From the Department of Cell Biology and Biochemistry, Texas Tech University Health Sciences Center, Lubbock, Texas 79430
Received for publication, May 17, 2000, and in revised form, October 13, 2000
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ABSTRACT |
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RUSH proteins are SWI/SNF-related transcription
factors with RING finger signatures near their COOH termini. Long
suspected of mediating protein-protein interactions, the RING motif was used to clone a binding partner. The RING finger binding protein (RFBP)
is a Type IV P-type ATPase, a putative phospholipid pump, with
conserved sequences for two loop segments, an ATP-binding site, a
phosphorylation domain, and transmembrane passes potentially involved
in substrate binding and translocation. However, RFBP differs from all
other Type IV P-type ATPases in three ways. It has only three of four
highly conserved NH2-terminal transmembrane passes,
it is located in the inner nuclear membrane, and it binds the RING
domain. Topographically the orientation of the adjacent hydrophilic
domains and the determinants of transport specificity are altered. As a
result, the small, hydrophilic loop extends into the perinuclear space
that is contiguous with the lumen of the endoplasmic reticulum. The
large, conformationally flexible loop extends into the
nucleoplasm to contact euchromatin. Competitive reverse
transcriptase-polymerase chain reaction and high performance liquid
chromatography analysis revealed that endometrial RFBP mRNA
expression is hormonally regulated. The physical association of a
hormone-dependent RING finger-binding protein with
transcriptionally active chromatin supports the speculation that RFBP
plays a role in the subnuclear trafficking of transcription factors
with RING motifs.
RUSH is an acronym for proteins with RING finger
motifs that bind to the uteroglobin promoter (1);
RUSH nucleophosphoproteins contain regions of homology with members of
the SWI/SNF superfamily of
DNA-dependent helicases/ATPases. The expression
of RUSH-1 Sequence alignment of homologs from rabbit, human, rodent, and plant
(3) showed that all RUSH proteins contain the RING finger motif
(C3HC4 or RING-HC), which binds two zinc ions
in a unique cross-braced system (4). RING fingers can be associated with other motifs to form larger, conserved domains such as the RING
finger-B box- It is generally accepted that the RING motif binds two zinc ions to
form an integrated structural unit that mediates protein-protein interactions (4, 7-9). The search for functional binding partners ultimately led to the demonstration that the RING domain in one protein
can associate with another RING-domain to promote homo- or
heterodimerization. Alternatively, the RING domain can also associate
with non-RING domains (10). The recent discovery of the functional link
between the ubiquitin-proteasome pathway and the RING-containing
protein Cbl has attracted considerable attention (11, 12). Although
these studies support the idea that the RING motif is involved in
ubiquitin-mediated proteolysis (11), Borden (9) speculates that the
RING finger may serve as a scaffold for the evolution of different
functions. Copps et al. (13) suggest that the RING motif may
play a regulatory role in the ordered assembly of factors. Borden
et al. (14) and Le et al. (15) used site-directed
mutagenesis to show that the RING finger motif of the promyelocytic
leukemia oncoprotein PML is necessary for the formation of
speckled nuclear bodies also known as promyelocytic oncogenic domains.
More recently, Cao et al. (16) show that mutations of the
RING finger resulted in the retention of the RET finger protein
in the cytoplasm even though the putative nuclear localization signal
was intact. These studies suggest that the RING finger plays a role in
nuclear targeting.
When the RING motif of the RUSH gene was used to clone a RING
finger-binding protein
(RFBP),1 a new Type IV P-type
ATPase was identified in the inner nuclear membrane. The topographical
orientation of the molecule allows the large conformationally flexible
loop portion of the protein to contact euchromatin. These physical
affiliations support the speculation that RFBP and RUSH are
functionally linked during transcription.
Reagents, Antibodies, and Cells--
cDNA Synthesis
System Plus, cDNA cloning system-
Rabbit antipeptide antibodies were made to a keyhole limpet
hemocyanin peptide at Research Genetics (Huntsville, Alabama). Amino acids 663-678 were selected because they displayed strong antigenicity according to the PeptideStructure program (Genetics Computer Group Software, Madison, WI), and because they are unique to
RFBP. They share only 3 of 16 amino acids common to any authentic Type
IV P-type ATPase in the GenBankTM data base. The
antipeptide antibody titer was determined with an enzyme-linked
immunosorbent assay with free peptide on the solid phase (1 µg/well),
goat anti-rabbit IgG-horseradish peroxidase conjugate as the secondary
antibody, and peroxidase dye. To reduce complications from nonspecific
binding, antibodies were affinity-purified. Horseradish
peroxidase-conjugated donkey anti-rabbit IgG was purchased from
Amersham Pharmacia Biotech. Midland Certified Reagent Co. (Midland, TX)
synthesized all PCR primers. Dr. J. Y. Chou, Human Genetics
Branch, NICHD, National Institutes of Health (Bethesda, MD), provided
HRE-H9 cells.
Cloning of the RING Motif--
For cloning, the RING motif was
amplified from 50 ng of a 1030-bp partial RUSH cDNA clone (2). The
50-µl PCR reaction mix contained LA PCR buffer (1X), TaKaRa ExTaq DNA
polymerase (2.5 units/50 µl), TaqStart antibody (0.55 µg/50 µl),
dNTPs (0.2 mM each), and primers (0.2 mM each).
The forward primer (5'-GCG
Recombinant protein with a T7 tag, a His tag, and an S tag at its
NH2 terminus was induced by exposure to
isopropyl- Cloning of the RING Finger Binding Partner--
A
A positive plaque was heated at 100 °C for 10 min, then amplified in
a 50-µl PCR reaction mix containing LA PCR buffer (1×), TaKaRa ExTaq DNA polymerase (2.5 units/50 µl), TaqStart antibody (0.55 µg/50 µl), dNTPs (0.2 mM each), and
Four different Marathon RACE reactions were performed to obtain
overlapping cDNA clones as described under "Results" and in Fig. 1. Poly(A+) RNA (1 µg) from HRE-H9 cells was used in
the preparation of adaptor-ligated cDNA libraries. For each PCR
reaction, 5 µl of diluted cDNA library was mixed with 45 µl of
a PCR reaction mix containing LA PCR buffer (1×), TaKaRa ExTaq
DNA polymerase (2.5 units/50 µl), TaqStart antibody (0.55 µg/50
µl), dNTPs (0.2 mM each), and primers (0.2 mM
each). In the first reaction (Fig. 1), RACE primer pair 1 consisted of
a forward gene-specific primer (5'-GTG CGT GGA CTC CCT ATG CTG TTT
CCC-3') and a reverse adaptor primer (AP1; 5'-CCA TCC TAA TAC GAC TCA
CTA TAG GGC-3'). A three-step, hot-start PCR reaction was performed
with the following conditions: 60 s at 95 °C followed by 5 cycles of 94 °C for 30 s, 72 °C for 60 s, 72 °C for
180 s, 5 cycles of 94 °C for 30 s, 71 °C for 60 s,
72 °C for 180 s, 25 cycles of 94 °C for 30 s, 70 °C
for 60 s, 72 °C for 180 s, and a final extension for 10 min at 72 °C. Samples were rapidly cooled to 4 °C. A single
1151-bp PCR product (Fig. 1) was cloned into pCR®II-TOPO and sequenced
in both directions by the dideoxy chain termination method.
