation of the receptor.
Reduced incorporation of HN into mutant virus particles at 39°C
In the present work, the question is addressed whether SeV HN with functional binding activity but defective NA is capable of receptor inactivation. It is well known that the first step in the receptor-destruction process is a temporary binding of HN to receptors, rapidly followed by cleavage of sialic acid by NA. These consecutive processes happen very quickly and could not be separated so far. Based on data on Sendai virus mutants from persistent infections , we suspected that for quantitative receptor inactivation, continuous binding to newly synthesized HN might be sufficient without any NA activity. To answer the question of whether NA-deficient HN mutants are able to inactivate receptors quantitatively, for the first time, superinfection assays were employed as a highly sensitive test system using eGFP-expressing Sendai virus as homologous challenge virus. These assays allow detection of single challenge virus entry via non-inactivated virus receptors on infected cells, which was not possible in earlier transduction or superinfection studies based on viral progeny [10, 15, 22].
Superinfection protection requires efficient binding of mutant virus to cells and efficient HN production in infected cells. The receptor-binding activity of mutated HN was demonstrated by determining infection rates of the mutant viruses, which were comparable to the wt virus. Normal quantities of mutant HN in the cytoplasm and on the surface of infected cells were detectable (Fig. 1a, c). In contrast to our approach, this state was not attained in cells transduced with wt hPIV3 HN or the NA-deficient mutant HN (C28a), since homologous superinfection was detectable . In order to achieve efficient superinfection protection, the time point of challenge virus addition has to be chosen carefully. After an infection time of 5 h, ca. 50% of the cells were unprotected against superinfection, whereas 24 h after primary infection, cells could no longer be infected by the challenge virus (Fig. 2a, b). We suppose that during progress of virus replication, the number of newly synthesized HN proteins exceeds that of the receptor molecules.
Newly synthesized HN 262+264+461 and 262+461 quantitatively blocked homologous superinfection of cells, and this was independent of the infection temperature (Fig. 3a), whereas the challenge virus alone efficiently expressed fluorescence in unprotected cells. The results of homologous (Fig. 3a) and heterologous superinfection (Fig. 3b) assays reveal that mutant HN blocks homologous superinfection specifically and not only due to cellular stress caused by the infection process. Hemadsorption on the cell surface can be restored by NA treatment and HN incorporation into viral progeny is restricted by continuous binding to sialylated receptors. Therefore, it is more likely that receptors are present but inactivated through binding to HN than that viral infection downregulates receptor synthesis, as believed in the case of the lentivirus CD4 receptor . These experiments clearly demonstrate that in the absence of NA activity, receptors remain bound to HN, leading to protection against superinfection, and that binding of mutant HN to receptors is reversible—by application of external neuraminidase.
Cells infected with HN mutant 262+264 at 33°C blocked superinfection almost completely, whereas at 39°C, infected cells were clearly superinfected (Fig. 3a). This result suggests that a HN phenotype with insufficient receptor-binding affinity was obtained at elevated temperature. The HN-binding activity by mutant 262+264 does not seem to be strong enough to inactivate receptors completely, thus allowing homologous superinfection.
A number of mutated HNs generated by different laboratories [3, 13, 34] were characterized in hemadsorption and NA assays as HN variants with simultaneously reduced binding and NA activity. These results are based on the assumption that the ligands had unrestricted accessibility to HN. However, when HN cannot be released from the receptor due to the lack of NA, HN, in turn, would not be available to bind other ligands, such as erythrocytes. Thus, interpretations of results from previous hemadsorption and NA assays typically employed in this type of study should be reconsidered [3, 34]. According to our results, newly synthesized HN is first targeted to binding to receptors. Consequently, only after NA is active and removed bound receptors can HN attain the ability to bind erythrocytes. The conclusion that HAd binding activity depends on the efficiency of NA in releasing HN from HN–receptor complexes was confirmed in various ways: (1) Most of the cells infected with the HN-262+264+461 or HN-262+461 mutant lost the HAd activity they had at 33°C when the infection temperature was increased, concomitantly with a loss of detectable NA activity (Figs. 1b, 4b). (2) When the deficiency in viral NA activity was compensated using bacterial NA, HN-262+264+461 and HN-262+461—bound to receptors—gain the ability to bind erythrocytes (Fig. 4a, c). The observations of Connaris et al.  and Mirza et al.  can be interpreted in the context of a similar NA-triggered hemadsorption activity. Reduced erythrocyte binding of mutated HN has been described to be accompanied by strongly reduced NA activity.
