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ORIGINAL PAPER
Multiple histone deacetylases are recruited by corepressor Sin3and contribute to gene repression mediated by Opi1 regulatorof phospholipid biosynthesis in the yeast Saccharomyces cerevisiae
Mathias Grigat • Yvonne Jaschke •
Felix Kliewe • Matthias Pfeifer •
Susanne Walz • Hans-Joachim Schuller
Received: 12 September 2011 / Accepted: 13 April 2012 / Published online: 28 April 2012
� Springer-Verlag 2012
Abstract Yeast genes of phospholipid biosynthesis are
negatively regulated by repressor protein Opi1 when pre-
cursor molecules inositol and choline (IC) are available.
Opi1-triggered gene repression is mediated by recruitment
of the Sin3 corepressor complex. In this study, we sys-
tematically investigated the regulatory contribution of
subunits of Sin3 complexes and identified Pho23 as
important for IC-dependent gene repression. Two non-
overlapping regions within Pho23 mediate its direct inter-
action with Sin3. Previous work has shown that Sin3
recruits the histone deacetylase (HDAC) Rpd3 to execute
gene repression. While deletion of SIN3 strongly alleviates
gene repression by IC, an rpd3 null mutant shows almost
normal regulation. We thus hypothesized that various
HDACs may contribute to Sin3-mediated repression of
IC-regulated genes. Indeed, a triple mutant lacking
HDACs, Rpd3, Hda1 and Hos1, could phenocopy a sin3
single mutant. We show that these proteins are able to
contact Sin3 in vitro and in vivo and mapped three distinct
HDAC interaction domains, designated HID1, HID2 and
HID3. HID3, which is identical to the previously described
structural motif PAH4 (paired amphipathic helix), can bind
all HDACs tested. Chromatin immunoprecipitation studies
finally confirmed that Hda1 and Hos1 are recruited to
promoters of phospholipid biosynthetic genes INO1 and
CHO2.
Keywords Histone deacetylase � Phospholipid
biosynthesis � Saccharomyces cerevisiae � Opi1 � Sin3 �Paired amphipathic helix
Introduction
Transcriptional corepressor complexes in eukaryotes are of
central importance for negative regulation of numerous
structural genes by creating a local structure of chromatin
inhibitory to gene expression. In the yeast Saccharomyces
cerevisiae, two pleiotropic corepressor complexes, Sin3
and Ssn6/Tup1, have been described (reviewed by Grzenda
et al. 2009; Silverstein and Ekwall 2005; Malave and Dent
2006), both of which execute gene repression by recruiting
histone deacetylases (Kadosh and Struhl 1997; Watson
et al. 2000; Davie et al. 2003). Since neither of these
complexes displays DNA binding, promoter targeting is
achieved through interactions with sequence-specific
DNA-binding proteins.
We have previously shown that the specific repressor
Opi1 of yeast phospholipid biosynthesis functions by
recruiting Sin3 and Ssn6 (Wagner et al. 2001; Jaschke et al.
2011). Structural genes of phospholipid biosynthesis such
as INO1, CHO1 and CHO2 are repressed when precursor
molecules inositol and choline (IC) are available in excess.
In contrast, limiting concentrations of IC allow activation
of these genes which is triggered by the heterodimeric
transcription factor Ino2/Ino4 (Schwank et al. 1995;
reviewed by Chen et al. 2007). Both Ino2 and Ino4 are
members of the basic helix-loop-helix (bHLH) family of
Communicated by H. Ronne.
M. Grigat and Y. Jaschke contributed equally to this work.
Electronic supplementary material The online version of thisarticle (doi:10.1007/s00438-012-0692-x) contains supplementarymaterial, which is available to authorized users.
M. Grigat � Y. Jaschke � F. Kliewe � M. Pfeifer � S. Walz �H.-J. Schuller (&)
Institut fur Genetik und Funktionelle Genomforschung,
Jahnstrasse 15a, 17487 Greifswald, Germany
e-mail: [email protected]
123
Mol Genet Genomics (2012) 287:461–472
DOI 10.1007/s00438-012-0692-x
DNA-binding proteins and specifically interact with the
UAS element ICRE (inositol/choline-responsive ele-
ment = UASINO; Schuller et al. 1992; Ambroziak and
Henry 1994; Hoppen et al. 2005) found upstream of
phospholipid biosynthetic genes. While Ino4 is responsible
for nuclear import of the heterodimer and its DNA binding
(Kumme et al. 2008), Ino2 mediates transcriptional acti-
vation (Schwank et al. 1995; Dietz et al. 2003) and regu-
latory input via its Opi1 interaction domain (Heyken et al.
2005). Thus, Opi1 as the specific repressor of ICRE-
dependent genes is indirectly recruited to target promoters
by activator Ino2 (Wagner et al. 2001).
Genetic analysis initially has shown that negative reg-
ulation of phospholipid biosynthetic genes by IC requires
the pleiotropic repressor Sin3, which can bind to the
N-terminus of Opi1 (containing OSID: Opi1-Sin3 interac-
tion domain; Slekar and Henry 1995; Wagner et al. 2001).
Sin3 contains four paired amphipathic helix motifs (PAH1–
PAH4; Wang et al. 1990) which via protein–protein
interactions support its function as a scaffold for various
unrelated regulatory networks. Interestingly, OSID is
responsible for interaction with PAH1 of Sin3 and for
contacting tetratricopeptide repeat motifs (TPR) of core-
pressor Ssn6 (Jaschke et al. 2011). Being recruited to
defined control regions via interaction with specific regu-
lators, Sin3 executes repression by associated histone
deacetylases (HDACs) such as Rpd3 in yeast (Kadosh and
Struhl 1997) and HDAC1 and HDAC2 in mammalian
systems (Laherty et al. 1997). Methods of proteomic
analysis led to the identification of two multiprotein com-
plexes (designated Sin3/Rpd3L and Sin3/Rpd3S; Loewith
et al. 2001; Carrozza et al. 2005b), varying with respect to
auxiliary proteins. While Rpd3L preferentially localizes to
promoter regions (Rundlett et al. 1998), Rpd3S is associ-
ated with transcribed regions (Joshi and Struhl 2005),
possibly preventing internal initiations. Importantly, the
genome of S. cerevisiae encodes five Zn2?-containing
HDACs which deacetylate histones by hydrolysis (Rpd3,
Hda1, Hos1, Hos2 and Hos3; Rundlett et al. 1996), while
Sir2 is a NAD-dependent enzyme. Based on sequence
similarities, HDACs have been classified into four groups
(class I, Rpd3, Hos1 and Hos2 in S. cerevisiae; class II,
Hda1 and Hos3; class III, Sir2 and related sirtuins; class
IV, no member in yeasts; reviewed by Hildmann et al.
