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Directedevolutionofahistoneacetyltransferase –
enhancing thermostability,whilstmaintaining catalytic
activity andsubstrate specificity
Hans Leemhuis
1
, Karl P. Nightingale
1,2
and Florian Hollfelder
1
1 Department of Biochemistry, University of Cambridge, UK
2 Chromatin and Gene Expression Group, Medical School, University of Birmingham, UK
The post-translational modification of the histone
N-terminal ‘tails’ plays a central role in the epigenetic
regulation of gene expression [1]. These processes are
highly integrated into transcriptional control mecha-
nisms, with many histone modifying enzymes being
associated with core components of the transcriptional
machinery. A diverse group of these enzymes generate
various marks in chromatin by the covalent modifica-
tion of the histone tails (i.e. phosphorylation, methyla-
tion, acetylation, etc.). The histone-code hypothesis
[2,3] suggests that these marks define the functional
status of the underlying DNA, leading to transcrip-
tional activation or silencing via the recruitment of
specific effector proteins.
Histone acetylation is the process of acetylation of
specific lysine residues in histones (Fig. 1) by a range of
histone acetyltransferase (HAT; EC 2.3.1.48) enzymes
and typically leads to gene activation. Histone acetyla-
tion exerts functional effects via two mechanisms. First,
it is associated with the charge neutralization of lysine
residues, thereby reducing the interaction of the lysine-
rich (and thus positively charged) histone tails with
Keywords
acetylation; chromatin; enzymology;
epigentics; protein engineering
Correspondence
F. Hollfelder, Department of Biochemistry,
80 Tennis Court Road, University of
Cambridge, Cambridge CB2 1GA, UK
Fax: +44 1223 766002
Tel: +44 1223 766048
E-mail: fh111@cam.ac.uk
Website: http://www.bioc.cam.ac.uk/uto/
hollfelder.html
(Received 1 August 2008, revised 5
September 2008, accepted 17 September
2008)
doi:10.1111/j.1742-4658.2008.06689.x
Histone acetylation plays an integral role in the epigenetic regulation of
gene expression. Transcriptional activity reflects the recruitment of oppo-
sing classes of enzymes to promoter elements; histone acetyltransferases
(EC 2.3.1.48) that deposit acetyl marks at a subset ofhistone residues and
histone deacetylases that remove them. Many histone acetyltransferases are
difficult to study in solution because of their limited stability once purified.
We have developed adirectedevolution protocol that allows the screening
of hundreds ofhistoneacetyltransferase mutants for histone acetylating
activity, and used this to enhance the thermostability of the human P ⁄ CAF
histone acetyltransferase. Two rounds ofdirectedevolution significantly
stabilized the enzyme without lowering the catalytic efficiency and substrate
specificity of the enzyme. Twenty-four variants with higher thermostability
were identified. Detailed analysis revealed twelve single amino acid mutants
that were found to possess a higher thermostability. The residues affected
are scattered over the entire protein structure, and are different from muta-
tions predicted by sequence alignment approaches, suggesting that sequence
comparison anddirectedevolution methods are complementary strategies
in engineering increased protein thermostability. The stabilizing mutations
are predominately located at surface of the enzyme, suggesting that the
protein’s surface is important for stability. The directedevolution approach
described in the present study is easily adapted to other histone modifying
enzymes, requiring only appropriate peptide substrates and antibodies,
which are available from commercial suppliers.
Abbreviations
DSC, differential scanning calorimetry; HAT, histone acetyltransferase; HDAC, histone deacetylase.
FEBS Journal 275 (2008) 5635–5647 ª 2008 The Authors Journal compilation ª 2008 FEBS 5635
DNA. The subsequent decreased compaction of chro-
matin facilitates access of DNA binding proteins (i.e.
transcription factors). Second, acetylated lysine residues
are recognized by ‘bromodomains’, a specific protein
fold found in many transcriptional regulators and
chromatin remodellers, suggesting that these proteins
are recruited to regions of acetylated chromatin, and
subsequently contribute to gene activation.
HAT andhistone deacetylase (HDAC) activities are
typically found in multi-subunit complexes, which are
recruited to their target loci by interactions with tran-
scriptional activators, or repressors, respectively [4].
Several classes ofhistone modification enzymes,
including HATs [5,6] andhistone demethylases, are
less active when studied in vitro (i.e. overexpressed as
an individual polypeptide in the absence of interaction
partners). A limitation of the biochemical characteriza-
tion of the HAT enzymes is their low activity and
stability in vitro. It is desirable to improve such mar-
ginally stable proteins in order to be able to use and
study them in biochemical experiments.
Proteins from thermophiles [7] have adapted various
strategies [8] to make them more thermostable, includ-
ing the incorporation of stabilizing structural features,
such as an increase in the number of charged residues
and ion pairs [9,10], increased a-helical content [11],
increased structural compactness [12] and entropic sta-
bilization due to an increased lysine to arginine ratio
[13]. Improved stability of proteins can be achieved by
design and library-based methods. Site-directed muta-
genesis based on sequence alignments and comparison
of 3D structures has been successful in creating pro-
teins with higher thermostability [14–19], although
many designed mutations had no stabilizing effect at
all. This emphasizes that our current ability to inte-
grate the lessons from naturally thermostable proteins
into engineering stable new structures is still far from
perfect [20] and has ensured that directedevolution is
increasingly being used to enhance the thermostability
of proteins. This approach involves the generation of
genetic diversity in the gene encoding the protein of
interest, followed by screening for mutant proteins
with the desired properties, and has been successfully
applied to change or improve enzyme function (sub-
strate selectivity and activity) and expression or to
enhance the stability of proteins [21–28]. The general
picture emerging from these studies is that just one or
a few amino acid substitutions can be sufficient to
increase the thermostability ofa protein by up to tens
of degrees Celsius and that it is generally hard to pre-
dict which mutations will be stabilizing.
In the present study, we describe a procedure that
uses random mutagenesis and subsequent screening to
identify substantially more thermostable mutants of
the catalytic domain of the human HAT P ⁄ CAF, with-
out affecting its catalyticactivity or substrate specific-
ity. P ⁄ CAF, p300 ⁄ CBP-associating factor, is a trans
criptional coactivator with a variable N-terminal, a
central HAT domain anda C-terminal bromodomain.
Several stabilizing mutations at multiple residues
throughout the protein were found to generate a more
thermostable HAT.
