THE JOURNAL OF BIOLOGICAL CHEMISTRY VOL. 282, NO. 1, pp. 353–363, January 5, 2007
© 2007 by The American Society for Biochemistry and Molecular Biology, Inc. Printed in the U.S.A.
Structural Characterization and Oligomerization of PB1-F2, a
Proapoptotic Influenza A Virus Protein*□
S
Received for publication, July 7, 2006, and in revised form, October 11, 2006 Published, JBC Papers in Press, October 19, 2006, DOI 10.1074/jbc.M606494200
Karsten Bruns‡§¶1, Nicole Studtrucker‡1, Alok Sharma‡¶, Torgils Fossen¶储, David Mitzner‡, André Eissmann‡,
Uwe Tessmer§, René Röder‡**, Peter Henklein**, Victor Wray¶, and Ulrich Schubert‡2
From the ‡Institute of Clinical and Molecular Virology, University of Erlangen-Nürnberg, Erlangen D-91054, Germany,
§
Heinrich-Pette-Institute, Hamburg D-20251, Germany, the ¶Department of Structural Biology, Helmholtz Centre for
Infection Research, Braunschweig D-38124, Germany, the 储Department of Chemistry, University of Bergen, N-5007 Bergen,
Norway, and the **Institute of Biochemistry, Humboldt University, Berlin D-10115, Germany
Recently, a novel 87-amino acid influenza A virus protein with
proapoptotic properties, PB1-F2, has been reported that originates from an alternative reading frame in the PB1 polymerase
gene and is encoded in most known human influenza A virus
isolates. Here we characterize the molecular structure of a biologically active synthetic version of the protein (sPB1-F2). Western blot analysis, chemical cross-linking, and NMR spectroscopy afforded direct evidence of the inherent tendency of
sPB1-F2 to undergo oligomerization mediated by two distinct
domains located in the N and C termini, respectively. CD and 1H
NMR spectroscopic analyses indicate that the stability of structured regions in the molecule clearly depends upon the hydrophobicity of the solvent. In aqueous solutions, the behavior of
sPB1-F2 is typical of a largely random coil peptide that, however, adopts ␣-helical structure upon the addition of membrane mimetics. 1H NMR analysis of three overlapping peptides afforded, for the first time, direct experimental evidence
of the presence of a C-terminal region with strong ␣-helical
propensity comprising amino acid residues Ile55–Lys85 connected via an essentially random coil structure to a much
weaker helix-like region, located in the N terminus between
residues Trp9 and Lys20. The C-terminal helix is not a true
amphipathic helix and is more compact than previously predicted. It corresponds to a positively charged region previously shown to include the mitochondrial targeting sequence
of PB1-F2. The consequences of the strong oligomerization
and helical propensities of the molecule are discussed and
used to formulate a hypothetical model of its interaction with
the mitochondrial membrane.
* This work was supported by a grant from the research network FORINGEN,
funded by the State of Bavaria, Germany, by German Human Genome
Research Project Grant IE-S08T06, and by German Research Council Grants
SFB 466-A11, SFB 643-A1, and GRKK 1071. The costs of publication of this
article were defrayed in part by the payment of page charges. This article
must therefore be hereby marked “advertisement” in accordance with 18
U.S.C. Section 1734 solely to indicate this fact.
The atomic coordinates and structure factors (code 2HN8) have been deposited
in the Protein Data Bank, Research Collaboratory for Structural Bioinformatics, Rutgers University, New Brunswick, NJ (http://www.rcsb.org/).
□
S
The on-line version of this article (available at http://www.jbc.org) contains
supplemental Fig. S1 and Table S1.
1
Both authors contributed equally to this work.
2
To whom correspondence should be addressed: Institute for Clinical and
Molecular Virology, University of Erlangen-Nürnberg, Schlossgarten 4,
D-91054 Erlangen, Germany. Tel.: 49-9131-85-26478; Fax: 49-9131-8526182; E-mail: ulrich.schubert@viro.med.uni-erlangen.de.
JANUARY 5, 2007 • VOLUME 282 • NUMBER 1
Influenza A virus (IAV)3 is one of the most common pathogens threatening humans and animals, with the potential to
cause disastrous pandemics. In the last century, it was the origin
of at least three pandemics, the most serious outbreak being the
“Spanish flu” (1918 –1919) that claimed 20 –50 million casualties worldwide (for a review, see Ref. 1). Apart from various
mammals, IAV also infects avian hosts, and particularly aquatic
birds have been shown to be the primary reservoir. Sporadically, some of these avian strains acquire the capability to infect
other mammals or humans either as a whole or more likely
upon genetic reassortment with prevailing human IAV strains.
This process termed antigenic (viral) shift appears to occur
via the pig as an intermediate host and “mixing vessel” and can
lead to new IAV subtypes of mixed surface antigens (2, 3).
The genome of IAV, a representative of the orthomyxoviruses, consists of eight separate linear segments of negative
sense RNA and was thought to encode 10 gene products. Only
very recently, while screening for major histocompatibility
complex class I epitopes derived from out-of-frame viral
polypeptides, an 11th IAV gene product, named PB1-F2, was
incidentally discovered (4). Like the two proteins M1 (matrix
protein) and M2 (ion channel) encoded on the M gene segment
and the two nonstructural proteins NS1 and NS2 encoded on
the NS gene segment, respectively, PB1-F2 was found to be
expressed as a second protein from the PB1 (RNA polymerase
basic protein 1) gene segment. In contrast to NS2 and M2,
which are derived from spliced mRNAs, PB1-F2 is the only
influenza A virus protein that originates from an alternative
(⫹1) open reading frame of the PB1 gene. PB1-F2 was characterized as an 87-amino acid residue protein and originally discovered for IAV strain A/Puerto Rico/8/34(H1N1), also termed
IAVPR8. However, whereas the pb1-f2 open reading frame was
identified in the majority of analyzed IAV subtypes, it is not
present in the influenza B virus genus (4).
A major part of IAV replication occurs in the nucleus, where
viral RNA is produced through the concerted action of three
polymerase subunits (polymerase acidic protein, PB1, and
PB2), together with the nucleoprotein. At a late stage of infection, M1 and NS2 proteins enter the nucleus, where, among
3
The abbreviations used are: IAV, influenza A virus; DSS, disuccinimidyl suberate; NOE, nuclear Overhauser enhancement; NOESY, nuclear Overhauser
enhancement spectroscopy; sPB1-F2, synthetic PB1-F2; TFE, trifluoroethanol; TOCSY, total correlation spectroscopy.