2007; Yang and Seto 2008).
Previous work focusing on the negative regulatory ele-
ment URS1 and its specific binding factor Ume6 proposed
the simple regulatory hierarchy URS1-Ume6-Sin3-Rpd3
(Kadosh and Struhl 1997). However, a more complex sit-
uation may be effective with other genes repressed by Sin3.
Our previous analysis of ICRE-dependent gene regulation
showed that repression by IC is severely alleviated in a sin3
null mutant, while loss of Rpd3 causes almost no change
(Wagner et al. 2001). We thus hypothesized that Sin3
should be able to recruit not only Rpd3, but also additional
HDACs which together may be required to transform
chromatin into a repressed state. In this study, we indeed
could show that loss of HDACs Rpd3, Hda1 and Hos1
phenocopies deletion of SIN3. This genetic result is further
confirmed by demonstration of physical interaction of Sin3
with Rpd3, Hda1 and Hos1 in vitro and in vivo. Finally, we
identify two additional HDAC interaction domains within
Sin3.
Materials and methods
Yeast strains, media and growth conditions
All strains of the yeast S. cerevisiae used in this study are
isogenic to the regulatory wild-type SIRP3 (Schwank et al.
1995), containing a chromosomally integrated ICRE-CYC1-
lacZ reporter gene. Strains differ with respect to the status of
subunits of Sin3 complexes and HDACs. Strains SIRP3.-
Dopi1, SIRP3.Dsin3, SIRP3.Dume6 and SIRP3.Drpd3 have
been described (Wagner et al. 2001). Null mutations were
introduced into SIRP3 by transformation with deletion
mutant alleles described below. Transformants obtained
were verified for the presence of the desired mutant allele
and the absence of the wild-type allele. Yeast extracts used
for protein–protein interaction assays were prepared from
strain C13-ABY.S86, lacking four vacuolar proteinases
(pra1 prb1 prc1 cps1; De Antoni and Gallwitz 2000). A
compilation of strains and genotypes is available as sup-
porting online Table 1.
Synthetic complete (SC) media used for selective
growth of transformants and conditions of IC repression or
derepression have been described (Schuller et al. 1992).
Although doubling times of mutants lacking multiple
HDACs were severely delayed with respect to the wild
type (275 min for the rpd3 hda1 hos1 triple mutant com-
pared with 100 min for the wild type), strains were uni-
formly harvested at a cell density of 2 9 107 cells/ml.
Plasmid constructions
The following plasmids were constructed by established
procedures to disrupt genes encoding subunits of Sin3
complexes and HDACs: pRH2 (Dsap30::HIS3), pRH4
(Dsds3::HIS3), pRH6 (Dpho23::kanMX), pSW2 (Ddep1::
LEU2), pSW21 (Dume1::LEU2), pTN2 (Drxt2::LEU2),
pTN4 (Deaf3::LEU2), pYJ11 (Dhos1::TRP1), pYJ16
(Dhos3::LEU2), pYJ18 (Dhda1::HIS3), pYJ20 (Dhos2::
hph) and pSS20 (Dino2::LEU2). To construct these plas-
mids, flanking sequences upstream and downstream of the
respective coding regions were amplified by PCR and
462 Mol Genet Genomics (2012) 287:461–472
123
inserted on both sides of the selection marker, allowing
total deletion of reading frames.
To perform interaction assays, Escherichia coli expres-
sion plasmids (derived from pGEX-2TK; GE Healthcare)
encoding various glutathione S-transferase (GST) fusions
were constructed. Length variants of coding regions of
PHO23, SDS3, SAP30, RPD3, HDA1 and HOS1 were
amplified by PCR and fused behind GST. Similarly,
HA-tagged length variants of Sin3 representing PAH and
HID domains were expressed in yeast using plasmid
p426-MET25HA (Mumberg et al. 1994). For bacterial
expression of selected Sin3 variants, plasmid pASK-IBA5
(tetR-regulated; IBA, Gottingen, Germany) was used.
Plasmid constructs encoding minimal length variants used
for interaction studies were verified by DNA sequencing to
confirm authenticity of gene fragments obtained by PCR.
Plasmid names and fused sequences are mentioned in the
legends of figures.
In vitro interaction assays (GST pull-down)
GST- and HA-tagged proteins used for interaction assays
by affinity chromatography were synthesized by E. coli
strain BL21 (Stratagene/Agilent). The tac promoter con-
trolling GST fusion genes was induced with 1 mM IPTG.
Similarly, tetR-dependent gene expression was activated
by 0.2 mg/l anhydrotetracycline. Derepression of MET25-
dependent gene fusions was achieved by cultivating yeast
transformants in the absence of methionine.
GST fusion proteins synthesized in E. coli were released
by sonication, immobilized on glutathione (GSH) Sephar-
ose and subsequently incubated with yeast or bacterial total
protein extracts containing HA fusions. To avoid unspecific
interactions, protein extracts were pre-cleared by treatment
with GSH Sepharose beads prior to incubation with GST
fusions. Details on washing steps at intermediary strin-
gency have been described (Wagner et al. 2001). After
release of GST fusions with free GSH (10 mM), eluates
were separated by SDS/PAGE and proteins transferred to a
filter. Following incubation with anti-HA-peroxidase con-
jugate, HA fusion proteins were detected with POD
chemiluminescent substrate (antibody conjugate and sub-
strate from Roche Biochemicals).
Two-hybrid assays
To perform two-hybrid assays, strain PJ69-4A was used
(MATa trp1 leu2 ura3 his3D gal4D gal80D GAL2-ADE2
LYS2::GAL1-HIS3 met2::GAL7-lacZ; James et al. 1996).
DNA fragments encoding interaction domains of Sin3,
Hda1, Hos1 and Rpd3 were inserted into plasmids pGBD-
C1 (2 lm GAL4DBD TRP1) and pGAD-C1 (2 lm GAL4TAD
LEU2), respectively. Double-transformed strains containing
both types of fusion plasmids were first selected on med-
ium lacking leucine and tryptophan (-L-T) and subse-
quently transferred to medium devoid of adenine (-L-T-A).
Chromatin immunoprecipitation
Essentially, chromatin immunoprecipitation (ChIP) analy-
sis followed the procedure described by Cobb and van
Attikum (2010). Chromosomal loci HDA1 and HOS1 were
modified such that they expressed His-tagged Hda1 and
Hos1 without alteration of gene copy number or control
region. Tagging was performed by transformation of strain
C13-ABY.S86 with a gene-specific modification fragment
and selection for resistance against geneticin. The modifi-
cation fragment was amplified by PCR, using gene-specific
primers and plasmid pU6H3HA as a template (contains a
His6-HA3-kanMX cassette; De Antoni and Gallwitz 2000).
