Method Article

Reconstitution of Nucleosomes with Differentially Isotope-labeled Sister Histones

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DOI:

10.3791/55349

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March 26th, 2017

1Department of Structural Biology, Leibniz Institute of Molecular Pharmacology (FMP-Berlin)

In This Article

Summary

This protocol describes the reconstitution of nucleosomes containing differentially isotope-labeled sister histones. At the same time, asymmetrically post-translationally modified nucleosomes can be generated after using a premodified histone copy. These preparations can be readily used to study modification crosstalk mechanisms, simultaneously on both sister histones, by using high-resolution NMR spectroscopy.

Abstract

Asymmetrically modified nucleosomes contain the two copies of a histone (sister histones) decorated with distinct sets of Post-translational Modifications (PTMs). They are newly identified species with unknown means of establishment and functional implications. Current analytical methods are inadequate to detect the copy-specific occurrence of PTMs on the nucleosomal sister histones. This protocol presents a biochemical method for the in vitro reconstitution of nucleosomes containing differentially isotope-labeled sister histones. The generated complex can be also asymmetrically modified, after including a premodified histone pool during refolding of histone subcomplexes. These asymmetric nucleosome preparations can be readily reacted with histone-modifying enzymes to study modification cross-talk mechanisms imposed by the asymmetrically pre-incorporated PTM using nuclear magnetic resonance (NMR) spectroscopy. Particularly, the modification reactions in real-time can be mapped independently on the two sister histones by performing different types of NMR correlation experiments, tailored for the respective isotope type. This methodology provides the means to study crosstalk mechanisms that contribute to the formation and propagation of asymmetric PTM patterns on nucleosomal complexes.

Introduction

Eukaryotic DNA is tightly packaged within cell nuclei into chromatin. The fundamental building block of chromatin is the nucleosome core particle that contains ~147 bp of DNA wrapped around an octameric complex made up of two copies each of the four core histones (H3, H4, H2A, H2B). Histone proteins harbor a plethora of Post-translational Modifications (PTMs). These covalent substitutions induce alterations in chromatin structure, both directly by affecting the physical chemistry of the system and indirectly by recruiting chromatin-remodeling activities1,2,3. By those means, histone PTMs control chromatin accessibility and, hence, regulate all DNA-based cellular functions4.

PTMs are installed by histone-modifying enzyme systems mainly on the unstructured N-terminal segments (tails) of nucleosome-incorporated core histones. Due to the many modification sites on the relatively short sequence of histone tails, PTMs influence each other by inducing or blocking subsequent modification reactions, an effect known as modification cross-talk5. Because of the overall symmetric architecture of the nucleosome, modification reactions and crosstalk mechanisms were thought to occur similarly onto the two copies of each nucleosomal histone (sister histones). This concept was recently challenged and subsequently disproved. Particularly, in vitro enzymatic assays on free histone H3 tail peptides and on nucleosomes demonstrated that a set of H3 kinases introduced phosphorylation in an asymmetric manner6. Additionally, affinity-purification-based LC-MS/MS analysis revealed the existence of asymmetrically H3-methylated nucleosomes in several types of eukaryotic cells7. Thus, asymmetrically modified nucleosomes constitute novel species, and tools are needed to uncover the mechanisms that control their formation and to analyze the crosstalk effects that this asymmetry might exert.

Commonly, Western Blotting (WB) and Mass Spectrometry (MS) analysis have been used to detect histone PTMs. Despite its easy application, WB suffers from specificity/cross-reactivity problems. On top of that, it is incapable of performing simultaneous multi-PTM analysis and direct quantification of the modification reactions8. On the other hand, MS analysis employs sophisticated instrumentation that requires high-level training, but provides high specificity as well as simultaneous mapping and quantification of multiple PTMs9. However, both methods are disruptive and the nucleosomal complexes are dissociated before analysis, giving rise to a mixture of histones and/or histone-derived peptides. This manipulation removes the ability to distinguish independent modification reactions that occur on each of the two sister histones and to report the copy-specific modification status of the nucleosomal histones.

Nuclear Magnetic Resonance (NMR) spectroscopy evolved as an alternative method to map PTM reactions. NMR is nondisruptive and thus allows the monitoring of PTM events in a real-time manner in reconstituted mixtures, and even in intact cells10,11. The development of routines for fast data acquisition as well as for high-resolution mapping based on 2D hetero-nuclear correlation methods of isotope-labeled (15N and/or 13C) samples12 allowed the simultaneous mapping of different types of PTMs, such as serine/threonine/tyrosine phosphorylation, lysine acetylation/methylation, and arginine methylation13. Depending on the PTM under investigation, 15N- or 13C-labeling protocols can be employed to mark the protein functional group that serves as a modification reporter. Consequently, PTM mapping can be performed by following the characteristic chemical shift displacement of the corresponding functional group 'sensing' the alteration on the chemical environment. In most cases, both N-H and C-H chemical groups can be used to report the evolution of the PTM of interest.

