# Membraneless organelles restructured and built by pandemic viruses: HIV-1 and SARS-CoV-2

Viviana Scoca, Francesca Di Nunzio

► To cite this version:

Viviana Scoca, Francesca Di Nunzio. Membraneless organelles restructured and built by pandemic viruses: HIV-1 and SARS-CoV-2. Journal of molecular cell biology, 2021, 10.1093/jmcb/mjab020. pasteur-03214326

HAL Id: pasteur-03214326

https://pasteur.hal.science/pasteur-03214326

Submitted on 1 May 2021

HAL is a multi-disciplinary open access
archive for the deposit and dissemination of sci-
entific research documents, whether they are pub-
lished or not. The documents may come from
teaching and research institutions in France or
abroad, or from public or private research centers.

L'archive ouverte pluridisciplinaire HAL, est
destinée au dépôt et à la diffusion de documents
scientifiques de niveau recherche, publiés ou non,
émanant des établissements d'enseignement et de
recherche français ou étrangers, des laboratoires
publics ou privés.

<figure><img src="image_1.png" /></figure>

Distributed under a Creative Commons Attribution 4.0 International License
<figure><img src="image_2.png" /></figure>

<figure><img src="image_3.png" /></figure>
# Review

## Membraneless organelles restructured and built by pandemic viruses: HIV-1 and SARS-CoV-2

Viviana Scoca<fnref n="1" />,<fnref n="2" /> and Francesca Di Nunzio<fnref n="1" />,*

### Abstract

Viruses hijack host functions to invade their target cells and spread to new cells. Specifically, viruses learned to usurp liquid-liquid phase separation (LLPS), a newly exploited mechanism, used by the cell to concentrate enzymes to accelerate and confine a wide variety of cellular processes. LLPS gives rise to actual membraneless organelles (MLOs), which do not only increase reaction rates, but also act as a filter to select molecules to be retained or to be excluded from the liquid droplet. This is exactly what seems to happen with the condensation of SARS-CoV-2 nucleocapsid protein to favor the packaging of intact viral genomes, excluding viral subgenomic or host cellular RNAs. Another older pandemic virus, HIV-1, also takes advantage of LLPS in the host cell during the viral cycle. Recent discoveries highlighted that HIV-1 RNA genome condensates in nuclear MLOs accompanied by specific host and viral proteins, breaking the dogma of retroviruses that limited viral synthesis exclusively to the cytoplasmic compartment. Intriguing fundamental properties of viral/host LLPS remain still unclear. Future studies will contribute to deeply understanding the role of pathogen-induced MLOs in the epidemic invasion of pandemic viruses.

**Keywords:** LLPS, MLO, HIV-1, SARS-CoV-2

<footnote n="1">¹ Advanced Molecular Virology and Retroviral Dynamics group, Department of Virology, Pasteur Institute, Paris, France</footnote>

<footnote n="2">² BioSPC Doctoral School, Université de Paris, Paris, France</footnote>

<footnote>* Correspondence to: Francesca Di Nunzio, E-mail: dinunzio@pasteur.fr</footnote>
**Introduction**

Eukaryotic cells evolved mechanisms to ensure the performance of complex cellular functions in a limited space and in a spatiotemporal manner. Macromolecule condensates in cells, typically termed liquid-like droplets, are generated by liquid-liquid phase separation (LLPS). LLPS is based on multivalent interactions among intrinsically disordered regions (IDRs) and/or modular interacting domains of some components (Bergeron-Sandoval et al., 2016; Banani et al., 2017; Shin and Brangwynne, 2017). IDRs do not have a well-defined structural conformation and usually contain repeated low-complexity sequences that favor transient intermolecular interactions such as aromatic, polar, and charge-charge (Bergeron-Sandoval et al., 2016; Banani et al., 2017; Shin and Brangwynne, 2017). As an example, IDRs characterize many RNA-binding proteins involved in the formation of large ribonucleoprotein (RNP) complexes. These proteins can form membraneless organelles (MLOs) using different RNA forms, including messenger RNA (mRNA), ribosomal RNA (rRNA), long non-coding RNA (lncRNA), small nuclear RNA, and small nucleolar RNA, as molecular scaffold for their condensation (Shin and Brangwynne, 2017; Fay and Anderson, 2018). Thus, MLOs are typically formed via LLPS, generated by an equilibrium between particular molecules concentrated in a liquid-like compartment and the surrounding liquid milieu (Banani et al., 2017; Shin and Brangwynne, 2017). This cellular organization allows a range of distinct cellular functions in a confined space (Boeynaems et al., 2018). MLOs have aroused the interest of many scientists from different disciplines, because they are critical for many biological phenomena. Some studies suggest an old origin of MLOs; indeed, they can be composed of simple heterogeneous polymer systems similarly to synthetic products from early Earth (Yoshizawa et al., 2020).

MLOs include biomolecular condensates, such as processing bodies (PBs), stress granules (SGs), nuclear pore complexes (NPCs), paraspeckles, speckles, promyelocytic leukemia nuclear bodies (PML NBs), the nucleolus, DNA damage foci, transcription factories, and germline granules. It has been observed that the composition of MLOs can be responsible for their distinct biological functions and their dynamic state (Alberti and Hyman, 2016; Kaganovich, 2017). In fact, condensates can play divergent biological roles (Roden and Gladfelter, 2020): (i) triggering the interaction between factors by bringing them closer to each other (Seydoux and Braun, 2006; Lee et al., 2013; Wang and Seydoux, 2014; Lee et al., 2015; Langdon and Gladfelter, 2018), (ii) serving as sink for chemical reactions (Lu et al., 2018), (iii) enhancing enzymatic rates (Hnisz et al., 2017; Cho et al., 2018), and (iv) acting as stress sensors (Riback et al., 2017; Du and Chen, 2018). Phase separation plays also a role in cargo trafficking pathways, such as docking cargos to mediate their transport across membranes and shuttling cargos through the NPC. Importantly, membrane-bound and membraneless organelles orchestrate
actions to guarantee spatiotemporal control of multiple cellular functions. In fact, LLPS plays broad roles with membrane-associated structures, such as post synaptic density (PSD) in neurons and T cell signaling. Phase separation-mediated PSD assembly can determine the physiological functions of synapses (Dustin and Choudhuri, 2016; Dustin and Kam, 2016; Zeng et al., 2016; Courtney et al., 2018). New evidences show that membrane-bound organelles and membraneless condensates closely interact, regulating various functions of both types of organelles that can be usurped by viruses for their replication (Zhao and Zhang, 2020). Study based on advanced electron microscopy revealed that positive-sense RNA viruses, such as picornaviruses, hepatitis C virus, noroviruses, and coronaviruses usurp host membranes to generate viral replication organelles (ROs), inducing encapsulated spherules or double-membrane vesicles (DMVs) for viral RNA (vRNA) synthesis (Knoops et al., 2008; Maier et al., 2013; Zhang et al., 2018; Snijder et al., 2020; Wolff et al., 2020). However, it is still unclear how critical DMVs are for effective viral spread, which is a vital notion for the design of broad-acting antivirals. Phase separation plays a key role in genome organization and gene expression; in fact, the nucleus optimizes its intricate function through its own compartmentalization. For instance, the genomic 3D organization is pivotal not only for the packaging of several Mb of DNA in the small nuclear volume, but also for short- and long-range interactions between regulatory sequences and genes. Nuclear architecture is dynamically coordinated by DNA-interacting proteins, which cleverly cluster the chromatin for the best purpose. The assembly of a large amount of specific nuclear factors, which transiently or permanently interact with DNA and/or RNA, generate well-defined nuclear domains (nuclear bodies). Even though biomolecular condensates miss an actual barrier from the surrounding environment, they represent actual independent ‘factories’. Overall, it is extremely advantageous for the cell exploiting these structures to quickly respond to different environmental inputs and/or to cellular perturbations, such as viral invasion. Indeed, viruses evolved multiple mechanisms to adapt and co-exist with the host to be able to release their new progeny. For example, DNA and RNA viruses learned to build or restructure MLOs to replicate.