The resulting strains FKY40 (HDA1-His6-HA3) and
FKY42 (HOS1-His6-HA3) and their isogenic ino2 deriva-
tives FKY44 and FKY46 grew until mid-log phase and
were treated with formaldehyde for 15 min. The cross-
linking reaction was subsequently quenched for 5 min by
addition of glycine to a final concentration of 125 mM.
After lysis, cells were sonicated five times for 30 s to shear
chromatin, using a Bandelin Sonoplus UW 70 microtip
(35 % power). After sonication, lysates were centrifuged
for 10 min at 16,0009g to remove insoluble material and
incubated for at least 4 h with His-Tag Dynabeads�
(Invitrogen/Dynal�). After elution of affinity-purified pro-
teins and bound DNA with a buffer containing 300 mM
imidazole, cross-linking was reversed by heating to 65 �C
overnight. DNA was recovered and analyzed by PCR (27
amplification cycles), using specific primers against INO1
(-315/?5) and CHO2 (-360/-40) promoters or ACT1
gene (?841/?1165) as a control.
Miscellaneous procedures
Transformation of S. cerevisiae strains, PCR amplification
and b-galactosidase assays have been described (Schwank
et al. 1995; Wagner et al. 2001). Oligonucleotides used in
this study are presented in supporting online Table 2.
Results
Importance of Sin3 binding proteins and multiple
HDACs for ICRE-dependent gene expression
We have previously shown that repression of ICRE-
dependent genes requires recruitment of pleiotropic
corepressor complexes Sin3 and Ssn6/Tup1 by the path-
way-specific repressor Opi1 (Wagner et al. 2001; Jaschke
Mol Genet Genomics (2012) 287:461–472 463
123
et al. 2011). We thus asked whether additional subunits of
Sin3 complexes, Rpd3L and Rpd3S (Carrozza et al. 2005a,
b), also contribute to repression of ICRE-dependent genes.
The possible importance of subunits Ash1, Raf60, Dot6
and Tod6 (Colina and Young 2005; Shevchenko et al.
2008) also identified in the Rpd3L complex was not
characterized in this study. For this investigation, we
constructed a set of isogenic single mutants, each con-
taining a synthetic minimal promoter, solely driven by
ICRE activating motifs (integrated ICRE-CYC1-lacZ
reporter gene; Schwank et al. 1995). To avoid confusion
among two regulatory pathways comprising Sin3, we did
not use an INO1-lacZ reporter gene, which in addition to
ICRE motifs is also affected by the URS1-Ume6-Sin3
pathway (Lopes et al. 1993; Kadosh and Struhl 1997). As a
means of deregulation in mutants, we used the ratio of
b-galactosidase activities assayed in cells grown under
derepressing and repressing conditions, respectively (D/R).
As is apparent from data shown in Table 1, subunits of
Sin3 complexes unequally affect ICRE-dependent gene
expression. In agreement with previous results (Wagner
et al. 2001), Sin3 is clearly of outstanding importance
(D/R = 2.0), but loss of subunits Pho23 (4.4) and Sap30
(6.1) also weakens the degree of regulation and increases
gene expression under repressing conditions at least by
1.5-fold.
It has been suggested that Sin3 executes its regulatory
influence by recruiting the HDAC Rpd3 (Kadosh and
Struhl 1997). In contrast to what was shown for a sin3
mutant, regulated expression of the reporter gene was not
significantly altered in an rpd3 null mutant (Wagner et al.
2001; Table 2). Apparently, Opi1-dependent repression of
Ino2-activated ICRE motifs is still effective even in the
Table 1 Subunits of Sin3/Rpd3 complexes differently influence
ICRE-dependent gene expression
Genotype (complex) Specific b-gal. activity (U/mg) D/R
D (SD) R (SD)
Wild type 220 (35) 20 (4) 11.0
sin3 (3L/3S) 86 (28) 44 (7) 2.0
rpd3 (3L/3S) 125 (20) 15 (2) 8.3
pho23 (3L) 215 (40) 49 (15) 4.4
sap30 (3L) 197 (35) 32 (8) 6.1
sds3 (3L) 191 (74) 28 (6) 6.8
dep1 (3L) 157 (40) 20 (5) 7.8
rxt2 (3L) 205 (25) 25 (6) 8.2
rxt3 (3L) 188 (36) 25 (3) 7.5
cti6 (3L) 293 (55) 26 (4) 11.3
ume6 (3L) 170 (35) 29 (3) 5.9
ume1 (3L/3S) 309 (32) 31 (3) 10.0
rco1 (3S) 345 (45) 35 (5) 9.9
eaf3 (3S) 245 (45) 20 (4) 12.2
Mutants used are deleted for a single gene and contain a chromo-
somally integrated ICRE-CYC1-lacZ reporter gene. Strains were
grown under repressing (R, 200 lM inositol ? 2 mM choline) and
derepressing conditions (D, 5 lM inositol ? 5 lM choline). Specific
b-galactosidase activities are given in nmol oNPG hydrolyzed per
min per mg of protein (U/mg). Each experiment represents the mean
value of at least 12 independent strain cultivations and enzyme
assays. 3L and 3S refer to complexes Rpd3L and Rpd3S, respectively
SD standard deviation
Table 2 Loss of HDACs, Rpd3, Hda1 and Hos1, imitates the
regulatory defect of a sin3 null mutation
Genotype Specific b-gal. activity (U/mg) D/R
D (SD) R (SD)
Wild type 220 (35) 20 (4) 11.0
opi1 240 (30) 250 (35) 1.0
sin3 86 (28) 44 (7) 2.0
rpd3 125 (20) 15 (2) 8.3
hda1 172 (30) 20 (3) 8.6
hos1 260 (30) 20 (2) 13.0
hos2 165 (25) 15 (2) 11.0
hos3 245 (35) 23 (3) 10.6
rpd3 hda1 113 (28) 33 (8) 3.4
rpd3 hos1 146 (30) 22 (5) 6.6
rpd3 hos2 67 (15) 8 (2) 8.4
rpd3 hos3 174 (25) 26 (5) 6.7
hda1 hos1 226 (28) 29 (4) 7.8
hda1 hos2 223 (30) 20 (4) 11.2
hda1 hos3 307 (38) 38 (6) 8.1
hos1 hos2 259 (24) 20 (4) 13.0
hos1 hos3 219 (32) 15 (3) 14.6
hos2 hos3 123 (20) 11 (2) 11.2
rpd3 hda1 hos1 80 (25) 42 (8) 1.9
rpd3 hda1 hos3 91 (27) 24 (5) 3.8
rpd3 hos1 hos2 90 (25) 11 (3) 8.2
rpd3 hos1 hos3 59 (17) 6 (2) 9.8
rpd3 hos2 hos3 59 (14) 8 (2) 7.4
hda1 hos1 hos2 215 (30) 21 (4) 10.2
hda1 hos1 hos3 260 (42) 22 (3) 11.8
hda1 hos2 hos3 94 (18) 6 (3) 15.7
hos1 hos2 hos3 56 (10) 5 (2) 11.2
rpd3 hda1 hos1 hos3 73 (20) 33 (8) 2.2
hda1 hos1 hos2 hos3 36 (15) 18 (6) 2.0
Strains with various combinations of HDAC gene deletions contain a
chromosomally integrated ICRE-CYC1-lacZ reporter gene. Strains
were grown under repressing (R, 200 lM inositol ? 2 mM choline)
and derepressing conditions (D, 5 lM inositol ? 5 lM choline).
