Melbournevirus encodes a shorter H2B-H2A doublet histone variant that forms structurally distinct nucleosome structures

Melbournevirus encodes a shorter H2B-H2A doublet histone variant that forms structurally distinct nucleosome structures | bioRxiv /* */ /* */ <!-- <!-- /*! * yepnope1.5.4 * (c) WTFPL, GPLv2 */ (function(a,b,c){function d(a){return"[object Function]"==o.call(a)}function e(a){return"string"==typeof a}function f(){}function g(a){return!a||"loaded"==a||"complete"==a||"uninitialized"==a}function h(){var a=p.shift();q=1,a?a.t?m(function(){("c"==a.t?B.injectCss:B.injectJs)(a.s,0,a.a,a.x,a.e,1)},0):(a(),h()):q=0}function i(a,c,d,e,f,i,j){function k(b){if(!o&&g(l.readyState)&&(u.r=o=1,!q&&h(),l.onload=l.onreadystatechange=null,b)){"img"!=a&&m(function(){t.removeChild(l)},50);for(var d in y[c])y[c].hasOwnProperty(d)&&y[c][d].onload()}}var j=j||B.errorTimeout,l=b.createElement(a),o=0,r=0,u={t:d,s:c,e:f,a:i,x:j};1===y[c]&&(r=1,y[c]=[]),"object"==a?l.data=c:(l.src=c,l.type=a),l.width=l.height="0",l.onerror=l.onload=l.onreadystatechange=function(){k.call(this,r)},p.splice(e,0,u),"img"!=a&&(r||2===y[c]?(t.insertBefore(l,s?null:n),m(k,j)):y[c].push(l))}function j(a,b,c,d,f){return q=0,b=b||"j",e(a)?i("c"==b?v:u,a,b,this.i++,c,d,f):(p.splice(this.i++,0,a),1==p.length&&h()),this}function k(){var a=B;return a.loader={load:j,i:0},a}var l=b.documentElement,m=a.setTimeout,n=b.getElementsByTagName("script")[0],o={}.toString,p=[],q=0,r="MozAppearance"in l.style,s=r&&!!b.createRange().compareNode,t=s?l:n.parentNode,l=a.opera&&"[object Opera]"==o.call(a.opera),l=!!b.attachEvent&&!l,u=r?"object":l?"script":"img",v=l?"script":u,w=Array.isArray||function(a){return"[object Array]"==o.call(a)},x=[],y={},z={timeout:function(a,b){return b.length&&(a.timeout=b[0]),a}},A,B;B=function(a){function b(a){var a=a.split("!"),b=x.length,c=a.pop(),d=a.length,c={url:c,origUrl:c,prefixes:a},e,f,g;for(f=0;f<d;f++)g=a[f].split("="),(e=z[g.shift()])&&(c=e(c,g));for(f=0;f<b;f++)c=x[f](c);return c}function g(a,e,f,g,h){var i=b(a),j=i.autoCallback;i.url.split(".").pop().split("?").shift(),i.bypass||(e&&(e=d(e)?e:e[a]||e[g]||e[a.split("/").pop().split("?")[0]]),i.instead?i.instead(a,e,f,g,h):(y[i.url]?i.noexec=!0:y[i.url]=1,f.load(i.url,i.forceCSS||!i.forceJS&&"css"==i.url.split(".").pop().split("?").shift()?"c":c,i.noexec,i.attrs,i.timeout),(d(e)||d(j))&&f.load(function(){k(),e&&e(i.origUrl,h,g),j&&j(i.origUrl,h,g),y[i.url]=2})))}function h(a,b){function c(a,c){if(a){if(e(a))c||(j=function(){var a=[].slice.call(arguments);k.apply(this,a),l()}),g(a,j,b,0,h);else if(Object(a)===a)for(n in m=function(){var b=0,c;for(c in a)a.hasOwnProperty(c)&&b++;return b}(),a)a.hasOwnProperty(n)&&(!c&&!--m&&(d(j)?j=function(){var a=[].slice.call(arguments);k.apply(this,a),l()}:j[n]=function(a){return function(){var b=[].slice.call(arguments);a&&a.apply(this,b),l()}}(k[n])),g(a[n],j,b,n,h))}else!c&&l()}var h=!!a.test,i=a.load||a.both,j=a.callback||f,k=j,l=a.complete||f,m,n;c(h?a.yep:a.nope,!!i),i&&c(i)}var i,j,l=this.yepnope.loader;if(e(a))g(a,0,l,0);else if(w(a))for(i=0;i (function(w,d,s,l,i){w[l]=w[l]||[];w[l].push({'gtm.start':new Date().getTime(),event:'gtm.js'});var f=d.getElementsByTagName(s)[0];var j=d.createElement(s);var dl=l!='dataLayer'?'&l='+l:'';j.src='//www.googletagmanager.com/gtm.js?id='+i+dl;j.type='text/javascript';j.async=true;f.parentNode.insertBefore(j,f);})(window,document,'script','dataLayer','GTM-M677548'); Skip to main content Home About Submit ALERTS / RSS Search for this keyword Advanced Search New Results Melbournevirus encodes a shorter H2B-H2A doublet histone variant that forms structurally distinct nucleosome structures View ORCID Profile Alejandro Villalta , View ORCID Profile Hugo Bisio , View ORCID Profile Chelsea M. Toner , View ORCID Profile Chantal Abergel , View ORCID Profile Karolin Luger doi: https://doi.org/10.1101/2025.01.15.633200 Alejandro Villalta 1 Department of Biochemistry, University of Colorado Boulder , Boulder, CO 80309, USA 2 Howard Hughes Medical Institute, University of Colorado Boulder , Boulder, CO 80309, USA Find this author on Google Scholar Find this author on PubMed Search for this author on this site ORCID record for Alejandro Villalta Hugo Bisio 3 Aix–Marseille University, Centre National de la Recherche Scientifique, Information Génomique & Structurale, Unité Mixte de Recherche 7256 (Institut de Microbiologie de la Méditerranée, FR3479, IM2B) , 13288 Marseille Cedex 9, France Find this author on Google Scholar Find this author on PubMed Search for this author on this site ORCID record for Hugo Bisio Chelsea M. Toner 1 Department of Biochemistry, University of Colorado Boulder , Boulder, CO 80309, USA Find this author on Google Scholar Find this author on PubMed Search for this author on this site ORCID record for Chelsea M. Toner Chantal Abergel 3 Aix–Marseille University, Centre National de la Recherche Scientifique, Information Génomique & Structurale, Unité Mixte de Recherche 7256 (Institut de Microbiologie de la Méditerranée, FR3479, IM2B) , 13288 Marseille Cedex 9, France Find this author on Google Scholar Find this author on PubMed Search for this author on this site ORCID record for Chantal Abergel Karolin Luger 1 Department of Biochemistry, University of Colorado Boulder , Boulder, CO 80309, USA 2 Howard Hughes Medical Institute, University of Colorado Boulder , Boulder, CO 80309, USA Find this author on Google Scholar Find this author on PubMed Search for this author on this site ORCID record for Karolin Luger For correspondence: karolin.luger{at}colorado.edu Abstract Full Text Info/History Metrics Preview PDF Abstract Unique among viruses, some giant viruses utilize histones to organize their genomes into nucleosomes. Melbournevirus encodes a distinct H2B-H2A histone doublet variant in addition to the canonical H4-H3 and H2B-H2A doublets. This viral histone variant has a truncated H2B portion and its amino acid sequence deviates from that of the main viral H2B-H2A throughout the entire coding region. It is less abundant than the main H2B-H2A doublet, is essential for melbournevirus fitness, and is conserved in all Marseilleviridae . The cryo-EM structure of a nucleosome-like particle reconstituted with this H2B-H2A variant and viral H4-H3 reveals that only 90 base pairs of DNA are stably bound, significantly less than in eukaryotic nucleosomes and viral nucleosomes made with the main fused viral histone