This review focuses on the interplay between MLOs and two pandemic viruses: HIV-1 and SARS-CoV-2. HIV-1 virions carry two copies of RNA genome that should be retrotranscribed to allow viral integration into the host chromosomal DNA. Thus, HIV-1 replicates in the nucleus of the host cell. Contrary to HIV-1, SARS-CoV-2, which has a genome formed by single stranded positive-sense RNA, replicates in the host cytoplasm (Zhou et al., 2020). This is also the case of SARS-CoV and SARS-related bat coronaviruses. Despite the differences in the cell cycle of those two categories of viruses, HIV-1 and SARS-CoV-2, recent studies highlight that both benefit from MLOs to replicate (Cubuk et al., 2020; Iserman et al., 2020; Perdikari et al., 2020; Rensen et al., 2020; Savastano et al.,
2020; Scoca et al., 2020). This review aims to discuss the most important strategies evolved by these two pandemic viruses to interact with MLO components for an efficient sabotage of the cellular compartments to their own benefit.

# HIV-1 and SARS-CoV-2 interplay with the host MLOs.

## SGs

Phase separation dictates the principles of cell organization, governing cell function and survival (Uversky, 2017), for instance, generating SGs in response to environmental and stress factors (Franzmann and Alberti, 2019). Of note, SGs can be induced by cellular stress, specifically triggered by translational silencing, causing accumulation of cellular mRNA. In most of the cases, the block of translation is due to the phosphorylation of the translation eukaryotic initiation factor 2α (eIF2α) (Protter and Parker, 2016). Different eIF2α kinases can sense environmental stress, like protein kinase RNA-dependent (PKR) in response to viral double-stranded RNA (dsRNA) sensing (Bou-Nader et al., 2019) and PERK/PEK (PKR-like ER kinase) in response to hypoxia and misfolded proteins in the endoplasmic reticulum (Harding et al., 2000).

Numerous viruses, however, inhibit SG assembly to evade the antiviral response (Poblete-Duran et al., 2016). An example is HIV-1 that evolved multiple mechanisms to block the assembly of SGs through the interplay between the viral structural precursor polyprotein (pr55Gag) and several host factors such as eEF2, G3BP1, CypA, and eIF4E (Cinti et al., 2016). Interestingly, it has been proposed that during HIV-1 replication, an equilibrium exists between SG assembly and disassembly (Rao et al., 2018). More recently, it has been identified that a prion-like IDR conserved among retrovirus Gag proteins regulates their zinc-dependent LLPS. This LLPS drives nucleocapsid-stress granule (NC-SG) formation and, in the presence of vRNA, viral RNP assembly. The chelation of the Zn²⁺ blocks the development of these MLOs and induces a relocalization of nucleocapsid and viral genomic RNA (NC-vRNA). The infection outcome seems to be based on the NC-vRNA/NC-SGs balance, which is due to the ordered Zn²⁺ LLPS of NC proteins that contributes to viral assembly, while the NC-SGs avoid an excessive accumulation, as NC proteins have a tendency to multimerize (Table 1; Monette et al., 2020).

Apart from HIV-1, several studies have been performed on the interplay of SARS-CoV with SGs. The infection, as for many other viruses, activates PKR and PERK kinases inducing SG assembly, but viral replication is not affected by eIF2α hyperphosphorylation, meaning that the viral expression is optimized in other ways, overcoming the induced cellular stress (Krahling et al., 2009). It has been
observed that the host cell translation is hampered by mechanisms involving nonstructural protein 1(nsp1) in SARS-CoV-infected cells (Kamitani et al., 2006; Narayanan et al., 2008; Kamitani et al., 2009; Lokugamage et al., 2012), which leads to stress-induced RNA accumulation (Anderson and Kedersha, 2008). *In vitro*, it has been observed that the nucleocapsid protein of SARS-CoV (SARS-CoV N protein) is recruited to SGs via its SR-domain that can be phosphorylated at multiple sites by SRPK1 (Peng et al., 2008), the mammalian homolog of a yeast SR-kinase that regulates SGs (Shattuck et al., 2019). Of note, the protein N can interact with the granule-associated protein hnRNPA1 (Luo et al., 2005) and other SG and phase-separating proteins (Molliex et al., 2015).

With COVID-19 outbreak, new research lines opened in the field of SARS-CoV-2 cellular stress. Similarly to the HIV-1 NC protein, the SARS-CoV-2 N protein undergoes phase separation with RNA *in vitro* (Perdikari et al., 2020). It has been hypothesized that this process facilitates SARS-CoV-2 replication by recruiting the excess of cytoplasmic proteins induced by the viral stress, like heterogeneous nuclear RNPs (hnRNPs), as hubs to assemble dense N protein-viral genomic RNA (N-vRNA) phases to promote viral replication (Table 1; Perdikari et al., 2020). Importantly, proteomic studies performed on a putative SARS-CoV-2 protein interaction map identified some RNA processing factors and SG regulation factors, such as G3BP1/2, to be the epicenter of the N interactome (Gordon et al., 2020). In fact, G3BP1 and G3BP2, which drive the formation of SGs (Guillen-Boixet et al., 2020; Sanders et al., 2020; Yang et al., 2020), co-precipitate with the N protein (Gordon et al., 2020).

Taking into account studies on SARS-CoV, several models can be foreseen to explain the N protein role in SARS-CoV and SARS-CoV-2 life cycle: (i) N protein is passively recruited by SGs exercising no effect on them or it can actively play a role in turning down the host translation in favor of viral replication (Peng et al., 2008; Krahling et al., 2009); (ii) non-canonical SGs can be restructured and built during infection for viral replication or viral mRNA translation (Piotrowska et al., 2010; Scholte et al., 2015; Hou et al., 2017; Hosmillo et al., 2019; Brocard et al., 2020; Burke et al., 2020); and (iii) N protein may inhibit the formation of SGs via the sequestration of critical SG components, such as G3BP1, G3BP2, and hnRNPA1 (Cascarina and Ross, 2020). The relevance of the role of N protein for SARS-CoV-2 viral life cycle shed light on potential treatments that can be foreseen to target the interaction between N protein and host cell kinases or virus-induced MLOs to combat SARS-CoV-2 infection.

## NPC

The NPC regulates the exchange of components between the cytoplasm and the nucleus and represents the first barrier that viruses encounter to pass through the nuclear membrane. It is composed by ~30
nucleoporins (Nups) (D'Angelo and Hetzer, 2008), which cover several functions, from the static scaffolding to the dynamic shuttling of cargos (Rabut et al., 2004) through the inner channel of ~ 39 nm (Pante and Kann, 2002). One third of Nups contain phenylalanine–glycine (FG) repeats (Raices and D'Angelo, 2012), which represent low-complexity IDRs. Most IDRs have a relatively low hydrophobicity and high net charge (Uversky et al., 2000), preventing the collapse into water insoluble aggregates, allowing the maintenance of their unfolded state in solution under physiological conditions (Monsellier and Chiti, 2007). A recent manuscript (Celetti et al., 2020) demonstrated that FG-Nups can undergo LLPS and form liquid droplets that mimic permeability barrier properties of intact NPCs. Thus, the authors evaluated whether the liquid Nup droplets have NPC-like permeability barrier properties, similarly to their solid counterparts. Liquid FG-Nup drops were rapidly penetrated by cargo–nuclear transport receptor (NTR) complexes, but only in the presence of the correct nuclear localization signal (NLS) and cognate NTR. Interestingly, this behavior was also observed for much larger cargo model, the recombinant capsid from MS2 bacteriophage; when surrounded by NLSs and importin α/β, this gigantic cargo was able to accumulate in FG-Nup drops (Celetti et al., 2020).

Nups are responsible for the static scaffolding of the NPC, as well as its dynamic transporter aspect. The dynamic and flexible nature of the NPC regulates the nuclear passage of viral complexes, such as for HIV-1 (Di Nunzio, 2013). The viral capsid is the determinant for HIV-1 nuclear import. Indeed, it has been demonstrated that the viral capsid directly docks at the NPC by engaging Nup358/RanBP2, located in the cytoplasmic side of the complex, by interacting with its Cyp-like domain (Di Nunzio et al., 2012). HIV-1 capsid also interacts with Nup153 (Table 1; Di Nunzio et al., 2013; Lelek et al., 2015), which is the most dynamic Nup, located in the nuclear side of the nuclear basket (D'Angelo and Hetzer, 2008). Interestingly, all Nups carrying FG domains can bind to HIV-1 capsid, probably helping the efficiency of viral nuclear entry and, likely, post-nuclear entry steps (Buffone et al., 2018). Thus, HIV-1 capsid penetrates the liquid Nup droplets, likely formed by Nup153 (Celetti et al., 2020).