In the second reaction (Fig. 1), RACE primer pair 2 consisted of a
degenerate forward primer (5'-GAY AAR ACN GGN ACN YTN ACN-3', Y = pyrimidine, R = purine, and N = A, T, G, or
C) and a reverse gene-specific primer (5'-CGC TTT CTG CAG TGG TGC CAT
ACG ACA GC-3'). A four-step, hot-start PCR reaction was performed with
the following conditions: 30 s at 94 °C followed by 5 cycles of
94 °C for 5 s, 65 °C for 240 s, 5 cycles of 94 °C
for 5 s, 60 °C for 240 s, 5 cycles of 94 °C for 5 s, 55 °C for 240 s, 20 cycles of 94 °C for 5 s,
50 °C for 240 s, and a final extension for 10 min at 68 °C.
Samples were rapidly cooled to 4 °C. A single 1185-bp PCR product
was cloned into pCR®II-TOPO and sequenced in both directions by the
dideoxy chain termination method.
The third reaction actually consisted of a primary reaction followed by
a nested secondary reaction (Fig. 1). In the primary reaction, the RACE
primer pair consisted of the forward AP1 primer and a reverse,
gene-specific primer (5'-CAG TGT GAC AGA GAC TGA CTG C-3'). The
hot-start PCR reaction was performed with the following conditions:
30 s at 94 °C followed by 30 cycles of 94 °C for 5 s,
62.5 °C for 240 s, and a final extension for 10 min at
68 °C. Samples were rapidly cooled to 4 °C. Products from this
reaction were used in a nested PCR reaction with RACE primer pair 3 (Fig. 1), which consisted of forward adaptor primer 2 (AP2; 5'-ACT CAC TAT AGG GCT CGA GCG GC-3') and a reverse gene-specific primer (5'-CCT
TCT GAA GAA TCT GGT GTC GGT CC-3'). The hot start PCR reaction was
performed with the following conditions: 30 s at 94 °C followed
by 25 cycles of 94 °C for 5 s, 66.5 °C for 240 s, and a
final extension for 10 min at 68 °C. Samples were rapidly cooled to
4 °C. A single 992-bp PCR product was cloned into pCR®II-TOPO and
sequenced in both directions by the dideoxy chain termination method.
The fourth reaction also consisted of a primary reaction followed by a
nested secondary reaction (Fig. 1). In the primary reaction, the RACE
primer pair consisted of forward AP1 and a reverse gene-specific primer
(5'-CAA GGC CAC CAC TTC GAA CAA CAT AAA CAG G-3'). A six-step, hot
start PCR reaction was performed with the following conditions: 30 s at 94 °C followed by 5 cycles of 94 °C for 5 s, 70 °C
for 150 s, 5 cycles of 94 °C for 5 s, 69 °C for
150 s, 5 cycles of 94 °C for 5 s, 68 °C for 150 s,
5 cycles of 94 °C for 5 s, 67 °C for 150 s, 5 cycles of
94 °C for 5 s, 66 °C for 150 s, 15 cycles of 94 °C
for 5 s, 65 °C for 150 s, and a final extension for 10 min
at 68 °C. Products from this reaction were used in a nested PCR
reaction with RACE primer pair 4 (Fig. 1), which consisted of forward
AP2, and a reverse gene-specific primer (5'-GTC TCA ACC AAT CTT CGT ACC
CCT G-3'). A six-step, hot-start PCR reaction was performed with the
following conditions: 30 s at 94 °C followed by 5 cycles of
94 °C for 5 s, 68 °C for 120 s, 5 cycles of 94 °C
for 5 s, 67 °C for 120 s, 5 cycles of 94 °C for 5 s, 66 °C for 120 s, 5 cycles of 94 °C for 5 s, 65 °C
for 120 s, 5 cycles of 94 °C for 5 s, 64 °C for
120 s, 10 cycles of 94 °C for 5 s, 63 °C for 120 s, and a final extension for 10 min at 68 °C. Samples were rapidly
cooled to 4 °C. A single 314-bp PCR product was cloned into
pCR®II-TOPO and sequenced in both directions by the dideoxy chain
termination method.
Genomic Cloning--
An amplified rabbit genomic library in the
EMBL3 SP6/T7 vector was screened with the 992-bp PCR product of the
third PCR reaction described above and in Fig. 1. Nitrocellulose filter
replicas were prepared from Subcellular Fractionation of Endometrium--
Rabbit endometrium
was homogenized (11 strokes) in 3 volumes (w/v) of buffer (10 mM Tris-HCl, pH 8.0, 100 mM KCl, 3 mM MgCl2, 250 mM sucrose, and 5 mM dithiothreitol) using a Potter-Elvejhem motor-driven
Teflon pestle at 4 °C. To test in vitro protein-protein interactions, Nonidet P-40 was added to an aliquot of the whole tissue
homogenate to a final concentration of 1%. This detergent lysate was
re-homogenized (5 strokes) and centrifuged at 2000 × g
to remove cellular debris. The supernatant fraction was used as a
source of protein (28.5 µg/µl) in glutathione
S-transferase (GST) pull-down assays. The remaining whole
tissue homogenate was fractionated by
centrifugation/ultracentrifugation to obtain nuclear (2000 × g), mitochondrial (10,000 × g), microsomal
(165,000 × g), and postmicrosomal supernatant
fractions for Western analysis. Detergent lysates (1% Nonidet P-40) of
the nuclear fraction were also prepared as a source of protein (22.5 µg/µl) in GST pull-down assays. The protein concentrations for all
fractions were determined according to Lowry et al. (17)
using bovine serum albumin as the standard.