JOURNAL OF BIOLOGICAL CHEMISTRY
353
Structure and Oligomerization of Influenza A Virus PB1-F2
other functions, they induce the shutdown of viral RNA synthesis and promote the export of newly assembled cores through
the cytosol to the plasma membrane, where progeny virions
bud from the membrane (reviewed in Ref. 5). IAV infection
generally activates several host cell antiviral mechanisms that
are in part counteracted by accessory IAV proteins, like the NS1
protein that is involved in the inhibition of type I interferon
response (6, 7). PB1-F2 appears to represent another tool by
which IAV regulates the host’s immune response to virus infection
(4). It is assumed that PB1-F2 removes host immune cells responding to IAV infection either by functioning as an endogenously
expressed apoptosis stimulator in infected cells or in an exogenous
form when the protein is released from infected cells or from disintegrated virus particles similar to the function of the proapoptotic human immunodeficiency virus-1 protein Vpr (8, 9).
With the goal of understanding the molecular mechanism
involved in the biological function of the regulatory IAV protein PB1-F2, we describe here the first structural characterization of the molecule derived from the IAVPR8 isolate. Although
the molecule investigated exhibits a high degree of flexibility in
pure aqueous environment, PB1-F2 adopts extended ␣-helical
structures in the presence of organic solvents that mimic the
membrane environment. According to high resolution NMR
data, PB1-F2 consists of two independent structural domains,
two closely neighboring short helices at the N terminus, and an
extended C-terminal helix. Both helical domains are connected
by a flexible and unstructured hinge region. Furthermore, we
observed that the PB1-F2 molecule has an intrinsic strong propensity to form oligomeric structures, a characteristic that supports the recent observation that the molecule can form membrane pores in planar lipid bilayers (10). The major
oligomerization domain is located in the C-terminal helix,
whereas both N- and C-terminal domains exhibit separate oligomerization capacity.
EXPERIMENTAL PROCEDURES
Peptide Synthesis and Purification—The synthesis, purification, and molecular characterization of sPB1-F2 and the three
related fragments PB-(1– 40), PB-(30 –70), and PB-(50 – 87)
derived from influenza A virus strain A/Puerto Rico/8/34(H1N1)
(isolate IAVPR8) (4) are described in detail elsewhere (11).
CD Spectroscopy—CD spectra of the protein and related peptides were recorded at room temperature and a concentration
of 0.2 mg/ml in 0.5-mm cuvettes on a Jasco J-810 spectropolarimeter in a wavelength range from 260 to 180 nm at various
TFE concentrations as described previously (8). The resulting
curves were smoothed using a high frequency filter, and secondary structure elements were quantified by deconvoluting
the measured ellipticity using the DICROPROT 2000 program.
1
H NMR Spectroscopy—One- and two-dimensional 1H NMR
spectra were recorded at various temperatures between 293
and 323 K on a Bruker Avance DMX 600 NMR spectrometer
using a triple resonance probe head with a gradient unit.
sPB1-F2 was dissolved at a concentration of 1 mM (10 mg/ml)
without pH adjustment in 90% H2O, 10% D2O, and in 50 and
90% aqueous TFE-d2 to give final volumes of 600 l. Spectra of
the fragments, PB-(1– 40), PB-(30 –70), and PB-(50 – 87), were
recorded in 50% aqueous TFE-d2 at 300 K of 2 mM solutions.
354 JOURNAL OF BIOLOGICAL CHEMISTRY
Spectra were referenced to either the water signal or to the
residual TFE-d2 signal at 3.95 ppm. Two-dimensional measurements without spinning were accumulated with mixing times of
110 ms for the TOCSY and 250 ms for the NOESY spectra, respectively. Spectra were processed on a Silicon Graphics INDY work
station using XWIN-NMR 1.3. The percentages of the proline cisisomer content were determined from comparison of resolved signal intensities in the spectra of PB-(30–70) and PB-(50– 87) and
the small 10-mer peptides PB-(3–12) and PB-(23–32).
The unambiguous amino acid spin systems, sequential
assignments, and final nuclear Overhauser enhancements
(NOEs) of the three fragments were established using a standard procedure (12) that has been used by us previously (13). The
complete signal assignments and 1H chemical shifts of PB-(1–
40), PB-(30 –70), and PB-(50 – 87) have been deposited in the
Biological Magnetic Resonance Data Bank under accession
numbers 7289, 7290, and 7258, respectively.
The volumes of the integrated cross-peaks from the NOESY
spectrum with a mixing time of 250 ms of PB-(50 – 87) were
determined and converted to interproton distances by calibration against the side chain Gln or Asn amide protons (0.19 nm)
using the AURELIA 2.7.9 program (14). Structures were then
generated using the standard protocol embodied in the CNSsolve 1.0 software package starting from an extended peptide
backbone as described previously (13). The 20 structures with
the lowest energy terms were chosen for the final analysis.
Structure fitting criteria were objectively derived using a consecutive segment approach described by us previously (15).
Final structures were displayed and manipulated on an Silicon
Graphics OCTANE-work station using the program BRAGI
(16). Structure superposition was performed with the same
program and r.m.s. deviations for the regions of interest were
calculated using LSQMAN (Uppsala Software Factory). The
final structure of PB-(50 – 87) has been deposited in the Protein
Data Bank under code 2HN8 and RCSB ID RCSB038537.
Chemical Cross-linking of sPB1-F2 and Detection by Western
Blotting—For chemical cross-linking, sPB1-F2 and the overlapping fragments PB-(1– 40), PB-(30 –70), and PB-(50 – 87) were
incubated at room temperature in phosphate-buffered saline,
usually at a final protein concentration of 5 g/ml, with varying
concentrations of different cross-linkers: bis(sulfosuccinimidyl)suberate (Pierce), ethylene glycol disuccinate di(N-succinimidyl)ester (Pierce), glutaraldehyde (Pierce), and disuccinimidyl suberate (DSS) (Pierce). After 30 min, the cross-linking
reaction was terminated by the addition of glycine and 10 l of
SDS sample buffer (2% SDS, 1% -mercaptoethanol, 10% glycerol in 65 mM Tris/HCl, pH 6.8). The samples were denatured
(5 min, 95 °C) and subjected to electrophoresis on a 12% SDSPAGE. Following electrotransfer onto nitrocellulose membranes, proteins were stained by Western blotting using antisera (anti-FL) raised in rabbits against the full-length molecule
sPB1-F2 as described previously (11). To follow the oligomerization of sPB1-F2 by Coomassie staining, the peptide was incubated at room temperature in PBS to a final protein concentration of 250 g/ml. DSS was added at a 2- or 20-fold molar ratio,
respectively. After 30 min, the reaction was quenched using
glycine at a final concentration of 25 mM. The cross-linking
samples were boiled in SDS buffer (0.2% SDS, 10% glycerol, 65
VOLUME 282 • NUMBER 1 • JANUARY 5, 2007
Structure and Oligomerization of Influenza A Virus PB1-F2
FIGURE 1. Structural predictions of PB1-F2 and synthetic peptides used.