Results
Generating P
⁄
CAF mutants with increased
thermostability
One thousand variants of the catalytic domain of
P ⁄ CAF generated by error-prone PCR mutagenesis
were screened for HAT activity following a mild heat
challenge (22 °C for 2 h), as shown in Fig. 2. This
Fig. 1. The acetylation ofa lysine residue catalysed by P ⁄ CAF
using acetyl-CoA as the acetyl donor.
A
B
Fig. 2. Screening procedure used to generate thermostable P ⁄ CAF
variants. (A) Acetylation of lysine residues is detected by an ELISA
protocol using an antibody specific for acetylated lysine residues.
The signal is amplified by a secondary antibody conjugated to
horseradish peroxidase. (B) Overview of the selection procedure.
Step 1: microtitre plates with liquid medium (200 lL) were inocu-
lated with single transformants and grown overnight. Step 2: 25 lL
of culture was transferred to a second plate containing fresh med-
ium with isopropyl thio-b-
D-galactoside to induce protein expres-
sion. Step 3: cells were harvested by centrifugation and lysed with
BugBuster. Following a heat challenge, the lysates were directly
used to detect histoneacetyltransferase activity, as shown in (A).
Stabilizing a human histoneacetyltransferase H. Leemhuis et al.
5636 FEBS Journal 275 (2008) 5635–5647 ª 2008 The Authors Journal compilation ª 2008 FEBS
procedure yielded 24 P ⁄ CAF mutants with an
increased resistance to thermal inactivation. Even the
relatively mild screening conditions applied were able
to reduce the activityof wild-type P ⁄ CAF by approxi-
mately 90%, allowing the identification of mutations
that detectably improved the thermostability. Of the
24 selected variants, twelve carried a single mutation
and twelve carried two to four mutations. Twenty-four
different amino acid mutations were identified in total
(Table 1). The observation that the screening ofa rela-
tively small number of library members (1000) lead to
a high percentage of variants displaying higher thermo-
stability may be a reflection of P ⁄ CAF being mono-
meric under the assay conditions, whereas it is likely
to be part of multi-subunit complexes in vivo. Most
mutations were charge neutral. Three mutations intro-
duced a charge, four mutations removed a charge and
two mutations switched a positive and negative charge.
At this stage, one of the mutants (V582A) was intro-
duced into the pREST-P ⁄ CAF vector, purified and
shown to have an apparent melting temperature that
was 3 °C higher than the wild-type catalytic domain of
P ⁄ CAF (Fig. 3), demonstrating the feasibility of creat-
ing thermostable P ⁄ CAF mutants by directed evolu-
tion.
Second round ofdirected evolution
To further increase the thermostability of P ⁄ CAF, a
second round ofevolution was performed by randomly
recombining all 24 selected P ⁄ CAF mutants using
DNA shuffling. Here, a more stringent heat challenge
was applied, with a 75 min incubation at 37 °C.
Screening of 700 variants yielded seven mutants with
enhanced resistance to thermal inactivation compared
to the best mutant (V582A) selected in the first round
of directed evolution. Sequencing revealed that four
double and three triple mutants had been selected, that
all seven variants were combinations of mutations
selected in the first round ofdirected evolution
(Table 1) and that no additional mutations were intro-
duced during the shuffling procedure.
Characterization of selected P/CAF variants
To investigate the thermostability of the selected
mutants in more detail, two double and one triple
mutant enzymes were expressed and purified to homo-
geneity. Differential scanning calorimetry (DSC) was
used to measure directly the thermal denaturation of the
proteins, giving the apparent melting temperature (T
m
).
All P ⁄ CAF enzymes tested showed irreversible thermal
unfolding, prohibiting the calculation of the free energy
(DG) of unfolding. All selected variants unfolded at
higher temperatures than wild-type P⁄ CAF, with the
L503P ⁄ D601G ⁄ Y612C and V582A ⁄ D639E mutants
having the highest apparent denaturation temperatures
(Fig. 3 and Table 2). At this stage, we aimed to deter-
mine the contribution of the individual mutations to
thermostability, and constructed the L503P, D601G
and D639E mutants by site-directed mutagenesis.
DSC of the single mutants showed that D601G,
V582A and D639E made a large contribution to the
increased denaturation temperature of the selected
P ⁄ CAF variants (Fig. 3). The Y612C mutation repro-
ducibly had the opposite effect, slightly lowering the
apparent melting temperature. This mutant was still
selected because it is stabilizing compared to the wild-
type enzyme, under the screening conditions, where
there is acetyl-CoA. By contrast, the DSC measure-
ments are made in the absence of acetyl-CoA, explain-
ing the effect of the Y612C mutation.
Table 1. Mutations identified in P ⁄ CAF variants displaying higher
thermostability under screening conditions. The second column
gives the relative solvent accessibility score as calculated by the
software
ASA-VIEW [35].
Mutant
a
Solvent accessibility score (%)
First round (22 °C)
L503P ⁄ D601G 50-91
N504I ⁄ Q519L ⁄ V572A ⁄ V582A 100-14-8-94
I511T ⁄ M529I 7-16
Q519R 14
H524Q 79
T535A ⁄ D551G 38-63
K542E ⁄ D639E 60-56
V582A 94
V582D 94
H592R 42
H600R 54
F605L 0
E611K 65
Y612C 87
K627R ⁄ D639E 36-56
D639V 56
E649D 77
P655R –
b
Second round (37 °C)
L503P ⁄ D601G ⁄ Y612C 50-91-87
K542E ⁄ D601G ⁄ Y612C 60-91-87
D551G ⁄ V582A ⁄ D639E 63-94-56
V582A ⁄ Y612C 94-87
V582A ⁄ D639E 94-56
V582D ⁄ D639V 94-56
Y612C ⁄ P655R 87-
b
a
Some mutations were found more than once: L503P ⁄ D601G (·2),
V582A (·4), Y612C (·2) and K627R ⁄ D639E (·2).
b
Pro655 is not vis-
ible in the structure.
H. Leemhuis et al. Stabilizing a human histone acetyltransferase
FEBS Journal 275 (2008) 5635–5647 ª 2008 The Authors Journal compilation ª 2008 FEBS 5637
Thermal inactivation
Resistance to thermal inactivation of the P ⁄ CAF
mutants was determined by heating protein samples
for 5 min at various temperatures and measuring resi-
dual activity. In this case, the reduction in activity
corresponds to the percentage of enzyme molecules
undergoing irreversible inactivation. We found that the
temperature at which enzymes lost 50% of their activ-
ity (T
50
) was increased for all mutants examined
(Fig. 4 and Table 2), with the triple mutant
L503P ⁄ D601G ⁄ Y612C having the highest T
50
value.