If on one side, HIV-1 exploits the NPC for its pre-integration complex import in the nucleus, on the other, SARS-CoV-2 influences the functionality of the nuclear pore in a direct or indirect way. Nsp1 of SARS-CoV-2 is able to disrupt Nup93 localization around the nuclear envelope without triggering its proteolytic degradation or perturbation of the nuclear lamina. However, being the nuclear–cytoplasmic exchange altered probably due to Nup93 impairment, a redistribution of the RNA binding protein nucleolin was observed (Gomez et al., 2019). Another recent study reported that ORF6 of SARS-CoV and SARS-CoV-2 inhibits STAT1 nuclear translocation to impede IFN signaling. Importantly, ORF6 localizes at the NPC where it directly interacts to the Nup98–Rae1 complex to
target the nuclear import pathway to overcome the antiviral action of IFN (Table 1; Miorin et al., 2020). Additional research might address more details on how SARS-CoV-2 can alter host nuclear import/export, through interaction with the NPC.

## Nucleolus

The nucleolus exemplifies the nucleolar MLO per excellence, which is further structured in three function-specific compartments, fibrillar centers (FCs), dense fibrillar component (DFC), and granular component (GC), all involved in different steps of rRNA biogenesis (Scheer and Hock, 1999). The nucleolar factors are condensed around the tandemly repeated ribosomal DNA (rDNA) and at the boundary between the FCs. In the DFC, there is a high concentration of Pol I for rDNA transcription; on the other hand, fibrillarin and small nucleolar RNPs (snoRNPs) are also enriched in the DFC, ready to process pre-rRNAs, which eventually are assembled in the GC (Boisvert et al., 2007). Nucleolar RNPs constitute a complex network of functions that several viruses exploit to replicate, especially RNA viruses whose cycle mainly occurs in the cytoplasm, but, unexpectedly, many viral components import in the nucleus and interact with nucleolar factors (Hiscox, 2007).

Mostly, the N protein and core proteins appear to exploit their ability to bind to the RNA molecule to interact with the nucleolar RNA and specifically localize there. This is the case for the majority of coronaviruses (Wurm et al., 2001), whose N protein probably share a so-called nucleolar retention signal (NoRS) sequence (Reed et al., 2006). Studies with deletion mutants and complementation assays coupled to imaging techniques suggest that the N protein may act as cytoplasm/nucleolus shuttle protein (Timani et al., 2005). The relocation of the N protein to the nucleolus seems cell cycle-dependent, with a greater accumulation in G2/M phase (Cawood et al., 2007). Not only N protein but aslo nsp3b (ORF3b) protein of SARS-CoV was found to colocalize with C23 (nucleolin) and B23 (nucleophosmin) (Yuan et al., 2005). So far, for the newly discovered SARS-CoV-2, it is still under investigation where N proteins may localize to the nucleolus. Of note, Wu et al. (2020), through a machine-learning approach, predicted the 5' and 3' SARS-CoV-2 genomic untranslated regions to be enriched in the host mitochondrial matrix and nucleolus (Table 1). Therefore, the localization of SARS-CoV-2 genetic material to the nucleolar body might be essential for viral life cycle, but more extensive research is demanded to clarify the interplay between SARS-CoV-2 N protein and the nucleolus.

HIV-1 has, as well, evolved mechanisms that involve the nucleolus; indeed, both Tat and Rev proteins have been characterized with a nucleolar localization signal (NoLS) since the end of last century (Cochrane et al., 1990; Siomi et al., 1990). Tat constitutive expression in T cells resulted in a
specific nucleolar proteomic profile with 49 proteins displaying a significant fold change compared to control. The ribosomal proteins and ribosomal biogenesis enzymes were in the top 20 most enriched ones, suggesting an HIV-induced upregulation and usurpation of ribosomal cellular machinery (Jarboui et al., 2012). On the other hand, since Rev protein is involved in intron-containing vRNA export, it was speculated that the nucleolus might be the platform for the assembly of RNP particles containing HIV-1 RNA genome and viral/cellular factors, which were then exported to the cytoplasm (Table 1; Michienzi et al., 2000). Indeed, upon Rev expression, the relocation of the nucleoporins Nup98 and Nup214 was observed, along with the export-aiding protein CRM1 in the nucleolus of HeLa cells (Zolotukhin and Felber, 1999). In particular, it was shown in live that Rev multimerizes in the nucleolus (Daelemans et al., 2004). Because of the relevance of Tat and Rev in a relatively early stage of viral replication, it has been proposed to target their activity for therapeutic purposes. Lastly, in the recent years, HIV-1 NC was also found to have a nuclear and nucleolar localization (Yu et al., 2016), but while several studies are carried on to determine its functions in the nucleus, little is known about the functional characterization of nucleolar nucleocapsid localization. Even if at first sight the nucleolus might be only a ‘ribosomal machine’, it seems that viruses have interest to interact with nucleolar proteins and accumulate viral components there.

Overall, the data accumulated so far highlight not only the importance of the impairment and reprogramming of cellular protein synthesis for viral life cycle, but also the exploitation of this nuclear MLO for genomic and subgenomic storage and/or as RNP assembly platform for nuclear export, facilitating vRNA trafficking.

## PML NBs

PML NBs were identified by electron microscopy in several cell types (de et al., 1960) and may vary from 0.1 to 1.0 µm in diameter size. These nuclear super-structures are formed by the phase separation of multiple cellular proteins, which accumulate to be SUMOylated (Bernardi and Pandolfi, 2007). The key proteins of these structures are Sp100, hDaxx, and PML. Because of the importance of SUMOylation in the regulation of a variety of cellular functions, PML NBs are involved in stress-related as well as homeostatic processes: stress response, oncogenesis, gene regulation, cell senescence, DNA damage repair, apoptosis, and antiviral response. In the context of viral infection, it has been demonstrated that PML and Sp100 expression is directly induced by IFN treatment (Everett and Chelbi-Alix, 2007). Recent studies show how PML NBs may have a role in HIV-1 persistence, since silenced HIV-1 proviruses are found in close proximity to PML in T lymphocytes (Table 1; Lusic et al., 2013). The HIV-1/PML proximity is lost upon chemical cell-activation or upon inhibition of
Class I HDACs. Indeed, HIV-1 activation is induced by PML knockdown and seems very specific and related to the loss of PML-associated repressive chromatin modifications, such as H3K9me2. With a view to novel therapeutic targets, the importance of oxidative stress and iron metabolism in HIV-1 infection has been highlighted and PML NBs seem to be the central players (Shytaj et al., 2020). Particularly, upon infection, PML proteins are hyper-SUMOylated and degraded with concomitant active viral expression; on the contrary, upon antioxidant treatment or iron chelation, HIV-1 reestablishes a latent phenotype and PML levels are restored (Shytaj et al., 2020).