Secondary structure prediction for PB1-F2 with the sequence MGQEQDTPWI11LSTGHISTQK21RQDGQQTPKL31EHRNSTRLMG41HCQKTMNQVV51MPKQIVYWKQ61WLSLRNPILV71FLKTRVLKRW81RLFSKHE derived from the IAV strain
A/Puerto Rico/8/34(H1N1) and the three synthetic fragments used in this
study is shown.
mM Tris/HCl, pH 6.8, with or without 5% -mercaptoethanol
for 5 min, at 55 °C, and separated by electrophoresis in a 15%
SDS-PAGE. After Coomassie staining (0.5% Coomassie Brilliant Blue G-250, 10% acetic acid, 25% isopropyl alcohol), the
gel was destained (25% methanol, 10% acetic acid), and processed for imaging.
RESULTS
sPB1-F2 Has a Strongly Environmentally Dependent Secondary Structure—As a prerequisite for structural and functional
studies on the small IAV regulatory protein PB1-F2, we have
established solid phase peptide synthesis protocols for the production of milligram amounts of full-length synthetic (s) peptide, sPB1-F2, and several fragments thereof on a routine basis
in highly pure and biologically active form (4, 10, 11). The
sequence of the sPB1-F2 molecule used in the present investigation corresponds to the strain IAVPR8 (4, 11). Although relatively small quantities of PB1-F2 have been produced by recombinant methods as a GST fusion protein (17), large scale
production of recombinant PB1-F2 sufficient for structural
studies is difficult both because of its inherent tendency for
aggregation and interactions with hydrophobic components of
the producer cell as well as its cytotoxicity causing altogether
low expression levels. Here we have used our synthetic material
to investigate the oligomerization and structure of PB1-F2.
Based on secondary structure prediction, the molecule was subdivided into three similarly sized domains, and three overlapping fragments were synthesized, comprising the 40 N-terminal residues (PB-(1– 40)), the central residues (PB-(30 –70)),
and the 38 C-terminal residues (PB-(50 – 87)) (11). Although no
clear structure was calculated for the N terminus, strong helical
regions were predicted for the central and particularly the
C-terminal domain (11, 18), as shown in Fig. 1.
Self-association of sPB1-F2 Is Regulated by Disulfide Bond
Formation and by Two Distinct Oligomerization Domains—
The first evidence for self-association of sPB1-F2 originates
from our previous studies demonstrating oligomers of sPB1-F2,
or the viral counterpart expressed in IAVPR8-infected cells, that
were detected without any chemical fixation even under denaturating conditions of the SDS-PAGE (11). Further, it was
shown that sPB1-F2 induces pore formation in planar lipid
bilayers, a characteristic of membrane-interacting proteins that
tend to form oligomeric structures (10). Direct evidence for the
existence of oligomeric structures of sPB1-F2 is now provided
by chemical cross-linking. In a first set of experiments, the peptide was exposed to various chemical cross-linkers, which
clearly resulted in the fixation of a ladder of high molecular
weight complexes with pronounced signals in the molecular
JANUARY 5, 2007 • VOLUME 282 • NUMBER 1
weight range of dimers to pentamers. In Fig. 2A, the results are
shown for exposure of sPB1-F2 to increasing concentrations,
ranging from 10⫺3- to 103-fold molar excess, of the cross-linking reagents bis(sulfosuccinimidyl)suberate, ethylene glycol
disuccinate di(N-succinimidyl)ester, glutaraldehyde, and DSS.
The most effective stabilization of oligomers was achieved with
DSS and bis(sulfosuccinimidyl)suberate, where trimers were
stabilized starting at a 10⫺1-fold molar excess of the cross-linking reagent, whereas dimers were observed for all cross-linkers
used, even at their lowest concentration.
Next, we investigated the oligomerization of individual fragments of sPB1-F2. According to secondary structure prediction, the N-terminal ⬃40 residues are mainly random coil,
whereas the C terminus has a high propensity for ␣-helix formation that should support protein interactions (Fig. 1).
Indeed, we found that the C-terminal fragment PB-(50 – 87)
displayed the highest capacity to form oligomeric structures
when compared with the N-terminal fragment PB-(1– 40).
First, titration experiments similar to that shown for full-length
sPB1-F2 (Fig. 2A) revealed oligomeric forms of PB-(1– 40)
starting at a 102-fold molar excess of DSS, whereas the oligomerization of PB-(50 – 87) was observed already at a 10-fold
molar ratio (Fig. 2B). The formation of dimers (marked with an
asterisk) was much more pronounced even at the lowest concentration of DSS for PB-(50 – 87) compared with PB-(1– 40)
(Fig. 2B). Further, using 1-molar excess DSS ratios, oligomers of
PB-(50– 87) were detected already at 100 ng of the peptide,
whereas 400 ng of PB-(1–40) were required per cross-linking reaction in order to stabilize a similar pattern of oligomers (Fig. 2C).
Similar cross-linking analyses were also conducted with the
middle fragment, PB-(30 –70). Although this fragment contains
only one cysteine residue at position 42 and has the inherent
capacity to form disulfide-linked dimers, it does not exhibit
significant oligomerization capacity compared with the N- and
C-terminal fragments (data not shown). Thus, the self-association of sPB1-F2 is mediated by both the N- and C-terminal
domains, with the C-terminal domain showing a higher propensity for oligomerization than the N-terminal domain.