Note that these T
50
temperatures are close to the
denaturating temperatures for the corresponding
enzymes, and that the stabilizing effect (as measured in
°C) for both methods is similar (Table 2). Interestingly,
the Y612C mutant displayed an increased T
50
tempera-
ture, consistent with selection in the thermostability
screen, despite its lower apparent T
m
temperature.
Next, we investigated whether the cofactor acetyl-
CoA stabilizes P ⁄ CAF against thermal inactivation, as
observed for two other HATs [29,30], and evaluated
whether the effect is comparable for wild-type and
mutant enzymes. Inactivation experiments were
repeated in the presence of saturating acetyl-CoA
(100 lm), revealing a large stabilizing effect for acetyl-
CoA (5.4–8.7 °C) for all enzymes examined (Fig. 4 and
Table 2). Comparison of the T
50
and T
50
AcCoA
values
indicated that acetyl-CoA binding is particularly stabi-
lizing for the V582A, Y612C and V582A ⁄ D639E
mutants.
The time taken for temperature-dependent inactiva-
tion was assessed by measuring the activity half-life
(t
1 ⁄ 2, 48 °C
), which was determined at 48 °C. All
mutants showed longer activity half-lives than wild-
type P ⁄ CAF (Table 2), with the most stable mutants
having 60- to 70-fold larger t
1 ⁄ 2, 48 °C
values, broadly
following the trend seen for the T
50
and T
m
tempera-
tures. The stabilizing effects of single mutations are
A
B
Fig. 3. Thermal denaturation traces mea-
sured by differential scanning calorimetry.
(A) Multiple P ⁄ CAF mutants and (B) single
P ⁄ CAF mutants (compared to wild-type,
wt). Conditions: 20 l
M P ⁄ CAF protein in
50 m
M sodium phosphate (pH 7.5), 150 mM
NaCl anda scan rate of 1 °CÆmin
)1
.
Table 2. Stability parameters of purified P ⁄ CAF and selected
mutants. Measurements were performed under the following con-
ditions: 50 m
M sodium phosphate (pH 7) and 150 mM NaCl. T
m
,
apparent melting temperature; T
50
, temperature at which half of
the initial activity is lost in 5 min; T
50
AcCo
, temperature at which half
of the initial activity is lost in 5 min in the presence of acetyl-CoA;
t
1 ⁄ 2, 48 °C
, activity half-life at 48 °C. Errors for T
m
and T
50
values are
less than 0.5 °C.
T
m
b, c
(°C)
T
50
(°C)
T
50
AcCoA
(°C)
t
1 ⁄ 2, 48 °C
(min)
Wild-type 46.2 48.5 53.9 5.0 ± 0.1
L503P 47.0 48.1 54.9 9.9 ± 0.4
V582A 49.3 52.4 59.9 60 ± 3
D601G 52.3 53.5 59.3 315 ± 10
Y612C 45.0 49.4 57.5 17 ± 1
D639E 49.1 50.3 56.3 32 ± 2
Y612C ⁄ P655R
a
49.5 50.5 57.2 35 ± 5
L503P ⁄ D601G ⁄ Y612C
a
54.2 55.4 61.4 315 ± 12
V582A ⁄ D639E
a
52.4 53.2 61.9 347 ± 16
a
Mutants selected in second round ofdirected evolution.
b
For
thermal inactivation curves, see Fig. 4.
c
Measured by differential
scanning calorimetry.
Stabilizing a human histoneacetyltransferase H. Leemhuis et al.
5638 FEBS Journal 275 (2008) 5635–5647 ª 2008 The Authors Journal compilation ª 2008 FEBS
approximately additive in the double and triple
mutants for all stability measurements, as expected for
mutations that are far apart in the structure. Overall,
the inactivation experiments clearly demonstrate that
the selected P ⁄ CAF mutants have a strongly enhanced
resistance towards thermal inactivation.
Catalytic properties andspecificityof the P/CAF
enzymes
The kinetic parameters of the wild-type and mutant
P ⁄ CAF enzymes for acetylation of the histone H3 and
H4 peptides were determined using a continuous assay
and synthetic peptide substrates. Wild-type P ⁄ CAF has
k
cat
and K
M
values of 12 min
)1
and 53 lm with the H3
peptide and 0.29 min
)1
and 194 lm with the H4 pep-
tide, whereas the K
M
for acetyl-CoA was 0.28 lm
(Table 3). Note that the H3 peptide is a much better
substrate for the enzyme, with k
cat
⁄ K
M
of 3774 s
)1
Æm
)1
versus 25 s
)1
Æm
)1
for the H4 peptide, in agreement
with histone H3 being the physiological substrate for
P ⁄ CAF [31]. The mutations had no significant effect
on the k
cat
H3
values but the V582A and Y612C muta-
tions increased the K
M
H3
value by ten-fold (Table 3).
An overlay of the P ⁄ CAF structure and the Tetrahy-
mena HAT, with a bound H3 peptide shows that
Tyr612 is located in the binding groove for the peptide
substrate, which may explain the higher K
M
H3
observed with the Y612C mutant. By contrast, the
basis of the high K
M
H3
of the V582A mutant is unclear
because Val582 is far away from the peptide binding
groove. The Y612C mutation reduced the k
cat
H4
by
three-fold, whereas the other mutations had no signifi-
cant effect on k
cat
values (Table 3).
Histone acetylation at distinct histone residues is
thought to have variable functional effects. We there-
fore examined whether the thermostable P ⁄ CAF
mutants affected the specificityof HAT activity.
Recombinant histone H4 [32,33] (containing minimal
endogenous post-translational modifications) was incu-
bated with wild-type and four single mutant P ⁄ CAF
enzymes and the specificityof acetylation was assessed
by western blotting using antibodies specific for
A
B
D
C
Fig. 4. Thermal inactivation curves of P ⁄ CAF and selected
mutants. In the absence (A, B) and presence (C, D) of 100 l
M ace-
tyl-CoA, used to determine T
50
(Table 2). Conditions: 10 lM P ⁄ CAF
protein in 50 m
M sodium phosphate (pH 7.5) and 150 mM NaCl
was incubated for 5 min at various temperatures before measuring
the residual activity by ELISA. The activity measured without a heat
challenge was set to 100%. The values derived from these curves
are given in Table 2.