GST Pull-down Assays and Immunoblotting--
The RING motif was
amplified from 50 ng of a 1030-bp partial RUSH cDNA clone (2), as
described above with a forward primer (5'-GCG
BLR(DE3)pLysS host cells were transformed with either the pGEX-2TK
control or the pGEX-2TK-RING recombinant. Individual cultures were
grown to an A260 of 0.6, and
isopropyl-
Membranes from Western (2) and GST pull-down assays were blocked in
Tris-buffered saline (150 mM NaCl, 20 mM
Tris-HCl, pH 7.6) with 0.1% Tween 20 (TBST) and 2% powdered milk.
Membranes were incubated overnight at 4 °C in the same buffer
containing affinity-purified anti-RFBP antibodies (1:50,000). Membranes
were washed 3 × 30 min in TBST and incubated in TBST with
horseradish peroxidase-conjugated donkey anti-rabbit IgG (1:5,000) for
90 min at room temperature. Membranes were subsequently washed 3 × 30 min in TBST. Specific signals were detected by chemiluminescence using Renaissance reagents.
For coimmunoprecipitation assays, aliquots of whole tissue homogenates
were incubated overnight at 4 °C with anti-RFBP then incubated for
2 h at 4 °C with a 50% slurry of protein A-Sepharose. Proteins
were fractionated by SDS/polyacrylamide gel electrophoresis in 10%
gels and transferred to nitrocellulose membrane. Membranes were
processed exactly as for Western analysis except they were incubated
with affinity-purified anti-RUSH-2 antibodies (1:100) as described
(2).
Immunoelectron Microscopy--
Nuclei from endometrium of
progesterone-treated rabbits were isolated ± 0.1% Triton X-100
on sucrose cushions containing protease inhibitors (24). Nuclear
pellets were resuspended in phosphate-buffered paraformaldehyde (4%)
and fixed for 30 min. Nuclei were dehydrated in a graded series of
ethanol and embedded in LR white resin (50 °C). Thin sections
(600-800 Å) were mounted on nickel grids, blocked with 5% normal
goat serum, and incubated in antipeptide antibody (1:100 with 5%
normal goat serum) overnight at 4 °C. Grids were rinsed and
incubated with goat anti-rabbit IgG conjugated to 6- or 15-nm gold
(1:25 with 5% normal goat serum) for 2 h at 37 °C. Grids were
fixed with phosphate-buffered glutaraldehyde (3%) for 5 min, stained
with uranyl acetate and lead citrate, and viewed with a Hitachi 600 electron microscope operated at 75 kV.
Animal Treatments--
All studies were conducted in accord with
the National Institutes of Health Guidelines for the Care and Use of
Laboratory Animals as reviewed and approved by the Animal Care and Use
Committee at Texas Tech University Health Sciences Center. Adult New
Zealand White rabbits (6 months of age) were housed for 3 weeks before experimentation. Seventeen estrous animals were divided into two groups. For group one, endometrium from six animals was pooled, and RNA
was isolated using a cold precipitation method (25). For group two, the
rabbits were used in three experimental subgroups (n = 3 animals/subgroup; 5 animals in the progesterone treatment category).
Animals were injected every 24 h with hormones and killed 24 h after the last injection. Treatments (2, 24, 26) included
subcutaneous injections of progesterone (3 mg/kg/day for 5 days),
prolactin (2 mg/day for 5 days), or prolactin (5 days) followed by
progesterone (5 days). For group 2 animals, total RNA was isolated from
individual endometrial samples in Tri-Reagent according to Chomczynski
and Sacchi (27). RNA concentrations for all samples were determined
spectrophotometrically (A260). Electrophoretic
fractionation and ethidium bromide staining confirmed the integrity of
each sample. Two animals in the progesterone treatment category were
used for subcellular fractionation of uterine endometrium and for
nuclear isolation.
Competitive RT-PCR--
The CLONTECH MIMIC
system was used to develop a heterologous competitor RNA. Competitor
construction required two PCR amplification reactions. In the primary
reaction, composite primers consisting of RFBP-specific sequence
contiguous with 20 bp of MIMIC-specific sequence were designed to
hybridize to opposite strands of the MIMIC DNA template, a 576-bp
BamHI/EcoRI fragment of the v-erbB gene. For each
50-µl PCR reaction, MIMIC DNA template (2 ng) was mixed with TaKaRa
ExTaq DNA polymerase (2 units/50 µl), TaqStart antibody (0.44 µg/50
µl), deoxynucleoside triphosphates (0.2 mM each), and 0.4 µM each composite primer. The MIMIC sequence in each
composite primer is underlined: forward, 5'-GTG CGT GGA CTC CCT ATG CTG
TTT CCC AGC GCA AGT GAA ATC TCC TCC G-3' and reverse, 5'-GGA GAG AGT CAA GAT GCT CCT GTC GTT GGT TTC ATC TCC CTG TAT
AAC A-3'. A total of 26 PCR cycles were performed for 45 s
at 94 °C, 45 s at 50 °C, and 90 s at 72 °C. Analysis
of PCR products by agarose gel (1.5%) electrophoresis revealed a
single 258-bp amplicon. A 1:100 dilution of this product was amplified
again with gene-specific primers.
This secondary PCR reaction was performed in a 100-µl PCR reaction
with TaKaRa ExTaq DNA polymerase (3 units/100 µl), TaqStart antibody
(0.66 µg/100 µl), deoxynucleoside triphosphates (0.2 mM
each), and 0.4 µM each RFBP-specific primer. The
RFBP-specific primers were forward, 5'-GTG CGT GGA CTC CCT ATG CTG TTT
CCC AG-3', and reverse, 5'-GGA GAG AGT CAA GAT GCT CCT GTC GTT GG-3'. A
total of 18 PCR cycles were performed as described above. The quality and size of the final reaction product was again verified by gel electrophoresis. The PCR product was subcloned into pCR®II-TOPO, and
closed circular DNA was purified by equilibrium centrifugation in
CsCl-ethidium bromide gradients. The identity of the MIMIC competitor
was confirmed by sequencing in both directions by the dideoxy chain
termination method.