In an additional set of cross-linking experiments, we investigated the interaction of individual domains of sPB1-F2 with the
full-length molecule. Increasing concentrations of PB-(1– 40)
(Fig. 2D) or PB-(50 – 87) (Fig. 2E) were mixed with 100 ng of
sPB1-F2 and subjected to the cross-linking reaction with an
equimolar ratio of DSS with respect to sPB1-F2. Most strikingly, both the N-terminal and the C-terminal fragments
caused significant changes in the pattern of the sPB1-F2 oligomers. In addition to the monomeric, dimeric, and trimeric
forms of sPB1-F2 migrating at ⬃11, ⬃23, and 34 kDa (Fig. 2, D
and E, marked with an asterisk), hetero-oligomeric adducts of
the full-length sPB1-F2 and the N- and C-terminal fragments
were detected (Fig. 2, D and E, marked with arrows). The intensities of these hetero-oligomers clearly increased with higher
concentration of the fragments PB-(1– 40) or PB-(50 – 87)
added to the cross-linking reactions (Fig. 2, D and E). In the case
of the C-terminal fragment, the maximum formation of heterooligomers, consisting of sPB1-F2 and PB-(50 – 87), already
occurred at 200 ng of PB-(50 – 87) (Fig. 2E), whereas ⬃5-fold
more of the N-terminal fragment PB-(1– 40) was required to
JOURNAL OF BIOLOGICAL CHEMISTRY
355
Structure and Oligomerization of Influenza A Virus PB1-F2
FIGURE 2. Oligomerization of PB1-F2. A, 100 ng of sPB1-F2 was subjected to cross-linking with increasing concentrations of bis(sulfosuccinimidyl)suberate (BS3),
ethylene glycol disuccinate di(N-succinimidyl)ester (EGS), glutaraldehyde (GA), and DSS, ranging from 103- to 10⫺3-fold molar excess (lanes a– g). Half of each crosslinking reaction was resolved in 12% SDS-PAGE, transferred to nitrocellulose membrane, and stained with anti-FL antibodies. B, N- and C-terminal fragments, PB-(1– 40)
and PB-(50 – 87), were cross-linked with varying concentrations of DSS as in A and detected by Western blot using anti-N for PB-(1– 40) and anti-FL for PB-(50 – 87). In
the lower panel of the PB-(50 – 87) section, 50 ng of peptide was separated per lane, whereas 25 ng of peptide was separated in all other lanes in B. It should be noted
that at the highest cross-linker concentrations, extremely high molecular weight complexes are formed that cannot be further resolved in the gel system, thus
reducing the detection of the cross-linked peptides in the high molecular weight range. C, 0.1–1 g of PB-(1– 40) or PB-(50 – 87) was cross-linked with one molar excess
of DSS, resolved in a 12% SDS-PAGE, and stained in Western blot as for B. Increasing concentrations of PB-(1–40) (D) or PB-(50–87) (E) were mixed with 100 ng of sPB1-F2 and
subjectedtothecross-linkingreactionwithanequimolarratioofDSSandstainedinWesternblotwithanti-FL.Evidenceofhetero-oligomersformedbetweensPB1-F2andthe
fragments are marked by arrows. Monomeric, dimeric, and trimeric forms of sPB1-F2 are marked with asterisks. F, 100 ng of sPB1-F2 were treated with a 2-fold molar excess of
dithiothreitol (DTT) and then subjected to the cross-linking reaction with an equimolar ratio of DSS, resolved in 12% SDS-PAGE, and stained in Western blot with anti-FL. For
control, the peptide solution was cross-linked without prior dithiothreitol treatment. G, 2.5 g of sPB1-F2 were cross-linked with 2- or 20-fold molar excess of DSS, resolved in
15% SDS-PAGE under reducing and nonreducing conditions, and stained with Coomassie Blue. ME, -mercaptoethanol.
356 JOURNAL OF BIOLOGICAL CHEMISTRY
VOLUME 282 • NUMBER 1 • JANUARY 5, 2007
Structure and Oligomerization of Influenza A Virus PB1-F2
mation of trimers and tetramers was
slightly decreased under reducing
conditions (Fig. 2F).
In a further set of confirmatory
cross-linking studies, we followed
the oligomerization of sPB1-F2
directly by staining the peptide in
SDS-PAGE (Fig. 2G) as opposed to
using antibody reactions. In contrast to the detection of oligomers of
sPB1-F2 by Western blot (Fig. 2A),
approximately a 100-fold higher
concentration of the peptide was
necessary for each cross-linking
reaction in order to allow detection
by Coomassie Blue staining. Nevertheless, a similar pattern of oligomers was detected, using various
molar ratios of the cross-linking
reagent DSS, when compared with
those found above using the more
sensitive Western blot analysis, suggesting that most of the possible oligomeric structures were reactive
with the antibodies used in the
above experiments (Fig. 2A).
Clearly, at a 20-fold molar excess of
DSS, high order oligomers of sPB-F2
were
stabilized, most of which were
1
1
FIGURE 3. H NMR spectral changes under various solution conditions. The H NMR spectra of sPB1-F2 are
shown. The low field region of the one-dimensional 1H spectra in aqueous solution containing 0, 50, and 90% barely separated in the higher
TFE-d2 at 323 K is shown.
molecular weight range of the SDSPAGE. In gels lacking -mercaptoachieve the same intense hetero-oligomerization (Fig. 2D), fur- ethanol, sPB1-F2 forms stable dimers even in the absence of
ther supporting the notion that the strongest oligomerization cross-linkers (Fig. 2G). Also, the extent of stabilization of
domain is located within the C-terminal region of sPB1-F2.
dimers by cross-linking was more evident when the cross-linkIn order to try to locate more specifically which residues are ing reaction was resolved in the absence of reducing reagent,
the underlying cause of this phenomenon, we have used the indicating that at least dimeric forms of sPB1-F2 were stabilized
statistical mechanics algorithm TANGO, which identifies by disulfide bonds. In summary, our comprehensive cross-linkaggregation-prone regions of peptides and denatured proteins ing data provide compelling evidence that sPB1-F2 is a moleusing a set of balanced physico-chemical parameters (19, 20). cule with an unusually high propensity for oligomerization that
According to the TANGO algorithm, a score of ⱕ0.02% indi- in addition is capable of forming a disulfide-linked dimer. It has
cates no aggregation, 0.02–5.0% indicates moderate aggrega- two distinct oligomerizing domains, with the most efficient one
tion, and ⱖ5.0% indicates high aggregation propensities. The being located in the C-terminal half of the molecule, that can be
application of this program predicted two regions of five resi- attributed to specific regions in the molecule. Both oligomerizing
dues populating the oligomerization state to more than 5% per domains can form independent homo-oligomers when shorter
residue, 54 –58 (1.34 –9.83% per residue) and 68 –72 (93.01– peptide fragments of sPB1-F2 are present and have the ability to
97.25% per residue) under variable conditions. A further oli- form hetero-oligomers with the full-length molecule sPB1-F2.
gomerization domain was predicted with much lower scores
Secondary Structure in sPB1-F2 Is Essentially Localized in the
(1.38 –1.36% per residue) for the N-terminal region extending C-terminal Domain and Is Dependent on Solution Conditions—
from residue 9 to 13. Thus, there is a good correlation between the Although no structure was calculated for the N terminus, the
predicted regions and the trends in the experimental cross-linking helical regions were predicted for both the central and the
data with specific 5-residue regions being predicted to be respon- C-terminal domains (11, 18) (Fig. 1). To analyze the impact of
sible for the differences in the oligomerization behavior.
the solvent conditions on the folding of the molecule, a considFurther, to analyze the potential of disulfide bridge forma- erable number of one- and two-dimensional 1H NMR spectra
tion by the single cysteine residue in position 42 of sPB1-F2, the of 1 mM solutions of sPB1-F2 were recorded in both pure aquepeptide was studied in the presence of 1 mM dithiothreitol and ous and aqueous TFE-d2 containing solutions at temperatures
subjected to the cross-linking reaction. As demonstrated in Fig. varying between 293 and 323 K (Fig. 3). TFE-d2 was chosen,
2F, the same pattern of oligomers was observed, albeit the for- since it not only functions as a membrane mimetic but also
JANUARY 5, 2007 • VOLUME 282 • NUMBER 1
JOURNAL OF BIOLOGICAL CHEMISTRY
357
Structure and Oligomerization of Influenza A Virus PB1-F2
content up to 90% (Fig. 3C) again
affects the dispersion of the signals
but also appears to lead to poorer
resolution, particularly apparent for
the signals at the low field edge of
the envelope. The fact that the
intensities, widths, and positions of
the four tryptophan signals are
strongly dependent on the solution
conditions was also confirmed for
the same set of solutions at 300 K
(data not shown). Thus, the evidence of these NMR experiments
(Fig. 3) are consistent with the
assumption that sPB1-F2 exhibits a
high tendency for self-association.