H. Leemhuis et al. Stabilizing a human histone acetyltransferase
FEBS Journal 275 (2008) 5635–5647 ª 2008 The Authors Journal compilation ª 2008 FEBS 5639
acetylation at distinct histone H4 lysines (K5, K8, K12
and K16). Figure 5 shows the specificity profiles of
wild-type P ⁄ CAF and its mutants, normalized using
the H4K16ac (i.e. the most physiologically abundant
acetyl isoform). Broadly, the wild-type and mutant
enzymes yield very similar patterns of lysine specificity,
indicating that the individual mutations do not impact
on substrate recognition. This may be expected
because the immediate sequence environments of many
of these residues are similar [e.g. for H4K5, 8 and 12
GK(ac)-G].
Discussion
Location of mutations in the P/CAF structure
Analysis of the location of the thermostabilizing
mutations identified, and comparison with homolo-
gous HAT sequences, shows that they are scattered
throughout the enzyme structure (Fig. 6), largely
occurring at nonconserved amino acid residues, with
only two conserved residues being mutated (see
Fig. S1). Close examination of the P ⁄ CAF crystal
structure [34] reveals that almost all of these stabiliz-
ing mutations are on the surface of the enzyme. This
observation is reinforced by comparison of the distri-
butions of solvent accessible residues in the entire
proteins versus the residues selected by directed evolu-
tion. The proportion of exposed residues (calculated
with the programme asa-view) [35] is markedly
increased in the selected set (see Fig. S2 and
Table S1). Together with the analysis of the individual
mutations, this suggests that the raised thermostablity
is brought about by optimization of surface residues.
Table 3. Kinetic parameters of the wild-type and mutant P ⁄ CAF enzymes at 25 °C and pH 7.5 in 150 mM Mes buffer.
k
cat
H3
(min
)1
) K
M
H3
(lM) k
cat
H4
(min
)1
) K
M
H4
(lM) K
M
AcCoA
(lM)
a
Wild-type 12 ± 1 53 ± 10 0.29 ± 0.02 190 ± 30 0.28 ± 0.03
L503P 12 ± 1 54 ± 14 0.32 ± 0.02 210 ± 30 0.33 ± 0.03
V582A 11 ± 1 560 ± 80 0.29 ± 0.02 500 ± 50 0.36 ± 0.06
D601G 12 ± 1 55 ± 11 0.33 ± 0.02 250 ± 20 0.34 ± 0.02
Y612C 11 ± 1 165 ± 29 0.11 ± 0.01 120 ± 30 0.41 ± 0.03
D639E 12 ± 1 39 ± 10 0.35 ± 0.03 150 ± 40 0.27 ± 0.02
Y612C ⁄ P655R 12 ± 1 62 ± 15 0.21 ± 0.01 140 ± 20 0.29 ± 0.03
L503P ⁄ D601G ⁄ Y612C 12 ± 1 64 ± 15 0.18 ± 0.02 110 ± 30 0.27 ± 0.03
V582A ⁄ D639E 13 ± 1 460 ± 60 0.37 ± 0.01 310 ± 20 0.34 ± 0.06
a
K
M
AcCoA
was determined using the H3 peptide.
Fig. 5. Lysine specificityof wild-type (wt) and mutant P ⁄ CAF
enzymes on histone H4. Acetylation of lysines 4, 8, 12 and 16 of
histone H4 was measured by western blotting using site specific
anti-acetyl sera. The degree of acetylation was normalized to that
detected at lysine 16, which was given a value of 1.0.
Fig. 6. Location of thermostabilizing mutations. Cartoon represen-
tation of the catalytic domain of P ⁄ CAF (crystal structure 1CM0 of
the Protein Data Bank) [34]. Residues mutated in variants with
higher thermostability are indicated by sticks. Magenta indicates
the residues shown to be stabilizing as a single mutant and grey
indicates that the residue was found mutated only in combination
with one or more other mutations. The catalytic glutamate residue
is shown in green and the bound coenzyme A molecule is shown
in black.
Stabilizing a human histoneacetyltransferase H. Leemhuis et al.
5640 FEBS Journal 275 (2008) 5635–5647 ª 2008 The Authors Journal compilation ª 2008 FEBS
The high rate of surface mutations is consistent with
the likely scenario that P⁄ CAF is part of larger multi-
subunit complexes in vivo. Directedevolutionof the
monomeric P ⁄ CAF under the conditions described
here then replaces the residues originally responsible
for potential binding interactions to partner proteins
by stabilizing residues.
The mutations that are most effective in raising the
thermostability of the catalytic domain of P ⁄ CAF
(V582A, D601G and D639E) are discussed in more
detail below. Mutation V582A introduced a smaller
alanine residue at the position of Val582, a residue
strictly conserved among HATs. This residue is in the
vicinity of the coenzyme A molecule bound to
the enzyme and is solvent exposed, indicating that the
V582A mutation increases thermostability by lowering
the hydrophobicity of the protein’s surface. The analo-
gous V582D mutation is also likely to derive its
stabilizing effect as a result of reduced surface hydro-
phobicity. Alternatively, the effect of this mutation
may be explained by modulating the surface charge
distribution, electrostatic interactions, or a combina-
tion of these effects. Similarly, the thermostabilizing
mutation D601G is located in a short loop connecting
an a-helix anda b-strand at the surface of the protein,
with the Asp601 side-chain solvent being exposed. The
observation that the D601G mutation is stabilizing is
noteworthy because the introduction of glycines is usu-
ally not considered to be stabilizing [20]. Asp601 is not
conserved among GCN5 HAT enzymes, anda glycine
at the equivalent position is found in a few other
HATs (see Fig. S1). The source of stabilization is
likely to arise from optimization of the surface charge
distribution by removing the negatively charged aspar-
tate side-chain. Alternatively, the release of conforma-
tional strain allowed by the extra flexibility of the
glycine residue may lead to better protein packing and
increased thermostability. The latter mechanism of sta-
bilization has been discussed in more detail by Veille
and Zeikus [10].
A D639E mutation significantly increased the ther-
mostability of P⁄ CAF. This aspartate residue is found
in most GCN5 HATs (see Fig. S1) and is part of a
loop region at the surface of the enzyme with its side
chain solvent being exposed. Different conformations
have been observed for this loop in crystal structures
of GCN5 HAT enzymes anda recent study demon-
strated that the movement of this loop correlates with
the different stages of the acetylation reaction [36]. A
possible explanation for the stabilizing effect of D639E
is that the longer glutamate side chain provides more
opportunities for salt bridge formation on the surface
of the protein.