The current protocol describes the generation of nucleosomes containing differentially isotope-labeled sister histones. It combines the flexibility of NMR spectroscopy to map PTMs using both 1H-15N and 1H-13C correlation spectra with the utilization of different protein affinity tags for purification of the selected reconstituted histone complexes. Notably, the protocol employs two different pools of a particular histone for nucleosome reconstitution. These pools are differentially isotope-labeled (one with 15N, the other with 13C), and they are fused to a polyhistidine and a streptavidin affinity tag, respectively. A tandem affinity purification scheme with Ni-NTA and streptavidin-based chromatography initially used by Voigt et al.7 is employed to purify asymmetric species from symmetric counterparts (Figure 1A). Asymmetric histone octamers are used subsequently to reconstitute equivalent nucleosomal complexes (Figure 1B), using the standard salt dialysis method14. Additionally, through the same procedure and by having one of the histone pools pre-modified, a PTM can be incorporated asymmetrically onto the resulting nucleosomes. The reaction of these substrates with histone-modifying enzymes and subsequent NMR-mapping of modification events enable the characterization of crosstalk mechanisms both in-cis (premodified histone copy) and in-trans (unmodified histone copy) (Figure 1C).

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Protocol

1. Reconstitution of Nucleosomes with Differentially Isotope-labeled (and Asymmetrically Modified) Sister Histones

NOTE: The current protocol describes the reconstitution of nucleosomes with differentially isotope-labeled histone H3. To this end, two pools of histone H3 were used; one was 15N-labeled and contained a 6xHis-tag at the N-terminus and the second was 13C-labeled and contained the Strep peptide (WSHPQFEK) fused at the N-terminus. Both tags were separated from the native H3 sequence with a Tobacco Etch Virus (TEV) protease recognition site. To prepare additional asymmetrically modified nucleosomes, one of the two H3 pools is included in a premodified form. Premodification of a histone pool can be performed by reacting the isotope-labeled histone of interest with the respective histone-modifying enzyme in the presence of the necessary for each type of reaction cofactors/PTM donors16. The efficient placement of the respective PTM can be assessed by NMR spectroscopy or mass spectrometry. The amounts of histones/DNA used here are rough recommendations to obtain a nucleosome preparation with an approximate concentration of 10 µM (measured as DNA concentration at 260 nm).This final yield is sufficient to record good quality NMR spectra with relatively short acquisition times.