doublets. The reduced ability to bind DNA can be attributed to structural differences between variant and main H2B-H2A. Variant melbournevirus nucleosomes are less stable, possibly aiding rapid genome unpacking to initiate gene expression. Our results highlight the remarkable propensity of giant viruses to appropriate the utility of histones for their specialized purposes. Introduction All eukaryotes organize their genomes into nucleosomes, a complex of four types of conserved histones (two copies each of H2A, H2B, H3, and H4) that wrap 147 base pairs of DNA 1 . Nucleosomes are the repeating structural unit of eukaryotic chromatin and contribute to the regulation of genome accessibility in major ways. This strategy, which was originally thought to be an exclusive feature of eukaryotes, is now increasingly found in non-eukaryotic organisms such as archaea, bacteria, and even viruses. Most representatives of the domain of Archaea encode at least one minimalist histone that forms histone fold dimers with strong structural homology to the eukaryotic histone pairs H2A-H2B and H3-H4. Archaeal histones are much less conserved across the domain compared to their eukaryotic counterparts and typically lack N-terminal tails and other extensions 2 , 3 . Rather than forming defined particles, these histones organize DNA into slinky-like hypernucleosomal structures of variable size 4 – 6 . Histone-like proteins were also identified in some bacterial clades, and in some cases significant amounts of the histone are associated with the bacterial genome 7 – 9 . Recently, some double-stranded DNA viruses, particularly in members of the phylum Nucleocytoviricota (encompassing the ‘giant viruses’) were also found to encode histone-like proteins 10 . Nucleosome-like particles (NLPs) with histones encoded by the giant viruses melbournevirus and medusavirus have been structurally characterized 11 – 13 . While medusavirus encodes single copies of homologs for the four core histones H2A, H2B, H3, and H4, histones from representatives of the distantly related Marseilleviridae (including melbournevirus) are encoded as doublets, linking H4 to H3, and H2B to H2A (mel_368 and mel_369, respectively) 11 , 12 , 13 . The NLPs from both viruses exhibit distinct structural features and are more unstable in vitro than their eukaryotic counterparts. The essential nature of histones has yet to be determined for histone-encoding viruses other than melbournevirus 12 , and to date no evidence for epigenetic histone modifications has been found in the few giant viruses that have been studied. In eukaryotes, the replacement of the canonical, replication-dependent core histones with histone variants (which are best described as ‘special histones for special occasions’) contributes in significant ways to gene regulation and chromosome organization, by conveying unique features to the nucleosome 14 . Well-characterized histone variants include H2A.Z (associated with active transcription), H2A.B, and the H3 variant CenpA (located exclusively at centromeres of eukaryotic chromosomes) 14 . Deletion of the genes encoding histone variants is embryonic-lethal in most cases, indicating that the subtle structural differences of the variant nucleosomes convey specific functions. Histone variants have expression patterns that are distinct from the replication-dependent major-type histones, and they utilize separate mechanisms for their integration into nucleosomes 15 . Intriguingly, melbournevirus (MV) encodes a gene (mel_149; originally annotated as a “histone 2A-domain-containing protein”) that we suspected to be the first virally encoded histone variant. The protein product was found in the virion of melbournevirus, together with the H4-H3 and H2B-H2A proteins, and was shown to be associated with melbournevirus chromatin 12 , 16 . Proteomic analysis of the melbournevirus virion revealed that the mel_149 gene product is 30 times less abundant than H4-H3 (mel_368) and ∼10 times less abundant than H2B-H2A (mel_369) 12 . Mel_149 is highly conserved across the entire Marseilleviridae family ( Extended Figure 1 ). Here we show that mel_149 is essential for melbournevirus fitness. We determined the structure and thermal stability of an NLP reconstituted from H4-H3 (mel_368) and the putative H2B-H2A variant (mel_149). A structural comparison with our previously published structure of a nucleosome reconstituted with the two main melbournevirus histone doublets sheds light on the potential role of the H2B-H2A variant in the organization and regulation of the Melbournevirus genome. Results Melbournevirus encodes a conserved shorter H2B-H2A doublet variant that is essential for viral fitness We suspected that the mel_149 gene product might be a virally-encoded H2B-H2A variant as it shares less than 31% identity with mel_369 (MV-H2B-H2A) and less than 23% identity with mel_368 (MV-H4-H3) ( Extended Table 1 ). This gene has no recognizable homology to histone H2B. Indeed, the H2A region of mel_149 is ∼ 40% identical to H2A encoded by the amoeba host Acanthamoeba castellanii (‘amoeba’), to Xenopus laevis H2A, and to the H2A region of MV-H2B-H2A ( Extended Table 1 ). In contrast, the H2B portion does not have any similarity with Xenopus laevis H2B, amoeba H2B, or with the H2B region of MV-H2B-H2A. Additionally, no homolog for the isolated H2B portion was found in the entire amoeba genome. The melbournevirus variant-H2B-H2A, with 168 amino acids (aa)) is much shorter than the main MV-H2B-H2A doublet (269 aa). We will refer to the mel_149 gene product as MV-varH2B-H2A to distinguish it from MV-H2B-H2A. Distinct features of the MV-varH2B-H2A amino acid sequence are its shorter predicted tail regions compared to MV-H2B-H2A (10 aa shorter H2B N-terminal tail, and 70 aa shorter H2A C-terminal tail), and the shortened H2BαC helix ( Figure 1 ). Additionally, the linker region between H2B and H2A in the variant is also predicted to be shorter by 10 aa. These features of MV-varH2B-H2A are highly conserved across the entire Marseilleviridae family ( Extended Figure 1 ), suggesting functional roles. Download figure Open in new tab Figure 1: Melbournevirus encodes an H2B-H2A histone variant. The amino acid sequence of MV-H2B-H2A (mel_369, secondary structure elements taken from pdb 7N8N shown in dark red for H2B, and yellow for H2A) and MV-varH2B-H2A (mel_149, predicted secondary structure elements shown