In order to obtain experimental evidence for the nature of the structure
present in sPB1-F2, we investigated
the folding of the molecule and its
fragments by CD spectroscopy
under different solution conditions.
When sPB1-F2 was initially analyzed in pure water, the spectrum
showed little evidence of stable secondary structure formation, and
deconvolution resulted in only 7%
helical content (Fig. 4, A and E).
However, upon the addition of 20%
TFE and even more pronounced at
50% TFE, there was a substantial
change in the shape of the CD
FIGURE 4. Environmental dependence of secondary structure formation in sPB1-F2. Far-UV CD spectra of curves showing negative ellipticities
sPB1-F2 (A) and related overlapping fragments PB-(1– 40) (B), PB-(30 –70) (C), and PB-(50 – 87) (D) were recorded
at 221 and 207 nm and a strong posin pure water and in 20 and 50% TFE. E, percentage helical content of the various solutions.
itive band at 192 nm (Fig. 4A), indicating the presence of significant
usually suppresses intermolecular interactions that support oli- amounts of helical structure upon deconvolution (Fig. 4E).
gomerization and hence affords better resolved NMR spectra Thus, consistent with the one-dimensional NMR experiments
(21). Initially, one-dimensional 1H NMR spectra of the aro- (Fig. 3), the CD measurements demonstrate that the solution
matic and NH region were recorded at 323 K for 0, 50, and 90% conditions can profoundly affect the folding of sPB1-F2; the
aqueous TFE-d2 solutions of sPB1-F2 (Fig. 3). When sPB1-F2 peptide is almost completely in the random coil conformation
was analyzed in water alone (Fig. 3A), broad poorly resolved in pure aqueous environment, whereas adding a membrane
signals were observed, with a limited dispersion of the back- mimetic, such as TFE or phospholipids (see below and Fig. 1 of
bone NH signals between 8.6 and 7.2 ppm that are, altogether, the supplemental data), strongly stabilizes secondary structure
characteristic of an oligomeric and random coil peptide confor- that is mainly ␣-helical in character. TFE is known to favor
mation. The indole 1NH signals of the aromatic side chains of intramolecular interactions and therefore stabilizes helix forthe tryptophan residues appear as unresolved signals centered mation only in those parts of a protein that have the inherent
at 10.0 ppm, and similarly broad signals are observed for the propensity to adopt helical structures (21).
carbon-bound side chain protons of the aromatic residues trypA similar set of spectra was recorded for the three overlaptophan, phenylalanine, tyrosine, and histidine between 7.7 and ping peptide fragments (Fig. 4, B–D), and quantitative esti7.2 ppm. The addition of 50% TFE-d2 (Fig. 3B), however, mates of the corresponding ␣-helical contents were deterimproves the resolution of all signals and affords an increased mined in TFE solutions (Fig. 4E). Similar qualitative changes in
dispersion of the signals in the region 8.7 to 6.2 ppm, providing the CD curves are observed for PB-(50 – 87) in phospholipid
evidence of a significant decrease in self-association. In the solutions (supplemental Fig. 1), indicating that helical secondpresence of 50% TFE-d2, the best resolved signals in this region ary structure is also stabilized under these conditions that
are those of the aromatic side chains and four distinct signals mimic the membrane hydrophobic environment.
characteristic of the indole 1NH group of tryptophan residues
The C-terminal fragment, PB-(50 – 87), shows the largest
between 9.8 and 9.5 ppm. A further increase in the TFE-d2 helical content, which changes little upon going from 20 to 50%
358 JOURNAL OF BIOLOGICAL CHEMISTRY
VOLUME 282 • NUMBER 1 • JANUARY 5, 2007
Structure and Oligomerization of Influenza A Virus PB1-F2
TFE. The central fragment, PB-(30 –70), shows a much smaller
helical content that is more susceptible to the amount of TFE
present, whereas the N-terminal fragment, PB-(1– 40), has only
a minor helical content even at the highest TFE level. Thus, the
CD data indicate that the major helical structure is concentrated in the C-terminal region of the molecule, which is consistent with the previous calculations where the major secondary structure was predicted for the C-terminal domain of
PB1-F2 (11, 18). However, unlike the predicted structures, the
CD data indicate that a minor helical region might be present in
the very N terminus and that, furthermore, the secondary
structure of PB1-F2 is extremely sensitive to the environment
and will only be stabilized under suitable membranous solution
conditions.
Identification of Structural Elements in PB-(1–40), PB-(30–70),
and PB-(50– 87) by 1H NMR Spectroscopic Characterization—It is
unlikely that structural details of full-length sPB1-F2, 87 amino
acids in length, can be enumerated at the atomic level using homonuclear 1H NMR techniques at the field strengths currently available. Clearly, signal overlap, evident in Fig. 3A or from preliminary
two-dimensional 1H TOCSY spectra conducted on sPB1-F2
recently (11), will prevent unambiguous signal assignments. Such a
study of the full-length molecule would require heteronuclear
NMR approaches. However, recombinant PB1-F2 with uniform
13
C/15N labeling has not been produced as yet, but the availability
of the three moderately sized overlapping fragments PB-(1–40),
PB-(30–70), and PB-(50– 87) allowed us to probe structural
details using two-dimensional 1H NMR techniques.
According to the preliminary one-dimensional NMR and CD
analyses of the full-length molecule, the best resolved NMR
spectra were obtained in 50% TFE-d2, which also corresponds
to conditions showing the most structured and least oligomerized state of the peptide. Indeed, dynamic light scattering data
indicate that all of the molecules investigated were monomeric
under these conditions (data not shown). Detailed analyses of
the two-dimensional 1H TOCSY and NOESY NMR spectra of
three overlapping fragments of sPB1-F2 in 50% TFE-d2 at 300 K
and pH ⬃3 afforded complete assignments of all amino acid
spin systems in each of the peptides PB-(1– 40), PB-(30 –70),
and PB-(50 – 87) investigated. Qualitative information about
the nature and position of secondary structure for such molecules in aqueous solution is readily deducible from the ␣-proton chemical shifts, since upfield shifts of these occurring in
four adjacent residues relative to the random coil values (12) are
indicative of local helical structure, whereas the downfield shift
of three adjacent residues is indicative of -sheets (22). In the
present case, the 1H chemical shift differences experimentally
obtained for 50% TFE-d2 solutions of each of the fragments are
shown in Fig. 5, A–C, whereas values for the full-length molecule (Fig. 5D) were derived by combining the shifts of the individual fragments with averaging in the overlapping regions
Leu30–Gly40 and Val50–Val70, respectively. The data clearly
imply that sPB1-F2 has a long stretch of continuous helical secondary structure located in the C-terminal section of the molecule between residues Lys53 and Ser84. In contrast, the N
terminus appears to have two short, weak helical regions
(Trp9–Thr13, Ile16–Lys20), each of approximately five residues
in length, that were not predicted empirically (11, 18). FurtherJANUARY 5, 2007 • VOLUME 282 • NUMBER 1
more, there is no evidence of any secondary structure in the
region between residues Arg37 and Gln48 that was previously
predicted for high propensity of helix formation (11, 18) and
that is experimentally part of the unstructured central section
Arg21 to Met51 of the molecule (Fig. 5E).