Specific b-galactosidase activities are given in nmol oNPG hydro-
lyzed per min per mg of protein (U/mg). Each experiment represents
the mean value of at least 12 independent strain cultivations and
enzyme assays
SD standard deviation
464 Mol Genet Genomics (2012) 287:461–472
123
absence of Rpd3. We thus reasoned that a functional
redundancy among yeast HDACs, Rpd3, Hda1, Hos1, Hos2
and Hos3, may exist (Rundlett et al. 1996; no consideration
of Sir2 and related NAD-dependent HDACs). Conse-
quently, we constructed deletion cassettes for HDAC genes
to obtain all viable combinations of mutations rpd3, hda1,
hos1, hos2 and hos3. However, we failed to obtain the
following combinations of mutant alleles: triple mutant
rpd3 hda1 hos2; quadruple mutants rpd3 hda1 hos1 hos2,
rpd3 hda1 hos2 hos3 and rpd3 hos1 hos2 hos3; pentuple
mutant rpd3 hda1 hos1 hos2 hos3.
In contrast to HDAC single mutants which showed
normal repression, gene expression of the rpd3 hda1 dou-
ble mutant under repressing conditions was increased
(D/R = 3,4; cf. Table 2). Importantly, the triple mutant
rpd3 hda1 hos1 (1.9) copied the regulatory phenotype of a
sin3 null mutant (2.0), indicating that the corresponding
HDACs may be recruited by Sin3 to trigger repression of
ICRE-dependent genes.
Two non-overlapping sequences of Pho23 directly
interact with Sin3
Pho23 is required for negative regulation of ICRE-depen-
dent gene expression (Table 1). Interestingly, the C-ter-
minal region of Pho23 (amino acids 276-330) comprising
the zinc finger-related C4-HC3 plant homeodomain (PHD)
shows strong similarity to the mammalian family of ING
tumor suppressor proteins (inhibitor of growth) involved in
control of cellular proliferation. We thus wished to inves-
tigate whether Pho23 binds to Sin3 and to establish a
physical map of interacting domains in both proteins.
A GST-Pho23 fusion protein (full-length) immobilized at
glutathione (GSH) Sepharose was incubated with
HA-tagged Sin3, synthesized either in E. coli or in S. cerevi-
siae. As shown in Fig. 1, Sin3 from either source could
bind to Pho23, arguing for a direct interaction of both
proteins. For a more precise mapping, GST fusions with
Pho23 length variants were incubated with Sin3. Interest-
ingly, two non-overlapping domains of Pho23 outside of
ING similarity could bind to Sin3, each independent of the
other. These domains were designated PSID1 and PSID2
(Pho23-Sin3 interaction domain; amino acids 80-151 and
208-250, respectively).
Vice versa, we also mapped Sin3 domains required for
Pho23 interaction. GST fusions of Pho23 comprising either
PSID1 or PSID2 were incubated with HA-tagged length
variants of Sin3. Sin3 fragments used for the interaction
assay represent individual structural and functional domains
described previously (PAH1-PAH4, HID). As shown in
Fig. 2, both PSID sequences could bind aa 801-1100 of
Sin3 but not aa 601-950, indicating aa 951-1100 as the Sin3
core domain responsible for Pho23 recruitment. Thus, nei-
ther PAH domain is required for binding of Pho23, but
instead sequences following the HDAC interaction domain
are involved.
Although deregulation of ICRE-dependent genes was
less evident for sap30 and sds3 mutants than with a pho23
mutant, we also investigated whether the corresponding
proteins could directly interact with Sin3. Similar to what
was found for Pho23, GST fusions of full-length Sds3 and
Sap30 were able to bind HA-tagged Sin3 from yeast and
bacterial protein extracts, arguing for direct interaction
(Fig. 3a, b). The C-terminus of Sds3 (aa 201-327) interacts
with the same internal domain of Sin3 which is also bound
by Pho23 (aa 801-1100). The importance of the C-terminus
of Sds3 for binding Sin3 agrees with the existence of a
shortened protein in the yeast Saccharomyces kluyveri (173
amino acids; Cliften et al. 2003) lacking aa 1-144 of Sds3
from S. cerevisiae.
PS1 PS2
1
1
1
1 330
151
100
PHD
Pho23interactionwith Sin3
1 200
1 200
+Ec
+Sc
+Sc
Sc
Ec
++
Sc
80
330
151 +Sc
+Sc330154
330208 +Sc
330251 Sc
200154 Sc
+Sc250154
+Sc250
330208 +Ec
208
ScGST vector
Input HA3-Sin3
Input HA3-Sin3
Sc
Ec
Fig. 1 Mapping of Pho23 domains responsible for interaction with
Sin3. Length variants of Pho23 were fused with GST, immobilized on
GSH Sepharose and incubated with full-length HA3-Sin3 in total
protein extracts, synthesized by S. cerevisiae (Sc, strain C13-
ABY.S86, plasmid pCW117) or E. coli (Ec, strain BL21, plasmid
pSW11). GST-Pho23 fusions are encoded by plasmids pSW5 (aa
1-330), pSW23 (aa 1-100), pSW24 (aa 1-151), pSW25 (aa 1-200),
pSW26 (aa 251-330), pSW27 (aa 208-330), pSW28 (aa 154-330),
pSW32 (aa 208-250), pSW33 (aa 154-200), pSW35 (aa 154-250) and
pSW40 (aa 80-151). Input controls are shown at the bottom of the
figure (20 % of protein used for the interaction assay). PS1, PS2
(=PSID1, 2): Pho23-Sin3 interaction domains 1 and 2; PHD plant
homeodomain
Mol Genet Genomics (2012) 287:461–472 465
123
HDAC Hda1 binds to Sin3 via new interaction domains
As shown above, the absence of Rpd3, Hda1 and Hos1
imitates the regulatory defect observed in a strain lacking
Sin3. Thus, in addition to Rpd3, HDACs Hda1 and Hos1
may also directly contact the Sin3 corepressor to induce a
more compact chromatin. Class II HDAC Hda1 contains a
long C-terminus of unknown function. To investigate
a possible interaction of Hda1 with Sin3, we used GST-Hda1
fusions comprising amino acids 1-353 and 354-706,
respectively. Indeed, the N-terminus of Hda1 with its
deacetylase domain could bind HA-Sin3 full-length protein
(cf. Fig. 4a). In subsequent studies, we therefore used the
GST-Hda1 (1-353) fusion plasmid to map the Sin3 domain
required for interaction. To allow a high resolution of
mapping, HA-tagged length variants of Sin3 described
above together with smaller fragments each synthesized in
yeast were used for the interaction assay. As is shown in
Fig. 4a, two non-overlapping Sin3 fragments representing
amino acids 301-600 and 1101-1536 (comprising PAH2
and PAH4, respectively) were able to bind to Hda1.