in light red and light yellow for H2B and H2A respectively). Dark blue highlighted amino acids (aa) are conserved between the two proteins; similar hydrophobic amino acids are shown in light blue (V/I or F/W/Y), and conserved positively charged aa (R/K) are highlighted in green. We have shown previously that the genes encoding MV-H4-H3 and MV-H2B-H2A (mel_368 and mel_369 gene products) are essential in melbournevirus, suggesting key roles for the two histone doublets in the viral life cycle 12 . To investigate the importance of the putative variant H2B-H2A for viral fitness, we proceeded to knock out mel_149 from the melbournevirus genome, as described previously 12 . We used the resultant recombinant viruses to infect the host organism Acanthamoeba castellanii . As was observed for the deletion of MV-H4-H3, the recombinant viruses were quickly lost and outcompeted by wild-type virus. To verify that this is a direct effect of the missing mel_149 gene, we infected amoebae that had been transfected with an expression vector containing the mel_149 gene encoding MV-varH2B-H2A. In these strains, the recombinant viruses are not outcompeted by wild-type viruses ( Figure 2 ). The persistence of the virus in the complementing amoebae confirms that MV-varH2B-H2A is also essential for MV and has functions that cannot be executed by major-type H2B-H2A or host histones. Download figure Open in new tab Figure 2: mel_149 is an essential gene of melbournevirus. (A) PCR amplifications of mel_149 at three cellular passages of A. castellanii, complemented with mel_149 or wildtype. (B) DNA map of the genomic region where the gene of interest is located, showing the expected size when the knockout of the gene is performed or in the case of wildtype. MV-varH2B-H2A and MV-H4-H3 assemble into structurally unique nucleosome-like particles (NLPs) To investigate whether the putative histone variant MV-varH2B-H2A can form viral NLPs with MV-H4-H3, we used our standard procedure to assemble nucleosomes with a 147 bp DNA fragment (Widom 601 positioning sequence). MV-varH2B-H2A behaved like MV-H2B-H2A during reconstitution, and the two NLPs migrate similarly on a native gel ( Extended Figure 2A ). Mass photometry analysis shows that the complex has a size of 157 ± 33 kDa, well within the error of the expected size of 133.5 kDa, confirming the assembly of the viral variant NLPs with a full complement of histones ( Extended Figure 2B ). Just as canonical MV-NLP, variant NLP is destabilized compared to eukaryotic nucleosomes, as demonstrated by a thermal shift assay 17 . This assay monitors the dissociation of histones from the DNA by measuring the exposure of hydrophobic amino acids to SYPRO Orange. MV-varNLP (with a melting temperature of 49.5±0.55°C) is destabilized compared to MV-NLP (52.8±0.4°C), and this difference, although relatively modest, is statistically significant ( Extended Figure 2C-E ). Both values are significantly lower than what is observed for eukaryotic nucleosomes, consistent with our experience that crosslinking is necessary to maintain intact viral NLPs on cryo-EM grids 12 . Both MV-NLPs are characterized by a denaturation curve that is qualitatively distinct from that of human nucleosomes. These typically show two distinct denaturing events: the first at around 75±0°C corresponding to H2B-H2A dissociation, and the second at 86.2±0.4°C corresponding to H4-H3 dissociation, as previously published 17 . In contrast, both variant and canonical MV-NLPs dissociate either in a single step or in two concurrent steps that are indistinguishable in our assays ( Extended Figure 2C, D ). To stabilize variant-NLP for cryo-EM, we crosslinked samples using a GraFix protocol that we previously optimized for MV-NLP 12 . We were able to determine the structure of MV-varNLP to an overall resolution of 4.4 Å ( Extended Figure 3 , Extended Table 2 ), with higher resolution observed for the protein core, while parts of the DNA and the tail regions are less well defined. MV-varNLP contains the requisite two copies of MV-H4-H3 and MV-varH2B-H2A (although one copy is better resolved than the other), and binds DNA in the canonical superhelical configuration typical for all nucleosomes. However, only about 90 bp of DNA are represented by density in MV-varNLP, compared to 124 bp in the MV-NLP density, and 147 bp in most canonical eukaryotic nucleosome structures ( Figure 3 ). Download figure Open in new tab Figure 3: MV-varNLP is structurally similar to MV-NLP. Experimental electron density and model of (A) MV-varNLP, and (B) MV-NLP (PDB: 7N8N). The histone fold regions of H2B are shown in red, H2A in yellow, H4 in green and H3 in blue, with helices not belonging to the histone fold in grey. (C) Superposition of MV-varNLP with MV-NLP. Here, only half of the nucleosome is shown for clarity. Superhelix locations (SHL) are numbered as previously defined 1 . The four-helix bundle region tethering H4 to H2B, and the ‘knuckle domain’ that binds DNA in MV-NLP are indicated by black and blue boxes, respectively. The arrow corresponds to the H2B α3-αC helix interface. In our structure, density for the first 14 amino acids are missing for the MV-H4-H3 portion, and the entire 30 amino acid connector between H4 and H3 is too disordered to confidently be built from the map, even though these regions were visible in our previously published maps of MV-NLP 12 . MV-varH2B-H2A is well resolved, and only the first four amino acids are not represented by density. Overall, the histone portions of variant and major-type MV-NLPs superimpose with a root mean square deviation (r.m.s.d.) of 1.76 Å. This can be mostly attributed to structural differences between the H2B-H2A portion (r.m.s.d. of 1.6 Å), while the H4-H3 portion, where the amino acid sequence is identical between the two structures, exhibits closer similarity (r.m.s.d. of 1.2 Å; Figure 3C ). The incomplete wrapping of DNA in MV-varNLP is caused by sequence differences between variant and main H2B-H2A. The H2B region of the variant histone doublet provides the requisite configuration for a stable four-helix bundle interface with the H4 portion of MV-H4-H3, and strong contacts with the DNA are established at this site (SHL ±3.5, Figure 3C ). The L2 loop connecting α1 to α2 in MV-varH2B is shorter by two amino acids but maintains interactions with its MV-varH2A L1 counterpart and with DNA. This is the last contact observed