Further noticeable features in Fig. 5 are the unusual low field
shifts of the ␣-protons of residues Thr27, Met51, and Asn66, all
of which precede proline residues in the sequence. We have
noted this phenomenon previously in similar NMR experiments during the study of cis/trans peptidyl-prolyl isomerism
in proline residues located in the N-terminal region of the
human immunodeficiency virus-1 accessory protein Vpr (13).
In these analyses, it was observed that proline substitution in
the trans-conformation causes an inherent downfield shift of
the ␣-proton belonging to the adjacent preceding residue in the
sequence of ⫹0.28 ⫾ 0.1 ppm and smaller shifts of ⫹0.08 ⫾ 0.03
ppm for these two residues toward the N terminus (13). Furthermore, this phenomenon occurs independently of the type
of secondary structure in the vicinity of proline residues (13).
Such effects clearly rationalize the shifts observed here for residues Thr27 and Met51 and imply that Asn66 should exhibit a
more negative shift difference. Taking this into account, the
C-terminal helix appears to be almost continuous without any
pronounced break.
Solution Structure of PB-(50 – 87)—Finally, we have determined the high resolution structure of the long C-terminal
helix using the NOE data of PB-(50 – 87) (Fig. 6A). Quantitative
NOE data derived from spectra recorded for PB-(50 – 87) in
50% TFE-d2 were used as distance constraints in molecular
dynamics/energy minimization calculations using a standard
protocol (23).
A total of 754 distance constraints from 373 intraresidue, 192
sequential, and 189 medium range NOEs, which are evenly distributed throughout the molecule (Fig. 6B), were used to generate 100 conformations. The 20 conformations with the lowest
NOE (ENOE ⫽ 237.0 ⫾ 5.4 kJ/mol) and total energies (Etotal ⫽
739.6 ⫾ 6.3 kJ/mol) and showing no constraint violations
greater than 0.2 Å were used for the final fitting analysis (see
supplemental Table 1). As we have shown previously, the identity and heterogeneity within a final set of molecular conformations can be visualized using the consecutive segment
approach. This method provides a relative measure of how well
the backbone atom positions for each amino acid are defined in
all of the final structures and thereby allows the determination
of an appropriate fitting region (15). Consequently, such a comparison provides an objective method for the recognition of
stable structural elements in the ensemble of final structures,
since the lower the mean root mean square deviations are, the
more similar are the conformations in the final structures. Such
an analysis (Fig. 6C) showed that the best defined region of the
molecule, with the lowest root mean square deviation (⬍0.2 Å),
is located between and includes residues Ile55–Lys85, which
corresponds to a well defined ␣-helix, as shown by superposition of the finally refined structures (Fig. 7).
In summary, the CD data for both the intact molecule and its
three overlapping fragments combined with the qualitative and
quantitative NMR data obtained for the three fragments indicate that sPB1-F2 requires the presence of a hydrophobic enviJOURNAL OF BIOLOGICAL CHEMISTRY
359
Structure and Oligomerization of Influenza A Virus PB1-F2
FIGURE 5. Localization of secondary structures in sPB1-F2. Shown are 1H chemical shift differences of the ␣-protons between the experimental values and
those for residues in a random coil for PB-(1– 40) (A), PB-(30 –70) (B), PB-(50 – 87) (C), and the combined data (D), where the average values have been taken for
the overlapping positions. E, final structural model of PB1-F2 in 50% TFE solution.
360 JOURNAL OF BIOLOGICAL CHEMISTRY
VOLUME 282 • NUMBER 1 • JANUARY 5, 2007
Structure and Oligomerization of Influenza A Virus PB1-F2
FIGURE 7. Structure of the C-terminal helix of PB1-F2. Superposition of the
20 best final refined structures after alignment of the backbone atoms of
residues Ile55 to Lys85 in PB-(50 – 87).
FIGURE 6. Structure of the C-terminal fragment PB-(50 – 87) in 50% TFE
from quantitative 1H NOE data. A, summary of the observed short and
medium range NOEs for PB-(50 – 87) in 50% TFE at 300 K. B, number of NOEs
against the sequence. C, mean r.m.s. deviations for the backbone atoms of
PB-(50 – 87) in each residue, calculated using a consecutive segment method
that averages the differences for segments 2–5 residues in length, plotted
against the residue number for the 20 final structures in 50% TFE.
ronment to adopt structured domains. Under such conditions,
there is strong circumstantial evidence that the molecule consists of a two-domain structure (Fig. 5E) with a relatively stable
31–32-residue helical structure at the C terminus (Fig. 7) connected by an unstructured central region to the N terminus,
which contains very little structure apart from a section with
two weak and neighboring helical regions, each 5 residues in
length.
DISCUSSION
Originally, the proapoptotic PB1-F2 protein was serendipitously discovered as an 87-amino acid protein encoded by a
JANUARY 5, 2007 • VOLUME 282 • NUMBER 1
cryptic open reading frame in the PB1 gene of the IAVPR8 isolate (4). Due to the very recent discovery of the protein, the
evolution and function of the PB1-F2 protein are not fully
understood yet, and several aspects are still under debate.
Although the protein has originally been described to induce
apoptosis, it has now been shown that PB1-F2 more likely acts
as an apoptosis promoter in concert with other apoptosis-inducing agents (4, 17). The finding that PB1-F2 is under positive
selection pressure among highly pathogenic IAVs of the H5N1
lineage has been questioned recently (24, 25). However, in vivo
data in mice infected with virus mutants lacking PB1-F2 indicate that the protein may play a critical role in IAV-induced
apoptosis (26). The ongoing discussion about PB1-F2 function
highlights the need to understand the structural behavior of
this novel protein. In consideration of the potential role of
PB1-F2 in IAV pathogenesis, particularly its apoptosis-promoting activities on mitochondria (4, 17, 18, 27), we sought to
investigate the molecular characteristics of this small regulatory protein.
The first insight into the structure-function correlation of
PB1-F2 domains stems from recent mutagenesis studies using
GFP-PB1-F2 fusion proteins that mapped the inner mitochondrial membrane localization signal to a possible putative
amphipathic and positively charged helix located near the C
terminus of PB1-F2 (18). However, no structural investigation
on PB1-F2 has been reported so far.