  1. Reconstitution of a histone octamer with differentially isotope-labeled (and asymmetrically modified) histone H3
    NOTE: Recombinant histone proteins can be produced in mg quantities in BL21(DE3)plysS cells14. To obtain isotope-labeled histones, the same expression/purification protocol is followed with the exception of using for bacterial growth a minimal medium containing 15NH4Cl and/or 13C-Glucose as nitrogen and carbon sources, for 15N- or 13C-labeling respectively. Purified histones are extensively dialyzed against 5 mM β-mercaptoethanol and stored lyophilized before use.
    1. Dissolve lyophilized histone aliquots, containing ~5 mg of each histone in 1 mL of unfolding buffer (7 M Guanidinium-HCl, 20 mM Tris pH 7.5, 10 mM DTT). Include both types of histone H3. Mix by pipetting and do not vortex. Keep the tubes on ice for 30 min to allow complete unfolding.
    2. Determine the exact concentration of each histone by measuring the absorbance at 280 nm against unfolding buffer and using extinction coefficients calculated with the ProtParam tool of the ExPASy portal.15
    3. Mix the core histones to equimolar ratios, keeping in mind to include 50% each of the two histone H3 pools. Start by using the whole content of the less concentrated histone and add all of the others accordingly.
    4. Adjust final protein concentration to approximately 1 mg/mL using unfolding buffer.
    5. Transfer the mixture to a 6 kDa-cutoff dialysis membrane and dialyze against 1-2 L of chilled refolding buffer (10 mM Tris pH 7.5, 2 M NaCl, 1 mM EDTA, 2 mM DTT) at 4 °C. Change the buffer at least once after dialysis has proceeded for a minimum of 3 h. Perform a final dialysis O/N at 4 °C.
    6. Collect dialyzed material and remove any precipitates by centrifugation in a microfuge for 5 min at 4 °C on maximum speed (normally no precipitation should be observed). Determine octamer concentration by measuring the absorbance at 280 nm. In the calculations, use the added extinction coefficients of histones, keeping in mind to double each value.
    7. Concentrate to a final volume of ~2 mL using a 10 kDa-cutoff centrifugal filter unit. Recalculate octamer concentration and estimate loss. At this point, an octamer concentration between 50 - 100 µM should be obtained.
    8. Connect the gel filtration column (stated in the Table of Materials) to an FPLC system and equilibrate with 2 column volumes (CV) of 0.22 µm-filtered and degassed refolding buffer at a flow rate of 1 mL/min and a pressure limit of 0.5 MPa.
      NOTE: The gel filtration run should be performed in the cold room or in a cold cabinet.
    9. Inject concentrated material using a flow rate of 1 mL/min and collect 1.0 - 1.5 mL fractions.
    10. Follow the chromatographic profile and observe histone octamer elution at ~65 - 68 mL.
      NOTE: A small shoulder of the elution peak and a peak at ~80 mL indicates the existence of free H3-H4 tetramers and H2A-H2B dimers, respectively.
    11. Run 20 µL of each collected fraction in an 18% SDS-PAGE gel.
      NOTE: Dilute the samples by a factor of at least 2 with water before loading them on the gel to reduce the high salt concentration and thus, avoid distortions. The same applies for subsequent SDS-PAGE analyses of samples in refolding buffer.
    12. Pool relevant fractions containing pure octamers judged by the equal distribution of the 4 histones on the stained gel and determine concentration as before (step 1.1.7).
    13. Connect a 1 mL Ni-NTA column (Table of Materials) to an FPLC system and equilibrate with 10 CV of 0.22 µm-filtered and degassed refolding buffer at a flow rate of 1 mL/min.
      NOTE: The Ni-NTA chromatography should be performed in the cold room or in a cold cabinet.
    14. Pass purified octamer through the Ni-NTA using a flow rate of 1 mL/min.
    15. Collect flow-through and keep samples for SDS-PAGE/WB analysis (20 µL and 4 µL, respectively). Subsequently, wash column with 10 CV of refolding buffer or until a baseline signal is reached.
    16. Elute with 10 CV of refolding buffer containing 250 mM imidazole using a flow rate of 1 mL/min. Keep samples for SDS-PAGE/WB analysis (20 µL and 4 µL, respectively).
    17. Equilibrate a 1 mL affinity column of a commercial streptavidin (Table of Materials) with 10 CV refolding buffer containing 250 mM imidazole using a batch/gravity flow setup.