between histones and DNA in MV-varNLP ( Figure 3C ). The MV-varH2B α3 helix is one turn shorter than in other H2B-like structures, and the adjacent αC helix which defines the surface of the nucleosome is two turns shorter than in any other H2B known to date. The interface between it and the H2B α3 helix is less pronounced, and it stops short of extending to the DNA ( Figure 3C , arrow). The orientation of MV-varH2B α1 has shifted. Its location is stabilized by a hydrophobic core composed of amino acids from the connector linking H2B with H2A that is distinct from MV-H2B-H2A and particularly conserved among members of the Marseilleviridae variant histones ( Extended Figure 1 ). This helix is also shorter by one turn ( Figure 3 and 4 ), due to a highly conserved Proline (P16) that terminates it prematurely, and the loss of contacts with the H2A α2 helix in the histone fold arrangement. This causes the MV-varH2B α2 helix to run straight rather than bent as it is in most other nucleosome structures ( Figure 4A and B ). Download figure Open in new tab Figure 4: MV-varNLP and MV-NLP differ in their H2B portion and in the extent of DNA binding. Cartoon representation of parts of H2B and the H2A C-terminal tail and knuckle domain of (A, B) MV-varNLP, (C, D) MV-NLP (7N8N), and (E, F) the eukaryotic nucleosome (1AOI). Models are represented in transparent colors with solid colors at regions of interest (H2A, yellow; H2B, red; knuckle domain, gray). The connector between H2B and H2A is much shorter in the variant histone and fails to form the ‘knuckle domain’ that in MV-H2B-H2A contact DNA at SHL 4.5. This domain, which is also present in H2A of all eukaryotic nucleosome structure including those with H2A variants 18 , 19 , is formed by a short additional α helix that points its N-terminal end at the DNA ( Figure 4 ). Due to its absence in MV-varH2B-H2A, no contacts with DNA are established at SHL 4.5, even though this region maintains an overall positively charged surface ( Extended Figure 4 ). The H2A α1 helix in MV-varH2B-H2A exhibits a different conformation compared to MV-H2B-H2A. This region differs substantially in its amino acid sequence from the major-type histone, and is particularly well conserved among members of the Marseilleviridae ( Extended Figure 1 ). This helix bends approximately 17° towards the DNA, positioning its N-terminus to contribute to DNA binding through its positive dipole moment ( Figure 4 ). This might help compensate for the lack of interaction that would otherwise be provided by the longer H2B αC helix and the knuckle domain in canonical H2B-H2A, thereby maintaining some level of DNA binding and stabilization in the variant nucleosome. Indeed, weak density for the conventional DNA superhelical path is observed extending to SHL 5.5, suggesting residual DNA interactions ( Extended Figure 4E, F ). Interestingly, a conserved cysteine in the MV-varH2A L1 loop forms a disulfide bond with the second varH2A, supported by well-defined electron density ( Extended Figure 5A ), seemingly stapling together the two MV-varH2B-H2A-variant moieties. This cysteine is also present in main MV-H2A but due to differences in loop configuration does not engage in disulfide-bond formation, as shown in two independently determined structures) 11 , 12 . We were able to observe weak evidence for this disulfide bridge in solution within the MV-variant NLP ( Extended Figure 5B ), although the functional significance of this stapling interaction is currently unknown. This feature is not seen in any eukaryotic H2A histone sequence. Finally, the docking domain in MV-varH2A maintains its characteristic orientation in the portion that packs against the C-terminal region of H4 to stabilize the interaction with H4-H3. However, the ‘stem’ portion in MV-H2A and eukaryotic nucleosomes that provides further contacts with H4-H3 is missing in all viral variant H2A sequences, leading to a less-stable interaction of MV-varH2B-H2A with MV-H4-H3, and an altered nucleosome surface ( Figure 3 C ; Figure 4 ; Extended Figure 4 ). Melbournevirus NLPs can stack to form stable dinucleosomes in silico It has been suggested that melbournevirus nucleosomes are tightly packed within the virus with very little connecting linker DNA 16 . This could provide further stabilization of the particles in the virus. Human telomeric dinucleosomes (PDB: 7V96) represent a tentative starting model for this type of arrangement. Human telomeres are characterized by exceedingly short nucleosome repeat length, resulting in a ‘columnar stacking’ of nucleosomes rather than the more canonical ‘beads on a string’ arrangement observed in genomic nucleosomes 20 . We replaced the histones in the telomeric dinucleosome structure with a histone model taken from both experimentally determined MV-NLPs and completed the missing regions from an Alphafold predicted model, which was largely similar to the experimentally determined structure (r.m.s.d of 1.76, 1.58 and 1.51, for MV-NLP, MV-varNLP and human nucleosome, respectively). We conducted all-atom molecular dynamics simulations to assess the in-silico stability of the resulting viral dinucleosomal stacks. In this configuration, both MV-NLP and MV-varNLP are stable over time and remain stacked ( Figure 5 A, B ). This is despite differences in the makeup of the nucleosomal surface, caused by the divergent H2B αC helix which in the model is positioned to stabilize the stack. The H2A C-terminal tail, which in the predicted MV-NLP dinucleosome model also contributes to stacking stability, is missing in MV-varNLP. As such, the MV-varNLP dinucleosome stack is more affected in the simulation by severing the DNA than MV-NLP or telomeric eukaryotic nucleosomes, suggesting weakened histone-histone stacking interactions ( Figure 5 C, D ). We also performed a simulation of a hybrid MV-varNLP●MV-NLP dinucleosome stack. This hybrid dinucleosome was also stable over time, and its behavior lies between that of MV-NLP and MV-varNLP. Download figure Open in new tab Figure 5: MV-NLP can form nucleosome stacks in silico . Two parameters were measured to assess the stability of di-nucleosomes: (A, C) root mean square deviation (r.m.s.d) of the overall structure compared to the start of the simulation, and (B, D) the distance between the center of gravity of both nucleosomes on the structure. The mean variation of the (A) r.m.s.d and (B) distance are over the