Without direct experimental evidence, we and other groups
have applied a number of different algorithms to predict the
secondary structure in PB1-F2 (11, 18). These predictions for
the IAVPR8 isolate reveal a 9 –20-residue-long C-terminal helix
that in all algorithms is concluded at residue 83, a shorter central helix in the region of residues 37– 48 with a maximum
length of 12 residues, and a third helix of approximately the
same size as the latter centered on residue 58 (summarized in
Fig. 1). Clearly, all of these programs predict the molecule to be
divided essentially into two approximately equally sized
domains, corresponding to an N-terminal domain that shows
little secondary structure and a C-terminal domain that should
consist of pronounced ␣-helical structure. Such predictions are
limited, however, since any environmental dependence is not
taken into account.
As a small membrane-interacting proapoptotic protein,
recombinant PB1-F2 would be complicated to produce in
the large quantities required for spectroscopic analyses. For
molecular analysis, sPB1-F2 was completely synthesized as a
functional entity that exhibits various biological phenomena
that were also observed for its virally expressed counterpart
(11). Following microinjection, it localizes to mitochondria,
where it induces morphological alterations and causes cell
JOURNAL OF BIOLOGICAL CHEMISTRY
361
Structure and Oligomerization of Influenza A Virus PB1-F2
dues, as surmised previously from
sequence predictions (18), and two
differently charged surfaces as
shown in Fig. 8. Furthermore, there
is a relatively high number of positively charged side chains and tryptophan residues located within the
C-terminal helical region; within
this 38-residue domain, a total of 10
positive charges are found, with a
clustering of six in the region
72– 85. The three tryptophan residues at positions 58, 61, and 80 are
positioned on one surface of the
helix, with the majority of the positively charged residues on the opposite surface. In a cellular membrane,
such a distribution of residues
favors an in-plane orientation of the
helix through electrostatic interacFIGURE 8. Model based on the wheel projection of the C-terminal helix. A, primary amino acid sequence of tion of the positively charged surthe experimentally determined C-terminal helix (residues 53– 85) of PB1-F2 protein from the IAVPR8 isolate face of the helix with the negatively
showing hydrophobic and hydrophilic residues in blue and red. Plus and minus signs, positively and negatively
charged amino acids. MTS, mitochondrial targeting sequence. F, TANGO-predicted high aggregation propen- charged surface of the membrane
sity residues. B, helical wheel representation of the C-terminal fragment showing the experimentally deter- (Fig. 8). Although the helix is potenmined helical region under hydrophobic conditions. The proposed pseudoamphipathic helix can be divided
into upper hydrophobic and lower hydrophilic surfaces, as shown by the dotted line. It is assumed that the tially long enough to span a lipid
bilayer in trans, the charge distribulower hydrophilic, relatively more positively charged surface would interact with the membrane.
tion would disfavor such a trans
death (4). It also induces transmembrane conductance of membrane orientation. Hence, under these conditions, PB1-F2
planar lipid bilayers and exhibits a behavior similar to other would adopt a C-terminal ␣-helix that anchors the molecule in
proapoptotic proteins (10). From this, it is legitimate to the plane of the membrane. However, our helical wheel repreassume that the molecular characteristics of the synthetic sentation reveals that the helix is not truly amphipathic in
peptide sPB1-F2 are comparable with those of its viral nature but has a unique, biased distribution of hydrophilic and
counterpart.
hydrophobic residues, which finally results in two distinct surThe high occurrence of cationic amino acids together with faces (Fig. 8B).
In such an in-plane orientation, the six positively charged
␣-helical structure within the C-terminal region suggests a
model of the entire molecule that is partially amphipathic in residues are oriented toward the membrane with the three
character. Such molecules typically form helical structures tryptophan side chains and one phenylalanine (residue 83)
only in a hydrophobic environment that is encountered bio- exposed as two pairs of aromatic residues (Trp58–Trp61,
logically in lipid membranes or when bound to the hydro- Trp80–Phe83) on adjacent turns toward each end of the helix.
phobic patches of interacting proteins and can be stimulated Presumably, any intermolecular interaction involving this
experimentally with solutions of organic solvents or lipids region of the membrane-associated PB1-F2 must occur
(21). Indeed, the experimental CD and NMR spectroscopic through interaction of the exposed hydrophobic surface.
data clearly demonstrate the structural variability of PB1-F2 Residues predicted to be responsible for oligomerization in
and its ready adaptability to solution conditions. In its most the C-terminal domain (Fig. 8) are distributed over the surstructured form in the model hydrophobic environment of face of the helix but only partially buried through interaction
50% TFE, the molecule shows a C-terminal ␣-helix ⬃32 res- with the membrane. However, even in this anchored
idues in length bound to an essentially unstructured N ter- arrangement, the N-terminal domain of PB1-F2 would still
minus apart from a region with relatively weak helical pro- be unstructured, apart from a potential short helical section,
pensity (residues 9 –20). The experimentally observed and thus freely available for further inter- and intramolecuC-terminal helix is shorter than the combined three empir- lar interactions.
Cross-linking and NMR experiments revealed a strong
ically predicted helices and is terminated at its N terminus by
proline 52. These helical structures gradually disappear tendency of sPB1-F2 to self-associate in pure aqueous soluupon increasing the hydrophilicity of the solution until in tion without any sign of precipitation even at a millimolar
pure aqueous solution the molecule exhibits a random coil concentration suitable for NMR spectroscopy. In contrast,
increasing the hydrophobicity of the solvent stabilized conconformation.
The helical wheel representation of the experimentally siderable amounts of ␣-helical structure, with the molecule
determined ␣-helical region of the C-terminal fragment of undergoing a transition from an oligomeric unstructured
PB1-F2 has a bias toward an amphipathic distribution of resi- state in water to a less oligomeric, more structured molecule.
362 JOURNAL OF BIOLOGICAL CHEMISTRY
VOLUME 282 • NUMBER 1 • JANUARY 5, 2007
Structure and Oligomerization of Influenza A Virus PB1-F2
Clearly, since the highly flexible molecule is prone to protein-protein interactions, we conducted a thorough oligomerization study of the full-length molecule and fragments thereof. The data suggest that the molecule has two
independent oligomerization domains: an N-terminal and a
stronger C-terminal region. Both are separated by a central
section incorporating a cysteine residue at position 42 that
allows the formation of disulfide-linked dimers. Cross-linking data indicate both the N- and the C-terminal fragments
can interact with the full-length molecule, suggesting that
the two distinct oligomerization domains are freely accessible and are able to interact with one another. Although Cys42
probably contributes to the dimerization of PB1-F2, the Nand the C-terminal domains can interact independently of
each other and must be considered the major force that
drives the inherent self-association of the molecule. Complementary data from the program TANGO identified three
sets of 5 residues that are predicted to contribute qualitatively and quantitatively to the oligomerization phenomenon. The strongest of these is the 68ILVFL72 motif centered
in the C-terminal helix (Fig. 8).