Importantly, these fragments do not contain the previously
characterized HDAC interaction domain (HID, aa
729-1048). By using N- and C-terminal truncations of the
fragment 301-600, we were able to show that it was not
PAH2 (406-472), but instead a region in its C-terminus (aa
473-600) that was sufficient to bind Hda1. The same result
was obtained with the Sin3 fragment comprising aa
1101-1210. We thus conclude that PAH4 (core sequence:
aa 1131-1208) can also bind to Hda1. Obviously, Sin3
contains at least three HID regions which we now desig-
nate HID1 (former HID), HID2 and HID3 (cf. Fig. 4).
We next wanted to map the region within Hda1 which is
required for interaction with Sin3. Length variants of Hda1
were fused with GST and used for interaction assays with
Sin3 sequences representing HID2 and HID3 (aa 301-600
and 1101-1300, respectively). Hda1 fragments aa 201-300
and aa 251-353 could interact with HID2 and HID3 of Sin3
(Fig. 5a), indicating that the region of aa 251-300 may
function as the core binding domain. Since identical results
were obtained with proteins entirely produced in E. coli,
we concluded that aa 251-300 of Hda1 mediated its inter-
action with HID2 and HID3 of Sin3.
HDAC Hos1 also binds to HID2 and HID3 within Sin3
In further studies, we investigated whether class I HDAC
Hos1 could also bind to Sin3. Immobilization of GST-Hos1
(full-length) on GSH Sepharose indeed allowed retention of
full-length Sin3. Subsequently, HA-tagged length variants
1
1 1536
Sin3 bait proteins
301 600
601 950
300
15361101
InputSin3
Pho23PSID1
Pho23PSID2
+ +
P1 P2 P3 P4
801 1100 + +
Fig. 2 Mapping of Sin3 domains interacting with PSID1 and PSID2
of Pho23. GST-Pho23 fusion plasmids pSW25 and pSW32 were used
to synthesize residues 1-200 (comprising PSID1) and 208-250
(comprising PSID2). The following expression plasmids representing
individual PAH domains were used for synthesis of HA-tagged Sin3
length variants in S. cerevisiae: pCW117 (aa 1-1536), pCW83 (aa
1-300), pYJ91 (aa 301-600), pYJ90 (aa 601-950), pYJ89 (aa
801-1100) and pMP20 (aa 1101-1536). For input controls (shown in
the right panel of the figure), 20 % of protein used for the interaction
assay was analyzed. P1, P2, P3 and P4 (=PAH1-4): paired amphi-
pathic helices 1–4
1
1 327
Sds3 Interaction with Sin3
1 200
201 327
+Ec
+
+
Sc
Sc +
327
Sc 1 - 1536
1 - 1536
1 - 1536
1 - 1536
801 - 1100201 327
1
1 201
Sap30 Interaction with Sin3
++
201
Sc 1 - 1536
1 - 1536
1 - 1536GST vector
(a)
(b)
Ec
Sc
Sc
GST vector 801 - 1100Sc
Fig. 3 Direct interaction of Sds3 (a) and Sap30 (b) with Sin3.
Fusion proteins GST-Sds3 (aa 1-327, encoded by pSW4), GST-Sds3
(aa 1-200, pMG4), GST-Sds3 (aa 201-327, pMG6) and GST-Sap30
(aa 1-201, pSW3), respectively, were immobilized on GSH Sepharose
and incubated with protein extracts containing epitope-tagged length
variants of Sin3. Protein extracts were prepared from transformants of
S. cerevisiae (Sc, plasmids pCW117 or pYJ89, 801-1100 of Sin3) or
E. coli (Ec, pSW11). Sin3 input controls are shown in Figs. 1 and 2
466 Mol Genet Genomics (2012) 287:461–472
123
of Sin3 described above were also used to map minimal
interaction domains. As is shown in Fig. 4b, minimal
fragments of Sin3, comprising HID2 and HID3 (=PAH4),
were also able to bind to Hos1, while HID1 again failed to
interact with Hos1. Thus, an identical interaction pattern
was observed for Hda1 and Hos1. Similar to what was
found for Hda1, the enzymatic deacetylase core domain of
Hos1 (amino acids 236-400) is sufficient for this interaction
(Fig. 5b). Again, binding of the Hos1 core region also
occurs with HID2 and HID3 of Sin3 synthesized in E. coli,
arguing for a direct interaction.
HDACs, Rpd3, Hda1 and Hos1, all bind to HID3/PAH4
of Sin3
Initially, HID(1) was identified as a conserved region of
mSin3A (amino acids 524-851, similar to aa 729-1048 of
1
1 1536
Interactionwith Hda1
301 600
601 950
300
InputSin3
P1 P2 P3 P4
801 1100
472301
600473
575473
15361101
13001101
12101101
13001140
+
+
+
+
+
+
1
1 1536
Interactionwith Hos1
301 600
601 950
300
801 1100
600473
15361101
12101101
+
+
+
H2
++
Sin3
(a) Pull-down assays with GST-Hda1
1
Interactionwith Rpd3
301 600
601 950
300
+++
++
15361101
12101101
H1(= H3)
13001101
801 1100
(b) Pull-down assays with GST-Hos1
(c) Pull-down assays with GST-Rpd3
Fig. 4 Mapping of Sin3 domains interacting with histone deacety-
lases Hda1, Hos1 and Rpd3. a GST-Hda1 fusion protein (residues
1-353 of Hda1, plasmid pMP1) was immobilized on GSH Sepharose
and incubated with yeast protein extracts containing epitope-tagged
length variants of Sin3. The following plasmids were used for
synthesis of Sin3 length variants: pCW117 (aa 1-1536), pCW83 (aa
1-300), pYJ91 (aa 301-600), pYJ90 (aa 601-950), pYJ89 (aa
801-1100), pMP20 (aa 1101-1536), pYJ105 (aa 301-472), pMG7
(aa 473-600), pMG8 (aa 473-575), pMP22 (aa 1101-1300), pMG13
(aa 1101-1210) and pMG15 (aa 1140-1300). b Incubation of
immobilized GST-Hos1 full-length fusion protein (470 amino acids,
plasmid pYJ26) with yeast protein extracts containing epitope-tagged
length variants of Sin3. c Incubation of immobilized GST-Rpd3
fusion protein (residues 141-300 of Rpd3, plasmid pMG17) with yeast
protein extracts containing epitope-tagged length variants of Sin3.