simulation time are plotted for the human telomeric dinucleosome (7v96) (green), MV-NLP (blue), MV-varNLP (red) and MV-hybridNLP (purple), the lighter area around the mean curve correspond to the standard variation around the mean curve. The larger r.m.s.d variations in the beginning of the simulation for the human telomeric complex are due to the long tails that collapse onto the DNA, as previously observed for eukaryotic mono-nucleosomes 21 . The lighter area around the mean curve corresponds to the standard variation around the mean curve, from three replicates. Individual tracks are found in Extended Figure 6 . Discussion Since their discovery, ‘giant viruses’ have continued to surprise the scientific community with their remarkable size, complex life cycles and unique genetic features that are characterized by a large number of ORFans (genes with no known homologs or function). Even viral proteins with assigned functions exhibit unexpected and intriguing properties. A prime example is the presence of genes encoding histones, histone variants, and in some instances even putative linker histones in a subclass of the Nucleocytoviricota 13 , 22 . The fusion of histones into doublets in melbournevirus likely facilitates the obligatory pairing of histones H2B with H2A, and histones H4 with H3, perhaps to decrease the reliance on histone chaperones. Recent analyses of many giant virus metagenomes unearthed a wide variety of histone fusions, indicating that this might not be an isolated incident 10 . Here we show that melbournevirus encodes an H2B-H2A variant in addition to the highly abundant main H2B-H2A doublet. Both H2B-H2A doublets, as well as the H4-H3 doublet are essential for viral fitness, as deletion of any of the three genes results in virus that is not infectious (this study and reference 13). This indicates that the variant H2B-H2A histone doublet has functions that cannot be fulfilled by the main histone H2B-H2A doublet or by amoeba host histones, despite its much lower abundance in the virus. Genes for this variant are present across the entire Marseilleviridae family and its distinct features are highly conserved. The nucleosomes that it forms with the H4-H3 doublet are structurally distinct from the canonical melbournevirus NLPs. The histone H2B-H2A variant has an H2B region that can be barely classified as such based on its sequence, yet assembles into a protein core with the full complement of histones, with the characteristic positively charged helical ramp around its outside. Nevertheless, this protein core stably binds only ∼90 bp of DNA, and the terminal 25 base pairs of DNA are not represented by density in our maps. This is also reflected by the reduced resistance of these nucleosomes against thermal melting. The diminished contacts between DNA and protein beyond SHL ±3.5 are due to a shorter H2B αC helix, a redirected and shorter connector between H2B and H2A, and by a missing portion of the H2A docking domain that in other structures stabilizes the H3 αN helix to interact with the penultimate 10 bp of DNA. Lower degrees of wrapping of in vitro assembled variant MV-NLPs were also observed by others through MNase protection assays 16 . We would have expected these features to decrease the overall stability of MV-varNLP (compared to MV-NLP) to a higher degree than what we determined experimentally. We hypothesize that the presence of the conserved disulfide bond stapling together the two MV-varH2B-H2A moieties, not present in MV-H2B-H2A or any other H2A known to date, might counteract these destabilizing features. In eukaryotes, histone H2A variants in particular are known for forming nucleosomes that organize less DNA (see, for example, the human histone H2A variant H2A.B; PDB: 6M4H 18 ), and as such the melbournevirus H2B-H2A variant fits into this category of nucleosome-destabilizing histone variants. Intriguingly, when determining the structure of nucleosomes containing the human histone variant H2A.B, an artificial H2B-H2A.B doublet had to be made, and the resulting nucleosomes had to be further stabilized by GraFix prior to structure determination by cryo-EM 18 . As such, the fusion of histones into doublets, observed as a natural occurrence for all histones in melbournevirus, might aid nucleosome assembly in absence of histone chaperones and assembly factors. This is consistent with the finding that multi-histones organization of metagenomic giant virus histone sequences appears to facilitate self-assembly of nucleosomes in E. coli 10 . In a biological context, nucleosomes are surrounded by other nucleosomes and form closely packed higher order structures. In eukaryotic chromatin, genomic nucleosomes are separated by linker DNA ranging in length between 15 and 65 bp 23 , resulting in a beads-on-a-string appearance of nucleosomal arrays in their most relaxed states. The melbournevirus genome appears to be densely packaged by nucleosomes with an exceedingly short repeat length of 121 bp, without connecting linkers and apparently not even providing the requisite 147 bp for a full nucleosomal superhelix 16 . This could result in stacking of nucleosomes to promote DNA-histone contacts beyond the 90 bp observed in the structure, as the DNA would already be partially constrained and twisted by neighboring nucleosomes. This could compensate for the lack of protein-DNA interactions beyond SHL ±4.5. Indeed, our MD simulations suggest that both canonical and variant melbournevirus nucleosomes can stably stack as di-nucleosomes similar to human telomeric nucleosomes, despite pronounced differences in nucleosomal surface and histone tails 16 . It is, however, important to point out that the conclusions from these simulations must be verified experimentally. In the melbournevirus capsid, MV-varH2B-H2A (mel_149) is ∼10 times less abundant than the main H2B-H2A doublet (mel_369). This means that MV-H2B-H2A is the main constituent of viral chromatin, while MV-varH2B-H2A is either randomly interspersed or clustered in the genome. Unfortunately, experimental maps of the genomic distribution of MV-varH2B-H2A are not yet available. Difficulties in obtaining ChIP-quality antibodies that are specific to viral histones, and the inability of generating viable viruses with tagged histone doublets have hampered these efforts. Members of the family Marseilleviridae possess all genes necessary to transcribe their genes and cap