## Nuclear speckles

Nuclear speckles (NSs) are highly versatile condensates of about 0.3 to 3 µm. Their characterization started with two major discoveries by Ramón and Cajal ('El nucleo de las celulas piramidales del cerebro humano y de algunos mamiferos', 1910) and independently, later on, by Swift (1959), who identified through electron microscopy structures that he named 'interchromatin granule nuclear clusters' (IGCs). The nowadays term was given by Beck (1961). Anatomy and function of NSs started to become clearer when these structures were re-identified through immune-labelling of some components of the pre-mRNA splicing machinery, like snoRNPs, spliceosome subunits, and other splicing factors, as well as through the highlighting of clusters of polyA+ RNAs (Spector et al., 1991; Carter et al., 1993). The functions of NSs are still under investigation, but they oscillate between two major processes: the storage and post-translational modification of splicing machinery components, which is supported by the presence of several phosphatases and kinases in NSs, and the ability of being molecular hubs of transcriptional expression linking different loci to the same RNA-processing factory (Sutherland and Bickmore, 2009). Key components of NSs are the protein SC35, the scaffolding protein SON (Sharma et al., 2010), and the lncRNA MALAT-1 (Fei et al., 2017); the latter is highly enriched in NSs and has a role in the recruitment of splicing factors to nascent transcripts. The splicing is an essential step for HIV-1 replication. Indeed, some studies identify a link between speckles factors and HIV-1 infection. Two to three-fold increase in the expression of SC35 RNA was detected upon infection (Maldarelli et al., 1998), indicating that HIV infection alters speckle factors and probably their composition. In fact, in human macrophages, SC35 protein levels were upregulated in the first weeks of infection probably favoring the splicing of vRNA, while hnRNPs, which are inhibitory factors, were downregulated. In addition, a correlation with Tat expression was observed when SC35 levels were higher (Dowling et al., 2008), supporting the role of splicing factor levels in HIV-1 replication–persistence balance.
Pandemic viruses trigger the formation of condensates as the scaffold for their replication

Condensation and coalescence of host/viral components can create a favorable environment for viral
replication. This microenvironment is formed by MLOs created from LLPS enhanced by viral
infection. Recently, it has been surprisingly found that HIV-1 infection remodels the nuclear
intra-compartments. In particular, HIV-1 relocates and condensates a paraspeckle factor, CPSF6, in a
different MLO enriched in speckle factors, such as SC35 (Francis et al., 2020; Rensen et al., 2020;
Scoca et al., 2020). This viral action most probably turns the host speckles in new hubs for viral
replication. Despite the fact that the HIV was discovered in 1983 (Barre-Sinoussi et al., 1983), only
recently, new insights into reverse transcription were tracked down. The reverse transcriptase (RT)
enzyme was at the basis of HIV discovery, thanks to the detection of RT activity in the supernatant of
cellular culture, which permitted to understand the nature of the isolated retrovirus, directly from a
lymph node biopsy of a HIV-infected patient. HIV-1 relies on the retro-transfer of RNA genetic
information to DNA to be able to integrate into the host genome to ensure viral persistence. Notably,
the ‘central dogma’ based on the concept that the genetic information could be carried only by the
DNA was revised. Historically, the discovery of RT (Baltimore, 1970; Temin and Mizutani, 1970) has
been considered a milestone of molecular biology and biotechnology, enabling scientists to set up new
tools that heavily influenced cloning, analysis of gene expression, the study of RNA biology, and the
development of state-of-the-art technologies and the modern medicine. Of note, the RT discovery has
been recompensed with the Nobel Prize to three scientists: Renato Dulbecco, Howard Temin, and
David Baltimore. HIV RT has been the most exploited antiviral drug target ever and, to date, 12
anti-RT drugs have been developed: nucleoside RT inhibitors (NRTIs) and nonnucleoside RT
inhibitors (NNRTIs). So far, the RT activity has been considered a process that begins and ends in the
cytoplasmic compartment of the host cell. However, a recent study directly highlights the presence of a
nuclear RT activity in the nucleus of infected macrophages, revisiting the HIV RT dogma considering
that retrotranscription can occur exclusively in the cytoplasm of the host infected cell (Rensen et al.,
2020). Of note, in the HIV-1-induced CPSF6-SC35 MLOs, newly synthesized viral DNA (vDNA) was
found (Rensen et al., 2020; Scoca et al., 2020). These results point out that, at least in macrophages, the
nuclear reverse transcription can occur, likely ending inside the nucleus, contrary to the current belief.
Other recent studies (Burdick et al., 2020; Dharan et al., 2020; Selyutina et al., 2020) supported similar
conclusions on the spatiotemporal action of RT. This surprising discovery of the new cellular
compartment where retrotranscription can occur has been elucidated only after 37 years from HIV
discovery (Barre-Sinoussi et al., 1983) and after 50 years from the stunning finding of the
RNA-dependent DNA polymerase RT (Baltimore, 1970; Temin and Mizutani, 1970). Interestingly, the
HIV genomic RNA has been observed in the host nuclei from several groups, suggesting that RT
completion is dispensable for nuclear entry (Burdick et al., 2013; Burdick et al., 2017; Bejarano et al.,
2019; Burdick et al., 2020; Dharan et al., 2020; Selyutina et al., 2020). However, the physiological role
of the presence of RNA inside the nucleus of infected cells was obscure. The discovery of the
formation of RNA genome clusters englobed in nuclear MLOs gave the opportunity to visualize for the
first time the presence of a nuclear RT activity using cutting-edge imaging technologies (Table 1;
Rensen et al., 2020). HIV genomes cluster together with host factors, such as CPSF6 and SC35, usually
located in distinct nuclear locations, paraspeckles and speckles, respectively. This finding supports the
hypothesis that HIV generates novel MLOs for its own aim or induced by the host to control the fuel of
infection (Figure 1). Several speculations can be proposed to explain the presence of these viral/host
nuclear structures: (i) to serve as nuclear microreactors that condensate RT enzymes and host factors to
promote vDNA synthesis in macrophages; (ii) to serve as microenvironments that include viral and
host factors required for the generation of new viral progeny and/or to hide the virus from cellular
defense mechanisms (Schmid et al., 2014; Lahaye et al., 2018); (iii) related to the finding that large
amounts of unintegrated vDNA cluster in the nucleus, probably forming viral reservoirs, which
constitute the bottleneck for a cure against HIV; and (iv) HIV-induced MLOs located in the nucleus
could serve as source of storage of viral genomes ready to be packed to spread as new progeny. HIV
genome clusters co-localize with condensates formed by SC35, a known speckle factor (Francis et al.,
2020; Rensen et al., 2020). Whether or not speckles have a role in HIV integration and transcription
still should be clarified, because current technologies used to visualize HIV DNA, such as click
chemistry based on EdU incorporation during the ongoing RT, interfere with viral transcription and are
not sufficiently sensitive to visualize an individual viral genome (Rensen et al., 2020). However, this
technology can successfully label nascent HIV DNA in non-dividing cells. In fact, episomal forms of
HIV DNA containing EdU have been visualized in MLOs enriched with CPSF6 and SC35 (Rensen et
al., 2020). On the other hand, more powerful imaging technologies are needed to identify the location
of viral proviruses, in particular by using live imaging. HIV-1 ANCHOR technology offers good
potentiality to investigate this important step of viral life cycle, because it allows the visualization of
single pre-integration complex (Blanco-Rodriguez et al., 2020; Scoca et al., 2020) using live imaging.
Recent results show that HIV-1 infection induced remodeling of pre-existing MLOs generating HIV-1
MLOs, thus it is possible that the remodeling of the nucleus by HIV-1 (Table 1; Scoca et al., 2020)
regulates viral transcription. Future studies will aim to define whether speckles or HIV-induced nuclear
MLOs are involved in fueling viremia or in the persistence process promoted by HIV to ensure its own
survival in the host. Additionally, LLPS contributes to the formation of heterochromatin and
nucleosomes, which have the intrinsic property to phase separate from the rest of the nuclear environment. The phase-separating properties of several chromatin-binding proteins seem to be essential for the regulation of chromatin dynamics and transcription (Hnisz et al., 2017; Larson et al., 2017; Strom et al., 2017; Boehning et al., 2018; Boija et al., 2018; Cho et al., 2018; Sabari et al., 2018; Nair et al., 2019; Plys et al., 2019; Zhang et al., 2019). For example, the transcriptional repressor HP1 mediates the formation of heterochromatin by its ability of phase separating (Larson et al., 2017; Strom et al., 2017) as well as CBX2 subunit of Polycomb-repressive complex 1 can phase separate *in vitro* (Plys et al., 2019). In contrast, other chromatin factor, such as the transcriptional coactivator BRD4, a well-known marker of euchromatin, is able to induce the formation of liquid-like condensates at super-enhancer regions (Sabari et al., 2018). Importantly, it has been reported that HIV-1 recurrently targeted host genes (RIGs) are proximal to super-enhancers genomic elements with BRD4 signature. Those RIGs cluster in particular spatial locations during the activation of T cells (Lucic et al., 2019). Whether euchromatin- or heterochromatin-related nuclear factors can establish condensates that may play a role in HIV-1 gene expression is a fascinating new perspective. The interplay between MLOs and HIV-1 genome puts forward new frontiers for future research. New results in this field could unveil mechanisms related to HIV-1 MLO function and the remodeling to regulate viral latency and viral rebound.