Implications for protein thermostability
engineering
Generally, only a few mutations are sufficient to
increase the thermostability ofa protein by as much as
tens of degrees Celsius [37–40] but the prediction of
the these mutations proves to be a challenge. One
might assume (e.g. for structure-based computational
approaches that are especially advantageous when no
straightforward screening or selection systems are
available) that surface residues should not be targeted
to increase thermal stability because their interactions
with the solvent were expected to be similar in the
native and unfolded state of the protein. Instead, inter-
nal residues have been preferred targets as in the com-
putational optimization of protein structures [41–43].
Our study suggests that surface residues play a more
important role in P ⁄ CAF: such mutations occurred in
residues with a clearly higher solvent accessibility rela-
tive to the average residue of this protein: 51.7% ver-
sus 34.1%; scale 0–100%; as calculated with asa-view
[35]. For the single mutations shown to be stabilizing
in the present study (eleven in total, excluding P655R,
which showed no electron density in the crystal struc-
ture), the solvent accessibility was even higher at
59.6% (see Fig. S2 and Table S1). Other directed evo-
lution studies aimed at the generation of thermostable
proteins also frequently identify surface mutations [27];
seven out of eight in the case of an esterase [44], three
out of three for an a-glucan phosphorylase [24] and
ten out of 12 for a phosphite dehydrogenase [45].
Computational optimization of surface charge–charge
interactions was able to predict site-directed mutants
with increased thermostabilities for five small proteins
(with < 100 amino acid residues) [46]. This preference
for surface mutations may be explained by (a) the rela-
tively high percentage of residues located at the protein
surface, (b) surface residues forming proportionally
fewer interactions than ‘internal’ residues, and there-
fore being less likely to cause detrimental effects that
offset gains by mutation, or (c) that the surface is rela-
tively important to thermostability of proteins. In
addition, (d) protein surfaces have been suggested to
be important for thermostability of proteins showing
irreversible unfolding [47] as in the case with P ⁄ CAF.
This scenario may involve partial unfolding of the
protein surface structure that would be addressed by
surface mutations.
Sequence comparison approaches in the design of
proteins with enhanced stability are based on the
assumption that there is a positive correlation between
the conservation ofa residue and its contribution to
the stability of the protein. Thus, substituting poorly
H. Leemhuis et al. Stabilizing a human histone acetyltransferase
FEBS Journal 275 (2008) 5635–5647 ª 2008 The Authors Journal compilation ª 2008 FEBS 5641
conserved residues for more conserved residues is
expected to increase the thermostability ofa protein,
as shown for GroEL minichaperone [14], immuno-
globulin domains [48], phytase [49] anda few other
proteins [20,50,51]. To investigate whether the stabi-
lized P ⁄ CAF mutants carry mutations predicted by
sequence comparison, the sequences of 15 homologous
HAT proteins, sharing approximately 25% sequence
identity, were aligned (see Fig. S3). We then matched
the stabilizing single mutants with the sequence align-
ment. The sequence comparison showed that 31 resi-
dues out of 167 (or 19%) in P ⁄ CAF, were different
from the amino acid most frequently found at this
position. Thus, according to the sequence comparison
approach, these 31 residues are the most likely to be
mutated. However, of the twelve stabilizing mutations
found by directed evolution, only the D601G muta-
tion was marginally predominant (with five glycine
versus three aspartate residues at this position). All
other stabilizing mutations introduced less conserved
residues (H600R, F605L, D639E and P655R) or resi-
dues not seen in any of the HATs (Q519R, H524Q,
V582A, H592R, E611K, Y621C and E649D). Muta-
tion V582A even substituted the completely conserved
Val582. These results emhasize the effectiveness of
directed evolution in the identification of thermostabi-
lizing mutants that cannot be predicted by rational
protein design. Because the effects of stabilizing muta-
tions are often additive, a combination of sequence
comparison anddirectedevolution may create even
more stable proteins by combining the advantages of
both methods.
Conclusions
Proteins have evolved to be stable and biologically
active under conditions imposed by the cellular envi-
ronment and the habitat of the organism; however,
there is little evolutionary advantage in being more
stable than required. Because the majority of muta-
tions are destabilizing, most proteins will be only mar-
ginally stable [52–54]. This implies that there is ample
sequence flexibility available to stabilize proteins,
whilst retaining their catalytic capacity. In the present
study, we have shown that mutations stabilizing the
catalytic domain of the human histone acetyltransfer-
ase P ⁄ CAF are readily identified by directed evolu-
tion. These mutations have either no or minimal
effects on the catalytic properties andspecificity of
this enzyme. The directedevolution method described
is able to generate stable histone modifying enzymes
in a straightforward procedure. Furthermore, histone
modifying enzymes are potential targets for drug
screening in ‘epigenetic therapies’ for a range of dis-
eases, notably cancers and acute myeloid leukaemia
[55–58]. A more thermostable target enzyme with
identical catalytic properties will facilitate high-
throughput drug screening and allow biochemical
experiments to be carried out in the absence of poten-
tial binding partners that are stabilizing the protein
in vivo.
The ELISA screening approach described in the
present study is easily adapted to investigate other
histone modifying enzymes simply by using another
appropriate histonesubstrateand antibody, which are
widely available from commercial suppliers. This there-
fore represents a general protocol to improve the sta-
bility ofa wide range ofhistone modification enzymes
for in vitro applications.
Experimental procedures
Antibodies and peptides
Polyclonal rabbit antibodies specific for the recognition of
acetylated lysine residues in histone tails (H4K5ac,
H4K8ac, H4K12ac and H4K16ac) were kindly provided by
Bryan Turner (University of Birmingham, UK). Goat anti-
(rabbit IgG) serum conjugated to horseradish peroxidase
was purchased from Sigma (St Louis, MO, USA). Histone
tail peptides were synthesized by the PNAC facility (Cam-
bridge University, UK): H3, ARTKQTARKSTGGKAPR
KQLC, and H4, SGRGKGGKGLGKGGAKRHRKV
GGK. The H4 peptide is biotinylated at its C-terminus to
allow attachment to streptavidin coated microtitre plates.