The pCR®II-TOPO vector containing the MIMIC competitor cDNA insert
was linearized with the restriction enzyme EcoRV, and
competitor RNA was transcribed. RNA was precipitated with isopropanol
to prevent the coprecipitation of free nucleotides, resulting in a more
accurate estimation of the RNA yield at 260 nm. Serial dilutions of
competitor RNA (6, 3, 1.5, 0.6, 0.3, and 0.1 pg) were combined with
poly(A)+ RNA (1 ng) from HRE-H9 cells and
reverse-transcribed with Moloney murine leukemia virus and random
hexamers for 30 min at 42 °C. Products from this reaction were
heated to 99 °C and cooled to 4 °C. Then 40 µl of a PCR mix
containing Amplitaq gold DNA polymerase (1 units/50 µl) and 0.25 µM each RFBP-specific primer described above were added
to each reaction tube. PCR cycle parameters included a hot start at
95 °C for 2 min, 36 cycles of 45 s at 94 °C, 45 s at
67 °C, and 60 s at 72 °C. Samples were subjected to a final extension at 72 °C for 5 min before rapid cooling to 4 °C.
Amplified products were quantified by means of a binary gradient HPLC
system. Briefly, an aliquot (10 µl) of each RT-PCR reaction was
injected onto a DNASep column containing an alkylated
polystyrene-divinylbenzene packing and eluted in a 4-min gradient of
acetonitrile in 0.1 M triethylammonium acetate (pH 7.0) at
a flow rate of 1 ml/min at room temperature. The amounts of native
(166-bp) and competitor (258-bp) products were determined by on-line UV
absorbance detection at 254 nm. This titration analysis was repeated 5 times to show the preservation of slope and linearity in the
quantification of the native product amounts. Next, a single dose of
competitor was mixed with a fixed amount of poly(A)+ RNA
from the HRE-H9 cells. Estimation of the amount of native transcript
gave a value similar to that from the titration analysis, confirming
the precision of the single-tube measurement with the denaturing HPLC
quantification system. The repeated analysis (n = 10)
of RNA from HRE-H9 cells yielded a coefficient of variation of 8.4%.
The single tube analysis was then used to determine the relative
expression of native RFBP in rabbit tissues.
To test the hypothesis that the RING domain is involved in unique
protein-protein interactions, the region of the RUSH cDNA that
encodes the RING finger motif was obtained by PCR with primers that
contained unique restriction enzyme sites. A single 142-bp PCR
product was subcloned into pCRTMII, excised with
appropriate restriction enzymes, and directionally subcloned into
SacI-HindIII sites of the pSCREEN-1b(+)
expression vector. Insert orientation was confirmed by sequencing in
both directions by the dideoxy chain termination method. The resultant recombinant protein with a T7 tag, a His tag, and an S tag at its
NH2 terminus was used in a novel cloning strategy (19) to identify protein binding partners. Filters with recombinant proteins from a
INTRODUCTION
TOP
ABSTRACT
INTRODUCTION
EXPERIMENTAL PROCEDURES
RESULTS
DISCUSSION
REFERENCES
(1005-amino acids, 113 kDa) and RUSH-1
(836 amino
acids, 95 kDa) is regulated by a steroid-dependent
alternative splicing mechanism (2) in which
is the
progesterone-dependent splice variant, and
is the
estrogen-dependent splice variant. Thus, the acronym acknowledges that in a changing hormonal milieu transcription is
bypassed by alternative splicing, and the response of individual target
genes is accelerated or "RUSHed."
-helical coiled-coil (RBCC) domain (4). Some changes
have occurred in the RING such that RING-H2
(C3H2C3) designates a subclass in
which a histidine residue was substituted for the fourth cysteine
residue. The U-box (UFD2 homology domain) is a degenerate version of
the RING motif that lacks the signature metal-chelating residues (5,
6). Unlike the authentic RING finger that is stabilized by binding zinc
ions, it has been inferred from the PROMODII model that the U-box is
maintained by a system of salt bridges and hydrogen bonds (6).
EXPERIMENTAL PROCEDURES
TOP
ABSTRACT
INTRODUCTION
EXPERIMENTAL PROCEDURES
RESULTS
DISCUSSION
REFERENCES
gt11, Sequenase Version 2.0 DNA
sequencing kit, pGEX-2TK vector, glutathione-Sepharose 4B, protein
A-SepharoseTMCL-4B, isopropyl-
-D-thiogalactopyranoside, and the following isotope were purchased from Amersham Pharmacia Biotech: [
-35S]dATP, 1000 Ci/mmol, for sequencing. The
SMART rapid amplification cDNA ends (RACE) and
MarathonTMcDNA amplification kits, polymerase chain
reaction (PCR) MIMIC construction kit, Rabbit genomic library, TaqStart
antibody, Tth Start antibody, Advantage genomic PCR kit, and Advantage
Tth polymerase mix were purchased from CLONTECH
Laboratories, Inc. (Palo Alto, CA). TaKaRa ExTaq enzyme and 10× LA PCR
buffer were purchased from PanVera Corp. (Madison, WI). The GeneAmp RNA
PCR core kit and Amplitaq gold DNA polymerase were purchased from
PerkinElmer Life Sciences. The vector pSCREEN-1b(+), thrombin
cleavage capture kit, T7-Tag antibody alkaline phosphatase conjugate,
S-protein alkaline phosphatase conjugate, and BLR(DE3)pLysS cells were
purchased from Novagen (Madison, WI). The pCRTMII and pCR®II-TOPO
vectors are components of individual TA cloning kits, which were
purchased from Invitrogen (San Diego, CA). MetaPhor-agarose was
purchased from BioWhittaker Molecular Applications, Inc.
(Rockland, ME). A 1-kb ladder was purchased from Promega
(Madison, WI). The binary gradient HPLC system was purchased from
Rainin Instrument Co., Inc. (Woburn, MA), and the DNASep columns
containing alkylated polystyrene-divinylbenzene packing were purchased
from Transgenomic, Inc. (San Jose, CA). Kodak X-Omat AR film was
purchased from Eastman Kodak Co. Renaissance chemiluminescence
reagents were purchased from PerkinElmer Life Sciences.
Nitrocellulose transfer/immobilization membranes were purchased from
Schleicher & Schuell. Tri reagent was purchased from Molecular Research
Center, Inc. (Cincinnati, OH). LR White resin and goat
anti-rabbit IgG conjugated to 6- or 15-nm gold were purchased from
Electron Microscopy Sciences (Ft. Washington, PA).