Similar to HIV-1, SARS-CoV-2 seems to use LLPS to spread, but in a different cellular compartment. It has been reported that N protein forms condensates in the presence of SARS-CoV-2 genome. In particular, there are several evidences suggesting that the serine-arginine (SR)-rich sequence of N protein serves as a key regulatory hub. Likely, N protein is linked to the function of the replication transcription complex (RTC). It has been observed that at early time post infection, SR regions of N protein are phosphorylated at multiple sites by cytoplasmic kinases (Cong et al., 2020). The phosphorylated N protein associates with the RNA helicase DDX1, which induces RNA structural changes required for transcription of subgenomic RNAs (Wu et al., 2014; Carlson et al., 2020). Interestingly, a liquid-like matrix composed of phosphorylated N protein, linked to RTC membranes by Nsp3, creates a compartment to concentrate and protect the viral replication and transcription machinery. Similar mechanisms have been highlighted for negative-sense RNA viruses, where replication depends on dynamic biomolecular condensates (Table 1; Cubuk et al., 2020; Iserman et al., 2020; Perdikari et al., 2020; Savastano et al., 2020). Of note, it has been elegantly shown by the group of Gladfelter that genomic RNA carrying 5' and 3' ends promotes condensates in the presence of nucleocapsid. Contrariwise, host RNA and viral subgenomic RNA are excluded from LLPS (Iserman et al., 2020; Figure 1). This is an appealing model for viral replication based on liquid-like droplets as
hubs of viral progeny. Future studies will clarify whether this exciting model can be validated in the context of a real infection with SARS-CoV-2.

## Conclusions

A role of LLPS in pandemic viruses, such as HIV-1 and SARS-CoV-2, has been highlighted by several studies. In particular, the establishments of new condensates during viral infection formed by viral factors with or without the host factor contribution seem to be key for viral replication. Interestingly, viruses evolved independent strategies to replicate by forming condensates in the host cells. The N protein of SARS-CoV-2 condensates in the cytoplasm with the viral genome to favor viral assembly in the cytoplasmic compartment (Figure 1). The evolving research on SARS-CoV-2 replication cycle will address important mechanisms of establishment of viral MLOs. In contrast to SARS-CoV-2, HIV-1 replicates in the nuclear compartment inducing new MLOs (Figure 1), containing HIV-1 RNA genome, capsid, and integrase from the incoming viral particles together with host nuclear factors. Several important functions have been attributed to these viral/host nuclear organelles, such as HIV-1 RNA genome sequestration, RT activity, and interaction with host factors, such as splicing components (Figure 1). These HIV-induced MLOs locate in SC35-speckle regions to reprogram pre-existing organelles to obey to the viral needs. Thus, viral MLOs could represent a new frontier of therapeutic targets to block viral replication either at early or late stages of viral life cycle.

## Funding

Work in the authors' laboratories was supported by the Agence Nationale de Recherche sur le SIDA (ANRS) grant ECTZ88162 with a nominative PhD student fellowship ECTZ88177 for V.S. and by the Pasteur Institute.

**Conflict of interest:** none declared.

## References

Alberti, S., and Hyman, A.A. (2016). Are aberrant phase transitions a driver of cellular aging? Bioessays **38**, 959-968.

Anderson, P., and Kedersha, N. (2008). Stress granules: the Tao of RNA triage. Trends Biochem Sci **33**, 141-150.

Baltimore, D. (1970). RNA-dependent DNA polymerase in virions of RNA tumour viruses. Nature **226**, 1209-1211.
Banani, S.F., Lee, H.O., Hyman, A.A., et al. (2017). Biomolecular condensates: organizers of cellular biochemistry. Nat. Rev. Mol. Cell Biol. 18, 285-298.

Barre-Sinoussi, F., Chermann, J.C., Rey, F., et al. (1983). Isolation of a T-lymphotropic retrovirus from a patient at risk for acquired immune deficiency syndrome (AIDS). Science 220, 868-871.

Beck, J.S. (1961). Variations in the morphological patterns of 'autoimmune' nuclear fluorescence. Lancet 1, 1203-1205.

Bejarano, D.A., Peng, K., Laketa, V., et al. (2019). HIV-1 nuclear import in macrophages is regulated by CPSF6-capsid interactions at the nuclear pore complex. Elife 8.

Bergeron-Sandoval, L.P., Safaee, N., and Michnick, S.W. (2016). Mechanisms and Consequences of Macromolecular Phase Separation. Cell 165, 1067-1079.

Bernardi, R., and Pandolfi, P.P. (2007). Structure, dynamics and functions of promyelocytic leukaemia nuclear bodies. Nat. Rev. Mol. Cell Biol. 8, 1006-1016.

Blanco-Rodriguez, G., Gazi, A., Monel, B., et al. (2020). Remodeling of the core leads HIV-1 pre-integration complex in the nucleus of human lymphocytes. J. Virol. 94, e00135-20.

Boehning, M., Dugast-Darzacq, C., Rankovic, M., et al. (2018). RNA polymerase II clustering through carboxy-terminal domain phase separation. Nat. Struct. Mol. Biol. 25, 833-840.

Boeynaems, S., Alberti, S., Fawzi, N.L., et al. (2018). Protein Phase Separation: A New Phase in Cell Biology. Trends Cell Biol. 28, 420-435.

Boija, A., Klein, I.A., Sabari, B.R., et al. (2018). Transcription Factors Activate Genes through the Phase-Separation Capacity of Their Activation Domains. Cell 175, 1842-1855 e1816.

Boisvert, F.M., van Koningsbruggen, S., Navascues, J., et al. (2007). The multifunctional nucleolus. Nat. Rev. Mol. Cell Biol. 8, 574-585.

Bou-Nader, C., Barraud, P., Pecqueur, L., et al. (2019). Molecular basis for transfer RNA recognition by the double-stranded RNA-binding domain of human dihydrouridine synthase 2. Nucleic Acids Res. 47, 3117-3126.

Brocard, M., Iadevaia, V., Klein, P., et al. (2020). Norovirus infection results in eIF2α independent host translation shut-off and remodels the G3BP1 interactome evading stress granule formation. PLoS Pathog. 16, e1008250.

Buffone, C., Martinez-Lopez, A., Fricke, T., et al. (2018). Nup153 Unlocks the Nuclear Pore Complex for HIV-1 Nuclear Translocation in Nondividing Cells. J. Virol. 92, e00648-18.

Burdick, R.C., Delviks-Frankenberry, K.A., Chen, J., et al. (2017). Dynamics and regulation of nuclear import and nuclear movements of HIV-1 complexes. PLoS Pathog. 13, e1006570.

Burdick, R.C., Hu, W.S., and Pathak, V.K. (2013). Nuclear import of APOBEC3F-labeled HIV-1 preintegration complexes. Proc. Natl Acad. Sci. USA 110, E4780-4789.

Burdick, R.C., Li, C., Munshi, M., et al. (2020). HIV-1 uncoats in the nucleus near sites of integration. Proc. Natl Acad. Sci. USA 117, 5486-5493.

Burke, J.M., Lester, E.T., Tauber, D., et al. (2020). RNase L promotes the formation of unique ribonucleoprotein granules distinct from stress granules. J. Biol. Chem. 295, 1426-1438.

Carlson, C.R., Asfaha, J.B., Ghent, C.M., et al. (2020). Phosphoregulation of Phase Separation by the SARS-CoV-2 N Protein Suggests a Biophysical Basis for its Dual Functions. 80, 1092-1103.e4.

Carter, K.C., Bowman, D., Carrington, W., et al. (1993). A three-dimensional view of precursor messenger RNA metabolism within the mammalian nucleus. Science 259, 1330-1335.

Cascarina, S.M., and Ross, E.D. (2020). A proposed role for the SARS-CoV-2 nucleocapsid protein in the formation and regulation of biomolecular condensates. FASEB J. 34, 9832-9842.
Cawood, R., Harrison, S.M., Dove, B.K., et al. (2007). Cell cycle dependent nucleolar localization of the coronavirus nucleocapsid protein. Cell Cycle 6, 863-867.