H1, H2, H3, histone deacetylase interaction domains HID1-3; P1, P2,
P3 and P4: paired amphipathic helices PAH1-4
1
Hda1
Interaction with
354 706
201 353
353
DAC
201 300
+(301-600)
Sin3(301-600)
Sin3
+
+
+(1101-1300)
Sin3(1101-1300)
Sin3
+
+
EcInput HA3-Sin3
201 300 + +Ec
Sc
Sc
Sc
Sc
251 353 + +Sc
Hos1
Interaction with
236 470
DAC
236 400
+(301-600)
Sin3(301-600)
Sin3
++
(1101-1300)Sin3
(1101-1300)Sin3
+
1 470
1 350
n. t.
n. t.
n. t.
Sc
Sc
Sc
Sc
Ec + +236 400
Rpd3
Interaction with
141 300
DAC
+(801-950)
Sin3(801-950)
Sin3
++
(1101-1300)Sin3
(1101-1300)Sin3
+ScSc
Ec141 300
+
EcInput HA3-Sin3
(a) Pull-down assays with GST-Hda1 variants
(b) Pull-down assays with GST-Hos1 variants
(c) Pull-down assays with GST-Rpd3
Fig. 5 Mapping of HDAC domains interacting with Sin3 domains
HID1, HID2 and HID3. a Length variants of Hda1 were fused with
GST, immobilized on GSH Sepharose and incubated with protein
extracts from yeast or E. coli. The following GST expression
plasmids were used: pMP1 (aa 1-353), pMP2 (aa 354-706), pMP12
(aa 201-353), pMP14 (aa 201-300) and pMP15 (aa 251-353). Epitope-
tagged Sin3 domains representing HID2 and HID3 were expressed in
yeast (Sc; plasmids pYJ91, aa 301-600 and pMP22, aa 1101-1300,
respectively) or in E. coli (Ec; pMG22 and pMG23, respectively).
b Length variants of Hos1 fused with GST were incubated with
protein extracts from yeast or E. coli. The following GST expression
plasmids were used: pYJ26 (aa 1-470), pMP9 (aa 1-350), pMP4 (aa
236-470) and pYJ85 (aa 236-400). c GST-Rpd3 fusion representing
residues 141-300 of Rpd3 (plasmid pMG17) was incubated with
protein extracts from yeast or E. coli. The epitope-tagged Sin3
domain representing HID1 was expressed in yeast (Sc; plasmid
pYJ92, aa 801-950) or in E. coli (Ec; pMG26). Yeast input controls
are shown in Fig. 4. DAC deacetylase core domain, n. t. not tested
Mol Genet Genomics (2012) 287:461–472 467
123
yeast Sin3), which turned out as sufficient to bind the
Rpd3-related mammalian HDAC2 (Laherty et al. 1997).
We thus wished to test whether Rpd3 can also interact with
a second domain of Sin3 and to perform a more precise
mapping of the yeast HID1. Assuming that a conserved
segment within HDACs may be responsible for Sin3
binding, we constructed a GST-Rpd3 fusion containing
amino acids 141-300. Indeed, this fusion protein could
interact with two Sin3 fragments covering HID1 (aa
601-950 and aa 801-1100; Fig. 4c). Using proteins entirely
produced in E. coli, we could finally confirm that amino
acids 801-950 indeed defined the functional core of HID1,
which was directly bound by Rpd3 without yeast-specific
auxiliary factors (Fig. 5c). In addition, GST-Rpd3 was also
able to bind Sin3 fragments containing HID3/PAH4, syn-
thesized either in yeast or in E. coli. Consequently, HID3/
PAH4 functions as an interaction domain for at least three
HDACs from yeast.
In vivo interaction of Sin3 with various HDACs
In addition to in vitro interaction assays, we also performed
two-hybrid analyses to verify binding of Sin3 to HDACs,
Hda1, Hos1 and Rpd3. Length variants of Sin3 comprising
HID2 (aa 301-600) and HID1, HID2 and HID3 (aa
301-1536), respectively, were fused with the DNA-binding
domain (DBD) of Gal4. Core deacetylase domains of
Hda1, Hos1 and Rpd3 which have been shown to bind Sin3
in vitro were fused with Gal4 transcriptional activation
domain (TAD). Sin3-HDAC interactions in vivo should
reconstitute a functional Gal4 activator being able to
induce the GAL2-ADE2 reporter gene of the recipient
strain, thereby allowing growth of transformants in the
absence of adenine. As is shown in Fig. 6, both DBD
fusions of Sin3 in combination with empty TAD vector
were unable to mediate growth on a medium lacking ade-
nine. In contrast, co-transformation of DBD-Sin3 (aa
301-1536) with TAD fused to HDACs, Hda1, Hos1 or
Rpd3, restored growth on adenine-free medium. We con-
clude that Sin3 comprising HID1-3 is able to interact with
these HDACs in vivo. On the other hand, a minimal Sin3
(aa 301-600) with HID2 but devoid of HID1 and HID3
could interact with Hda1 and Hos1, but not with Rpd3.
To finally investigate whether Hda1 and Hos1 are
indeed recruited to ICRE-containing promoters regulated
by Ino2 and Opi1, we performed ChIP analyses. We thus
constructed strains containing variants of HDA1 and HOS1
which encode epitope-tagged proteins (His6). To analyze
protein occupation of ICRE-containing promoters, we
selected INO1 (biosynthesis of inositol; three ICRE motifs)
and CHO2 (biosynthesis of choline, three ICRE motifs).
The ACT1 gene encoding actin served as a negative con-
trol. As shown by pull-down experiments and two-hybrid
studies, binding of HDACs follows a defined order of
interaction events (ICRE-Ino2-Opi1-Sin3-HDACs; Wagner
et al. 2001; this work). We thus also constructed ino2
deletion strains which should no longer allow recruitment
of HDACs to ICRE-containing promoters. As shown in
Fig. 7, Hda1 and Hos1 indeed occupy ICRE-dependent
promoters INO1 and CHO2 under conditions of gene
repression by inositol and choline (lines 1 and 3; INO2
intact), while binding to ACT1 is substantially less effec-
tive. The figure also shows that binding of HDACs, Hda1
and Hos1, requires a functional INO2 gene (lines 2 and 4,
ino2 deletion mutants). These findings agree with results
derived from in vitro interaction studies and provide in
vivo evidence that ICRE-dependent promoters are affected
by more than a single histone deacetylase.