AGCT
CA TGT GCT ATA TGC TTG G-3') had a unique SacI site (bold), and
the reverse primer
(5'-GCA
AGCT
TC TGC ATA AAG GGC
AC-3') had a unique HindIII site (bold). A four-step,
hot-start PCR reaction was performed. The conditions were as follows:
45 s at 95 °C followed by 10 cycles of 94 °C for 45 s,
39.5 °C for 60 s, 72 °C for 60 s, 10 cycles of 94 °C
for 45 s, 38.5 °C for 60 s, 72 °C for 60 s, 10 cycles of 94 °C for 45 s, 55 °C for 60 s, 72 °C for
60 s, 20 cycles of 94 °C for 45 s, 54 °C for 60 s, 72 °C for 60 s, and a final extension for 5 min at 72 °C.
Samples were rapidly cooled to 4 °C. A single 142-bp PCR product was
cloned into pCRTMII, excised with appropriate restriction
enzymes, and directionally subcloned into the
SacI-HindIII sites of the pSCREEN-1b(+)
expression vector. Insert orientation was confirmed by sequencing in
both directions by the dideoxy chain termination method.
-D-thiogalactopyranoside (1 mM)
and purified by metal chelation chromatography. Briefly, recombinant
His-tag protein was eluted under native conditions (1 M
imidazole, 0.5 M NaCl, 20 mM Tris-HCl, pH 7.9),
dialyzed against water to remove excess salt, and lyophilized. The
protein concentration (1.05 mg/ml) was determined according to Lowry
et al. (17) using bovine serum albumin as the standard. The
leader sequence containing the T7 tag, and the His tag was removed by digestion with biotinylated thrombin. Biotinylated thrombin was separated from the remaining S-tag protein with
streptavidin-agarose.
gt11
cDNA expression library was prepared using mRNA isolated from
HRE-H9 cells (18) and screened according to Macgregor et al.
(19) to identify protein binding partners. Nitrocellulose filter
replicas were prepared from
gt11 recombinants (
3 × 104 plaque-forming units/plate) and processed with 6 M guanidine-HCL denaturation-renaturation (20, 21) to
ensure proper protein folding. The filters were then screened with the
recombinant RING finger protein (1 µg/ml) with ZnSO4 (10 µM) to maintain functional conformation (22, 23) and the
T7-tag antibody alkaline phosphatase conjugate (1:10,000). A single,
plaque-pure clone was rescreened with the thrombin-cleaved recombinant
protein (1 µg/ml) in the presence of ZnSO4 (10 µM) and the S-protein alkaline phosphatase conjugate
(1:5,000).
gt11
primers (0.2 mM each). Forward (5'-GGT GGC GAC GAC TCC TGG
AGC CCG-3') and reverse (5'-TTG ACA CCA GAC CAA CTG GTA ATG-3')
gt11
primers flank the insert sequence in the vector. Hot-start PCR
reactions were performed with the following conditions: 120 s at
95 °C followed by 35 cycles of 94 °C for 45 s, 54 °C for
60 s, 72 °C for 180 s, and a final extension for 10 min at
72 °C. Test and control reactions were rapidly cooled to 4 °C. A
single 1584-bp PCR product was cloned into pCRTMII and
sequenced in both directions by the dideoxy chain termination method.
gt11 recombinants (
3 × 104 plaque-forming units/plate) and screened with the
random-prime-labeled cDNA (specific activity = 3-6 × 108 CPM/µg). A genomic clone (
14 kb) was isolated and
used as template in a PCR reaction. A region of the genomic DNA (150 ng) was amplified in a 50-µl PCR reaction containing PCR buffer
(1×), magnesium acetate (1.1 mM), Tth DNA polymerase (0.1 units), TthStart antibody (0.01 µg/µl), dNTPs (0.2 mM
each), and primers (0.2 mM each). The forward (5'-CAG GGG
TAC GAA GAT TGG TTG AGA C-3') and reverse (5'-CTG TCA GCG TAC CCG TTT
TAT CTG TAA ACA C-3') primers matched sequence in the cDNA. The
hot-start PCR amplification reaction was performed as follows: 30 s at 94 °C, followed by 5 cycles of 94 °C for 5 s, 67 °C
for 360 s, 5 cycles of 94 °C for 5 s, 66 °C for
360 s, 5 cycles of 94 °C for 5 s, 65 °C for 360 s,
5 cycles of 94 °C for 5 s, 64.5 °C for 360 s, 20 cycles
of 94 °C for 5 s, 64 °C for 360 s, and a final
extension for 10 min at 68 °C. Samples were rapidly cooled to
4 °C. A single 742-bp PCR product was cloned into pCR®II-TOPO and
sequenced in both directions by the dideoxy chain termination method.
GATC
CG AAG AAT GTG CT-3')
that had a unique BamHI site (bold) and a reverse primer
(5'-GCG
AATT
CC ATG TAT ATC
ATT-3') that had a unique EcoRI site (bold). To accommodate the low melting temperature of this primer pair, a four-step touch-up PCR reaction was performed with a hot start. The conditions were as
follows: 30 s at 94 °C followed by 5 cycles of 94 °C for
5 s, 35 °C for 120 s, 5 cycles of 94 °C for 5 s,
40 °C for 120 s, 5 cycles of 94 °C for 5 s, 45 °C
for 120 s, 5 cycles of 94 °C for 5 s, 50 °C for
120 s, and a final extension for 10 min at 68 °C. Samples were
rapidly cooled to 4 °C. A single 161-bp PCR product was cloned into
pCRTMII, excised with appropriate restriction enzymes, and
directionally subcloned into the BamHI-EcoRI
sites of the pGEX-2TK vector. Insert orientation was confirmed by
sequencing in both directions by the dideoxy chain termination method.
-D-thiogalactopyranoside was added to a final
concentration of 1 mM. After 3 h of additional growth,
bacteria were pelleted by centrifugation at 5000 × g
for 10 min. Bacteria were resuspended in 1/10th volume of lysis buffer (50 mM Tris-HCl, pH 7.5, 100 mM NaCl, 1 mM EDTA, 0.5% Nonidet P-40, leupeptin (1 µg/ml),
antipain (2 µg/ml), benzamidine (10 µg/ml), chymostatin (10 µg/ml), pepstatin (10 µg/ml), and phenylmethylsulfonyl fluoride (2 mM)). Bacteria were lysed on ice with mild sonication and
centrifuged at 10,000 × g for 10 min. Pellets were
discarded, and supernatants (1 ml/each) were incubated with 25 µl of
glutathione-Sepharose (50% slurry in lysis buffer with 0.5% powdered
milk) for 90 min at 4 °C. GST and GST-RING were mixed with detergent
lysates containing RFBP at 4 °C for 90 min. Binding complexes were
washed 3× lysis buffer, fractionated by SDS/polyacrylamide gel
electrophoresis in 12.5% gels and transferred to nitrocellulose membrane.