Celetti, G., Paci, G., Caria, J., et al. (2020). The liquid state of FG-nucleoporins mimics permeability barrier properties of nuclear pore complexes. J. Cell Biol. 219.

Cho, W.K., Spille, J.H., Hecht, M., et al. (2018). Mediator and RNA polymerase II clusters associate in transcription-dependent condensates. Science 361, 412-415.

Cinti, A., Le Sage, V., Ghanem, M., et al. (2016). HIV-1 Gag Blocks Selenite-Induced Stress Granule Assembly by Altering the mRNA Cap-Binding Complex. mBio 7, e00329.

Cochrane, A.W., Perkins, A., and Rosen, C.A. (1990). Identification of sequences important in the nucleolar localization of human immunodeficiency virus Rev: relevance of nucleolar localization to function. J. Virol. 64, 881-885.

Cong, Y., Ulasli, M., Schepers, H., et al. (2020). Nucleocapsid Protein Recruitment to Replication-Transcription Complexes Plays a Crucial Role in Coronaviral Life Cycle. J. Virol. 94.

Courtney, A.H., Lo, W.L., and Weiss, A. (2018). TCR Signaling: Mechanisms of Initiation and Propagation. Trends Biochem. Sci. 43, 108-123.

Cubuk, J., Alston, J.J., Incicco, J.J., et al. (2020). The SARS-CoV-2 nucleocapsid protein is dynamic, disordered, and phase separates with RNA. bioRxiv, doi: https://doi.org/10.1101/2020.06.17.158121

D'Angelo, M.A., and Hetzer, M.W. (2008). Structure, dynamics and function of nuclear pore complexes. Trends Cell Biol. 18, 456-466.

Daelemans, D., Costes, S.V., Cho, E.H., et al. (2004). In vivo HIV-1 Rev multimerization in the nucleolus and cytoplasm identified by fluorescence resonance energy transfer. J. Biol. Chem. 279, 50167-50175.

de, T.H.E., Riviere, M., and Bernhard, W. (1960). Examination by electron microscope of the VX2 tumor of the domestic rabbit derived from the Shope papilloma. Bull. Assoc. Fr. Etud. Cancer 47, 570-584.

Dharan, A., Bachmann, N., Talley, S., et al. (2020). Nuclear pore blockade reveals that HIV-1 completes reverse transcription and uncoating in the nucleus. Nat. Microbiol. 5, 1088-1095.

Di Nunzio, F. (2013). New insights in the role of nucleoporins: a bridge leading to concerted steps from HIV-1 nuclear entry until integration. Virus Res. 178, 187-196.

Di Nunzio, F., Danckaert, A., Fricke, T., et al. (2012). Human nucleoporins promote HIV-1 docking at the nuclear pore, nuclear import and integration. PLoS One 7, e46037.

Di Nunzio, F., Fricke, T., Miccio, A., et al. (2013). Nup153 and Nup98 bind the HIV-1 core and contribute to the early steps of HIV-1 replication. Virology 440, 8-18.

Dowling, D., Nasr-Esfahani, S., Tan, C.H., et al. (2008). HIV-1 infection induces changes in expression of cellular splicing factors that regulate alternative viral splicing and virus production in macrophages. Retrovirology 5, 18.

Du, M., and Chen, Z.J. (2018). DNA-induced liquid phase condensation of cGAS activates innate immune signaling. Science 361, 704-709.

Dustin, M.L., and Choudhuri, K. (2016). Signaling and Polarized Communication Across the T Cell Immunological Synapse. Annu. Rev. Cell Dev. Biol. 32, 303-325.

Dustin, M.L., and Kam, L.C. (2016). Tapping out a mechanical code for T cell triggering. J. Cell Biol. 213, 501-503.

Everett, R.D., and Chelbi-Alix, M.K. (2007). PML and PML nuclear bodies: implications in antiviral defence. Biochimie 89, 819-830.

Fay, M.M., and Anderson, P.J. (2018). The Role of RNA in Biological Phase Separations. J. Mol. Biol. 430, 4685-4701.
Fei, J., Jadaliha, M., Harmon, T.S., et al. (2017). Quantitative analysis of multilayer organization of proteins and RNA in nuclear speckles at super resolution. J. Cell Sci. 130, 4180-4192.

Francis, A.C., Marin, M., Singh, P.K., et al. (2020). HIV-1 replication complexes accumulate in nuclear speckles and integrate into speckle-associated genomic domains. Nat. Commun. 11, 3505.

Franzmann, T.M., and Alberti, S. (2019). Protein Phase Separation as a Stress Survival Strategy. Cold Spring Harb. Perspect. Biol. 11, a034058.

Gomez, G.N., Abrar, F., Dodhia, M.P., et al. (2019). SARS coronavirus protein nsp1 disrupts localization of Nup93 from the nuclear pore complex. Biochem. Cell Biol. 97, 758-766.

Gordon, D.E., Jang, G.M., Bouhaddou, M., et al. (2020). A SARS-CoV-2 protein interaction map reveals targets for drug repurposing. Nature 583, 459-468.

Guillen-Boixet, J., Kopach, A., Holehouse, A.S., et al. (2020). RNA-Induced Conformational Switching and Clustering of G3BP Drive Stress Granule Assembly by Condensation. Cell 181, 346-361 e317.

Harding, H.P., Zhang, Y., Bertolotti, A., et al. (2000). Perk is essential for translational regulation and cell survival during the unfolded protein response. Mol. Cell 5, 897-904.

Hiscox, J.A. (2007). RNA viruses: hijacking the dynamic nucleolus. Nat Rev Microbiol 5, 119-127.

Hnisz, D., Shrinivas, K., Young, R.A., et al. (2017). A Phase Separation Model for Transcriptional Control. Cell 169, 13-23.

Hosmillo, M., Lu, J., McAllaster, M.R., et al. (2019). Noroviruses subvert the core stress granule component G3BP1 to promote viral VPg-dependent translation. Elife 8.

Hou, S., Kumar, A., Xu, Z., et al. (2017). Zika Virus Hijacks Stress Granule Proteins and Modulates the Host Stress Response. J. Virol. 91.

Iserman, C., Roden, C., Boerneke, M., et al. (2020). Specific viral RNA drives the SARS-CoV-2 nucleocapsid to phase separate. bioRxiv, doi: https://doi.org/10.1101/2020.06.11.147199

Jarboui, M.A., Bidoia, C., Woods, E., et al. (2012). Nucleolar protein trafficking in response to HIV-1 Tat: rewiring the nucleolus. PLoS One 7, e48702.

Kaganovich, D. (2017). There Is an Inclusion for That: Material Properties of Protein Granules Provide a Platform for Building Diverse Cellular Functions. Trends Biochem. Sci. 42, 765-776.

Kamitani, W., Huang, C., Narayanan, K., et al. (2009). A two-pronged strategy to suppress host protein synthesis by SARS coronavirus Nsp1 protein. Nat. Struct. Mol. Biol. 16, 1134-1140.

Kamitani, W., Narayanan, K., Huang, C., et al. (2006). Severe acute respiratory syndrome coronavirus nsp1 protein suppresses host gene expression by promoting host mRNA degradation. Proc. Natl Acad. Sci. USA 103, 12885-12890.

Knoops, K., Kikkert, M., Worm, S.H., et al. (2008). SARS-coronavirus replication is supported by a reticulovesicular network of modified endoplasmic reticulum. PLoS Biol. 6, e226.

Krahling, V., Stein, D.A., Spiegel, M., et al. (2009). Severe acute respiratory syndrome coronavirus triggers apoptosis via protein kinase R but is resistant to its antiviral activity. J. Virol. 83, 2298-2309.

Lahaye, X., Gentili, M., Silvin, A., et al. (2018). NONO Detects the Nuclear HIV Capsid to Promote cGAS-Mediated Innate Immune Activation. Cell 175, 488-501 e422.

Langdon, E.M., and Gladfelter, A.S. (2018). A New Lens for RNA Localization: Liquid-Liquid Phase Separation. Annu. Rev. Microbiol. 72, 255-271.

Larson, A.G., Elnatan, D., Keenen, M.M., et al. (2017). Liquid droplet formation by HP1α suggests a role for phase separation in heterochromatin. Nature 547, 236-240.