their mRNA, but do not carry the RNA polymerase subunits in their capsids. Instead, during the early infectious cycle they destabilize the host nucleus and transiently recruit the host machinery to the early viral factory until the virally encoded RNA polymerase is translated and localized to the viral factory 24 . We hypothesize that MV-varH2B-H2A forms nucleosomes over genes that need to be expressed early in the viral cycle, and that the rapid dissociation of MV-varNLP upon host infection allows speedy transcription by the host polymerase of early genes. Such a role in orchestrating gene transcription would be in keeping with the function of many eukaryotic histone variants. Proteins organizing DNA in recently studied giant viruses seem to share a common feature of inherent instability. For instance, the Mimivirus genomic fiber is designed to disassemble quickly to unlock the RNA polymerase and initiate rapid gene transcription, facilitating the viral propagation cycle 25 . Medusavirus encodes histones to organize its DNA, and like melbournevirus, its nucleosomes are less stable than eukaryotic nucleosomes 13 . We hypothesize that DNA organizing proteins in giant viruses have adapted to package and protect the genome within the capsid, and to rapidly dissociate once the viral infection cycle has begun. To date, it is unknown whether any of the viral histones harbor post-translational modifications that in eukaryotes are used for gene expression regulation, even though is noteworthy that melbournevirus does encode for a methyltransferase. It is also unknown whether host-encoded ATP-dependent chromatin remodelers are recruited from the compromised host nucleus and are utilized to free up the genome, or whether viral nucleosomes, unlike their eukaryotic counterparts, are self-assembling and self-organizing. It is also unknown whether the H2B-H2A is placed randomly or whether it is targeted to specific regions of the viral genome by dedicated assembly factors. It is entirely possible that novel components of a viral chromatin maintenance machinery are hiding amongst the many viral ORFan genes whose functions are currently unknown. Methods Generation of vectors Melbournvirus mel_149 knockout vector: Gene knockout strategy was performed as previously described for pandoravirus and mimivirus 26 , 27 . The plasmid for gene knock-out was generated by sequential cloning of the 3’ UTR of mel_282, the promoter of mel_367 and a neomycin (NEO) selection cassette. Each cloning step was performed using the Phusion Taq polymerase (ThermoFisher) and InFusion (Takara). Finally, 500-bp homology arms were introduced at the 5’ and 3’ end of the cassette to induce homologous recombination with the viral DNA 28 . Before transfection, plasmids were digested with EcoRV and NotI. All primers are shown in ( Extended Table 3 ). MV-var-H2B-H2A expression vectors: the mel_149-GFP plasmid previously described 12 was modified as follows: 1) the neomycin selection cassette was replaced for a nourseothricin N-acetyl transferase (NAT) using the primers listed in Extended Table 3 . 2) A stop codon was added between the mel_149 and the GFP to allow expression of mini H2B-H2A without a tag using the primers in Extended Table 3 . Cell transfection and generation of trans-complementing lines 1.5×10 5 Acanthamoeba castellanii cells were transfected with 6 μg of MV-var-H2B-H2A ecnoding plasmid using Polyfect (QIAGEN) in phosphate saline buffer (PBS) according to the manufacturer’s instructions. Selection of transformed cells was initially performed at 30 μg/mL Nourseothricin and increased up to 100 μg/mL within a couple of weeks. The procedure is described step by step in 28 . Gene knock-out Gene knockout strategy was performed following our published protocol 28 . Briefly, 1.5×10 5 Acanthamoeba castellanii cells were transfected with 6 µg of linearized plasmid using Polyfect (QIAGEN) in phosphate saline buffer (PBS). One hour after transfection, PBS was replaced with PPYG, and cells were infected with 1.5 × 10 7 melbournvirus particles for 30 minutes with sequential washes to remove extracellular virions. 24 h after infection, the new generation of viruses (P0) was collected and used to infect new cells. An aliquot of P0 viruses was utilized for genotyping to confirm the integration of the selection cassette. Primers used for genotyping are shown in Extended Table 3 . The new infection was allowed to proceed for 30 minutes, then cells were washed to remove extracellular virions and geneticin was added to the media. Viral growth was allowed to proceed for 24 h. This procedure was repeated one more time before removing the geneticin selection to allow viruses to expand more rapidly. Once the viral infection was visible, the selection procedure was repeated one more time. Viruses produced after this new round of selection were used for genotyping and cloning, as previously described 28 . Melbournevirus histones doublet purification Mel_149 and mel_368 were cloned into a pET-28 plasmid to add an N-terminal 6-His tag. Vectors were transformed onto E. coli (DE3) Rosetta cells for expression after induction with 0.4 mM IPTG at 37 °C, for 2.5 h. Pellets from 1 L of E. coli cells were re-suspended and lysed with 40 mL of guanidinium lysis buffer (6 M Guanidinium HCl, 40 mM HEPES pH 6.8 and 500 mM NaCl) and sonicated four cycles for 30 s at 50 % strength (Branson Digital Sonifier). Lysate was spun at 16,000 rpm for 25 minutes using a JA-20 rotor (Beckman) on an Avanti J-20 XPI (Beckman). The supernatant was incubated with Nickel NTA Agarose Beads (GoldBio) for ∼ 30 min at room temperature (RT). Nickel beads were pelleted at 1,500 rpm for 2 minutes, the supernatant was discarded, and beads were resuspended with denaturing binding buffer (8 M Urea, 40 mM HEPES, 200 mM NaCl, pH 6.8). After gentle shaking for 2 hours at RT, beads were washed with denaturing wash buffer (8 M Urea, 40 mM HEPES, 200 mM NaCl, 200 mM Imidazole, pH 6.8). Proteins were batch-eluted using histone elution buffer (8 M Urea, 20 mM HEPES pH 6.8, 200 mM NaCl, and 500 mM imidazole). To refold histones doublets, samples were dialyzed against 1 M urea Buffer (1 M urea, 20 mM HEPES pH 6.8, 200 mM NaCl, pH 6.8) for 6 hours, followed by overnight dialysis against the same buffer without urea (1 mM EDTA, 20 mM HEPES and 200 mM NaCl, pH 6.8). Precipitated protein was removed by centrifugation, and the supernatant was concentrated and run over a size-exclusion column S200 16/60 (Cytiva) equilibrated in 20 mM HEPES and 200 mM NaCl, pH 6.8. Samples were stored in 20% glycerol at −80°C. Nucleosome reconstitution Purified and refolded MV-varH2B-H2A (or MV-H2B-H2A as controls), MV-H4-H3 and a 147 bp DNA fragment (601 Widom) were mixed at a ratio of histone doublet to DNA = 2:2:1. Samples were dialyzed overnight against a gradient buffer (2-0.25 M NaCl, 10 mM MES, 1 mM DTT, pH 6.5) starting at 2 M NaCl and going to 0.25 M NaCl with an exchange flowrate of 1.5 ml/min using an Econo gradient pump (BioRad). The reconstituted products were analyzed by 5% native-PAGE. Sucrose gradient and crosslinking (GraFix) A linear 5-40 % sucrose gradient was prepared by pouring 6 ml of 5 % sucrose buffer (50 mM NaCl, 20 mM HEPES, 0.1 mM EDTA, pH 6.5, 5 % sucrose and 0.16 % glutaraldehyde) into a centrifugal tube (Beckman, 331372). 