RESULTS
TOP
ABSTRACT
INTRODUCTION
EXPERIMENTAL PROCEDURES
RESULTS
DISCUSSION
REFERENCES
gt-11 expression library prepared from HRE-H9 cells were denatured-renatured with guanidine hydrochloride to ensure proper protein folding (20, 21). The filters were then screened with the
recombinant RING finger protein in the presence of ZnSO4
(10 µM) to maintain functional conformation (22, 23). The
single phage clone (1.6-kb cDNA insert), depicted in Fig.
1, was identified with the T7-tag
antibody alkaline phosphatase conjugate. Because the His tag is known
to bind heavy metals, it was removed along with the T7 tag by enzymatic
cleavage with thrombin. The truncated recombinant protein with its S
tag was then used with the S-protein alkaline phosphatase conjugate to
confirm the identity of the positive clone in a secondary
screen.
View larger version (13K):
[in a new window]
Fig. 1.
Strategy for RACE and competitive RT-PCR
reactions. The open box depicts the original 1.6-kb
clone with the stop (TAA) codon. Large arrowheads mark the
locations of the primer pairs used in the RACE procedure. Small
arrowheads mark the location of the primer pair used in
competitive RT-PCR reactions. The sizes of the overlaps between known
sequence and additional sequences obtained as single reaction products
by 5'- and 3'-RACE are provided in bp. Region C and the putative
phosphorylation (P) site are provided for orientation. The
poly(A) tail (A23) is indicated at the end of the
3'-RACE product.
The cDNA insert in the phage clone was amplified by PCR and subcloned into pCRTMII. Sequence analysis revealed the presence of a partial cDNA that contained a single open reading frame and a TAA stop codon but lacked an initiator codon. Northern analysis of rabbit endometrial mRNA with this clone revealed a strong 5.3-kb band. As shown in Fig. 1, RACE was used to extend the 5'-end of the cDNA and to obtain the entire 3'-end of the cDNA. The 5' region, which encodes the initiator methionine, is missing. Repeated attempts to obtain this sequence using 5'-RACE and SMART RACE met with no success.
The composite cDNA sequence (4286 bp) and the predicted amino acid
sequence (1107 amino acids) for RFBP (GenBankTM accession
number AF236061) are shown in Fig. 2. The
incomplete protein has a predicted molecular mass of 126 kDa. A
computer search of sequence data bases (SWISS-PROT + PIR + PRF and
GenBankTM) was conducted with the BLAST 2.0.12 program at
the National Center for Biotechnology Information. This search revealed
the predicted RFBP protein is 50% similar and 34% identical to Type IV P-type ATPases from Bos taurus (protein ID AAD03352),
Mus musculus (protein ID AAB18627), and Saccharomyces
cerevisiae (protein ID L01795). RFBP and the partial cDNA
sequence for human KIAA0956 (GenBankTM accession number
AB023173) are 92% identical using the BLAST algorithm for pairwise
DNA-DNA sequence alignment, whereas the amino acid sequences are 93%
identical and 95% similar. Such comparisons indicate that KIAA0956 is
the human homolog of RFBP. A position-specific iterated BLAST
(PSI-BLAST) program (28), which is sensitive to weak but biologically
relevant sequence similarities, identified 597 hits. All of the hits
were ATPases, and 289 of them had statistically significant expectation
(e) values greater than the 0.001 threshold.
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Although the coding sequence for RFBP is incomplete by ~18 amino acids, the ClustalW alignment (29) with known Type IV P-type ATPases indicates that it has all of the diagnostic structural features including consensus sequences for the conformationally flexible loop, seven of eight core segments, the ATP binding domain, the highly conserved phosphorylation site (DKTGT(L/I)T), and nine transmembrane domains potentially involved in substrate binding and translocation. Transmembrane domain assignments were confirmed by analyses with the SOAP algorithm derived by Kyte-Doolittle (30), the Argos et al. (31) transmembrane analysis, the Tmpred program (can be located using Pedro's Biomolecular Research Tools website) and the SOSUI system. Conserved core regions A-H and the transmembrane domains are shown in Fig. 2. It is important to note that region D, which contains transmembrane domain 4, is absent from the RFBP cDNA sequence. However, to avoid confusion, the domains were numbered consecutively in Fig. 2.
All working models of membrane topology for P-type ATPases contain
an even number of transmembrane passes, with four of them highly
conserved at the NH2 terminus (32, 33). Thus, it was important to determine whether or not such an evolutionarily conserved domain that is missing from the cDNA was also missing from the gene. Primers that recognize cDNA sequence on either side of Region D in transmembrane domain 2 and core Region E were used in a PCR reaction with genomic DNA. Analysis of PCR reaction products by agarose
gel electrophoresis is shown in Fig.
3A. Gel electrophoresis with
MetaPhor agarose and ethidium bromide fluorescence allowed the
visualization of a single 742-bp reaction product. Genomic sequence
data provided in Fig. 3B has 100% identity with the
corresponding region of the cDNA. These data show that region D,
which contains transmembrane domain 4, is absent from the RFBP gene and
confirm that RFBP is not a splice variant.
|
Western analysis with affinity-purified, antipeptide (IgG) antibodies
prepared against RFBP amino acids 663-678 was used to identify a
128-kDa immunoreactive protein in nuclear fractions from endometrium
(Fig. 4A). In vitro
protein-protein interactions were verified by GST pull-down assays and
immunoblotting. As shown in Fig. 4B, the RING domain peptide
expressed as a GST fusion protein binds to native RFBP in a
dose-dependent manner. Moreover, the RING domain peptide
was able to bind RFBP isolated from nuclei (Fig. 4B). This
observation indicated RFBP is the first Type IV P-type ATPase to be
located in the nuclear membrane. Based on the ClustalW alignment, the
hydrophilicity plot, and the immunoanalysis data, RFBP would span the
nuclear membrane nine times leaving the NH2- and
COOH-terminal ends on opposite sides of the bilayer. Each transmembrane
domain is a 20-30-amino acid residue coiled into a single -helix
that approximates the thickness of the polar region of the lipid
bilayer (34). However, because the nuclear envelope is formed from two
concentric membranes, it was not possible to deduce the membrane
topology of RFBP from its primary structure alone. Because RFBP could
be located in either the inner or the outer nuclear membrane,
immunoelectron microscopy was used to show that RFBP is located in the
inner nuclear membrane of nuclei isolated from rabbit endometrium (Fig.