Lee, C., Occhipinti, P., and Gladfelter, A.S. (2015). PolyQ-dependent RNA-protein assemblies control symmetry breaking. J. Cell Biol. 208, 533-544.
Lee, C., Zhang, H., Baker, A.E., et al. (2013). Protein aggregation behavior regulates cyclin transcript localization and cell-cycle control. Dev. Cell **25**, 572-584.

Lelek, M., Casartelli, N., Pellin, D., et al. (2015). Chromatin organization at the nuclear pore favours HIV replication. Nat. Commun. **6**, 6483.

Lokugamage, K.G., Narayanan, K., Huang, C., et al. (2012). Severe acute respiratory syndrome coronavirus protein nsp1 is a novel eukaryotic translation inhibitor that represses multiple steps of translation initiation. J. Virol. **86**, 13598-13608.

Lu, H., Yu, D., Hansen, A.S., et al. (2018). Phase-separation mechanism for C-terminal hyperphosphorylation of RNA polymerase II. Nature **558**, 318-323.

Lucic, B., Chen, H.C., Kuzman, M., et al. (2019). Spatially clustered loci with multiple enhancers are frequent targets of HIV-1 integration. Nat. Commun. **10**, 4059.

Luo, H., Chen, Q., Chen, J., et al. (2005). The nucleocapsid protein of SARS coronavirus has a high binding affinity to the human cellular heterogeneous nuclear ribonucleoprotein A1. FEBS Lett. **579**, 2623-2628.

Lusic, M., Marini, B., Ali, H., et al. (2013). Proximity to PML nuclear bodies regulates HIV-1 latency in CD4⁺ T cells. Cell Host Microbe. **13**, 665-677.

Maier, H.J., Hawes, P.C., Cottam, E.M., et al. (2013). Infectious bronchitis virus generates spherules from zippered endoplasmic reticulum membranes. mBio **4**, e00801-00813.

Maldarelli, F., Xiang, C., Chamoun, G., et al. (1998). The expression of the essential nuclear splicing factor SC35 is altered by human immunodeficiency virus infection. Virus Res. **53**, 39-51.

Michienzi, A., Cagnon, L., Bahner, I., et al. (2000). Ribozyme-mediated inhibition of HIV 1 suggests nucleolar trafficking of HIV-1 RNA. Proc. Natl Acad. Sci. USA **97**, 8955-8960.

Miorin, L., Kehrer, T., Sanchez-Aparicio, M.T., et al. (2020). SARS-CoV-2 Orf6 hijacks Nup98 to block STAT nuclear import and antagonize interferon signaling. Proc. Natl Acad. Sci. USA **117**, 28344-28354.

Molliex, A., Temirov, J., Lee, J., et al. (2015). Phase separation by low complexity domains promotes stress granule assembly and drives pathological fibrillization. Cell **163**, 123-133.

Monette, A., Niu, M., Chen, L., et al. (2020). Pan-retroviral Nucleocapsid-Mediated Phase Separation Regulates Genomic RNA Positioning and Trafficking. Cell Rep. **31**, 107520.

Monsellier, E., and Chiti, F. (2007). Prevention of amyloid-like aggregation as a driving force of protein evolution. EMBO Rep. **8**, 737-742.

Nair, S.J., Yang, L., Meluzzi, D., et al. (2019). Phase separation of ligand-activated enhancers licenses cooperative chromosomal enhancer assembly. Nat. Struct. Mol. Biol. **26**, 193-203.

Narayanan, K., Huang, C., Lokugamage, K., et al. (2008). Severe acute respiratory syndrome coronavirus nsp1 suppresses host gene expression, including that of type I interferon, in infected cells. J. Virol. **82**, 4471-4479.

Pante, N., and Kann, M. (2002). Nuclear pore complex is able to transport macromolecules with diameters of about 39 nm. Mol. Biol. Cell **13**, 425-434.

Peng, T.Y., Lee, K.R., and Tarn, W.Y. (2008). Phosphorylation of the arginine/serine dipeptide-rich motif of the severe acute respiratory syndrome coronavirus nucleocapsid protein modulates its multimerization, translation inhibitory activity and cellular localization. FEBS J. **275**, 4152-4163.

Perdikari, T.M., Murthy, A.C., Ryan, V.H., et al. (2020). SARS-CoV-2 nucleocapsid protein phase-separates with RNA and with human hnRNPs. EMBO J. **39**, e106478.

Piotrowska, J., Hansen, S.J., Park, N., et al. (2010). Stable formation of compositionally unique stress granules in virus-infected cells. J. Virol. **84**, 3654-3665.
Plys, A.J., Davis, C.P., Kim, J., et al. (2019). Phase separation of Polycomb-repressive complex 1 is governed by a charged disordered region of CBX2. *Genes Dev.* **33**, 799-813.

Poblete-Duran, N., Prades-Perez, Y., Vera-Otarola, J., et al. (2016). Who Regulates Whom? An Overview of RNA Granules and Viral Infections. *Viruses* **8**, 180.

Protter, D.S.W., and Parker, R. (2016). Principles and Properties of Stress Granules. *Trends Cell Biol.* **26**, 668-679.

Rabut, G., Doye, V., and Ellenberg, J. (2004). Mapping the dynamic organization of the nuclear pore complex inside single living cells. *Nat. Cell Biol.* **6**, 1114-1121.

Raices, M., and D'Angelo, M.A. (2012). Nuclear pore complex composition: a new regulator of tissue-specific and developmental functions. *Nat. Rev. Mol. Cell Biol.* **13**, 687-699.

Rao, S., Cinti, A., Temzi, A., et al. (2018). HIV-1 NC-induced stress granule assembly and translation arrest are inhibited by the dsRNA binding protein Staufen1. *RNA* **24**, 219-236.

Reed, M.L., Dove, B.K., Jackson, R.M., et al. (2006). Delineation and modelling of a nucleolar retention signal in the coronavirus nucleocapsid protein. *Traffic* **7**, 833-848.

Rensen, E., Mueller, F., Scoca, V., et al. (2020). Clustering and reverse transcription of HIV-1 genomes in nuclear niches of macrophages. *EMBO J.* **40**, e105247.

Riback, J.A., Katanski, C.D., Kear-Scott, J.L., et al. (2017). Stress-Triggered Phase Separation Is an Adaptive, Evolutionarily Tuned Response. *Cell* **168**, 1028-1040.e19.

Roden, C., and Gladfelter, A.S. (2020). RNA contributions to the form and function of biomolecular condensates. *Nat. Rev. Mol. Cell Biol.* **22**, 183-195.

Sabari, B.R., Dall'Agnese, A., Boija, A., et al. (2018). Coactivator condensation at super-enhancers links phase separation and gene control. *Science* **361**, eaar3958.

Sanders, D.W., Kedersha, N., Lee, D.S.W., et al. (2020). Competing Protein-RNA Interaction Networks Control Multiphase Intracellular Organization. *Cell* **181**, 306-324.e28.

Savastano, A., Ibanez de Opakua, A., Rankovic, M., et al. (2020). Nucleocapsid protein of SARS-CoV-2 phase separates into RNA-rich polymerase-containing condensates. *Nat. Commun.* **11**, 6041.

Scheer, U., and Hock, R. (1999). Structure and function of the nucleolus. *Curr. Opin. Cell Biol.* **11**, 385-390.

Schmid, M., Speiseder, T., Dobner, T., et al. (2014). DNA virus replication compartments. *J. Virol.* **88**, 1404-1420.

Scholte, F.E., Tas, A., Albulescu, I.C., et al. (2015). Stress granule components G3BP1 and G3BP2 play a proviral role early in Chikungunya virus replication. *J. Virol.* **89**, 4457-4469.

Scoca, V., Louveaux, M., Morin, R., et al. (2020). Direct tracking of single proviruses reveals HIV-1/LEDGF complexes excluded from virus-induced membraneless organelles. *bioRxiv*, doi: https://doi.org/10.1101/2020.11.17.385567

Selyutina, A., Persaud, M., Lee, K., et al. (2020). Nuclear Import of the HIV-1 Core Precedes Reverse Transcription and Uncoating. *Cell Rep.* **32**, 108201.