Expression and purification
All (mutant) P ⁄ CAF proteins (20 kDa) were expressed in
Escherichia coli BL21(DE3) from pRSET-P ⁄ CAF in liquid
medium (10 gÆL
)1
NaCl, 10 gÆL
)1
yeast extract and
20 gÆL
)1
bacto tryptone) with 100 mgÆL
)1
ampicillin at
25 °C. This vector expresses the catalytic domain of
P ⁄ CAF. The proteins were purified by cation exchange and
size exclusion chromatography, as described previously [59].
In the latter column, P ⁄ CAF eluted as a monomer (at con-
centrations above those used in the stability and catalytic
assays), suggesting that any effects of mutations on the
oligomerization state can safely be excluded, thus simplify-
ing the analysis of stability-conferring mutations.
DNA manipulation
The gene encoding the catalytic domain (amino acids 492–
658) of P ⁄ CAF [60] was amplified from pRSET-P ⁄ CAF
using the primers P ⁄ CAF-for-BamHI and P ⁄ CAF-rev-PstI.
The resulting PCR product was restricted with BamHI and
Stabilizing a human histoneacetyltransferase H. Leemhuis et al.
5642 FEBS Journal 275 (2008) 5635–5647 ª 2008 The Authors Journal compilation ª 2008 FEBS
PstI and cloned into pMalC2x (New England Biolabs,
Beverly, MA, USA), yielding plasmid pMal-P ⁄ CAF. This
construct expresses P ⁄ CAF as C-terminal fusion to the
maltose binding protein (see Fig. S4). DNA sequencing was
carried out with the T7 or Seq oligonucleotides. L503P,
D601G and D639E mutations were introduced in pRSET-
P ⁄ CAF using the QuickChange system (Stratagene, La
Jolla, CA, USA). Oligonucleotide sequences are provided in
the Table S2.
First generation library construction
In the first round ofdirected evolution, the catalytic
domain of P ⁄ CAF was expressed as C-terminal fusion to
maltose binding protein to minimize the effects of the
random mutations on the amount of protein expressed.
Random mutations were introduced in the gene encoding
P ⁄ CAF by error-prone PCR amplification in the presence
of manganese chloride. Additional details on directed evo-
lution procedures are provided elsewhere [61]. Optimal
error-prone PCR conditions were determined by sequencing
P ⁄ CAF genes amplified at various MnCl
2
concentrations.
As expected, the number of nucleotide mutations increased
with increasing MnCl
2
concentrations with a clear prefer-
ence for T > C andA > G substitutions. The library con-
structed with 0.075 mm MnCl
2
was used for screening
because it had one to two nucleotide mutations per gene,
and two to four changes per 1000 bp. The gene for P ⁄ CAF
was amplified from plasmid pMal-P ⁄ CAF using primers
pMal-forII and pMal-revII (see Table S2), which anneal at
the BamHI and PstI restriction sites used for cloning; for a
schematic view of the gene and its flanking regions, see the
Fig. S4. PCRs (50 lL) contained: 1· Taq DNA polymerase
buffer, 0–0.5 mm MnCl
2
, 0.4 mm of each dNTP, 10 ng of
pMal-P ⁄ CAF template, primers at 0.5 lm and 4 U Taq
DNA Polymerase (New England Biolabs). The PCR pro-
gram used was: 1 min at 94 °C; 30 cycles each comprising
45 s at 94 °C, 45 s at 54 °C and 45 s at 72 ° C; followed by
5 min at 72 °C. PCR products were digested with BamHI
and PstI, purified with a QIAquick PCR purification Kit
(Qiagen, Valencia, CA, USA) and cloned into pMalC2x by
incubating overnight with T4 DNA ligase (New England
Biolabs) at 16 °C. Ligated plasmids were transformed into
E. coli DH5a cells (Invitrogen, Carlsbad, CA, USA) and
plated onto LB agar with 100 mgÆL
)1
ampicillin. Plasmids
were purified from pooled transformants and stored at
)20 °C.
Second generation library construction
Plasmid DNA of all 24 P ⁄ CAF variants selected in the first
round ofdirectedevolution were mixed and used as tem-
plates in a PCR with Pfu-DNA polymerase (Stratagene)
with primers pMal-for and pMal-rev. These primers anneal
approximately 100 bp upstream and downstream of the
gene for P ⁄ CAF (see Fig. S4). The PCR product, purified
with a QIAquick PCR Purification Kit (Qiagen) was
digested with DNAse (3 U; Promega, Madison, WI, USA)
at 15 °C for 3, 4 and 5 min. Digestion was stopped by add-
ing EDTA to 10 mm. Following separation on an agarose
gel (2%), fragments between 50 and 100 bp were isolated
with the Qiagen II gel extraction kit (Qiagen). A re-assem-
bly reaction (50 lL) contained 100 ng of DNA fragments,
0.4 mm of each dNTP, 1· Pfu reaction buffer and 2.5 U
Pfu DNA polymerase. The re-assembly reaction (1 min at
94 °C; 70 cycles each comprising 40 s at 94 °C, 30 s at
50 °C, 30 s at 94 °C; followed by 4 min at 72 °C) yielded a
product of expected size ( 750 bp) plus a smear of smaller
and larger products. Aliquots of this re-assembly reaction
were used as PCR templates to amplify the shuffled P ⁄ CAF
genes using Pfu-DNA polymerase and primers pMal-forII
and pMal-revII, obtaining a product of the expected size
( 550 bp). This fragment was digested with BamHI and
PstI and cloned into pRSET (Invitrogen). Ligated plasmids
were transformed into E. coli DH5a cells, plated onto LB
agar with 100 mgÆL
)1
ampicillin, and plasmids were purified
from the pooled transformants to yield the second genera-
tion library.
Screening procedure
The plasmid libraries were transformed into E. coli
BL21(DE3), plated on LB agar supplemented with
100 mgÆL
)1
ampicillin and resulting colonies were trans-
ferred to 200 lL of LB medium in 96-well plates. A sche-
matic view of the screening procedure is provided in
Fig. 2. After overnight incubation at 37 °C and shaking at
750 r.p.m., 25 lL was transformed to a fresh 96-well
plate containing 200 lL of LB and 0.25 mm isopropyl
thio-b-d-galactoside followed by incubation at 37 °C
(750 r.p.m. shaking speed) for 4 h. Cells were harvested by
centrifugation (4000 g). To release the P ⁄ CAF activity,
cells were broken by resuspension in a mixture of BugBust-
er (Novagen, Madison, WI, USA) and demineralized water
(40 : 60, v ⁄ v; total volume of 20 lL) and incubated at
room temperature (20–25 °C) for 15 min. The plates were
subsequently incubated for 2 h at 4 and 22 ° C, respec-
tively, or for 75 min at 37 °C. The remaining HAT activity
after exposure to elevated temperatures was determined by
ELISA, as described below. Plasmid DNA of clones
expressing a more stable P ⁄ CAF was isolated and used to
re-transform E. coli DH5a cells to verify the apparent
increase in thermal stability.