5A). More specifically, immunogold labeling was used to show that the conformationally flexible
loop extends into the nucleoplasm to contact euchromatin (Fig.
5B).
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|
The extensive sequence identity of RFBP with known P-type ATPases from Plasmodium falciparum and B. taurus suggests the protein may be highly conserved. Therefore, competitive RT-PCR (Fig. 1) and an ion-pair reversed-phase HPLC product purification and detection system was used to show that RFBP is ubiquitous in its expression (Table I). The CLONTECH MIMIC system was used in the development of a heterologous competitor template. Native and mutant products were identified and quantified by denaturing HPLC, an analytical technique that preserves the accuracy of competitive RT-PCR beyond the log-linear phase of the reaction (2, 35-36). A computer model of competitive PCR was used to show an 8-fold range in the amounts of RFBP, with some of the highest values recorded for organs of the reproductive tract.
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Because RUSH, the RFBP binding partner, is hormonally regulated in the
endometrium (2, 37), it was important to determine whether
hormone-dependent changes in the amount of RFBP message corresponded to a similar pattern of change in RUSH message expression. Quantification of competitive RT-PCR reactions by ion-pair
reversed-phase HPLC was used to show that message expression is
increased (p < 0.05) in response to treatment with
progesterone (Fig. 6). Prolactin plus
progesterone further increased (p < 0.05) the amount
of message over the value for progesterone alone. Without progesterone,
the inclusion of prolactin in the treatment protocol resulted in RFBP levels comparable with estrous controls. This indicates that there is
tight regulation between the expression of the RING finger containing
RUSH protein and its binding partner.
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DISCUSSION |
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P-type ATPases comprise an evolutionarily diverse superfamily of nearly 200 ATP hydrolysis-driven ion pumps (33, 38). Structurally related to hydrolases (39), P-type ATPases are thought to share a common catalytic mechanism with these enzymes. Because P-type ATPases show very little similarity to each other (<15%), they were originally described as P1ATPases (heavy metal pumps), P2-ATPases (nonheavy metal pumps and phospholipid translocases), and P3-ATPases (bacterial K+ pumps). However, when arranged phylogenetically according to substrate specificity and sequence alignment, P-type ATPases can be divided into five main groups. The groups are designated Type I (heavy metal pumps), Type II (Ca2+, Na+/K+, and H+/K+ pumps), Type III (H+ and Mg2+ pumps), Type IV (phospholipid pumps), and Type V (no assigned substrate specificity). Type IV, the most recently discovered group is found only in eukaryotes and appears to be very distinct from the metal ion transporters that dominate this enzyme class. The absence of Type IV from prokaryotes supports the hypothesis that P-type ATPases are evolving at a variable rate and that Type IV enzymes have evolved more recently than their counterparts (33).
All working models of membrane topology for P-type ATPases contain
8 or 10 clearly defined transmembrane passes with four highly conserved
spans at the NH2 terminus (32-33, 40). Collectively these
transmembrane helices anchor the protein in the lipid bilayer, orient
the hydrophilic domains of the protein at the membrane surface, and
assemble into channel-like structures to regulate transport. As shown
in Fig. 7, the hydrophilic portions of
the protein, which include its NH2 and COOH termini and two
loop segments, are located on the same side of the plasma membrane and
therefore in the same subcellular compartment (41). This topology
preferentially exposes the small, strongly hydrophilic loop (Regions
A-C) between transmembrane domains 2 and 3 and the large
conformationally flexible loop (Regions D-H) between transmembrane
domains 4 and 5 to the cytoplasm. Regions A-C have been assigned a
role in energy transduction that may be as simple as maintaining the
stability of the ATPase structure. Transmembrane domain 4 is thought to
be directly involved in energy transduction. The sequences that link
transmembrane domain 4 to the phosphorylation site, i.e.
regions D and E, are two of the three most highly conserved regions in
ATPases. Mutations in this region cause a significant reduction in the
transport capabilities of H+-ATPase (42). The
conformationally flexible loop that accounts for 45% of the
polypeptide contains highly conserved phosphorylation and ATP-binding
sites. The function of the phosphorylation site in all P-type ATPases
is the same, i.e. the transfer of -phosphate from ATP to
the aspartate residue in the phosphorylation site. In fact, P-type
ATPases were named for the participation of a high energy
aspartyl-phosphoryl enzyme intermediate in their catalytic cycle (38,
43). Phosphorylation of the aspartate (D) residue in the invariant
sequence DKTGT(L/I)T distinguishes P-type ATPases from V-type and
F0F1-ATPases.
|
The newly identified RFBP differs from all described previously Type IV P-type ATPases in three important ways. The most striking feature of this putative phospholipid pump is an odd number of transmembrane domains resulting from the absence of Region D and transmembrane domain 4. Because of the highly conserved nature of the NH2 terminus, the absence of the fourth membrane-embedded domain alters both the orientation of the adjacent hydrophilic domains and the determinants of transport specificity. Deletion of this region alters the conformational dynamic that functionally links the transport site in the membrane with the site of ATP hydrolysis and strongly suggests that RFBP is not involved in phospholipid transport. In the larger scheme of evolutionary advantage, altered substrate specificity requires a change in structural constraint resulting from a dramatic change in primary structure (33). Such a change in substrate specificity is likely to result from the absence of Region D and the PEGL motif, which is considered to play a critical role in energy transduction (44).
Our first thought was that the endometrial RFBP might be the product of an alternative splice event. Once considered to be the exception to the rule (one gene, one protein), alternative splicing is known to regulate ~5% of all genes (45). It is an economical way to produce different products from the same gene (46-47). A survey on intron and exon length by Hawkins (48) indicated that although introns in vertebrates vary in size from 40 to greater than 3000 nucleotides, the largest single size range is 80-90 nucleotides. Region D and its included transmembrane domain 4 are encoded by 72 nucleotides that could easily participate in the simplest of alternative splicing events, i.e. splice/don't splice. However, sequences from genomic clones confirmed that Region D and transmembrane domain 4 are absent from the RFBP gene. These results support a working model for membrane topology (Fig. 7) in which the NH2 and COOH termini of RFBP are located on opposite sides of the membrane.