Discussion
The importance of Sin3 as a pleiotropic corepressor for
several regulatory systems of gene expression in eukary-
otes is well known (Grzenda et al. 2009). The existence of
Growth on-L -T -L -T -A
Opi1 (1-106)
Sin3 (301-1536)
Sin3 (301-1536)
Sin3 (301-1536)
Sin3 (301-1536)
Sin3 (301-600)
Sin3 (301-600)
Sin3 (301-600)
Sin3 (301-600)
DBD fusion
Sin3 (1-300)
-
Hda1 (201-353)
Hos1 (236-400)
Rpd3 (141-300)
-
Hda1 (201-353)
Hos1 (236-400)
Rpd3 (141-300)
TAD fusion
Fig. 6 Interaction of Sin3 with various HDACs shown by two-
hybrid assays. The Gal4 DNA-binding domain (DBD) was fused with
Sin3 fragments comprising HDAC interaction domains to give
plasmids pMG42 (aa 301-600) and pJW31 (aa 301-1536). Corre-
spondingly, Gal4 transcriptional activation domain (TAD) was fused
with HDAC fragments to give pMG41 (Hda1, aa 201-353), pMG40
(Hos1, aa 236-400) and pMG39 (Rpd3, aa 141-300). Plasmids
encoding fusions DBD-Opi1 and TAD-Sin3 (pJW8 and pJW1,
respectively; Wagner et al. 2001) were used as a positive control.
As a negative control, empty TAD vector pGAD-C1 was used. DBD
and TAD pairs of fusion plasmids (selection markers: TRP1 and
LEU2, respectively) were co-transformed into strain PJ69-4A,
containing a GAL2-ADE2 fusion which allows growth in the absence
of adenine when a functional Gal4 activator is reconstituted. Selection
plates (-L -T and -L -T -A; absence of leucine, tryptophan and
adenine) were incubated for 48 h
468 Mol Genet Genomics (2012) 287:461–472
123
structural motifs suitable for protein–protein interactions
suggested that Sin3 functioned as a recruiting platform for
effector enzymes (e.g., HDAC Rpd3), allowing their access
to specific promoter regions. In this study, we have
investigated the influence of subunits of the Sin3 complex
for regulation of phospholipid biosynthetic genes. Char-
acterization of various combinations of HDAC mutations
led us to conclude that Rpd3 was not the sole enzyme
responsible for gene repression mediated by Sin3. This
hypothesis is further confirmed by our demonstration of
physical interaction of Sin3 with HDACs, Rpd3, Hda1 and
Hos1. The existence of three non-overlapping HDAC
interaction domains (HID1, HID2 and HID3) indicates that
a greater combinatorial variety of Sin3-containing com-
plexes than previously assumed is able to contribute to
target gene repression.
The Sin3/Rpd3L complex comprises at least 12 subunits
which may stabilize interactions of Sin3 with specific
repressors and thus unequally influences different regula-
tory pathways. Surprisingly, phenotypes of the corre-
sponding null mutants differ with respect to the regulatory
system, leading to enhanced repression of yeast silent
mating type loci and at telomeric positions, but increased
initiation at the PHO5 promoter and URS1-containing
promoters (Vannier et al. 1996; Zhang et al. 1998; Sun and
Hampsey 1999; Loewith et al. 2001). To investigate the
importance of 13 subunits identified in complexes Rpd3L
and Rpd3S for ICRE-dependent gene expression, we used
single null mutants for analyzing the regulation of a syn-
thetic minimal promoter which did not contain a URS1
motif such as the widely used INO1 control region. Besides
sin3, deregulation was most apparent with a pho23 mutant,
which was initially isolated because of increased expres-
sion of the PHO5-encoded acid phosphatase (Lau et al.
1998). Pho23 is especially interesting due to the similarity
of its C-terminal PHD finger with mammalian tumor sup-
pressors of the ING family. This structural motif strongly
binds to trimethylated lysine of histone H3 (H3K4me3) and
mediates recruitment of Sin3/Rpd3L to the repressed
PHO5 promoter (Shi et al. 2006; Wang et al. 2011). Our
results show that Pho23 contains two non-overlapping
domains which both can directly bind to a domain of Sin3
close to HID1. In contrast to Rpd3, Pho23 interacts with aa
801-1100 but not with aa 601-950, suggesting that aa
951-1100 are at least necessary for binding of Pho23.
Similarly, Sds3 also binds to aa 801-1100 of Sin3 (sum-
marized in Fig. 8a). We could also demonstrate that Sds3
and Sap30 directly interact with Sin3. For the mammalian
ING1b protein, association with Sin3 through direct inter-
action with Sap30 has been shown (Kuzmichev et al.
2002).
Importantly, comparison of ICRE-dependent gene reg-
ulation in sin3 and rpd3 null mutants revealed a striking
difference, indicating that Rpd3 could not be responsible
for the entire repressing influence of the Sin3 complex.
Inspection of the data published by Kadosh and Struhl
(1997) on URS1-Ume6 dependent repression showed that
similarly loss of gene repression in a sin3 mutant was
clearly stronger than in an rpd3 mutant. Both findings can
be explained by assuming a separate repressing activity
within the Sin3 complex which is not mediated by histone
deacetylation or, alternatively, triggered by recruitment of
HDAC isoenzymes. Our first evidence supporting the latter
view resulted from construction of multiple HDAC null
mutants and subsequent analysis of ICRE-dependent gene
expression. Although we failed to obtain certain combi-
nations of mutant alleles (indicating that total loss of class I
and class II HDACs leads to synthetic lethality), a triple
mutant rpd3 hda1 hos1 showed deregulation similar to that
observed with a sin3 single mutant.
Our studies with the ICRE-dependent reporter gene
revealed that repression and derepression were affected in
the sin3 strain and in several mutants lacking multiple
HDACs (cf. Table 2). These data could mean that activa-
tors as well as repressors may utilize Sin3, as it has been
shown for the Ssn6/Tup1 corepressor which also acts as a
positive cofactor of Gcn4 activator (Kim et al. 2005).
Similarly, a positive role of Sin3-Rpd3 for activation of
osmosensitive genes such as HSP12 has been shown (de
Nadal et al. 2004). Alternatively, pleiotropic deregulation
in a sin3 strain affecting carbon and nitrogen metabolism
may cause a general shortage of important metabolites,
indirectly leading to less efficient derepression.