ELISA procedure
ELISA plates were prepared by incubating clear 96-well
streptavidin coated microtitre plates (SigmaScreen; Sigma)
with biotinylated H4 peptide (0.5 lgin50lL NaCl ⁄ P
i
per
well) at room temperature for 30 min. After rinsing with
H. Leemhuis et al. Stabilizing a human histone acetyltransferase
FEBS Journal 275 (2008) 5635–5647 ª 2008 The Authors Journal compilation ª 2008 FEBS 5643
water (·4), plates were blocked with BSA in NaCl ⁄ P
i
(3%,
w ⁄ w) at room temperature for 1 h. Plates were then rinsed
with water (·4) and HAT reactions were started by the
addition of reaction buffer [5 · reaction buffer: 250 mm
Tris ⁄ HCl (pH 8.0), 5 mm dithithreitol, 0.5 m m EDTA and
50% glycerol (v ⁄ v), 200 lm acetyl-CoA (Sigma)] and either
purified enzyme or lysate of E. coli cells expressing P ⁄ CAF
protein. Reactions were continued for 10–45 min at room
temperature and stopped by washing (·5) with water. The
degree of acetylation was determined using an antibody
specific for acetylated K8 in the H4 peptide, by diluting the
antibodies 200-fold in NaCl ⁄ P
i
with 3% BSA and incubat-
ing at room temperature for 1 h. Plates were washed with
NaCl ⁄ P
i
⁄ 0.5 m NaCl ⁄ 1% Tween-20 (·2), NaCl ⁄ P
i
⁄ 1%
Tween-20 (·2) and water (·3). The secondary antibody, an
anti-(rabbit IgG) horseradish peroxidase conjugate, was
added at a dilution of 1000-fold in NaCl ⁄ P
i
with BSA (3%,
w ⁄ w) and incubated for 30 min. Following washing with
NaCl ⁄ P
i
⁄ 1% Tween-20 (·3) and water (·4), 100 lLof
peroxidase substrate (tetramethylbenzidine; KPL, Silver
Spring, MD, USA) was added and incubated for 5–10 min.
This peroxidase reaction was stopped by the addition of
sulfuric acid (50 lL, 1 m) and A
450
was measured. Under
the conditions described above, the increase in absorbance
obtained from the ELISA is linear (for the wild-type with-
out the exposure to the high temperature) for the time
between 0 and 30 min for acetylation of K8 in the H4
peptide.
Continuous HAT assay
Progress curves as a measure of HAT activityof wild-type
and mutant P ⁄ CAFs were followed using a coupled enzyme
assay [62]. HAT activity generates CoA as a byproduct that
is converted back to acetyl-CoA by pyruvate dehydroge-
nase, which is accompanied by NAD
+
reduction to
NADH, thus increasing A
340
. An example ofa progress
curve is provided in the Fig. S3. Reactions were carried out
in 96-well plates at 25 °C. Reaction mixtures (300 lL)
contained Mes buffer (pH 7.5, 100 mm), H3 peptide (0–
500 lm) or H4 peptide (0–700 lm), acetyl-CoA (0–
1000 lm), NAD
+
(0.2 mm), thiamine pyrophosphate
(0.2 mm), MgCl
2
(5 mm), dithiothreitol (1 mm), pyruvate
(2.4 mm) and pyruvate dehydrogenase (0.3 UÆmL
)1
; Sigma).
Reactions were initiated by the addition of P ⁄ CAF enzyme
(i.e. the catalytic domain as expressed from pREST-
P ⁄ CAF) at a concentration of 0.8–7 lm. Linear curves of
reaction progress over time were measured at 340 nm, con-
verted using a value of 5296 AbsÆM
)1
for e*d. The value of
e*d for NADH was determined from a calibration curve
with pure NADH in our microtitre plate setup. The time
traces gave initial rates that were fitted to the Michaelis–
Menten equation. The measured rates were corrected for
the spontaneous acetyl-CoA hydrolysis (obtained in the
absence of enzyme).
Stability assays
Resistance to thermal inactivation was determined by incu-
bating the P⁄ CAF protein in sodium phosphate (pH 7.5,
50 mm), NaCl (150 mm), dithithreitol (1 mm) and EDTA
(1 mm) buffer. All stability assays were performed with
P ⁄ CAF protein expressed from pRSET-P ⁄ CAF. Protein
samples (25 lL, 10 l m P ⁄ CAF) were incubated at various
temperatures in the range 0–67 °C for 5 min in a PCR
machine followed by incubation on ice for at least 30 min.
Residual activity was measured by ELISA. The activity
measured without a heat challenge was set to 100%. We
define the T
50
temperature as the temperature at which half
of the initial activity is lost in 5 min. The activity half-life
t
1 ⁄ 2, 48 °C
of the proteins was determined at 48 °C by incu-
bating the proteins for 0–1800 min at 48 °C, followed by
incubation on ice. Residual activity was determined by
ELISA and the activity half-life (t
1 ⁄ 2, 48 °C
) is defined as the
time in which the activity is reduced by 50%.
DSC
Thermal unfolding was measured using the MicroCal
VP-DSC microcalorimeter (MicroCal Inc., Northampton,
MA, USA), with a cell volume of 0.5 mL. Experiments
were carried out at a scan rate of 1 °CÆmin
)1
from 2–75 °C
at a constant over-pressure of 1.79 bar (26 psi). Samples
were degassed prior to the scan and contained 20 lm
(0.40 mgÆmL
)1
)P⁄ CAF protein (expressed from pRSET-
P ⁄ CAF) in sodium phosphate (pH 7.5, 50 mm), NaCl
(150 mm), dithiothreitol (1 mm) and EDTA (1 mm) buffer.
Samples were dialyzed against this buffer and the reference
cell contained the dialysis buffer of the last dialysis step.
The apparent melting temperature (T
m
) is defined as mid-
point of thermal unfolding as seen in a DSC thermogram.