Seydoux, G., and Braun, R.E. (2006). Pathway to totipotency: lessons from germ cells. *Cell* **127**, 891-904.

Sharma, A., Takata, H., Shibahara, K., et al. (2010). Son is essential for nuclear speckle organization and cell cycle progression. *Mol. Biol. Cell* **21**, 650-663.

Shattuck, J.E., Paul, K.R., Cascarina, S.M., et al. (2019). The prion-like protein kinase Sky1 is required for efficient stress granule disassembly. *Nat. Commun.* **10**, 3614.

Shin, Y., and Brangwynne, C.P. (2017). Liquid phase condensation in cell physiology and disease. *Science* **357**, eaaf4382.
Shytaj, I.L., Lucic, B., Forcato, M., et al. (2020). Alterations of redox and iron metabolism accompany the development of HIV latency. EMBO J. 39, e102209.

Siomi, H., Shida, H., Maki, M., et al. (1990). Effects of a highly basic region of human immunodeficiency virus Tat protein on nucleolar localization. J. Virol. 64, 1803-1807.

Snijder, E.J., Limpens, R., de Wilde, A.H., et al. (2020). A unifying structural and functional model of the coronavirus replication organelle: Tracking down RNA synthesis. PLoS Biol. 18, e3000715.

Spector, D.L., Fu, X.D., and Maniatis, T. (1991). Associations between distinct pre-mRNA splicing components and the cell nucleus. EMBO J. 10, 3467-3481.

Strom, A.R., Emelyanov, A.V., Mir, M., et al. (2017). Phase separation drives heterochromatin domain formation. Nature 547, 241-245.

Sutherland, H., and Bickmore, W.A. (2009). Transcription factories: gene expression in unions? Nat. Rev. Genet. 10, 457-466.

Swift, H. (1959). Studies on nuclear fine structure. Brookhaven Symp. Biol. 12, 134-152.

Temin, H.M., and Mizutani, S. (1970). RNA-dependent DNA polymerase in virions of Rous sarcoma virus. Nature 226, 1211-1213.

Timani, K.A., Liao, Q., Ye, L., et al. (2005). Nuclear/nucleolar localization properties of C-terminal nucleocapsid protein of SARS coronavirus. Virus Res. 114, 23-34.

Uversky, V.N. (2017). Intrinsically disordered proteins in overcrowded milieu: membrane-less organelles, phase separation, and intrinsic disorder. Curr. Opin. Struct. Biol. 44, 18-30.

Uversky, V.N., Gillespie, J.R., and Fink, A.L. (2000). Why are ‘natively unfolded’ proteins unstructured under physiologic conditions? Proteins 41, 415-427.

Wang, J.T., and Seydoux, G. (2014). P granules. Curr. Biol. 24, R637-R638.

Wolff, G., Melia, C.E., Snijder, E.J., et al. (2020). Double-Membrane Vesicles as Platforms for Viral Replication. Trends Microbiol. 28, 1022-1033.

Wu, C.H., Chen, P.J., and Yeh, S.H. (2014). Nucleocapsid phosphorylation and RNA helicase DDX1 recruitment enables coronavirus transition from discontinuous to continuous transcription. Cell Host Microbe. 16, 462-472.

Wu, K.E., Fazal, F.M., Parker, K.R., et al. (2020). RNA-GPS Predicts SARS-CoV-2 RNA Residency to Host Mitochondria and Nucleolus. Cell Syst. 11, 102-108 e103.

Wurm, T., Chen, H., Hodgson, T., et al. (2001). Localization to the nucleolus is a common feature of coronavirus nucleoproteins, and the protein may disrupt host cell division. J. Virol. 75, 9345-9356.

Yang, P., Mathieu, C., Kolaitis, R.M., et al. (2020). G3BP1 Is a Tunable Switch that Triggers Phase Separation to Assemble Stress Granules. Cell 181, 325-345 e328.

Yoshizawa, T., Nozawa, R.S., Jia, T.Z., et al. (2020). Biological phase separation: cell biology meets biophysics. Biophys. Rev. 12, 519-539.

Yu, K.L., Lee, S.H., Lee, E.S., et al. (2016). HIV-1 nucleocapsid protein localizes efficiently to the nucleus and nucleolus. Virology 492, 204-212.

Yuan, X., Yao, Z., Shan, Y., et al. (2005). Nucleolar localization of non-structural protein 3b, a protein specifically encoded by the severe acute respiratory syndrome coronavirus. Virus Res. 114, 70-79.

Zeng, M., Shang, Y., Araki, Y., et al. (2016). Phase Transition in Postsynaptic Densities Underlies Formation of Synaptic Complexes and Synaptic Plasticity. Cell 166, 1163-1175 e1112.

Zhang, W., Chen, K., Zhang, X., et al. (2018). An integrated analysis of membrane remodeling during porcine reproductive and respiratory syndrome virus replication and assembly. PLoS One 13, e0200919.
Zhang, Y., Bertulat, B., Tencer, A.H., et al. (2019). MORC3 Forms Nuclear Condensates through Phase Separation. *iScience* 17, 182-189.

Zhao, Y.G., and Zhang, H. (2020). Phase Separation in Membrane Biology: The Interplay between Membrane-Bound Organelles and Membraneless Condensates. *Dev. Cell* 55, 30-44.

Zhou, P., Yang, X.L., Wang, X.G., et al. (2020). A pneumonia outbreak associated with a new coronavirus of probable bat origin. *Nature* 579, 270-273.

Zolotukhin, A.S., and Felber, B.K. (1999). Nucleoporins nup98 and nup214 participate in nuclear export of human immunodeficiency virus type 1 *Rev. J. Virol.* 73, 120-127.
**Figure legend**

**Figure 1** MLOs induced by HIV-1 and SARS-CoV-2 to replicate. Left: HIV-1 infection prompts the formation of nuclear MLOs enriched in host factors, such as CPSF6 and SC35, and in viral components, such as vRNA, vDNA, capsid, and integrase. Right: SARS-CoV-2 N protein forms condensates in the cytoplasm to recruit exclusively intact vRNA genome against subgenomic vRNAs or host RNAs. Cartoon created with BioRender.com.
<table><caption>Table 1 Role of MLOs in viral infection of pandemic viruses HIV-1 and SARS-CoV-2.</caption><thead><tr><th>MLOs</th><th>Viruses: HIV-1 & SARS-CoV-2</th><th>Role of MLOs during infection</th><th>References</th></tr></thead><tbody><tr><td rowspan="2">SGs</td><td>HIV-1</td><td>Regulation of genomic RNA and trafficking</td><td>Rao et al., 2018<br>Monette et al., 2020</td></tr><tr><td>SARS-CoV-2</td><td>Role of N protein in SARS-CoV-2 viral genome packing</td><td>Perdikari et al., 2020<br>Iserman et al., 2020<br>Cubuk et al., 2020<br>Savastano et al., 2020</td></tr><tr><td rowspan="2">NPC</td><td>HIV-1</td><td>Nuclear import and integration site selection</td><td>Di Nunzio et al., 2013<br>Lelek et al., 2015<br>Buffone et al., 2018<br>Marini et al., 2015</td></tr><tr><td>SARS-CoV-2</td><td>Inhibition of IFN signaling</td><td>Miorin et al., 2020</td></tr><tr><td rowspan="2">Nucleolus</td><td>HIV-1</td><td>Viral RNP assembly platform</td><td>Michienzi et al., 2000</td></tr><tr><td>SARS-CoV-2</td><td>Untranslated viral genomic RNA accumulation</td><td>Wu et al., 2020</td></tr><tr><td>PML NBs</td><td>HIV-1</td><td>Silenced HIV-1 location</td><td>Lusic et al., 2013</td></tr><tr><td rowspan="2">NSs</td><td rowspan="2">HIV-1</td><td>Potential sites of the PIC maturation</td><td>Scoca et al., 2020</td></tr><tr><td>Nuclear reverse transcription</td><td>Rensen et al., 2020<br>Burdick et al., 2020<br>Dharan et al., 2020<br>Selyutina et al., 2020<br>Scoca et al., 2020</td></tr></tbody></table>
<figure><img src="image_4.png" /></figure>

<figure><img src="image_5.png" /></figure>