      NOTE: This chromatographic step should be performed in the cold room.
    18. Pass Ni-NTA elution through the commercial streptavidin affinity column.
    19. Collect flow through and keep samples for SDS-PAGE/WB analysis (20 µL and 4 µL, respectively). Subsequently, wash with 10 CV of refolding buffer.
    20. Elute with 10 CV of refolding buffer containing 2.5 mM desthiobiotin. Keep samples for SDS-PAGE/WB analysis (20 and 4 µL respectively).
    21. Measure octamer concentration, add 10 times less TEV protease and let reaction proceed overnight at 4 °C in a standard plastic centrifuge tube.
      NOTE: The necessary amount of TEV to obtain complete digestion (removal of the affinity tags) depends on the origin (construct) and on the activity (freshly made, recombinant TEV is more active compared to the one stored for prolonged periods at - 80 °C). Try initially adding 10 times less TEV compared to the octamer (estimated as protein concentrations) and adjust accordingly.
    22. Check for the efficient digestion by running 20 µL of the mixture prior and after TEV addition on an 18% SDS-PAGE gel. If digestion is not complete, add more TEV protease and continue incubation for another 3-4 h.
    23. Dialyze sample against refolding buffer using a 50 kDa-cutoff dialysis membrane to remove TEV protease and adjust buffer composition.
    24. Concentrate the purified asymmetric octamer using a 10 kDa-cutoff centrifugal filter unit (the same filter unit from step 1.1.7 can be also used) to a volume of 1.0-2.0 mL. Measure the final concentration. Either use soon after for nucleosome reconstitution or adjust to 50% (v/v) glycerol to store at -20 °C for longer periods. At this point and expecting at least 70% loss during the previous steps, the octamer concentration should be in the range of 20 - 50 µM.
  2. Nucleosome reconstitution
    1. If octamer was stored in 50% glycerol, dialyze overnight at 4 °C against refolding buffer before proceeding with nucleosome reconstitution.
    2. Adjust DNA (containing a nucleosome-positioning sequence) salt concentration to 2 M NaCl by using a 5 M NaCl stock solution.
      NOTE: The purified DNA either isolated after purification of a plasmid that contains multiple copies of the desired sequence or synthesized by PCR amplification should be stored concentrated to ~50 µM in water or a standard Tris-EDTA buffer.
    3. Mix octamer and DNA using the optimum ratio determined from a small-scale test. Use refolding buffer to adjust the final volume to ~3.0 mL. Always add the octamer last to prevent any possibility of mixing the octamer and the DNA at <2 M salt concentrations.
      1. Perform initial small-scale reconstitutions to determine the octamer:DNA ratio that leads to optimum nucleosome yields. For this, assemble three reactions of 0.9:1.0, 1.0:1.0, and 1.1:1.0 DNA:octamer ratios in a volume between 50-100 µL. Typically, use a concentration of 5 µM DNA.
      2. Proceed with reconstitution as described below (steps 1.2.4-1.2.8) and at the end, estimate the amount of soluble and good quality reconstituted nucleosome by measuring the DNA concentration at 260 nm and by running a 6% native-PAGE DNA gel, stained with ethidium bromide, respectively (Figure 5A).
    4. Transfer the mix to a 6 kDa-cutoff dialysis membrane and dialyze against 1 L of refolding buffer overnight at 4 °C.
    5. Reduce the salt concentration of the dialysis buffer in a step-wise manner from 2, to 0.85, 0.64, and 0.2 M NaCl respectively. Keep sample in each buffer for at least 3 h. Sometimes precipitate is formed after the last transition. In this case continue dialysis as planned and remove precipitate by microfuge centrifugation at the end of the next step.
    6. Transfer dialysis membrane in a beaker with 1 L of assay buffer (25 mM NaH2PO4/Na2HPO4 pH 6.8, 25 mM NaCl, 2 mM DTT) and continue dialysis O/N at 4 °C.
    7. Collect sample, remove any precipitate formed at step 1.2.5 by centrifugation in a microfuge for 5 min at 4 °C on maximum speed and concentrate using a 30 kDa-cutoff centrifugal filter unit to a final volume of ~300 µL.
    8. Measure DNA concentration at 260 nm, run an 18% SDS-PAGE protein gel (4 µL of sample) and a 6% native-PAGE DNA gel (0.2 µL of sample) and store sample at 4 °C for several weeks. The final concentration should be in the range of 10-20 µM.