Assessment of wild-type and mutant P/CAF
substrate specificity
Substrate specificityof wild-type and single substitution
P ⁄ CAF mutants (expressed from pRSET-P ⁄ CAF) was
assessed by western blotting using antibodies specific for
acetylation at distinct histone H4 lysines (H4K5ac,
H4K8ac, H4K12ac and H4K16ac). Histone acetyltransfer-
ase assays were performed using 20 lgofE. coli expressed
histone H4 substrate [32,33] and enzyme in reaction buffer
[50 mm Tris ⁄ HCl (pH 8.0), 1 mm dithiothreitol, 0.1 mm
EDTA, 200 lm acetyl-CoA] at 30 °C for 3 h. The reaction
was halted by addition of SDS loading buffer, and sepa-
rated on 15% acrylamide : bis-acrylamide (30 : 1) gel, prior
to transfer to nitrocellulose (Hybond-C; Amersham Phar-
macia, Piscataway, NJ, USA), western blotting and detec-
tion using a fluorescently tagged anti-rabbit secondary
(Licor, 800 nm).
Stabilizing a human histoneacetyltransferase H. Leemhuis et al.
5644 FEBS Journal 275 (2008) 5635–5647 ª 2008 The Authors Journal compilation ª 2008 FEBS
[...]... Sequence alignment of the catalytic domain of 14 histoneacetyltransferase sequences Stabilizing a human histoneacetyltransferase Fig S2 Relative solvent accessibility of amino acid residues of the catalytic domain of P ⁄ CAF Fig S3 Example for a reaction progress curve as a measure of HAT activity Fig S4 The gene for P ⁄ CAF and its flanking regions Table S1 Relative solvent accessibility of amino acids of. .. The Authors Journal compilation ª 2008 FEBS 5645 Stabilizing a human histoneacetyltransferase H Leemhuis et al 30 Herrera JE, Bergel M, Yang XJ, Nakatani Y & Bustin M (1997) The histoneacetyltransferaseactivityof human GCN5 and PCAF is stabilized by coenzymes J Biol Chem 272, 2725 3–2 7258 31 Schiltz RL, Mizzen CA, Vassilev A, Cook RG, Allis CD & Nakatani Y (1999) Overlapping but distinct patterns of. .. expression and stability Curr Opin Struct Biol 15, 1–7 24 Yanase M, Takata H, Fujii K, Takaha T & Kuriki T (2005) Cumulative effect of amino acid replacements results in enhanced thermostability of potato type L alpha-glucan phosphorylase Appl Environ Microbiol 71, 543 3–5 439 25 Hao J & Berry A (2004) A thermostable variant of fructose bisphosphate aldolase constructed by directedevolution also shows increased... Rogiers V & Vanhaecke T (2007) The pharmaceutical potential ofhistone deacetylase inhibitors Curr Pharm Des 13, 258 4–2 620 57 Mai A (2007) The therapeutic uses of chromatin-modifying agents Expert Opin Ther Targets 11, 83 5–8 51 58 Mai A, Massa S, Rotili D, Cerbara I, Valente S, Pezzi R, Simeoni S & Ragno R (2005) Histone deacetylation in epigenetics: an attractive target for anticancer therapy Med Res... 304, 3–1 9 34 Clements A, Rojas JR, Trievel RC, Wang L, Berger SL & Marmorstein R (1999) Crystal structure of the histoneacetyltransferase domain of the human PCAF transcriptional regulator bound to coenzyme A EMBO J 18, 352 1–3 532 35 Ahmad S, Gromiha MM, Fawareh H & Sarai A (2004) ASAView: solvent accessibility graphics for proteins BMC Bioinformatics 5, 51 36 Zheng Y, Mamdani F, Toptygin D, Brand L,... 1196 1–1 1969 61 Neylon C (2004) Chemical and biochemical strategies for the randomization of protein encoding DNA sequences: library construction methods for directedevolution Nucleic Acids Res 32, 144 8–1 459 62 Kim Y, Tanner KG & Denu JM (2000) A continuous, nonradioactive assay for histone acetyltransferases Anal Biochem 280, 30 8–3 14 Supporting information The following supplementary material is available:... 28 4–2 95 5 Akhtar A & Becker PB (2000) Activation of transcription through histone H4 acetylation by MOF, an acetyltransferase essential for dosage compensation in Drosophila Mol Cell 5, 36 7–3 75 6 Akhtar A, Zink D & Becker PB (2000) Chromodomains are protein-RNA interaction modules Nature 407, 40 5– 409 7 Sterner R & Liebl W (2001) Thermophilic adaptation of proteins Crit Rev Biochem Mol Biol 36, 3 9–1 06 8... discussions and anti -histone H4 sera References 1 Kouzarides T (2007) Chromatin modifications and their function Cell 128, 69 3–7 05 2 Strahl BD & Allis CD (2000) The language of covalent histone modifications Nature 403, 4 1–4 5 3 Turner BM (2007) Defining an epigenetic code Nat Cell Biol 9, 2–6 4 Lee KK & Workman JL (2007) Histoneacetyltransferase complexes: one size doesn’t fit all Nat Rev Mol Cell Biol 8, 28 4–2 95... Rev 25, 26 1–3 09 59 Leemhuis H, Packman LC, Nightingale KP & Hollfelder F (2008) The human histoneacetyltransferase FEBS Journal 275 (2008) 563 5–5 647 ª 2008 The Authors Journal compilation ª 2008 FEBS H Leemhuis et al P ⁄ CAF is a promiscuous histone propionyltransferase Chembiochem 9, 49 9–5 03 60 Tanner KG, Langer MR & Denu JM (2000) Kinetic mechanism of human histoneacetyltransferase P ⁄ CAF Biochemistry... JT & Cole PA (2005) Fluorescence analysis ofa dynamic loop in the PCAF ⁄ GCN5 histoneacetyltransferase Biochemistry 44, 1050 1–1 0509 37 Eijsink VGH, Veltman OR, Aukema W, Vriend G & Venema G (1995) Structural determinants of the stability of thermolysin-like proteinases Nat Struct Biol 2, 37 4–3 79 38 Williams JC, Zeelen JP, Neubauer G, Vriend G, Backmann J, Michels PA, Lambeir AM & Wierenga RK (1999) . Directed evolution of a histone acetyltransferase –
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Hans. CAF and its flanking regions.
Table S1. Relative solvent accessibility of amino acids
of the catalytic domain of P ⁄ CAF as calculated with
the program asa-view.
Table