Until the discovery of PB1-F2, the IAV-induced apoptosis
has been thought to be regulated by only extrinsic pathways
(e.g. Fas ligand-mediated apoptosis) (28 –30). Currently,
PB1-F2 is the only influenza A virus factor that can be
directly linked to mitochondrial localization (27). Conductance and ion permeability studies on planar lipid bilayer
membranes have indicated that sPB1-F2 shares similar
membrane destabilizing profiles with other proapoptotic
proteins, such as the Bcl-2 family of proteins, which result in
mitochondrial membrane instability and subsequently apoptosis (10). Our data unequivocally establish the unique oligomerization properties of PB1-F2 and indicate that these
are due to particular regions in the molecule. Consequently,
it seems probable that the formation of variably sized pores
that have been shown previously to induce membrane instability (10) is a direct result of oligomerization of PB1-F2. A
prerequisite for this to occur is location of the molecule at
the membrane surface, which we propose takes place as a
consequence of the cationic nature of the C-terminal helix.
Formation of helical secondary structure in the vicinity of
the membrane affords a unique arrangement of charges to
give one surface that is positively charged and favorable for
interaction with the negatively charged membrane. Interestingly, the other surface of the molecule contains more
hydrophobic residues and four of five high aggregation propensity residues. This will now allow interaction with other
PB1-F2 molecules and eventually lead to the formation of
pores in membranes of mitochondria and other cellular
compartments.
Acknowledgments—We thank Stephan Ludwig, Evelyn Schubert, and
Jimut K. Ghosh for helpful discussion and Prisca Kunert, Barbara
Brecht, Christel Kakoschke, and Stefanie Meier for excellent technical
assistance.
JANUARY 5, 2007 • VOLUME 282 • NUMBER 1
Addendum—While this manuscript was under review, Zamarin and
co-workers (26) reported that in IAV-infected cells, a C-terminal
domain of PB1-F2 with an approximate molecular mass of 6 kDa is
expressed from a downstream initiation codon and that this molecule is interacting with full-length PB1-F2.
REFERENCES
1. Lamb, R. A., and Takeda, M. (2001) Nat. Med. 7, 1286 –1288
2. Webster, R. G. (1997) Arch. Virol. Suppl. 13, 105–113
3. Webby, R. J., and Webster, R. G. (2001) Philos. Trans. R. Soc. Lond. B. Biol.
Sci. 356, 1817–1828
4. Chen, W., Calvo, P. A., Malide, D., Gibbs, J., Schubert, U., Bacik, I., Basta,
S., O’Neill, R., Schickli, J., Palese, P., Henklein, P., Bennink, J. R., and Yewdell, J. W. (2001) Nat. Med. 7, 1306 –1312
5. Neumann, G., Brownlee, G. G., Fodor, E., and Kawaoka, Y. (2004) Curr.
Top. Microbiol. Immunol 283, 121–143
6. Garcia-Sastre, A., Egorov, A., Matassov, D., Brandt, S., Levy, D. E., Durbin,
J. E., Palese, P., and Muster, T. (1998) Virology 252, 324 –330
7. Garcia-Sastre, A. (2001) Virology 279, 375–384
8. Henklein, P., Bruns, K., Sherman, M. P., Tessmer, U., Licha, K., Kopp, J., de
Noronha, C. M., Greene, W. C., Wray, V., and Schubert, U. (2000) J. Biol.
Chem. 275, 32016 –32026
9. Zhao, R. Y., Bukrinsky, M., and Elder, R. T. (2005) Indian J. Med. Res. 121,
270 –286
10. Chanturiya, A. N., Basanez, G., Schubert, U., Henklein, P., Yewdell, J. W.,
and Zimmerberg, J. (2004) J. Virol. 78, 6304 – 6312
11. Henklein, P., Bruns, K., Nimtz, M., Wray, V., Tessmer, U., and Schubert,
U. (2005) J. Pept. Sci. 11, 481– 490
12. Wüthrich, K. (1986) NMR of Proteins and Nucleic Acids, pp. 13–19,
40 – 43, and 130 –161, John Wiley & Sons, Inc., New York
13. Bruns, K., Fossen, T., Wray, V., Henklein, P., Tessmer, U., and Schubert, U.
(2003) J. Biol. Chem. 278, 43188 – 43201
14. Neidig, K. P., and Kalbitzer, H. R. (1990) J. Magn. Reson. 88, 155–160
15. Blankenfeldt, W., Nokihara, K., Naruse, S., Lessel, U., Schomburg, D., and
Wray, V. (1996) Biochemistry 35, 5955–5962
16. Schomburg, D., and Reichelt, J. (1988) J. Mol. Graphics 6, 161–165
17. Zamarin, D., Garcia-Sastre, A., Xiao, X., Wang, R., and Palese, P. (2005)
PLoS Pathog. 1, 40 –54
18. Gibbs, J. S., Malide, D., Hornung, F., Bennink, J. R., and Yewdell, J. W.
(2003) J. Virol. 77, 7214 –7224
19. Fernandez-Escamilla, A. M., Rousseau, F., Schymkowitz, J., and Serrano,
L. (2004) Nat. Biotechnol. 22, 1302–1306
20. Pande, V. S. (2004) Nat. Biotechnol. 22, 1240 –1241
21. Buck, M. (1998) Q. Rev. Biophys. 31, 297–355
22. Wishart, D. S., Sykes, B. D., and Richards, F. M. (1992) Biochemistry 31,
1647–1651
23. Brunger, A. T., Adams, P. D., Clore, G. M., DeLano, W. L., Gros, P.,
Grosse-Kunstleve, R. W., Jiang, J. S., Kuszewski, J., Nilges, M., Pannu, N. S.,
Read, R. J., Rice, L. M., Simonson, T., and Warren, G. L. (1998) Acta
Crystallogr. D Biol. Crystallogr. 54, 905–921
24. Obenauer, J. C., Denson, J., Mehta, P. K., Su, X., Mukatira, S., Finkelstein,
D. B., Xu, X., Wang, J., Ma, J., Fan, Y., Rakestraw, K. M., Webster, R. G.,
Hoffmann, E., Krauss, S., Zheng, J., Zhang, Z., and Naeve, C. W. (2006)
Science 311, 1576 –1580
25. Holmes, E. C., Lipman, D. J., Zamarin, D., and Yewdell, J. W. (2006) Science
313, 1573
26. Zamarin, D., Ortigoza, M. B., and Palese, P. (2006) J. Virol. 80, 7976 –7983
27. Lowy, R. J. (2003) Int. Rev. Immunol. 22, 425– 449
28. Takizawa, T., Matsukawa, S., Higuchi, Y., Nakamura, S., Nakanishi, Y., and
Fukuda, R. (1993) J. Gen. Virol. 74, 2347–2355
29. Takizawa, T., Fukuda, R., Miyawaki, T., Ohashi, K., and Nakanishi, Y.
(1995) Virology 209, 288 –296
30. Wada, N., Matsumura, M., Ohba, Y., Kobayashi, N., Takizawa, T., and
Nakanishi, Y. (1995) J. Biol. Chem. 270, 18007–18012
JOURNAL OF BIOLOGICAL CHEMISTRY
363