2. NMR Analysis of Modification Reactions on the Two Sister Histones

NOTE: Assignment of 2D 1H-15N correlation spectra of nucleosomal histone tails can be found at references16,17,18. Additionally, assignments of CHx groups of lysines, serines and threonines on 2D 1H-13C correlation spectra can be found at reference16.

  1. NMR setup and recording of reference spectra
    NOTE: Enzymatic assays were performed using 140 µL of the nucleosome sample in assay buffer into a 3-mm NMR tube at 300 K. Different NMR tubes with other sample volumes can be also used. The aforementioned temperature is appropriate to obtain good quality 1H-15N correlation spectra of nucleosomal histone tails and good enzymatic activities. 2D-SOFAST-HMQC 1H-15N and 2D-HSQC 1H-13C spectra were recorded respectively with a setup that confers similar acquisition times. Typical acquisition parameters are 128 transients with 1.024 (1H) x 128 (15N) complex points and 32 transients with 1.024 (1H) x 64 (13C) complex points for the two different types of correlation spectra. For both 2D spectra, the acquisition time was ~30 min.
    1. Set 300 K as the sample temperature in the spectrometer. Add 10% D2O (v/v) to the sample to be used for the spectrometer frequency lock.
    2. Place the sample in the spectrometer and perform basic operations (locking, tuning, shimming). Additionally, determine optimal pulse lengths and general acquisition parameters.
    3. Record 1D and 2D 1H-15N and 1H-13C reference spectra.
    4. Process reference spectra and ensure that the signals to be used for mapping the modification reactions are well resolved and have good intensities.
    5. Recover sample and transfer it to a microfuge tube.
  2. Setup of the enzymatic reaction, NMR monitoring and quantitative analysis
    1. Copy and arrange a series of interleaved 2D 1H-15N and 1H-13C spectra. Aim for a total acquisition time of several hours and adjust accordingly in a new run based on the enzymatic rates obtained from the first reaction.
    2. Add to the sample the necessary cofactors for the respective type of modification reaction (1 mM ATP/2 mM MgCl2 for phosphorylation, 1 mM acetyl-CoA for acetylation, 1 mM SAM for methylation, etc.).
    3. Add the enzyme of interest, mix by pipetting, transfer the sample back in the NMR tube and subsequently in the spectrometer (perform these operations quickly).
      NOTE: If there is no data about the expected enzymatic activity, adjust the substrate-to-enzyme molar ratio to 10:1. Perform a first trial run and adjust accordingly for the real run.
    4. Perform a fast automatic shimming and use the rest of parameters from the reference spectra.
    5. Initiate the series of the interleaved 2D 1H-15N and 1H-13C spectra.
    6. Follow the progression of the reaction in real-time and stop acquisition when the reaction reaches completion or a desired level.
    7. Process spectra as before with exactly the same parameters.
    8. Repeat the whole run using a different acquisition order for the two types of correlation spectra. If in the first experiment a 1H-15N correlation was first in the series, start now with a 1H-13C correlation. By this and having same acquisition time for both spectra, it is possible to plot and compare PTM reactions on both differentially isotope-labeled histones on the same time scale. Additionally, it is possible to calculate averages and plot error bars.
      NOTE: A thorough description of the methodologies for NMR signal analysis and subsequent quantification of enzymatic reactions can be found here19.
    9. Select NMR signals from each time-course NMR spectrum that report the progression of the reaction and calculate their relative signal intensities using a visualization and analysis software for NMR spectra. Do this for signals that report the unmodified as well as the modified state. Extract modification levels.
    10. Plot the calculated values of modification levels against the reaction time.

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Results

Properly refolded octameric species are isolated after a run of the reconstitution mixture through a gel filtration column (Figure 2). The reconstituted octameric pool containing the three different types of octamers is subjected to the tandem affinity purification scheme. Samples are collected from all the steps and analyzed by SDS-PAGE and subsequently WB. Verification of the correct execution of the protocol that results in the isolation of asymmetric species is achiev...

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Discussion

For nucleosome reconstitution, the current protocol utilizes a 165 bp long DNA template containing the 601-Widom nucleosome positioning sequence20, but similar performance is expected using various lengths of DNA templates. The protocol was designed and employed using asymmetric types of histone H3. With the same principle, the method can be applied also for the other core histones and additionally can be used to reconstitute complexes carrying two distinct core histones with different isotope lab...

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Disclosures

The author has nothing to disclose.

Acknowledgements

The author thanks Dr. Philipp Selenko (FMP-Berlin) for providing wet-lab space and infrastructure to perform experiments and Deutsche Forschungsgemeinschaft (DFG) for funding the work through a research grant (LI 2402/2-1).

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Materials

List of materials used in this article
NameCompanyCatalog NumberComments
Guanidinium HClApplichemA14199Use high quality Gu-HCl
Tris Roth4855.2
DTTApplichemA1101
NaClVWR chemicals27810.364
EDTARoth8043.2
Na2H2PO4ApplichemA1046
NaH2PO4ApplichemA3902
ImidazoleApplichemA1073
d-DesthiobiotinSigmaD1411
Ni-NTA SuperflowQiagen1034557
Strep-Tactin SuperflowIBA2-1207-001
His-probe antibodySanta Cruzsc-8036
Strep-tactin conjugated HRPIBA2-1502-001
Hi-Load 16/600 Superdex 200 pgGE Healthcare28-9893-35
6 - 8 kDa dialysis membraneSpectrumlabsspectra/por 1, 132650
50 kDa dialysis membraneSpectrumlabsspectra/por 7, 132129
10 kDa centrigugal filter unitMerck MilliporeUFC901024
30 kDa centrigugal filter unitMerck MilliporeUFC903024
Solution-state NMR spectrometer at least 500 MHz operating frequency, equipped with a triple-resonance cryoprobe
Buffer nameComponent
Unfolding Buffer7 M Guanidinium HCl
20 mM Tris, pH 7.5
10 mM DTT
Refolding Buffer10 mM Tris, pH 7.5
2 M NaCl
1 mM EDTA
2 mM DTT
Assay Buffer25 mM Na2H2PO4, pH 6.8
25 mM NaCl
2 mM DTT

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Nucleosome ReconstitutionIsotope labeled HistonesHistone H3Protein PurificationDialysis MembraneGel FiltrationAffinity ChromatographyNMR SpectroscopyPost translational Modifications

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