6 mL 40 % sucrose buffer (50 mM NaCl, 20 mM HEPES, 0.1 mM EDTA, pH 6.5, and 0.16 % glutaraldehyde) was slowly added from the bottom. The tubes were spun on a gradient maker (BioComp Gradient Master) to form a continuous gradient. Then, 200 μl of sample was loaded on top and spun at 4 °C for 18 h at 30,000 rpm (Beckman, Rotor SW-41Ti). The gradient was fractionated using a FC 203B Fraction collector (Gilson). The fractions were assessed by 5 % native-PAGE. The nucleosome-containing fractions were then pooled and dialyzed against 50 mM NaCl, 20 mM MES, 1 mM EDTA, pH 6.5 and 1 mM DTT to remove the sucrose. Cryo-electron microscopy (cryo-EM) single particle data collection and analysis Crosslinked nucleosomes were concentrated to 2-3 μM using Amicon Ultra-4 centrifugal filters (Ultracel 50K, Millipore). 4 µl of the concentrated sample were applied to glow discharged (40 mA, 30 s, EMItec, Lohmar, DE) C-Flat 1.2/1.3 (Cu) grids, and blotted for 4 s using a Vitrobot Mk IV (Thermo Scientific) using the following parameters: 4 °C, 100 % humidity, blotting force 1, wait time 30 seconds, and plunge frozen in liquid ethane cooled to liquid nitrogen temperature. Images were collected at nominal magnification of 130,000x (Pixel size: 0.97 Å) on a FEI Titan Krios (300 kV), equipped with a Falcon 4 Direct Detection Camera. The movies were captured in super resolution mode with a total dose of 50 e/Å 2 (electrons per Angstrom square). Defocus range was −1.0 to −2.5 μm. The dataset was pre-processed (motion correction and CTF estimation) and processed with CryoSPARC (v4) 29 , 30 . Particles were picked using Blob picker. Then 1,010,995 particles across 2,894 micrographs were extracted with a 448-pixel size box (up-sampling factor 2) after Inspect Picks. Particles were 2D classified into 400 classes, where only 12 classes were kept (85,405 particles). Five ab initio models were generated, followed by heterogeneous refinement, non-uniform refinement, as well as local refinement of the best ab initio model (36,051 particles), were performed to improve the density resolution to 4.41 Å, as estimated by GFSC. Model building and refinement Initial protein models were built using AlphaFold 2 which were fitted into the final 3D electron maps in UCSF ChimeraX 31 . These models were then iteratively refined by multiple runs in COOT 32 and PHENIX 33 . For the DNA, DNA from 7N8N was used as a starting model, followed by further iterative refinement in PHENIX. Molecular dynamics Initial models used for molecular dynamics simulations were made by taking the experimentally solved models and then using Alphafold 2 predictions models to fill the missing regions of the experimentally solved structures 34 . The terminal tails were manually adjusted in Chimera X 31 to avoid clashes with the DNA. Then, all-atom molecular dynamics simulations using explicit solvent were carried out using AMBER18 35 using the ff14SB, bsc1 and tip3p forcefields (for protein, DNA and water, respectively). Structures were protonated and hydrogen mass repartitioned (as implemented through ‘parmed’ in AMBER). Structures were placed in cubic boxes surrounding the structures by at least 25 Å, charge neutralized using potassium ions and hydrated with water molecules. The structures were energy minimized in two 5,000-step cycles, the first restraining the protein and DNA molecules to allow the solvent to relax and the second to allow the whole system to relax. Minimized structures were then heated to 300 K and slowly brought to 1.01325 atm. These systems were then simulated for 130 ns in 4 femtosecond steps. Simulations were carried out on NVIDIA GPUs (RTX6000s or A100s) using CU Boulder’s Blanca Condo cluster. Root mean square, deviations (RMSD), distance, angle and dihedral analysis were carried out using cpptraj through AMBER18 35 . Each simulation was carried out in triplicate; individual trajectories are shown in Extended Figure 6 . Structural characterization of the miniH2BH2A/H4-H3 nucleosome model Comparisons between nucleosome structures were conducted using UCSF ChimeraX 31 . The r.m.s.d between different models was calculated using COOT 32 . Thermal Shift Assay For thermal shift assays, we mixed nucleosome preparations at 2.25 µM with 5x SYPRO Orange in 20 µl final reaction mix, in 20 mM MES, 50 mM NaCl at pH 6.5. We used StepOnePlus Real-Time PCR unit (Applied Biosystems) to increase the temperature from 25 °C to 95 °C at a rate of 1 °C/min and measured the fluorescence at 560 nm every 1 °C. Normalized data was plotted by displaying relative fluorescence over temperature using GraphPad Prism version 10.3.1 for Windows (GraphPad Software, Boston, Massachusetts USA). The thermal melting point (Tm) ranges of each sample and replicate measured were determined by identifying the temperature at the lowest point of the fluorescence derivative (−d/dU RFU). Statistical analysis (t-test) was performed on GraphPad Prism version 10.3.1 for Windows. Data Availability The pdb coordinates and EM maps have been deposited (pdb: 9CVT; EMD-45966). Movies of MD simulation, and all raw data can be made available upon request during the review process, and will be made freely available at the final acceptance of the manuscript. Authors Contributions A.V: research conceptualization and design; research; data curation; validation; analysis; writing (original draft, review, and editing); visualization. H.B: research conceptualization and design; research; data curation; validation; analysis; visualization. C.M.T: research conceptualization; data curation; writing (review, and editing). C.A: research conceptualization; funding acquisition; writing (review, and editing). K.L: research conceptualization and design; funding acquisition; project administration; validation; analysis; writing (original draft, review, and editing), visualization. Extended data Tables View this table: View inline View popup Download powerpoint Extended Table 1: Identity percentage of mel_149 compared to other melbournevirus (MV) histones, and to Xenopus laevis and Acanthamoeba castellanii histones. Note the lack of any identity between the H2B portion of MV-varH2B-H2A and other H2B sequences. View this table: View inline View popup Download powerpoint Extended Table 2: MV-varNLP cryo-EM data statistics View this table: View inline View popup Download powerpoint Extended Table 3: Primers for genetic modification of melbournevirus Extended Data: Figures Download figure Open in new tab Extended Figure 1: the H2B-H2A histone variant is conserved among the Marseilleviridae . MAFFT 36 alignment of the putative H2B-H2A variant sequences in the family Marseilleviridae . Predicted secondary structure elements for melbournevirus protein are shown in light red and light yellow for H2B and H2A regions, respectively. Dark blue highlighted amino acids (aa) are conserved; similar hydrophobic aa are shown in light blue (V/I or F/W/Y), positively charged aa (R/K) are highlighted in green. Download figure Open in new tab Extended Figure 2: MV-varH2B-H2A form nucleosome-like particles. (A) 5% Native PAGE of major and variant nucleosome reconstituted with 147 bp Widom 601 DNA. –DNA: protein ratio: 1= 1:0.9:0.9; 2=1:1:1; 3= 1:1.25:1.25:1.25; 4=1:1.5:1.5; 5=1:1.75:1.75; 6=1:2:2 (major H2B-H2A in blue and H2B-H2A-variant in red). Putative subnucleosomal particles are formed with MV-varH2B-H2A and H4-H3 at low histone-to-DNA ratios. (B) Mass Photometry of MV-varNLP (assembled at a 1.6:1 protein:DNA ratio): a homogeneous peak at 157±33 kDa, within error of the calculated molecular weight of MV-varNLP (133.5 kDa) is observed. The minor peak at 33±14.9 kDa is likely from free histones. (C, D) Thermal shift assay of MV-varNLP (red), MV-NLP (blue) and human nucleosome (green). (C) raw normalized data and (D) derivative normalized data. (E) Difference (t-test) between melting temperature of MV-NLPs (6 replicates) and human nucleosomes (5 replicates). (*) correspond to a statistically significant difference (p-value <0.0001). Download figure Open in new tab Extended Figure 3. Cryo-EM analysis of MV-varNLP. (A) Single particle analysis CryoSPARC flow chart of MV-varNLP data processing. (B) Final map colored by its local resolution. (C) FSC curve of MV-varNLP map. Resolution was determined using DSC cutoff of 0.143. (D) Azimuth representation of viewing direction distribution. Download figure Open in new tab Extended Figure 4: Weak density suggests canonical DNA trajectory past SHL ±4.5 in MV-varNLP. Electrostatic surface of (A, C) MV-varNLP and (B, D) MV-NLP (PDB: 7N8N), Coulombic electrostatic potential values are between −10 kcal/(mol· e ) and 10 kcal/(mol· e ) at 298 K. (E) MV-varNLP and (F) MV-NLP in cartoon model fitted inside the MV-varNLP density. Spurious density for DNA following the canonical superhelical path is visible at low contour levels Download figure Open in new tab Extended Figure 5: MV-varH2B-H2A Cys103 form disulfide bridge stapling together the two varH2B-H2A moieties. (A) Cartoon representation of MV-varNLP (H2A: yellow, H2B: red, H3: blue, H4: green) fitted into its density map. The density for the disulfide bond is indicated by an arrow. (B) BisTris 4-12% SDS PAGE. Lane 1: molecular weight marker; 10-200 kDa; 2: MV-varNLP with reducing agent and boiling; 3: MV-varNLP without reducing agent, no boiling; 4: MV-varNLP without reducing agent, with boiling, (5) MV-varH2B-H2A with reducing agent and boiling, (6) MV-H4-H3 with reducing agent and boiling, (7) MV-varH2B-H2A with reducing agent and heat, (8) MV-varH2B-H2A without reducing agent and no heat. Download figure Open in new tab Extended Figure 6: Individual molecular dynamics data (all replicates). (A, C, E, G, I, K, M, O) root mean square deviation (r.m.s.d.) of the overall structure compared to the start of the simulation: (B, D, F, H, J, L, N, P) the distance between the center of gravity of both nucleosomes on the structure. Individual trajectories of the triplicate molecular dynamic simulations for the (A, B) MV-varNLP, (E, F) MV-NLP, (I, J) human telomeric nucleosomes (pdb: 7v98) and (M, N) MV-hybridNLP models and their respective DNA truncated models ( (C, D) MV-varNLP, (G, H) MV-NLP, (K, L) Human telomere and (O, P) MV-hybridNLP). Acknowledgements and funding We thank Garry Morgan and Johannes Rudolph for help with data collection, and Shawn Laursen for help with data analysis. Data collection was done at the Biochemistry Krios Electron Microscopy Facility (BioKEM) at CU Boulder (RRID: SCR_019057). We thank the Shared Instruments Pool (SIP) core facility (RRID: SCR_018986), Department of Biochemistry, University of Colorado Boulder, and Dr. Annette Erbse for the use of the shared research instrumentation infrastructure. The software used in this project was curated by SBGrid. This work utilized the CUmulus on-premise cloud service at the University of Colorado Boulder. Cumulus is jointly funded by the National Science Foundation (award OAC-1925766) and the University of Colorado Boulder. This work utilized the Blanca condo computing resource at the University of Colorado Boulder. Blanca is jointly funded by computing users and the University of Colorado Boulder. Data storage is supported by the University of Colorado Boulder PetaLibrary. This study was funded by the Howard Hughes Medical Institute (A.V., C.M.T., and K.L.), and the European Research Council (ERC) under the European Union’s Horizon 2020 research and innovation program (grant agreement No 832601; H.B and C.A.). We thank the Shared Instruments Pool (SIP) core facility (RRID: SCR_018986), Department of Biochemistry, University of Colorado Boulder, and Dr. Annette Erbse for the use of instrumentation infrastructure. The content is solely the responsibility of the authors and does not necessarily represent the official views of the funding agencies. References 1. ↵ Luger , K. , Mäder , A. 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