Similar regulatory phenotypes of mutants sin3 and rpd3
hda1 hos1 do not necessarily mean that the corresponding
HDA1 INO2
HDA1 Δino2
IN IP IN IP IN IP
INO1 CHO2 ACT1
HOS1 INO2
HOS1 Δino2
Fig. 7 In vivo binding of Hda1 and Hos1 to ICRE-containing
promoters INO1 and CHO2 shown by chromatin immunoprecipitation
(ChIP). INO2 wild-type strains FKY40 and FKY42 contain HDA1and HOS1 variants with C-terminal His6 and HA3 epitopes at their
natural chromosomal position. FKY44 and FKY46 were constructed
by subsequent introduction of an ino2 deletion allele. Strains were
grown under conditions of inositol/choline repression. Details of the
procedure are given in ‘‘Materials and methods’’. After reversal of
cross-linking, DNA samples were analyzed by PCR using gene-
specific primers which allow amplification of *320 bp fragments. INinput control (analysis of total lysate samples), IP immunoprecipitate
(analysis of samples enriched for His-tagged Hda1 and Hos1,
respectively)
Mol Genet Genomics (2012) 287:461–472 469
123
HDACs are indeed recruited by Sin3. We have previously
shown that repression by Opi1 is also mediated to a certain
degree by the Ssn6/Tup1 corepressor (Jaschke et al. 2011),
which can recruit HDACs, Rpd3, Hda1, Hos1 and Hos2
(Watson et al. 2000; Wu et al. 2001b; Davie et al. 2003).
Thus, glucose repression of the invertase gene SUC2 was
abolished in an rpd3 hos1 hos2 triple mutant. These results
clearly show that corepressor function may be indeed
mediated by more than a single HDAC, supporting the idea
of some redundancy among them. Consequently, we per-
formed interaction studies to decide whether Sin3 is also
able to recruit additional HDACs. According to the results
of our mutational analysis, we concentrated on HDACs,
Hda1 and Hos1. Indeed, GST fusions of both enzymes
were able to interact with full-length Sin3. In contrast, we
could not reproducibly show interaction of Hos2 and Hos3
with Sin3. These in vitro studies were confirmed in vivo by
two-hybrid experiments, using fusion plasmids which
encode domains of Sin3 and HDACs, Hda1, Hos1 and
Rpd3. Using ChIP analysis, we also demonstrate recruit-
ment of Hda1 and Hos1 to promoter regions of INO1 and
CHO2. We selected these genes because they show strong
regulation by inositol/choline which is mediated by three
ICRE upstream motifs (Hoppen et al. 2005; Kodaki et al.
1991). Promoter recruitment of HDACs required a func-
tional Ino2 activator which directly binds ICRE motifs and
establishes the core for subsequent interactions with Opi1,
Sin3 and finally Hda1/Hos1.
Detailed mapping experiments revealed that Sin3 not
only contains the single HDAC interaction domain initially
mapped in mammalian proteins (HID, aa 801-950 for the
yeast protein), but also two additional segments which we
designate HID2 (aa 473-600) and HID3 (aa 1101-1210; cf.
Fig. 8a). A hydrophobic-amphipathic sequence pattern
which is completely conserved between yeast and human
Sin3 proteins could be identified within the renamed HID1
(Fig. 8b). HID2 immediately follows the PAH2 domain
and may be specific for yeast Sin3 proteins. This conclu-
sion can be derived from the finding that mSin3 proteins
lack sequence motifs convincingly similar to HID2. In
contrast, HID3 which is identical to PAH4 is a conserved
structural feature of Sin3 proteins. The structural pattern of
PAH4 deviates from PAH1, PAH2 and PAH3 and its
function remained unclear. To our knowledge, the work
reported here is the first demonstration of a physical
function for PAH4 within yeast Sin3. For mammalian
mSin3A, interaction of PAH4 with TPR motifs of an
O-glycosyltransferase (OGT) specific for N-acetylgluco-
samine (NAG) has been demonstrated (Yang et al. 2002),
indicating that NAG transfer on transcription factors may
inhibit their activity. In conclusion, the existence of at least
three HDAC interaction domains indicates that a single
Sin3 protein could be able to simultaneously bind Rpd3,
Hda1 and Hos1. Alternatively, Sin3 may only interact with
a single HDAC isoenzyme, leading to the coexistence of
individual HDAC/Sin3 complexes. This latter view would
Sin3P1 P2 P3 P4HID2(HID3)
Opi1 Ume6
Hda1
Hos1
Sds3Sap30
Rpd3
Pho23
HID1 HCR
(a)
Rpd3Hda1Hos1
(b)
(c)
ScSin3HsSin3A
Fig. 8 a Summary of mapped interaction domains within Sin3. Data
were those presented in this work or taken from Wagner et al. (2001)
(for Opi1), Washburn and Esposito (2001) (for Ume6) and Xie et al.
(2011) (for Sap30). HCR highly conserved region of unknown
function, HID histone deacetylase interaction domains; P1, P2, P3 and
P4 (=PAH1-4): paired amphipathic helices 1–4. b Hydrophobic-
amphipathic pattern in an alignment of sequences from Sin3 HID1 of
yeast and H. sapiens. Hydrophobic residues at heptad positions 7/1
and 4/5 are shown in bold. c Hydrophobic-amphipathic pattern in an
alignment of sequences from HDACs, Rpd3, Hda1 and Hos1, shown
to bind Sin3 HID motifs. #, hydrophobic amino acids
470 Mol Genet Genomics (2012) 287:461–472
123
explain why previous purification procedures using tagged
Rpd3 failed to detect Hda1 and Hos1 within the complex
(Carrozza et al. 2005b). It should be mentioned that Hda1
also exists in a distinct complex together with non-catalytic
subunits Hda2 and Hda3 (Wu et al. 2001a).
Interaction experiments with HDAC length variants
showed that Sin3 binding maps within their catalytic
deacetylase domains. However, catalytic and binding
functions are not identical. Two histidine residues (H247,
H248 for Hda1) which are essential for binding the
substrates water and acetyllysine via hydrogen bonds lie
outside the core interaction domain of Hda1 (aa 251-300).
We also searched for hydrophobic-amphipathic sequence
motifs within HDACs which possibly could bind Sin3. As
shown in Fig. 8c, hydrophobic residues appear at positions
7 or 1 and 4 or 5 of heptad repeats placed above sequence
segments of Rpd3, Hda1 and Hos1. By using bacterial
protein extracts, we could show that Rpd3, Hda1 and Hos1
are able to directly interact with Sin3 domains. This does
not rule out that auxiliary proteins of the Sin3/Rpd3L
complex such as Pho23, Sds3 and Sap30 increase Sin3-
HDAC interaction in yeast. The interactions shown for
yeast Sin3 in this work and previous publications are
summarized in Fig. 8a.
Acknowledgments This work has been supported by the Deutsche
Forschungsgemeinschaft (DFG). We thank Marius Wanjek for valu-
able support.
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