The second, equally striking feature of RFBP is its exclusive presence in the nuclear membrane. Nicotera et al. (49) and Lanini et al. (50) identified a nuclear Type II P-type Ca2+-ATPase whose structure is that of a transporting pump. However, no Type IV P-type ATPases have been localized to the nuclear membrane. The use of immunoelectron microscopy to show RFBP is located in the inner nuclear membrane provides additional insights to its atypical structure. As shown in Fig. 7, the small hydrophilic loop (Regions A-C; 174 residues) extends into the perinuclear space that is contiguous with the lumen of the endoplasmic reticulum, and the large conformationally flexible loop (Regions E-H; 499 residues) extends into the nucleoplasm. Physical contact between the large loop and the euchromatin was confirmed with immunoelectron microscopy. A comparison (51-52) of the three-dimensional map of the neurospora plasma membrane H+-ATPase (53) with the map of the sarcoendoplasmic reticulum Ca2+-ATPase shows their transmembrane domains are similar, but their large loops differ substantially. The compact conformation of the Ca2+-ATPase contrasts with the relatively open conformation of the large cytoplasmic loop of the H+-ATPase, which extends to a maximum height of 80 Å above the membrane surface and measures 85 × 50 Å in cross-section (53). Such conformational differences can be attributed to major rigid body interdomain movements (52).
The third intriguing feature of RFBP is its ability to bind the RING finger, the common feature of a superfamily of nearly 200 otherwise nonhomologous proteins (4, 7, 14), many of which are transcription factors. Conventional approaches to understanding transcriptional regulation of target genes have been focused on the identification and characterization of promoter elements and their cognate binding proteins. However, it is biologically meaningful to investigate transcriptional activation and chromatin remodeling as interrelated processes within the context of nuclear architecture (54). Not only is intranuclear organization required for physiological control of normal gene expression, modifications in nuclear organization are linked to cancer and neurological disorders (55) and are likely to be linked to some forms of infertility. Multiple mechanisms are involved in the entry and trafficking of regulatory factors, and at least two signals are required, i.e. a nuclear localization signal and a nuclear matrix-targeting signal. Once inside the nucleus, proteins are targeted to unique, nonoverlapping sites where gene activation or suppression occurs. For example, gene regulatory factors (steroid receptors), chromatin-remodeling proteins (SWI/SNF), and processing factors (SC35) are found in discrete subnuclear foci, a unique subset of which is associated with RNA polymerase II (54, 55). The punctate distribution of regulatory proteins, some of which are members of the RING finger family, has provided experimental opportunities for exploring the mechanism for compartmentalization within the nucleus (54). Moreover, RING domains are thought to be molecular scaffolds responsible for the assembly of protein complexes (9). Although the biochemical basis for the RFBP-RING-euchromatin interaction remains obscure, these physical affiliations support the speculation that RFBP is part of a mechanism that coordinates the spatial organization of regulatory proteins with RING domains within the nucleus.
The potential for hormones to regulate the expression of ATPases
generally, and P-type ATPases specifically, remains relatively unexplored. A few studies consider the effects of hormones on ATPase
activity. For example, the demonstration that physiologically relevant
concentrations of estradiol increased the hydrolytic activity of rat
cortical Ca2+-ATPase (56) supports the idea that this
plasma membrane calcium pump is a nongenomic steroid target (56).
Menkes- and Wilson-ATPases have been implicated in human disorders of
copper homeostasis. In the case of the Menkes P-type ATPase, treatment
of human breast carcinoma cells, PMC42, with a combination of estrogen,
progesterone, and prolactin increased perinuclear (Golgi) and punctate
(endosome) protein, as measured by indirect immunofluorescence (57).
However, Northern analysis failed to show an effect of hormones on
mRNA expression. By comparison, we used competitive RT-PCR and an
ion-pair reversed-phase HPLC product purification and detection system to show that low abundance endometrial RFBP mRNA expression is regulated by progesterone and that prolactin augments the
progesterone-dependent increase in RFBP message. This is
the first demonstration that hormones regulate the expression of a
P-type ATPase in the uterus. The importance of ATPases in reproduction
is underscored by the recent demonstration (58) that the isoform of
the Na+/K+-ATPase plays a critical role in
sperm motility and fertilization.
Only the Type IV P-type ATPase from B. taurus (protein ID
AAD03352) has been authenticated at the biochemical level as a
phospholipid pump (59). Sequence similarity between this known
phospholipid transporter and RFBP supports the idea that RFBP may
regulate nuclear phospholipid composition such that levels of
intranuclear phospholipids are higher for active chromatin than for
repressed chromatin (60). However, the unique structure of RFBP coupled to its ability to bind the RING domain and contact euchromatin supports
the idea that it has a very different function. It is tempting to
speculate that RFBP is part of a molecular mechanism that targets
regulatory proteins, in this case transcription factors with RING
finger motifs, to specific domains within the nucleus.
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ACKNOWLEDGEMENTS |
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We thank Peter A. Doris, Institute of Molecular Medicine, University of Texas at Houston for help in developing the heterologous competitor RNA and for use of the HPLC quantification system. We also thank Benny C. Shaw, Jr. for artwork.
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FOOTNOTES |
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* This work was supported by National Institutes of Health Grant HD29457 (to B. S. C.).The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.
The nucleotide sequence(s) reported in this paper has been submitted to the GenBankTM/EMBL Data Bank with accession number(s) AF236061.
The amino acid sequence of this protein can be accessed through NCBI Protein Database under NCBI accession number AAF68024.
To whom correspondence and reprint requests should be addressed:
Dept. of Cell Biology and Biochemistry, Texas Tech University Health
Sciences Center, 3601 4th St., Lubbock, TX 79430. Tel.: 806-743-2709;
Fax: 806-743-2990; E-mail: beverly.chilton@ttmc.ttuhsc.edu.
Published, JBC Papers in Press, October 31, 2000, DOI 10.1074/jbc.M004231200
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ABBREVIATIONS |
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The abbreviations used are: RFBP, RING finger binding protein; PCR, polymerase chain reaction; kb, kilobase(s); bp, base pair(s); HPLC, high performance liquid chromatography; RACE, rapid amplification cDNA ends; GST, glutathione S-transferase; TBST, Tris-buffered saline with 0.1% Tween 20; RT, reverse transcription.
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