Until now, the functional relevance of amino acids 262, 264 and 461 was neither recognizable from their classification as highly conserved amino acids nor by identification as active site residues due to structure analysis data. However, an influence on NA activity could be suggested by the proximity of amino acids 262 and 264 to the “NRKSCS motif” at positions 254–259 in SeV HN, a highly conserved region among parainfluenzaviruses . Moreover, conformational implications could also be thought to have an influence, because positions 262 and 264 lie between C258 and C271, which form a disulfide bridge in the human parainfluenzavirus 3 HN protein, the closest “sequence” relative of the SeV HN .
Absence of NA activity was associated with a drastically reduced HN content in mutant progeny particles generated at 39°C (Fig. 5). This is in accordance with earlier results obtained with mutant ts 271. Reduced HN incorporation into ts 271 virus particles occurred in combination with significantly reduced NA activity at elevated temperature but without significantly reduced virus budding [30, 35]. We assume that HN incorporation into virus particles might be inhibited to the same extent that HN remains bound to sialylated cell-surface components. The receptor-cleavage function of newly synthesized HN seems to play an essential role with regard to the HN content of virus particles and consequently to the infectivity of viral progeny.
Based on our results, the two steps of HN–receptor interaction need to be interpreted in a new light: (1) HN binds very efficiently to receptors, thus leading to quantitative inhibition of receptor function, as demonstrated by superinfection protection. (2) By cleavage of a neuraminic acid residue by NA, the receptor is destroyed and, in parallel, HN is released from the complex, allowing it to be incorporated into new virus particles. This situation is thought to depend strictly on the amount of each of the two binding partners present during the viral life cycle. When, at the beginning of an infection, many receptors but only a few HN molecules are present, all of the HN should be bound to the receptors and have to be released by NA action. However, later during infection, when HN is expressed in excess, the majority of HN could follow the secretory pathway without binding to receptors. Finally, when HAd-competent HN molecules and destroyed receptors are detectable at the surface of wt infected cells, it is impossible to determine whether the HN and receptors came in contact early in their pathways or whether this interaction happened later on when receptors and HN were already inserted into the cell membrane, or even when HN was incorporated into the envelope of viral progeny.
Receptor inactivation in the absence of NA activity during infections with mutant HN-262+461 and HN-262+264+461 is a quantitative process. In order for this process to reach adequate efficiency, we conclude that it takes place soon after HN protein synthesis, before assembly of progeny virus particles. Therefore, the mechanism involved must differ from the receptor-destroying NA activity during budding and re-binding of virus particles . When functional receptors would have to be cleaved by newly assembled progeny virus as a requirement for their release from the cell, it would be difficult to explain for our mutant virus by which mechanism superinfection of cells is inhibited when NA is absent. The spread of paramyxoviruses in tissues depends on the efficient release of viral progeny from primary infected cells, leading to further cell infections. NA inhibitors are applied extracellularly to inhibit that viral spread to neighboring cells [1, 38]. When, as shown with our mutants, receptor inactivation and receptor destruction are already finished before the process of virus budding has started, the effects of antiviral drugs should be rather directed toward preventing paramyxoviral progeny from adsorption to new, uninfected cells. The principle of early receptor inactivation by intracellular HN–receptor binding—as supposed here—would allow virus particles unimpeded release from infected cells, and this would represent another example of viral evolution.
We thank A. Portner for providing anti-HN antibody S2. This work was supported by grants from the Bundesministerium für Bildung und Forschung (AZ: 0312193) and from the European Commission (QLK2-2002-01722).
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